N88S seipin-related seipinopathy is a lipidopathy associated with loss of iron homeostasis

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Ribeiro, Mafalda Oliveira, Verónica Nogueira, Vítor Costa, and 1 more This is a preprint; it has not been peer reviewed by a journal. https://doi.org/ 10.21203/rs.3.rs-5224286/v1 This work is licensed under a CC BY 4.0 License Status: Published Journal Publication published 07 Jan, 2025 Read the published version in Cell Communication and Signaling → Version 1 posted 15 You are reading this latest preprint version Abstract Background Seipin is a protein encoded by the BSCL2 gene in humans and SEI1 gene in yeast, forming an Endoplasmic Reticulum (ER)-bound homo-oligomer. This oligomer is crucial in targeting ER-lipid droplet (LD) contact sites, facilitating the delivery of triacylglycerol (TG) to nascent LDs. Mutations in BSCL2, particularly N88S and S90L, lead to seipinopathies, which correspond to a cohort of motor neuron diseases (MNDs) characterized by the accumulation of misfolded N88S seipin into inclusion bodies (IBs) and cellular dysfunctions. Methods Quantitative untargeted mass spectrometric proteomic and lipidomic analyses were conducted to examine changes in protein and lipid abundance in wild-type (WT) versus N88S seipin-expressing mutant cells. Differentially expressed proteins were categorized into functional networks to highlight altered protein functions and signaling pathways. Statistical comparisons were made using unpaired, two-tailed Student's t-tests or two-way ANOVA. P -values < 0.05 are considered significant. Results In a well-established yeast model of N88S seipinopathy, misfolded N88S seipin forms IBs and exhibits higher levels of ER stress, leading to decreased cell viability due to increased reactive oxygen species (ROS), oxidative damage, lipid peroxidation, and reduced antioxidant activity. Proteomic and lipidomic analyses revealed alterations in phosphatidic acid (PA) levels, associated with disrupted inositol metabolism and decreased flux towards phospholipid biosynthesis. Importantly, deregulation of lipid metabolism contributed to ER stress beyond N88S seipin misfolding and IB formation. Additionally, the model exhibited deregulated iron (Fe) homeostasis during lifespan. N88S seipin-expressing cells showed impaired ability to cope with iron deficiency. This was linked to changes in the expression of Aft1p-controlled iron regulon genes, including the mRNA-binding protein CTH2 and the high-affinity iron transport system member FET3 , in a p38/Hog1p- and Msn2p/Msn4p-dependent manner. Importantly, we unraveled a novel link between inositol metabolism and activation of the iron regulon in cells expressing the N88S seipin mutation. Despite iron accumulation, this was not associated with oxidative stress. Conclusions The study highlights that the effects of N88S seipin mutation extend beyond protein misfolding, with significant disruptions in lipid metabolism and iron homeostasis. This research marks a significant advance in understanding and defining the roles of proteins and signaling pathways that contribute to human seipinopathy. Altered cellular processes, as well as potential therapeutic targets and biomarkers, were identified and can be explored in translational studies using human cell models. lipid droplet seipin misfolding seipinopathy lipidopathy proteinopathy inositol iron Figures Figure 1 Figure 2 Figure 3 Figure 4 Figure 5 Figure 6 Figure 7 Figure 8 1. Introduction Lipid droplets (LDs) are ubiquitous cellular organelles responsible for fat storage, consisting of a core of triacylglycerols (TG) and sterol esters (SE) surrounded by a protein-decorated phospholipid monolayer membrane ( 1 – 3 ). LD dysfunction is linked to multiple diseases, making the study of LD biogenesis pivotal for understanding basic disease mechanisms. LDs are formed in the Endoplasmic Reticulum (ER), where enzymes like DGAT1 and DGAT2 (diacylglycerol acyltransferases, Dga1p and Lro1p in yeast) and ACAT1 and ACAT2 (acyl-coenzyme A: cholesterol acyltransferases, Are1p and Are2p in yeast) convert excess cellular fatty acids and cholesterol into TG and SE ( 4 – 6 ). These neutral lipids accumulate within the ER bilayer, coalescing to form an oil lens that grows and eventually buds off. Proteins such as fat storage-inducing transmembrane (FIT) proteins, perilipins, and the seipin complex (human BSCL2 and the Sei1p-Ldb16p complex in yeast) facilitate this process ( 4 – 6 ). Seipin, which is expressed in motor neurons of the spinal cord and cortical neurons in the frontal lobe, hypothalamus, and brainstem ( 7 ), and is essential for excitatory synaptic transmission and neurotransmitter release ( 7 ). This protein functions as a membrane protein featuring two transmembrane domains, a conserved luminal loop, and cytosolic domains that assembles into an oligomeric ring-like complex, which is essential for TG binding and proper LD budding and growth ( 8 – 13 ). For that reason, seipin plays a crucial role in the formation and maintenance of ER-LD contact sites. At these membrane junctions, seipin facilitates the transfer of neutral lipids from the ER to the forming LDs, ensuring efficient lipid storage and metabolism. In several organisms, deletion of seipin leads to severe cellular phenotypes, including the aberrant formation of LDs, which manifest as clustered or enlarged LDs ( 14 – 16 ), and impaired lipid homeostasis associated with altered cellular lipid profile and metabolic dysfunctions ( 7 , 17 ), as observed in severe congenital generalized lipodystrophy and other metabolic diseases. On the other hand, gain-of-function mutations in seipin, including N88S and S90L, are associated with autosomal dominant motor neuron diseases (MNDs), such as hereditary spastic paraplegias (Silver syndrome), Charcot-Marie-Tooth disease type 2, and distal hereditary motor neuropathy type V ( 18 – 21 ). This cohort of MNDs involve gradual involvement of both upper motor neurons (resulting in gait disturbances and pyramidal signs) and lower motor neurons (leading to amyotrophy of the peroneal muscles and small hand muscles), as well as pes cavus ( 22 ). By disrupting N -glycosylation, these mutations stimulate protein aggregation, resulting in ER stress and cell death ( 7 , 23 , 24 ). The molecular mechanisms underlying seipinopathy remain largely unresolved. Expression of dominant, unglycosylated N88L and S90L variants of seipin triggers a pronounced ER stress response by activating the unfolded protein response (UPR). This activation leads to the segregation of mutant seipin into inclusion bodies (IBs). The exact composition and characteristics of these IBs are still unclear. However, it is known that IBs do not colocalize with aggresomal markers such as pericentrin or vimentin ( 7 ). Despite these observations, the N88S seipin variant undergoes polyubiquitination and is subsequently targeted for degradation via the proteasome through the ER-associated degradation (ERAD) pathway ( 7 , 25 ). Neutral lipid metabolism, which drives LD biogenesis, is intricately linked to phospholipid biosynthesis pathways, as both processes are crucial for maintaining cellular lipid homeostasis and organellar membrane integrity ( 26 ). The synthesis of membrane phospholipids begins with the phospholipid phosphatidic acid (PA). In the de novo pathways, membrane glycerophospholipids are synthesized from PA through the liponucleotide intermediate CDP-diacylglycerol (CDP-DAG). It can also be channelled towards the synthesis of phosphatidylglycerol (PG). Additionally, CDP-DAG serves as a precursor for the synthesis of TG stored in LDs ( 26 ). Phospholipid synthesis is tightly regulated by modulating both enzyme expression and activity. This regulation is influenced by various factors such as carbon source, nutrient availability, growth stage, pH, and temperature ( 26 ). Key to this control are cis -acting elements like the inositol-responsive UAS INO , and transcription factors including the Ino2p-Ino4p complex and the transcriptional repressor Opi1p, which orchestrate the transcriptional regulation of phospholipid biosynthetic genes ( 27 , 28 ). Genes involved in the CDP-DAG pathway (e.g., CDS1, CHO1, PSD1, CHO2, OPI3 ), and in the synthesis of phosphatidylinositol (e.g., INO1 ) are regulated by UAS INO elements in their promoters ( 29 , 30 ). This element binds the Ino2p-Ino4p heterodimer, which activates transcription when inositol levels drop. However, when Opi1p binds to Ino2p, which essentially occurs in response to an increase in inositol levels, this activation is repressed ( 30 , 31 ). It is known that Opi1p transcriptional repressor activity is influenced by its cellular localization. Although Opi1p lacks a membrane-spanning domain, it associates with the nuclear/ER membrane through interaction with the integral membrane protein Scs2p and PA via electrostatic interactions ( 32 , 33 ). When PA levels decrease (e.g., in response to an increase in inositol levels), Opi1p is no longer anchored to the ER and is translocated into the nucleus to repress transcription of INO1 and UAS INO -containing phospholipid synthesis genes ( 31 ). Neurological issues have also been linked to dysregulated iron (Fe) metabolism, which can promote oxidative stress and cellular damage. Iron (Fe) is essential for various biological processes, including cell respiration, neurotransmitter synthesis, metabolism, lipid biosynthesis, and oxygen delivery ( 34 , 35 ). However, excessive iron can generate ROS, leading to the oxidation of proteins, lipids, and nucleic acids, which is harmful ( 36 , 37 ). Dysregulated iron metabolism in the brain is associated with neurological issues, promoting oxidative stress and cellular damage. Thus, cells have developed complex mechanisms to regulate iron levels ( 36 ). In yeast, the transcription factors Aft1p and its paralog Aft2p manage the cellular response to iron deficiency by activating genes of the iron regulon ( 37 , 38 ). These factors are transported into the nucleus by karyopherin Pse1p, where they bind to target genes to initiate transcription ( 36 , 39 ). Under iron deficiency, S. cerevisiae activates the Fe regulon to acquire iron from the environment via reductive and non-reductive pathways. In the reductive pathway, iron is reduced from the ferric (Fe 3+ ) to the ferrous (Fe 2+ ) state by Fre1-4p metalloreductases, and imported into the cytoplasm by a copper-dependent complex of Fet3p and Ftr1p. Copper activates Fet3p oxidase activity, aided by the copper chaperone Atx1p and the transporter Ccc2p ( 38 , 39 ). The non-reductive pathway imports siderophore-iron complexes retained by mannoproteins Fit1-3p and transported into the cell by Arn1-4p transporters ( 38 , 39 ). Iron homeostasis is also maintained by regulating iron-dependent metabolic processes. Non-essential pathways are downregulated, and iron is redirected to essential ones. Aft1p and Aft2p upregulate Cth2p, an mRNA-binding protein that restricts the expression of genes encoding iron-containing proteins or associated with iron-utilizing pathways ( 38 , 39 ). Cth2p also aids in prioritizing iron allocation towards specific pathways while stalling or inhibiting its mobilization in non-essential processes, including heme biosynthesis and mitochondrial respiration. The heme oxygenase Hmx1p degrades heme to free iron for essential pathways, helping cells survive under conditions of iron starvation ( 40 ). Under iron-replete conditions, Aft1p is transported from the nucleus into the cytosol in a process facilitated by Msn5p. This export mechanism requires proper biosynthesis of mitochondrial Fe-S clusters and their subsequent export to the cytoplasm, ensuring inhibition of Aft1p activity when iron is readily available ( 41 , 42 ). Importantly, Aft1p phosphorylation is negatively regulated by Mitogen-Activated Protein Kinase (MAPK) Hog1p/p38 in iron-replete conditions ( 43 ), and Slt2p/Mpk1p is also involved in maintaining iron levels by directly regulating Aft1p activity ( 44 ). More recently, we have developed a yeast model for N88S seipinopathy that recapitulates the cellular characteristics observed in human seipinopathy ( 45 ). This model exhibits increased ER stress levels with aging and the formation of IBs is also observed. Notably, cells expressing N88S homo-oligomers show reduced viability, increased oxidative damage from higher generation of reactive oxygen species (ROS), lipid peroxidation, and significantly decreased antioxidant activity ( 45 ). Using this system, we performed a multi mass spectrometry-based omics approach to investigate protein functions and delineate the signaling pathways involved in the pathological features of N88S seipinopathy. Altered cellular processes, as well as potential therapeutic targets and biomarkers, were identified and can be now explored in translational studies using human cell models. 2. Materials and Methods 2.1. Yeast strains and plasmids S. cerevisiae strains used in this study resulted from the W303α parental strain and are described in Table S1 . Protein tagging and individual gene deletions were performed by standard PCR-based homologous recombination ( 46 , 47 ). Primers were designed using Primers-4-Yeast ( 48 ) for pFA6 and pYM plasmid sets ( 46 , 47 ). Plasmids used in this study are listed in Table S2 . For cloning of CTH2- LacZ in the YEplac181 vector, pCM64-CTH2-FeRE-CYC1-LacZ plasmid ( 49 ) was digested with HindIII, and the insert was cloned into the HindIII restriction site of the YEplac181 vector. For cloning of ADH1pr- CDS1 -3HA into the pRS315-UPRE-LacZ vector ( 45 ), the plasmid UG75-ADH- CDS1 -3HA ( 50 ) was digested with SacII, and the resulting insert was cloned into the SacII restriction site of the pRS315-UPRE-LacZ vector. Plasmid YEplac181- FET3 -LacZ was generated by digesting p FET3 -LacZ ( 51 ) with ScaI and performing ligation into the SmaI restriction site of YEplac181. To produce plasmid YEplac181-GFP- AFT1 , pRS426-GFP- AFT1 ( 52 ) was cut with SacI and KpnI and the resulting insert was ligated into the same restriction sites of YEplac181. All constructs were verified either by sequencing (plasmids) or PCR (mutant strains). Strains were transformed using the standard lithium acetate procedure ( 53 ). 2.2. Culture media and growth conditions The yeast cells were grown aerobically at 26 ºC in a gyratory shaker at 140 rpm using Erlenmeyer flasks. A 1:5 proportion of growth media to flask volume was used. The liquid growth media used for yeast grown were: Yeast peptone dextrose (YPD) [1% (wt/vol) yeast extract (Conda Pronadisa), 2% (wt/vol) bacto peptone (LabM) and 2% (wt/vol) glucose (Fisher Scientific)], and synthetic complete (SC) medium [2% (wt/vol) glucose (Fisher Scientific) and 0.67% (wt/vol) yeast nitrogen base (YNB) without amino acids (BD BioSciences), supplemented with appropriate amino acids and nucleotides: (0.008% (wt/vol) histidine (Sigma Aldrich), 0.008% (wt/vol) tryptophan (Sigma Aldrich), 0.04% (wt/vol) leucine (Sigma Aldrich), 0.008% (wt/vol) uracil (Sigma Aldrich) and 0.008% (wt/vol) adenine (Sigma Aldrich)]. When indicated, YNB without aa and inositol was used (FORMEDIUM, ref: CYN3701) to prepare SC-glucose medium without inositol. For solid medium, 1.5% (wt/vol) agar (Conda Pronadisa) was added, supplemented or not with 3 µM FeSO 4 (II). Where indicated, myo-inositol (Sigma Aldrich) was used at a final concentration of 1 mM. The iron chelator bathophenanthrolinedisulfonate (BPS, Sigma Aldrich) was added to a final concentration of 100 µM in liquid medium to create iron-starvation conditions. Cells were grown to exponential (OD 600 ≈ 0,6), to the post-diauxic shift (PDS) phase (24 h after exponential phase) or to early stationary phase (48 h after exponential phase). 2.3. Proteomics analysis For proteome analysis, cells were grown to PDS phase in SC-glucose medium. Proteomics were performed by the company BGI on a commercial basis following standard protocols ( 54 ). The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE ( 55 ) partner repository with the dataset identifier PXD054826. 2.3.1. Protein preparation for proteomic analysis . Proteins were extracted with Lysis buffer (7 M urea, 2 M thiourea, 20 mM tris-HCl, pH 8.0), containing 1X Cocktail and 10 mM dithiothreitol (DTT). The samples were then sonicated on ice and centrifuged at 4°C, 25,000 g for 15 min. The supernatant was mixed with ice-cold acetone (1:5, v/v) containing 20 mM DTT and incubated at -20°C overnight. After centrifugation at 4°C, 25,000 g for 15 min, the precipitate was collected, washed twice with ice-cold acetone containing 20 mM DTT, and then air-dried. To reduce disulfide bonds, the dried samples were re-dissolved in Lysis buffer (without SDS) containing 10 mM DTT (final concentration) and incubated at 56°C for 1 h. Subsequently, 55 mM iodoacetamide (IAM, final concentration) was added to block the cysteines and the samples were further incubated for 1 h in the darkroom. Following the incubation, the samples were then precipitated with ice-cold acetone, air-dried, and finally dissolved in 0.5 M TEAB (tetraethyl ammonium bromide) (Applied Biosystems, Milan, Italy), before being used for protein quantification and subsequent iTRAQ labeling. 2.3.2. Peptide labeling . The protein (100 µg) was digested with Trypsin Gold (Promega, Madison, WI, USA) (30:1, protein: trypsin) at 37°C for 16 h. Digested samples were dried by vacuum centrifugation, reconstituted in 0.5 M TEAB and processed according to the manufacturer’s protocol for 6-plex iTRAQ reagent labeling (Applied Biosystems). The labeled peptide mixtures were then pooled and dried by vacuum centrifugation. 2.3.3. Peptide Fractionation. The Shimadzu LC-20AB liquid phase system was used, and the separation column was a 5 µm, 4.6x250 mm Gemini C18 column for liquid phase separation of the sample. The dried peptide samples were reconstituted with mobile phase A (5% acetonitrile, ACN pH 9.8), injected and eluted at a flow rate of 1mL/min using the following gradients: 5% mobile phase B (95% ACN, pH 9.8) for 10 min. 5–35% mobile phase B for 40 min, 35–95% mobile phase B for 1-min, mobile phase B for 3 min, and 5% mobile phase B for 10 min. The elution peak was monitored at a wavelength of 214 nm, and one component was collected per min. The samples were combined according to the chromatographic elution peak map to obtain 20 fractions, which were then freeze-dried. 2.3.4. LC-ESI-MS/MS analysis. The peptides were separated using a Thermo Easy nLC 1200 (Thermo Fisher Scientific, San Jose, CA) and loaded onto an analytical C18 column packed in-house (75 µm inner diameter, 1.8 µm column material particle size, 25 cm column length). The separation was carried out through the following effective gradient at a flow rate of 250 nL/min: 0 ~ 3 min, 5–10% mobile phase B (80% ACN, 0.1% FA); 3 ~ 43 min, mobile phase B increased linearly from 10–30%; 43 ~ 53 min, mobile phase B linearly increased from 35–44%; 53 ~ 63 min, mobile phase B increased from 40–100%; 63 ~ 70 min, 100% mobile phase B. The end of the nanoliter liquid phase separation was directly connected to the mass spectrometer. 2.3.5. Mass Spectrometry Detection. The eluate was subjected to nanoelectrospray ionization and entered into the tandem mass spectrometer Orbitrap Eclipse (Thermo Fisher Scientific, San Jose, CA) for DDA (Data Dependent Acquisition) mode detection. Main parameter settings: the scanning range of the primary mass spectrometer was 350 ~ 1,600m/z; the resolution was set to 60,000; the initial m/z of the secondary mass spectrometer was fixed at 100; the resolution was 15,000. The precursor ion screening conditions for secondary fragmentation were: charge 2 + to 7+, peak intensity over 25000, Data Dependent Mode set to Cycle Time, Time between Master Scans set to 2s. The ion fragmentation mode was HCD, the fragment ions were detected in Orbitrap, the fragmentation energy was 36, and the separation window was set to 0.7 m/z. The dynamic exclusion time was set to 45s. The AGC settings were: 1.2E6 for the first level and 5E4 for the second level. 2.3.6. Bioinformatics analysis . Protein identification was performed using Mascot search engine (version 2.3.02; Matrix Science, London, UK) against the Saccharomyces 811 (27719 sequences) database, after removal of redundant sequences). Search parameters were set as follows: monoisotopic mass; peptide mass tolerance at 10 ppm and fragment mass tolerance at 0.02 Da; trypsin as the enzyme; allowing one missed cleavage; +2 and + 3 as the peptide; oxidation (M), deamidated (NQ), Itraq8plex (Y) as the potential variable modifications, and carbamidomethyl (C), iTRAQ8plex (N-term), iTRAQ8plex (K) as fixed modifications. 2.3.7. Protein Quantification. An automated software called IQuant ( 56 ) was used to quantitatively analyzing the labeled peptides with isobaric tags. It integrates Mascot Percolator, a well performing machine learning method for rescoring database search results, to provide reliable significant measures. To assess the confidence of peptides, the peptide-spectrum matches (PSMs) were pre-filtered at a PSM-level false discovery rate (FDR) of 1%. Then, based on the "simple principle" (The parsimony principle), identified peptide sequences were assembled into a set of confident proteins. In order to control the rate of false-positive at protein level, a protein FDR at 1%, which is based on Picked protein FDR strategy ( 57 ), was estimated after protein inference (Protein-level FDR < = 0.01). The protein quantification process included the following steps: Protein identification, Tag impurity correction, Data normalization, Missing value imputation, Protein ratio calculation, Statistical analysis, Results presentation. The main IQuant quantification parameters were: Quant peptide: Use all Unique peptide; Quant number: at least one unique spectra; Normalization: VSN; Protein Ratio: Weighted average; Statistical Analysis: Permutation Test. In total, there were 4543 proteins identified, among which 97 and 115 were up or down regulated, respectively. Functional annotations of the proteins were conducted using Blast2GO program against the non-redundant protein database (NCBInr). The KEGG database ( http://www.genome.jp/kegg/ ) and the COG database ( http://www.ncbi.nlm.nih.gov/COG/ ) were used to classify and group these proteins. To identify significantly enriched GO terms and KEGG pathways, enrichment analyses will be performed based on the hyper-geometric test ( 58 ). 2.4. Lipid quantification by mass spectrometric analysis For lipidome analysis, cells were grown to PDS phase in SC-glucose medium. Lipidomics were performed by the company BGI on a commercial basis following standard protocols. Briefly, 20 mg cells were weighed and added into 2 mL thickened centrifuge tubes. Two steel balls and 800 µL of pre-chilled dichloromethane/methanol (3:1, v/v) precipitant were added into each sample, as well as 10 µL of the prepared internal standard. Samples were subjected to an ice bath ultrasound for 10 min and refrigerated overnight at -20°C. Samples were centrifuged at 25,000 × g for 15 min at 4°C and 500 µL supernatant were taken and drained in a freezer dryer. 500 µL lipid reconstituted solution (in isopropanol: acetonitrile: water = 2:1:1) was reconstituted and shaken for 30 sec. Then samples were implemented in ice bath ultrasound for 10 min and centrifuged at 25,000 × g for 15 min at 4°C. 20 µL of each sample was used and mixed as QC samples. For UPLC-MS Analysis, waters 2777c UPLC (waters, USA) in series with Q exactive HF high resolution mass spectrometer (Thermo Fisher Scientific, USA) was used for the separation and detection of metabolites. Chromatographic separation was performed on CSH C18 column (1.7 µm, 2.1x100 mm, Waters, USA). In positive ion mode, solvent A was 60:40 v / v acetonitrile:water with 10 mM ammonium formate and 0.1% formic acid and solvent B was 90:10 v / v isopropanol:acetonitrile with 10 mM ammonium formate and 0.1% formic acid. In negative ion mode, solvent A was 60:40 v / v acetonitrile:water with 10 mM ammonium formate and solvent B was 90:10 v / v isopropanol:acetonitrile with 10 mM ammonium formate. The gradient conditions were as follows: 40% ~43% B over 0 ~ 2 min, 43%~50% B over 2 ~ 2.1 min, 50%~54% B over 2.1 ~ 7 min, 54% ~70% B over 7ཞ7.1 min, 70% ~99% B over 7.1 ~ 13 min, 99%~40% B over 13 ~ 13.1 min, held constant at 99%~40% B over 13.1 ~ 15 min and washed with 40% B over 13.1–15 min. The flow rate was 0.4 mL/min and the injection volume was 5 µL. The instrument Q Exactive HF (Thermo Fisher Scientific, USA) was used for LC-MS analysis. The full scan range was 70–1050 m/z with a resolution of 120,000, and the automatic gain control (AGC) target for MS acquisitions was set to 3e6 with a maximum ion injection time of 100 ms. Top 3 precursors were selected for subsequent MSMS fragmentation with a maximum ion injection time of 50 ms and resolution of 30000, the AGC was 1e5. The stepped normalized collision energy was set to 15, 30 and 45 eV. ESI parameters were setting as: sheath gas flow rate: 40; aux gas flow rate: 10; spray voltage in positive ion mode: 3.80 V; spray voltage in negative ion mode: 3.20 V; capillary temperature: 320°C; aux gas heater temp: 350°C. For compound identification, full-scan and MS/MS analyses were performed using Lipidsearch v.4.1 (Thermo Fisher Scientific, USA) software. Metabolite ion peak extraction and metabolite identification for lipidomics, data preprocessing using metaX ( 59 ) and data visualization were performed as described ( 60 ). 2.5. Transcriptomics For transcriptomics analysis, cells were grown to exponential phase in SC-glucose medium, and then BPS was added to a final concentration of 100 µM. Cells were then incubated for additional 4 h. RNA extraction, library construction, and sequencing were performed by the BGI company following internal procedures. The raw and processed RNA sequencing data are available from the NCBI GEO repository under the accession number GSE273946. 2.5.1. RNA extraction . Cells were homogenized by mechanical disruption in 1.5 mL TRIzol lysis buffer. Samples were centrifuged at 12,000g for 5 min in 4ºC. The supernatant was transferred to new centrifuge tubes containing a chloroform/isoamyl alcohol (24:1) mix. After each shaking step, the samples were centrifuged at 12,000g for 8 min at 4ºC. Then, the supernatant was transferred to a new centrifuge tube containing isopropyl alcohol (2/3 vol/vol), gently shaken and cooled at -20ºC. Samples were then centrifuged for 25 min at 17,500 g (4ºC) and the supernatant was transferred to new microcentrifuge tubes, and combined twice with 75% (vol/vol) ethanol and mixed by pipetting. After centrifugation at 17,500 g for 3 min (4ºC), the supernatant was discarded, and the pellet was resuspended in 20–200 µL DEPC-H 2 O or RNase-free water. 2.5.2. Library construction methods. mRNA enrichment was performed on total RNA using oligo(dT)-attached magnetic beads. The enriched mRNA with poly(A) tails was fragmented using a fragmentation buffer, followed by reverse transcription using random N6 primers to synthesize cDNA double strands. The synthesized double-stranded DNA was then end-repaired and 5'-phosphorylated, with a protruding 'A' at the 3' end forming a blunt end, followed by ligation of a bubble-shaped adapter with a protruding 'T' at the 3' end. The ligation products were PCR amplified using specific primers. The PCR products were denatured to single strands, and then single-stranded circular DNA libraries were generated using a bridged primer. The constructed libraries were quality-checked and sequenced after passing the quality control. 2.5.3. Data filtering. Sequencing was performed on a DNBSEQ platform with PE150 (read length). The sequencing data was filtered with SOAPnuke ( 61 ) by: ( 1 ) removing reads containing sequencing adapter; ( 2 ) removing reads whose low-quality base ratio (base quality less than or equal to 15) is more than 20%; ( 3 ) removing reads whose unknown base ('N' base) ratio is more than 5%, afterwards clean reads were obtained and stored in FASTQ format. The subsequent analysis and data mining were performed on Dr. Tom Multi-omics Data mining system ( https://biosys.bgi.com ). 2.5.4. Structure variation detection. Saccharomyces_cerevisiae_S288C_559292.NCBI.GCF_000146045.2_R64.v2201 was used a reference from NCBI. The clean reads were mapped to the reference genome using HISAT2 ( 62 ). After that, Ericscript (v0.5.5) ( 63 ) and rMATS (V3.2.5) ( 64 ) were used to detect fusion genes and differential splicing genes (DSGs), respectively. 2.5.5. RNA identification . Bowtie2 ( 65 ) was applied to align the clean reads to the gene set, in which known and novel, coding and noncoding transcripts were included. 2.5.6. Gene quantification differential expression analysis . Expression level of gene was calculated by RSEM (v1.3.1) ( 66 ). The heatmap was drawn by pheatmap (v1.0.8) according to the gene expression difference in different samples. Essentially, differential expression analysis was performed using the DESeq2 (v1.4.5) ( 67 ) [or DEGseq (68) or PoissonDis ( 69 )] with Q value ≤ 0.05 (or FDR ≤ 0.001). 2.5.7. Gene annotation . To take insight to the change of phenotype, GO ( http://www.geneontology.org/ ) and KEGG ( https://www.kegg.jp/ ) enrichment analysis of annotated different expression gene was performed by Phyper ( https://en.wikipedia.org/wiki/Hypergeometric_distribution ) based on Hyper geometric test. The significant levels of terms and pathways were corrected by Q value with rigorous threshold (Q value ≤ 0.05, http://github.com/jdstorey/qvalue ). Genes meeting this criterion were considered significantly enriched in the candidate gene set. 2.6. β-Galactosidase (β-Gal) activity assay Cells harboring LacZ-reporter fusion plasmids were grown in SC-glucose medium. Cells were harvested by centrifugation, resuspended in breaking buffer (100 mM Tris, 1 mM DTT, 10% (vol/vol) glycerol) and protease inhibitors (Complete mini EDTA-free Protease cocktail inhibitor tablets) and mechanically lysed with zirconium beads for 5 min. Debris were pelleted at 12,044 g for 15 min at 4 ºC and the supernatant was collected for protein quantification. Total protein levels were quantified by the Lowry method using a bovine serum albumin standard curve. Volumes corresponding to 15–100 µg of total extract protein were diluted up to 800 µL with β-Gal buffer (60 mM Na 2 HPO 4 , 40 mM NaH 2 PO 4 , 10 mM KCl, 1 mM MgSO 4 , 50 mM β-mercaptoethanol). β-Galactosidase (β-Gal) activity was measured at 30°C using the substrate o -nitrophenyl-β-D-galactopyranoside (ONPG; Merck, Kenilworth, NJ, USA), as described previously ( 70 ). 2.7. Western blotting analysis For assessment of total protein levels of Ino1p, strains WT-VN WT-VC INO1-HA and N88S-VN N88S-VC INO1-HA were grown to exponential or PDS phases in SC-glucose medium. To evaluate the phosphorylation status and total protein levels of Aft1p, strains expressing pRS415-HA-AFT1 were grown to PDS phase in SC-glucose medium at 26 ºC. The cells were washed and harvested by centrifugation for 4 min at 4000 rpm (4 ºC). Proteins were extracted by alkaline lysis, and prepared in Laemmli sample buffer. Proteins were separated by SDS-PAGE, using 10% (Ino1p-3HA/HA-Aft1p total levels) and 6% (HA-Aft1p phosphorylation) polyacrylamide gels, and transferred to nitrocellulose membranes (Hybond-ECL GE Healthcare) in a semi-dry system for 1 h. Membranes were blocked with 5% (wt/vol) nonfat dry milk in TTBS (20 mM Tris, 140 mM NaCl, 0.05% (vol/vol), Tween-20 pH 7.6) for 1 h. Next, membranes were incubated with primary antibodies: mouse anti-HA tag antibody F-7 (1:1000, sc-7392 Santa Cruz Biotechnology) or mouse anti-Pgk1 (1:50,000, Molecular Probes). After washing with TTBS, membranes were incubated with the secondary antibody mouse IgG-peroxidase. Immunodetection was performed by chemiluminescence using WesternBright ECL reagent (Advansta) and exposing the membranes to LucentBlue X-ray films (Advansta). Band intensities were analyzed using the GS-900 Calibrated Densitometer (Bio-Rad). 2.8. Fluorescence microscopy To examine the intracellular localization of IBs using the Venus signal upon reconstitution of the VN and VC fragments, cells were grown to exponential phase in SC-glucose medium. To evaluate the localization of GFP-Aft1p, cells transformed with YEplac181-GFP- AFT1 were grown to the exponential phase in SC-glucose medium supplemented with 300 µM FeSO 4 (II). For nuclear staining, cells were incubated with 4 µg/mL of 4′-6-diamidino-2-phenylindole (DAPI, Molecular Probes, Invitrogen) for 15 min at room temperature, and protected from light. Cells were washed twice with PBS and observed by fluorescence microscopy (Zeiss Axio Imager Z1 Apotome or Leica TCS SP8). Z-stacks were acquired for DIC, DAPI and GFP/Venus channels. The output final images and colocalization analysis were performed using ImageJ 1.51k software. When applicable, all quantifications were performed from two independent experiments, and more than 100 cells per condition were scored. Values were recorded in Excel (Microsoft) and analyzed in Prism 8.0 (GraphPad Software). Brightness and contrast were adjusted using Inkscape (The Inkscape Project). 2.9. Iron Levels Total iron levels were quantified in yeast cells (3–7 × 10 7 cells mL − 1 ) grown in SC glucose medium to late exponential (OD 600 ≈ 2) and PDS (OD 600 ≈ 6-7.5) phases, using a colorimetric assay as described ( 43 ). 2.10. ROS staining and IB formation To assess ROS, cells grown in SC-glucose medium at specified phases were incubated with 5 µg/mL dihydroethidium (DHE, Molecular Probes) for 10 min at room temperature in the dark. The quantification of Venus fluorescence intensity, normalized to the number of cells, was used as a means to monitor IB formation ( 45 ). Then, cells were centrifuged, washed twice and resuspended in PBS ( 45 ). Flow cytometry analysis was performed using the FL1 (533/30) for IB monitoring, and FL3 (670 LP) channels (BD Accuri C6 Flow cytometer) for ROS quantification via DHE. Data were evaluated with FlowJow software (v. 10.6.1). 2.11. Yeast Spotting Assay The oxidative stress agents tert -Butyl hydroperoxide ( t -BOOH, Sigma Aldrich) and hydrogen peroxide (H 2 O 2 , Merck) were added at a final concentration of 50 µM and 250 µM to iron-supplemented SC-glucose plates. The iron chelator BPS was added to a final concentration of 30 µM. Growth assays were performed by spotting 1:10 serial dilutions of exponentially grown cell cultures onto SC-glucose plates and containing the specified compounds. The growth was observed and recorded after a 2-day incubation period at 26°C. 2.12. Bioinformatics Analysis In-silico analysis of transcriptional regulation of the FET3 promoter was carried out using the Yeast Search for Transcriptional Regulators and Consensus Tracking (YEASTRACT+) database ( 71 ). The search was performed to define unbiased regulatory associations between transcription factors (TFs) and the promoter region, either document or potential associations (based on TF binding sites). YEASTRACT + was also used to find genes encoding proteins found to be elevated in the mutant strain and regulated by Msn2/Msn4p. For that, documented associations between genes and transcription factors Msn2p and Msn4p were searched using the following parameters: 1) Simultaneous DNA binding and expression evidence and 2) Transcription factor acting as activator. 2.13. Aconitase activity assay The measurement of aconitase activity was performed as described ( 51 , 72 , 73 ), with minor modifications. Briefly, cells were grown to PDS phase in SC-glucose medium and harvested by centrifugation for 5 min at 4000 rpm (4 ºC). Cells were resuspended in aconitase buffer (100 mM Tris-HCl pH 7.4 and 0.6 M sorbitol) containing protease inhibitors (Complete, EDTA-free Protease Inhibitor Cocktail, Roche). The protein extracts were obtained by vortexing in the presence of glass beads for 10 min. Cell debris was removed by centrifugation at 3000 rpm for 15 min at 4 ºC, and protein concentration was determined by the method of Lowry, using bovine serum albumin as a standard. Cell lysates were assayed at 25°C in aconitase reaction buffer containing 100 mM Tris-HCl (pH 7.4), 1.2 mM cis -aconitate (Sigma-Aldrich) and 45 µL of protein sample. The lysis and enzymatic activity measurement steps were performed under an anaerobic atmosphere using buffers flushed with nitrogen gas. The decrease in absorbance at 240 nm was measured as a function of time (normalized to protein concentration), and an extinction coefficient of 3.6 (mM.cm) −1 was used to calculate the specific activity of aconitase. 1 unit of aconitase activity is defined as 1 nmol of cis -aconitate converted per minute and per mg of protein. 2.14. Statistical analysis Unless specified otherwise, the results were derived from a minimum of three independent experiments. The images shown are representative of these findings. Quantitative data are presented as the mean ± standard deviation (SD). Statistical comparisons were made using unpaired, two-tailed Student's t-tests or two-way ANOVA, conducted with Prism 8.0 software (GraphPad Software). P -values < 0.05 were considered significant: * p ≤ 0.05; ** p ≤ 0.01; *** p ≤ 0.001; **** p ≤ 0.0001. 3. Results 3.1. Lipid metabolism is altered in N88S seipin-expressing cells In this study, we employed comparative unbiased quantitative mass spectrometric proteomic analysis to examine changes in protein abundance and profile between the WT-VN WT-VC and N88S-VN N88S-VC strain at the post-diauxic shift (PDS) phase, when cells shifted from a fermentative (exponential phase) to aerobic utilization of non-glycolytic substrates (e.g. ethanol) by mitochondria. The goal was to define a set of differentially expressed proteins (DEPs - either up- or down-regulated) and sort into functional networks to highlight perturbed protein functions and signalling pathways contributing to disease-related phenotypes. We were able to identify 115 proteins with reduced abundance and 97 proteins with increased abundance in N88S seipin-expressing cells (Fig. 1A and Fig. S1 A, Tables S3 and S4). A volcano plot (Fig. 1B) is shown to highlight the differences in protein levels. Using YEASTRACT+ ( 74 ), a Gene Ontology (GO) analysis and KEEG pathway analysis for DEPs in biological processes revealed an enrichment in proteins related to ion transport (GO:0006811; p -value = 0.001380), phospholipid biosynthetic process (GO:0008654; p -value = 2.920 × 10 − 9 ) and lipid metabolic process (GO:0006629; p -value = 1.562 × 10 − 6 ) (Fig. S1 B-C and Fig. 1C). Notably, among the protein identified, eight showed reduced abundance, including seven key players in the phospholipid biosynthetic pathway: Cho1p, Cho2p, Opi1p, Opi3p, Psd1p, Cpt1p and Cds1p (Table S3 and Fig. 1D). This suggests potential alterations in the lipid profile, particularly in phospholipid and neutral lipids content. To investigate these changes, we conducted a quantitative lipidomic analysis at the same growth phase (PDS phase) to measure the levels of major phospholipids and their derivatives, inositol phosphates, and neutral lipids along with their corresponding precursors. We observed a decrease in 46 lipid metabolites, while 41 lipid molecules levels were increased (Fig. S2 A-B). The levels of fatty acids (Fig. S2 C) and of major phospholipids (PC, PE, PS and PI) remained essentially unaltered (Fig. 2A), however the levels of PG, which is derived from CDP-DAG, were decreased (Fig. 2A). The amount of ceramide (Fig. S2 D) and lysophospholipids (Fig. 2B) was increased, suggesting that the activity of lysophospholipid acyltransferases may be impaired in the mutant. Despite the fact of DG abundance was unchanged (Fig. 2C), the levels of PA and TG are increased (Fig. 2D-E), suggesting that PA and lipid precursors are being redirected towards neutral lipid synthesis. 3.2. Inositol metabolism is deregulated in cells expressing the mutant seipin Genes encoding enzymes in both the CDP-DAG ( CDS1, CHO1, PSD1, CHO2, OPI3 ) and Kennedy ( CPT1 ) pathways contain a UAS INO element in their promoters whose expression is transcriptionally repressed by Opi1p ( 31 , 75 ). To evaluate if their lower protein abundance in N88S seipin-expressing cells correlates with reduced transcription, we measured the transcription of Opi1p-dependent genes in WT and mutant cells, using an INO1 -LacZ transcriptional reporter during lifespan. We observed that INO1 expression remains unchanged in the WT, however there is a ~ 4-fold increase in N88S seipin-expressing cells at PDS and stationary phases (Fig. 3A). It was previously demonstrated that the accumulation of PA acts as the metabolic signal that triggers the derepression of INO1 ( 29 , 76 , 77 ). Therefore, a plausible explanation for lower Opi1p repressor activity is the retention of Opi1p in the ER potentiated by accumulation of PA as observed by lipidomic analysis (Fig. 2D), allowing the Ino2p-Ino4p heteromeric complex to stimulate the transcription of INO1 . We then conclude that post-transcriptional mechanisms may operate to control the steady protein levels of these phospholipid biosynthetic enzymes in response to changes in the lipid profile observed in the mutant strain (Fig. 1D). More recently, it was shown that the levels of PA (34:1) is correlated with optimal expression of INO1 irrespective of total PA content ( 78 ). We observed that the amount of the PA (34:1) is increased by ~ 7-fold at PDS phase in mutant cells, which coincides with the increase in INO1 expression at the same phase (Fig. S2 E). Next, we decided to evaluate if higher INO1 expression was correlated with changes in Ino1p protein levels during lifespan. For that, we analyzed Ino1p-HA levels at the exponential and PDS phases by Western Blotting. We observed increased protein levels starting at the exponential phase, which remained elevated during the PDS phase (Fig. 3B), where INO1 expression is largely derepressed in mutant cells (Fig. 3A). Ino1p is essential for the de novo biosynthesis of inositol, which is incorporated into phosphatidylinositol (PI) for the synthesis of phosphatidylinositol phosphates (PIP). In N88S seipin-expressing cells, we also observed changes in PI-derived lipids, including decreased levels of phosphoinositides (PIP and PIP 3 ). This indicates that PI metabolism is also deregulated (Fig. S2 F). We next tested whether cells expressing the seipin N88S mutation are responsive to changes in inositol levels. For that, cells expressing the INO1 -LacZ reporter fusion were grown to exponential phase in the absence of inositol and then shifted to medium containing inositol. While WT cells adapted to inositol by reducing INO1 expression, the mutant was unable to adapt and failed to repress INO1 expression (Fig. 3C). Importantly, in the absence of inositol, INO1 expression was lower in the mutant compared to WT cells which is reminiscent of the behavior displayed by the mutant Opi1 FFAT , in which the Opi1p-Scs2p interaction motif two phenylalanines ( FF ) in an a cidic t ract (FFAT) is absent, and the activity of Opi1p is mainly driven by the electrostatic interaction with PA is absent, and the activity of Opi1p is mainly driven by the electrostatic interaction with PA ( 79 ). Overall, we provide strong evidence that inositol and lipid metabolism is highly deregulated in the mutant. In summary, the results suggest that increased PA levels may be linked to decreased flux of lipid precursors into phospholipid biosynthesis, due to lower protein levels of key enzymes in this pathway. Consequently, accumulation of PA levels causes Opi1p to be retained in the ER, allowing the transcription of INO1 to be derepressed, thus leading to elevated Ino1p protein levels. Additionally, PA may be redirected towards the synthesis of neutral lipids, thus explaining the higher amount of TG exhibited by the mutant. 3.3. PA and impaired inositol metabolism contribute to ER stress independently of protein misfolding in mutant cells ER stress and UPR activation can influence cellular processes beyond ER protein folding, playing critical roles in lipid metabolism, as it constitutes a key site for lipid synthesis and storage ( 80 ). Previous studies showed that inositol depletion can trigger ER stress without causing a noticeable accumulation of unfolded proteins in the ER lumen ( 81 – 83 ). Instead, this stress response appears to activate the UPR via a membrane-based mechanism that functions independently of unfolded proteins ( 84 ). This offers an ideal framework to investigate whether deregulated lipid metabolism contributes to ER stress observed in the yeast model of N88S seipinopathy. We then evaluated how INO1 deficiency affects the activity of the UPRE-LacZ ER stress reporter. As previously described, N88S seipin-expressing cells displayed higher levels of ER stress (Fig. 3D) associated with elevated expression of the reporter fusion ( 45 ). Importantly, β-galactosidase activity further increased in mutant cells upon deletion of INO1 , although to lower extent, indicating that misregulation of INO1 expression and impaired inositol metabolism also contribute to ER stress. Notably, INO1 deletion is associated with reduced PI levels and accumulation of lipid precursors, including PA and CDP-DAG ( 31 ). This led us to investigate whether accumulation of PA is associated with higher induction of the UPR. When WT cells are grown in inositol-depleted conditions, PI levels remain low, leading to PA buildup ( 31 ). Importantly, under these conditions, N88S seipin-expressing cells exhibited higher UPR levels when grown in the absence of inositol in a INO1 -dependent manner (Fig. 3E). In the presence of exogenous inositol, where PA is consumed as a precursor to support PI biosynthesis, the β-galactosidase activity of the ER stress reporter remained unchanged in WT cells regardless of inositol levels, but decreased in the mutant (Fig. 3E). This reinforces the hypothesis that the response to changing PA levels involves the induction of the UPR in cells expressing N88S mutant seipin. Next, we tested how the overexpression of CDS1 affects the ER stress response. Cds1p is responsible for the synthesis of CDP-DAG from PA. Cds1p consumes the PA pools and channels the CDP-DAG pool towards PI biosynthesis under conditions of inositol surplus ( 85 ). However, in the absence of inositol, where PI biosynthesis is essentially halted, CDP-DAG derived from PA is channeled into the phospholipid biosynthetic pathway. Under inositol starvation, we observed that the UPR is significantly increased in WT cells, and even more induced in N88S seipin-expressing cells upon overexpression of CDS1 (Fig. 4A). Higher UPR induction in the mutant might be linked to reduced enzymatic capacity to promote phospholipid biosynthesis under these conditions, as the overall phospholipid biosynthesis rate is likely reduced due to decreased protein levels of key enzymes involved in the pathway (Fig. 1D). So, we tested whether stimulation of phospholipid biosynthesis by overexpressing CHO1 in WT and N88S mutant cells induces ER stress under the same conditions (in the absence of inositol). In this case, we observed no changes in the induction of the LacZ reporter fusion for all strains tested (Fig. 4B). Notably, overexpression of CDS1 , in contrast with CHO1 counterparts, leads to inositol auxotrophy and significant viability loss in the absence of inositol (Fig. 4C). Overall, the data support a model in which the accumulation of PA, whether due to a reduced rate of phospholipid biosynthesis or in response to changes in lipid flux upon inositol availability (Fig. 1D, 3C-E, and 4A-B), is a key feature of the ER stress response in N88S seipin mutant cells. This is particularly significant, as it demonstrates that lipid imbalance also contributes to the ER stress response beyond protein misfolding of seipin caused by the N88S mutation. In agreement with this idea, we found that INO1 deletion actually reduced IB formation by ~ 50% in N88S seipin-expressing cells, as monitored by fluorescence microscopy and flow cytometry (Fig. 4D-E), despite the earlier observation that the UPR is more strongly induced in cells grown under the same conditions (Fig. 3D). Finally, we tested the relationship between impaired lipid metabolism and ROS production in the mutant strain. For this purpose, cells were grown to stationary phase, and ROS levels were detected using the DHE probe. The results showed that INO1 deficiency reduced ROS levels by ~ 30% in WT cells, but did not affect ROS levels in mutant cells (Fig. S3 A). This indicates that oxidative damage is not directly linked to defects in membrane lipid metabolism in N88S seipin-expressing cells. 3.4. N88S seipin expressing cells are sensitive to iron deficiency conditions The proteomic analysis revealed that proteins involved in iron ion homeostasis, including Fit1p, Arn1p, Arn2p and Hmx1p, were present at lower levels in N88S seipin expressing cells (Fig. 1C and Table S3 ). This prompted us to investigate whether there were alterations in cellular iron levels during lifespan imparted by the N88S seipin mutation. The results revealed that cells expressing the N88S seipin mutant accumulated iron (Fe) at the exponential phase (Fig. 5A). Nevertheless, there was a significant decrease in Fe levels from the exponential to PDS phase in the mutant, suggesting that cells experience iron deficiency. It is known that the demand for iron increases during the diauxic shift, and Aft1p is responsible for the regulation of proteins involved in capturing, internalizing, and mobilizing Fe to meet the needs of mitochondria, DNA repair, and other cellular processes ( 86 – 88 ). Using a LacZ reporter where the Aft1p binding sequence from the CTH2 promoter is fused to the LacZ gene, we found that Aft1p transcriptional activity boosted ~ 15-fold in WT cells grown from exponential phase to PDS phase. In contrast, in N88S seipin-expressing cells, the increase was approximately 7-fold, about half of the one observed in WT cells (Fig. 5B). This is in agreement with decreased protein levels of Fit1p, Arn1p, Arn2p and Hmx1p observed in these cells at PDS phase as identified by proteomic analysis (Table S3 ), which collectively correspond to proteins whose genes are transcriptionally activated by Aft1p/Aft2p in response to iron deficiency ( 37 ). To test if this effect is related to impaired ability to activate the iron regulon, cells were grown to the exponential phase and treated with the iron chelator bathophenanthrolinedisulfonate (BPS), which limits iron availability and causes an iron deprivation condition. As expected, β-galactosidase activity was significantly increased in WT cells as an adaptive response to BPS-induced iron depletion, but the induction was lower by 50–60% in the mutant strain compared to WT cells (Fig. 5C). To further address how Aft1p deregulation affects the iron deficiency response in cells expressing mutant seipin, WT and N88S seipin-expressing cells were subjected to transcriptomic analysis under BPS-induced iron deprivation (Fig. S4 A-D). As expected, bioinformatic analysis revealed that GO functional categories were enriched among differentially expressed genes (DEGs) involved in iron-regulated processes and mitochondrial-related functions, namely tricarboxylic acid cycle and mitochondrial electron transport chain, iron-sulfur cluster assembly, sterol biosynthetic process and aminoacid metabolism (Fig. S4 A-D). The results revealed that 197 and 250 genes had lower and higher expression in the mutant respectively, when compared to WT cells (Tables S5 and S6). We thus focused our attention on transcripts that are transcriptionally regulated by Aft1p/Aft2p upon BPS treatment, as defined in a previous study ( 49 ). Of the DEGs, 10 out of 28 genes previously reported to be upregulated during Fe starvation in WT cells ( 49 ) are downregulated in N88S seipin-expressing cells, including members of the Fe regulon: CCC2, ARN1, FIT1 , FTH1 , OLE1 , FIT3, FET4 , ATX1, SIT1 and FTR1 (Fig. S4 E and Table S6 ). Conversely, 13 ( ISA1, COR1, PYC2, LEU1, RNR4, BIO2, CYC1, HAP4, NFU1, CCP1, CYT1, QCR2 and RIP1 ) out of 34 genes with reduced expression in WT cells under similar conditions ( 49 ) are increased in the mutant strain (Fig. S4 E and Table S5 ). Overall, these results suggest that the N88S mutation renders cells unable to effectively activate Aft1p-mediated transcription of the iron regulon in response to changes in iron levels during lifespan and in response to iron deficiency. We then propose that this defective response may contribute to the increased ROS generation and oxidative damage previously reported for the mutant strain ( 45 ). To test this, cells were incubated with BPS at different growth phases and then allowed to grow in medium for 48 hours. When treated with the iron chelator at the exponential phase, where iron accumulation was observed in mutant cells (Fig. 5A), both WT and N88S seipin-expressing cells exhibited an acute growth defect (Fig. 5D). Although an increase in ROS content was noted in BPS-treated WT cells, the mutant displayed similar levels of ROS regardless of the presence of BPS in the medium (Fig. 5D). When cells were incubated with BPS at the diauxic shift, we observed no changes in growth and ROS content in WT and mutant cells (Fig. 5E). Next, we evaluated the sensitivity of WT and mutant cells to the oxidants t -BOOH and H 2 O 2 , and determined if this was altered by the addition of BPS to the medium (Fig. 5F). We observed that N88S seipin-expressing cells were slightly more sensitive to the tested oxidants than WT cells, but their sensitivity was not significantly altered by BPS when compared to WT cells (Fig. 5F). In the absence of any oxidative stress but in the presence of BPS, N88S seipin-expressing cells also displayed a mild growth defect as previously reported for cth2 Δ cells ( 89 ), which is in agreement with lower Aft1p transcriptional activity and impaired response to iron deficiency (Fig. 5F). Overall, the data suggest that disruption of iron homeostasis is not the primary cause of oxidative damage in the yeast model of N88S seipinopathy. 3.5. The MAPK Hog1p/p38 contributes to impaired iron metabolism in cells carrying the seipin N88S mutation The regulation of Aft1p phosphorylation by the MAPK kinases Hog1p and Slt2p has been implicated in the control of iron homeostasis and associated stress response pathways ( 43 , 44 ). In particular, Hog1p negatively regulates Aft1p transcriptional activity, which allows its export from the nucleus to the cytosol under iron sufficient conditions ( 37 , 38 , 43 , 90 ). Based on this, we posit that reduced activation of the iron regulation by Aft1p might be associated with changes in Hog1p activation and/or Aft1p phosphorylation. Detailed proteomic analysis revealed increased levels of Sko1p (Table S4 ). Sko1p is a key transcription factor regulating osmostress-induced gene expression under the direct control of the Hog1p ( 91 ). Sko1p binds to cAMP-responsive element (CRE) sequences, and the expression analysis of CRE-driven reporter genes is used as a reporter of osmostress-activated expression, which depends solely on Sko1p and Hog1p proteins ( 92 – 94 ). Using a 2xCRE-LacZ reporter, we evaluated changes in Hog1p activation during lifespan. At the exponential phase, we observed no significant changes, however a higher activation of the reporter fusion was observed in N88S seipin-expressing cells at PDS phase, indicating higher Hog1p activation (Fig. 6A). This coincided with reduced Aft1p transcriptional activity at this phase (Fig. 5B). To evaluate changes in Aft1p phosphorylation, we analyzed the migration pattern of HA-tagged Aft1p using Western blotting at PDS phase (Fig. 6B). Although total Aft1p levels are slightly higher (but not statistically significant), no noticeable alterations in the phosphorylation mobility pattern of Aft1p were observed in the mutant compared to WT cells (Fig. 6B). As a result, we conclude that the Aft1p phosphorylation status is not a primary cause for defective activation of the iron regulon at PDS phase (Fig. 5B). The transcriptional activity of Aft1p is governed by its localization in the nucleus, which is controlled by several regulatory mechanisms involving a range of proteins. These interactions can result in alterations in the activation of the iron regulon. We thus investigated the localization of GFP-Aft1p in WT and mutant cells using fluorescence microscopy. Under iron-rich conditions, around 40% of wild-type cells displayed nuclear Aft1p, whereas only 21% of cells expressing the N88S seipin variant showed nuclear localization of the transcription factor (Fig. 6C). These data suggest increased export of Aft1p to the cytosol, which could explain why full activation of the iron regulon is hampered in the yeast model of N88S seipinopathy. We decided to extend our analysis of the contribution of Hog1p to the loss of iron homeostasis imparted by the N88S seipin mutation. Firstly, we measured iron levels during lifespan, and the results revealed that deletion of HOG1 in WT cells increased iron levels at the exponential phase, consistent with its role as a negative regulator of the iron regulon (Fig. 6D). Importantly, the absence of Hog1p suppressed the iron accumulation phenotype of the mutant, and restored its ability to maintain proper iron levels as observed in WT cells (Fig. 6D). Next, we analyzed the Aft1p transcriptional activity during lifespan and upon BPS treatment in cells expressing p CTH2 -LacZ. At PDS phase, we observed that deletion of HOG1 had no significant alterations in the β-galactosidase reporter activity in both WT and N88S seipin-expressing cells (Fig. 6E). This indicates that during lifespan, the activation of the iron regulon by Aft1p/Aft2p is mediated by other signal transduction pathways in addition to Hog1p regulation ( 37 , 38 ). However, under iron deprivation, CTH2 -LacZ expression was induced in WT cells and reached higher levels in the corresponding hog1 Δ mutant (Fig. 6F). Notably, the transcriptional activity of Aft1p in cells expressing the N88S mutation was restored to WT levels (Fig. 6F) in the absence of the MAPK, supporting the idea that Hog1p controls iron levels and the adaptive response to iron deficiency in the yeast model of N88S seipinopathy. We also decided to investigate whether Hog1p signalling also modulates IB formation in the mutant. For that, we followed intracellular localization of IBs using the Venus signal ( 45 ). We observed a reduction of number of cells displaying IBs upon deletion of either HOG1 or SKO1 (Fig. S5 A-B), indicating that Hog1p/p38 also promotes IB generation beyond iron imbalance in cells expressing mutant seipin. Finally, we decided to investigate if regulation of ER stress response is linked to loss of iron homeostasis observed in the mutant. To test this hypothesis, we analyzed CTH2 -LacZ reporter activity in cells shifted to SC-glucose medium with or without inositol, supplemented or not with BPS. In WT cells, shifting to inositol-containing medium did not result in measurable changes in the β-galactosidase activity. Notably, CTH2 -LacZ expression was induced only in the presence of BPS, with no significant changes due to inositol alone in these cells (Fig. S5 C). However, in N88S seipin-expressing cells, there was a subtle but consistent increase in Aft1p transcriptional activity when grown in inositol-containing medium supplemented with BPS, compared to cells grown without inositol plus BPS (Fig. S5 C). This finding is particularly important as it reveals a previously unexplored functional relationship between inositol and iron metabolism. It indicates that under conditions where PA is consumed and the ER stress response is attenuated in the mutant (Fig. 3E), there is higher activation of the iron regulon by Aft1p/Aft2p in the yeast model of N88S seipinopathy. 3.6. FET3 expression is altered in cells carrying the seipin N88S mutation The expression of FET3 , a gene involved in iron uptake, is also regulated by the transcription factor Aft1p ( 37 , 95 , 96 ). To evaluate if Aft1p inhibition in N88S seipin-expressing cells also affects FET3 expression, we used a construct containing the FET3 promoter (-863 bp to + 1) fused to the LacZ reporter gene (YEplac181- FET3 -LacZ) ( 51 ). In this construct, there is an identified functional Aft1p consensus site ( 96 ) located − 254 bp upstream of the ATG translation initiation codon, and a predicted Aft1p-binding site at position − 670 bp (GGCACCC) in the FET3 promoter ( 51 ). The impact of N88S seipin mutation on FET3 -LacZ expression was firstly assessed by measuring the β-galactosidase activity of the reporter during lifespan (Fig. 7A). The results showed no differences in the reporter gene expression in WT and N88S seipin-expressing cells at the exponential phase. We observed an increase in FET3 expression in WT cells at PDS phase, but the induction was higher in the mutant (Fig. 7A), which contrasts with reduced Aft1p-controlled CTH2 expression observed at the same phase (Fig. 5B). This suggests that in mutant cells, Aft1p regulates FET3 expression differently compared to other Aft1p-regulated genes. We also tested if this effect is also observed under BPS-induced iron deficient conditions. As expected, BPS treatment induced FET3 expression in WT cells, but the reporter fusion activity was even higher in N88S seipin expressing cells (Fig. 7B). Overall, the results indicate that CTH2 expression was reduced, whereas FET3 expression is increased at PDS phase and under iron-deficient conditions in cells expressing N88S mutant seipin. 3.7. In-silico analysis revealed the presence of a potential Msn2p/Msn4p binding site in the FET3 promoter It was previously shown that FET3 expression is not entirely dependent on Aft1p, and that the transcription factor Ace1p regulates the response to copper overload by limiting the expression of FET3 ( 51 ). To delineate potential promoter regions responsible for Aft1p-independent activation of FET3 , we performed an unbiased bioinformatic analysis of the FET3 promoter (-863 bp to + 1) to search for potential transcription factor binding sites using YEASTRACT+ ( 74 ). The results revealed more than 50 transcription factors that could potentially bind to the FET3 promoter (Table S7 ). The results identified the putative Aft1p/Aft2p binding sequence (-670 bp), the predicted Ace1p-like binding site (-783 bp) ( 51 ), and importantly a Msn2p binding sequence located upstream (-813 bp) on the FET3 promoter was now uncovered (Fig. 7C). In S. cerevisiae , the stress response involves a sophisticated network of sensing and signal transduction mechanisms, prominently featuring the transcriptional regulation of various genes. In yeast, the zinc-finger transcription factors Msn2p and Msn4p, which share 66% sequence homology, are key regulators of stress-responsive gene expression ( 97 – 102 ). They bind specifically to the stress response element (STRE) sequences 5′-AGGGG or 5′-GGGGA. Msn2p and Msn4p control the expression of over 90% of genes activated in response to heat stress, osmotic stress, and carbon starvation, and are essential for regulating chronological lifespan ( 97 – 102 ). Importantly, it was reported that overexpression of the plasma membrane receptor IZH2 inhibits FET3 expression via negative regulation of Msn2p/Msn4p transcriptional activation without requiring Aft1p-dependent induction of the iron-responsive element FeRE ( 103 ). Based on this study, we posit that overexpression of IZH2 should decrease the FET3- LacZ reporter gene expression if the latter relies on Msn2p/Msn4p activation. At the exponential phase, no significant differences were observed in all strains tested, but upon transition to PDS phase, we observed higher β-galactosidase activity of the FET3 -LacZ reporter in cells expressing mutant seipin cells, which was reduced to WT levels upon overexpression of IZH2 (Fig. 7D). Importantly, we observed a reduction in FET3 expression in WT cells when IZH2 was overexpressed (Fig. 7D), which is consistent with a negative regulation of FET3 expression by Izh2p. In keeping with a role for Msn2p/Msn4p in the regulation of FET3 expression, we further tested the expression of the pSTRE-LacZ reporter gene, which contains the STRE sequences from the CTT1 promoter regulated by these transcription factors ( 104 ). Here, we transformed both strains with the reporter, and β-galactosidase activity was measured during lifespan. We found that higher FET3 expression (Fig. 7A) paralleled the increased activation of Msn2p/Msn4p transcriptional activity at PDS phase in N88S seipin-expressing cells (Fig. 7E). In addition, a bioinformatic search for target genes with documented regulation by Msn2p/Msn4p identified genes encoding proteins whose levels were found to be higher at PDS phase by proteomic analysis (Table S4 ), including GRX2 , PUT3 , HXT1 , HXT7 , RAS2 , DIP5 , ARO10 , MAL12 and ARO9 (Table S8 ). Altogether, the data strongly suggest that stress responsive Msn2p/Msn4p transcription factors are activated and may positively regulate FET3 expression at PDS phase, thus compensating for the reduced Aft1p transcriptional activity (as observed for CTH2 -LacZ reporter) in N88S seipin-expressing cells (Fig. 5B). It is possible that FET3 expression acts as an adaptive response to partially counteract the reduced Aft1p-controlled CTH2 expression and lower protein levels of Fit1p, Arn1p, Arn2p, and Hmx1p. It is important to note that analysis of the CTH2 promoter used in the CTH2 -LacZ reporter fusion ( 49 ) did not reveal any binding sites for Msn2p/Msn4p using YEASTRACT+ (data not shown). 3.8. The induction of FET3 expression is associated with a reduction in aconitase activity in cells expressing N88S mutant seipin Cells respond to defective Fe-S cluster synthesis by accumulating iron both within the mitochondria and in the cell. It is known that reducing intracellular iron pool results in decreased activity of the Fe-S cluster enzyme aconitase and subsequently triggers FET3 expression ( 105 , 106 ). Based on this, we measured aconitase activity of WT and N88S seipin-expressing cells grown to PDS phase, when FET3 expression was increased for the mutant. Aconitase activity was decreased by ~ 40% in the mutant (Fig. 7F), suggesting that mitochondrial Fe-S cluster synthesis/assembly may signal the upregulation of FET3 expression at PDS phase, while compensating for the reduced activation of the iron regulon by Aft1p, in an attempt to reestablish homeostatic intracellular iron levels. In agreement with this hypothesis, we observed that many genes involved in Fe-S cluster assembly were among the most affected DEGs in cells expressing the N88S seipin mutation under conditions of Fe deprivation (Fig. S4 D). 4. Discussion In this project, we provide evidence that inositol and neutral lipid metabolism and cellular iron homeostasis are compromised in the yeast model of N88S seipinopathy (Fig. 8). Importantly, our results are consistent with a reduced rate of phospholipid biosynthesis and increased TG content coupled with PA accumulation. As a result, the activity of the Opi1p transcriptional repressor is impaired, leading to derepression of INO1 expression and increased levels of Ino1p. Nevertheless, we did not observe altered levels of major phospholipids, including PC, PE, PS or PI. It has been previously reported that about 10% of the WT level of activity of the phospholipid biosynthetic enzymes is sufficient to maintain normal growth and almost normal lipid composition ( 31 , 85 , 107 ). However, a decrease in the protein levels of these enzymes is expected to significantly influence the flux of lipid precursor at the PA metabolic branch point, where PA can be channeled towards TG synthesis at the expense of a reduced rate of de novo synthesis of phospholipids (Fig. 8). Curiously, PG levels which is derived from CDP-DAG, were reduced. One possibility is impaired synthesis of CDP-DAG, resulting from decreased activity of Tam41p, thereby reducing the substrate availability for PG production. Additionally, dysfunction of enzymes responsible for the biosynthesis of PG could also contribute to lower PG levels ( 108 ). PA increases membrane order in the ER, and its accumulation has been associated with the induction of the ER stress response and apoptosis under various conditions ( 109 , 110 ). It would then be interesting to further explore whether changes in ER ultrastructure could also contribute to ER stress beyond IB formation associated with seipin misfolding. In addition, we observed increased levels of the pro-apoptotic ceramide, indicating a degree of pathological convergence of ceramide accumulation observed in different MNDs ( 111 , 112 ). Interestingly, we observed increased levels of lysophospholipids, indicating that lysophospholipid:acyl-CoA acyltransferases (LPLATs) Slc1p and Ale1p activities are impaired. Of particular interest, dysfunction in LPA signaling has been associated with several neurological conditions, including Alzheimer’s disease and Parkinson’s disease, and other disorders ( 113 – 115 ). Moreover, LPC has been shown to contribute to pericyte loss, disruption of the vascular barrier, demyelination, and motor function impairments ( 116 – 118 ). Additionally, LPC exacerbates the neurotoxicity of amyloid β1–42 peptide oligomer formation and promotes neurotoxic protein aggregation, highlighting its potential as a therapeutic target for neurodegenerative diseases ( 119 , 120 ). Notably, one study found that patients with repetitive mild traumatic brain injury exhibited significantly elevated LPC levels ( 121 ). Unfortunately, search for diagnostic and prognostic biomarkers in seipinopathy and related MNDs is scarce, and there are currently no definitive molecular biomarkers associated with such disorders. Here, we propose that PA and lysophospholipids could serve as potential candidates for biomarkers of this cohort of diseases. Overall, we provide strong evidence that N88S seipinopathy is also a lipidopathy. In fact, deletion of INO1 increased basal levels of the ER stress response, however this was associated with reduced IB formation in N88S seipin-expressing cells. It should be noted that INO1 deletion did not affect ROS levels in mutant cells, suggesting that oxidative stress is not directly linked to lipid metabolism defects. In line with abnormal lipid profile observed in cells expressing N88S seipin, which influences the activation of the ER stress response, we posit that an imbalance in cellular lipid homeostasis is a potential major driver of the neurotoxic process in human seipinopathy, with N88S seipin misfolding acting as the initiating trigger. This aligns with seipin´s crucial role in phospholipid and neutral lipid metabolism. However, we cannot exclude the possibility that seipinopathy and related human MNDs may be defined as both proteinopathies and lipidopathies. A vicious cycle of dysregulation in protein folding and lipid metabolism might be initiated by early and subtle changes in either lipid or protein handling as previously proposed ( 45 ). Another interesting finding of this work was the loss of iron homeostasis in the yeast model of N88S seipinopathy (Fig. 8). Our proteomic analysis revealed that levels of iron homeostasis-associated proteins, including Fit1p, Arn1p, Arn2p, and Hmx1p, were reduced in cells expressing the N88S seipin mutation. The expression of these proteins is regulated by the major iron-sensing transcription factor Aft1p, a key transcription factor that manages the cellular response to iron deficiency. In this study, it was shown that Aft1p transcriptional activity is deregulated during lifespan and upon iron depletion, which likely contributes to a defective adaptive response, particularly under conditions of iron deficiency. We provide strong evidence that Aft1p localization was impaired under excess iron conditions, and importantly MAPK Hog1p/p38 was involved in the regulation of CTH2 expression in response to iron starvation, but not throughout lifespan. This indicates that other major signaling effectors (e.g., Snf1p/AMPK or PKA) might control the transcription of genes belonging to the iron regulon via regulation of Aft1p activation and its transcriptional activity ( 37 , 38 ). Yet, we found that the expression of the ferroxidase Fet3p, which is required for high affinity iron transport and also regulated by Aft1p, was increased. While both Cth1p and Cth2p are transcriptionally induced by Aft1p/Aft2p, FET3 expression appears to be adaptively regulated by multiple transcription factors in response to changes in iron and other ion levels, including Ace1p, Aft1p and Msn2p. Importantly, Cth1/2p functions post-transcriptionally by targeting and degrading RNA transcripts of nonessential proteins that require large amounts of iron ( 49 ). In contrast, Fet3p operates upstream by capturing iron to fulfil cellular iron needs, with its expression being more closely associated with the iron-sulfur (Fe-S) biogenesis machinery ( 105 , 106 ). Notably, defects in the assembly of cytosolic Fe-S cluster-containing proteins do not trigger activation of the iron regulon. Instead, alterations in mitochondrial iron-sulfur cluster assembly are important for signaling iron bioavailability to Aft1p or Aft2p ( 122 , 123 ). The activity of the mitochondrial Fe-S enzyme aconitase was inversely correlated with the expression of FET3 in the mutant, in agreement with previous findings ( 106 ). We currently envision a model where coupling transcription of the high affinity iron transport system Ftr1p/Fet3p to the Fe-S cluster activity may provide a potential link that might explain why FET3 expression increased via activation of stress responsive transcription factors Msn2p/Msn4p (Fig. 8), despite reduced Aft1p transcriptional activity and iron imbalance. Moreover, it is known that Fe-S clusters are primary targets of ROS, so impaired Fe-S metabolism, as suggested by partial loss of aconitase activity, could potentially contribute to ROS buildup and oxidative damage exhibited by the N88S mutant strain ( 45 ). Loss of aconitase activity may therefore reflect increased levels of cellular dysfunction due to oxidative damage or possibly changes in other cellular processes, as recently proposed for Parkinson´s disease ( 124 ). This could be relevant to human N88S seipinopathy pathogenesis as a biomarker candidate to improve diagnostics/disease progression. Whether mitochondrial mobilization of iron coupled with the synthesis of Fe-S clusters is altered in N88S seipin-expressing cells is currently undefined, and should be explored in future studies. 5. Conclusions This study presents compelling evidence that human N88S seipinopathy may also be a lipidopathy linked to the disruption of iron homeostasis. The accumulation of PA and TG, combined with a decreased rate of phospholipid synthesis, plays a crucial role in inducing ER stress. This underscores the potential therapeutic strategy of targeting phospholipid and neutral lipid metabolism to manage ER stress and cell death arising from disruption of inositol metabolism. Such an approach could benefit patients with seipinopathy and other MNDs. Although many neurodegenerative and neuromotor syndromes are mostly related to iron overload with its deleterious effects in proteotoxicity and oxidative damage, there is increasing evidence that response to both iron overload and iron deficiency affects signalling pathways contributing to neuronal death. For instance, patients carrying biallelic mutations in IREB2 (Iron Responsive Element Binding Protein 2) display neurological and haematological defects associated with iron deficiency, impaired transcriptional regulation of iron metabolism and mitochondrial dysfunction ( 125 ), which are neuropathological cellular phenotypes reminiscent of seipinopathy ( 45 ). More recently, the analysis of primary fibroblasts from a patient with a loss-of-function mutation in L-ferritin revealed reduced cellular iron levels, lower catalase activity, ROS accumulation and increased levels of oxidized proteins ( 126 ). We have also previously reported a loss of catalase activity associated with ROS generation in the yeast model of seipinopathy ( 45 ), indicating that in both cases, impaired response to iron deficiency is likely associated with the oxidative stress response. Whether these phenotypes are closely related to the development of neuromotor defects observed in patients with seipinopathy remains to be investigated, but emerges as a novel and exciting avenue for therapeutic intervention in this cohort of MNDs. To the best of our knowledge, this study represents the first detailed description of protein and lipid alterations in N88S seipinopathy using systems biology. Abbreviations ACAT - Acyl-coenzyme A: cholesterol acyltransferase; AGPAT - Acylglycerolphosphate Acyltransferase; BiFC - Biomolecular Fluorescence Complementation; BPS - Bathophenanthrolinesulfonate; BSCL2 - Berardinelli-Seip congenital lipodystrophy type 2; CDP-DAG - Cytidine Diphosphate-Diacylglycerol; CYC1t - CYC1 terminator; DEG - Differentially Expressed Genes; DEP - Differentially Expressed Protein; DG - Diacylglycerol; DGAT - Acyl-CoA Diacylglycerol Acyltransferase; DNA - Deoxyribonucleic Acid; ER - Endoplasmic Reticulum; ERAD - ER-Associated Degradation; EXP - Exponential Phase; Fe-S - Iron-Sulfur; FIT - Fat storage-inducing transmembrane; GO - Gene Ontology; GPAT - Glycerol-3 Phosphate Acyltransferase; GPDpr - GPD promoter; IB - Inclusion body; IREB2 - Iron Responsive Element Binding Protein 2; LA - Lithium Acetate; LD - Lipid Droplet; LPA - Lysophosphatidic Acid; LPC - Lysophosphatidylcholine; LPLAT - Lysophospholipid:acyl-CoA acyltransferases; MAPK - Mitogen-Activated Protein Kinase; MNDs - Motor Neuron Diseases; MS - Mass Spectrometry; ONPG - O-nitrophenylgalactopyranosyde; PA - Phosphatidic Acid; PC - Phosphatidylcholine; PE - Phosphatidylethanolamine; PG - Phosphatidylglycerol; PI - Phosphatidylinositol; PS - Phosphatidylserine; PDS - Post-diauxic shift; PEG - Polyethylene glycol; ROS - Reactive Oxygen Species; SC - Synthetic Complete; SE - Sterol Esters; STRE - Stress Response Element; TFs - Transcription Factors; TG - Triacylglycerol; UPR - Unfolded Protein Response; VC - Venus C-terminal fragment; VN - Venus N-terminal fragment; WT - Wild-type; YNB - Yeast Nitrogen Base; YPD - Yeast Peptone Dextrose. Declarations Competing interests : The authors declare that they have no known competing financial interests or personal relationships that could have appeared to influence the work reported in this paper. The funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript, or in the decision to publish the results. Funding: This work was funded by national funds through Foundation for Science and Technology (FCT), under the project 2022.02305.PTDC, CEECIND/00724/2017 and CEECIND/00724/2017/CP1386/CT0006, and EMBO Scientific Exchange Grant 9890. Author Contribution V. T. and V. C. conceived and supervised the project. V. T. and V. C. designed the experiments and analyzed most of the data. M. R., M. O. and V. N. performed most of the experiments. V. T. wrote the manuscript with input from all authors. 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Supplementary Files TablesRibeiroetal2024.docx G2VSG1DownTableS3.xls G2VSG1UpTableS4.xls 17231529012771c7f427daf001upRNAseqTableS5.xls 17231529726741c7f439499001downRNAseqTableS6.xls findregulatorsMsn2Msn4TableS8.xlsx LegendsMarianaetal2024final.docx SupFigure1.pdf SupFigure2.pdf SupFigure3.pdf SupFigure4.pdf SupFigure5.pdf Cite Share Download PDF Status: Published Journal Publication published 07 Jan, 2025 Read the published version in Cell Communication and Signaling → Version 1 posted Editorial decision: Revision requested 23 Nov, 2024 Reviews received at journal 18 Nov, 2024 Reviews received at journal 17 Nov, 2024 Reviews received at journal 17 Nov, 2024 Reviews received at journal 13 Nov, 2024 Reviews received at journal 06 Nov, 2024 Reviewers agreed at journal 05 Nov, 2024 Reviewers agreed at journal 04 Nov, 2024 Reviewers agreed at journal 04 Nov, 2024 Reviewers agreed at journal 03 Nov, 2024 Reviewers agreed at journal 16 Oct, 2024 Reviewers invited by journal 14 Oct, 2024 Editor assigned by journal 09 Oct, 2024 Submission checks completed at journal 09 Oct, 2024 First submitted to journal 08 Oct, 2024 You are reading this latest preprint version Research Square lets you share your work early, gain feedback from the community, and start making changes to your manuscript prior to peer review in a journal. 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Also discoverable on Platform About Our Team In Review Editorial Policies Advisory Board Help Center Resources Author Services Accessibility API Access RSS feed Manage Cookie Preferences © Research Square 2026 | ISSN 2693-5015 (online) Privacy Policy Terms of Service Do Not Sell My Personal Information {"props":{"pageProps":{"initialData":{"identity":"rs-5224286","acceptedTermsAndConditions":true,"allowDirectSubmit":false,"archivedVersions":[],"articleType":"Research Article","associatedPublications":[],"authors":[{"id":364133750,"identity":"93ce1b8c-396c-456f-8b09-5cefda575045","order_by":0,"name":"Mariana O. Ribeiro","email":"","orcid":"","institution":"Institute for Research and Innovation in Health","correspondingAuthor":false,"prefix":"","firstName":"Mariana","middleName":"O.","lastName":"Ribeiro","suffix":""},{"id":364133753,"identity":"46d063f5-20ba-4af2-93a7-b2da922776e7","order_by":1,"name":"Mafalda Oliveira","email":"","orcid":"","institution":"Institute for Research and Innovation in Health","correspondingAuthor":false,"prefix":"","firstName":"Mafalda","middleName":"","lastName":"Oliveira","suffix":""},{"id":364133754,"identity":"7f04715f-6a37-4a32-8727-e4619a5052ea","order_by":2,"name":"Verónica Nogueira","email":"","orcid":"","institution":"Institute for Research and Innovation in Health","correspondingAuthor":false,"prefix":"","firstName":"Verónica","middleName":"","lastName":"Nogueira","suffix":""},{"id":364133763,"identity":"d4ccd58f-dec0-48b8-b7af-58a3e7491b31","order_by":3,"name":"Vítor Costa","email":"","orcid":"","institution":"Institute for Research and Innovation in Health","correspondingAuthor":false,"prefix":"","firstName":"Vítor","middleName":"","lastName":"Costa","suffix":""},{"id":364133765,"identity":"be79178c-b6a3-4522-b0ef-e06662983877","order_by":4,"name":"Vitor Teixeira","email":"data:image/png;base64,iVBORw0KGgoAAAANSUhEUgAAAZAAAAAyAQMAAABI0h/eAAAABlBMVEX///8AAABVwtN+AAAACXBIWXMAAA7EAAAOxAGVKw4bAAAA+0lEQVRIie3RsWrDMBCA4TMCeTmq1cEhfoUTHhPSV3EwZM7oobQKAU+hWfU4EgJ3Cc0DOEsIZG6XTqU0xE2htLbXDvpBCCE+3SAAn+8/xr52fl4GYIJJP7kYupI5StVcRD1j6HpyF9hJ6EnYYwHvo5sot6642w2DjeHxAvb3rcQxJrdAKccqs9uqxjDKeKzh1DplsGJ8oIBmZbgmq3iNgQYeI7he8lAy8WLVxzPCznQTwRqS8XANdlkaBJP1klQqSmWJFdnlY45Sz1ZjTafzQ3/HhT0cVDFKEp0fX9Xb9DYRztaLYi/apjTRj1OgGJDpFr9i3x/q8/l8PoBPgLZJN/bDKFYAAAAASUVORK5CYII=","orcid":"","institution":"Institute for Research and Innovation in Health","correspondingAuthor":true,"prefix":"","firstName":"Vitor","middleName":"","lastName":"Teixeira","suffix":""}],"badges":[],"createdAt":"2024-10-08 10:08:23","currentVersionCode":1,"declarations":"","doi":"10.21203/rs.3.rs-5224286/v1","doiUrl":"https://doi.org/10.21203/rs.3.rs-5224286/v1","draftVersion":[],"editorialEvents":[{"content":"https://doi.org/10.1186/s12964-024-02007-9","type":"published","date":"2025-01-07T15:57:50+00:00"}],"editorialNote":"","failedWorkflow":false,"files":[{"id":66424096,"identity":"a54398b1-f31b-44da-80d6-a9707e9bccab","added_by":"auto","created_at":"2024-10-11 16:36:33","extension":"png","order_by":1,"title":"Figure 1","display":"","copyAsset":false,"role":"figure","size":177544,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cstrong\u003eProteomic analysis of WT and N88S seipin-expressing cells.\u003c/strong\u003e \u003cstrong\u003e(A) \u003c/strong\u003eNumber of proteins significantly up- or down-regulated in the mutant strain. \u003cstrong\u003e(B)\u003c/strong\u003e The volcano plot illustrates the differentially expressed proteins (DEPs) in the N88S seipin mutant compared to the WT strain. The x-axis represents the log2 fold-change, while the y-axis shows the -log\u003csub\u003e10\u003c/sub\u003e P-value, indicating the probability of differential expression. A P-value \u0026lt; 0.05 and a fold-change \u0026gt; 1.2 were used as the significance thresholds for differential expression. Points of interest, marked in red and blue, highlight proteins with both substantial fold-change and high statistical significance. Red dots and blue dots indicate significantly up-regulated and down-regulated proteins, respectively. Grey dots correspond to proteins that were not significantly differentially expressed. \u003cstrong\u003e(C) \u003c/strong\u003eGene Ontology (GO) term enrichment analysis on biological processes was conducted for proteins exhibiting statistically significant alterations in\u0026nbsp;N88S seipin-expressing cell samples. \u003cstrong\u003e(D) \u003c/strong\u003eHeat map analyses of total protein level changes of enzymes of the phospholipid biosynthesis pathway in WT and N88S seipin-expressing cells (for the 3 independent experiments for each strain).\u003c/p\u003e","description":"","filename":"Figure1.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/acecc7a5d529e6141b13f67d.png"},{"id":66425155,"identity":"c7e151e5-6e86-4caa-af73-33f23c837136","added_by":"auto","created_at":"2024-10-11 17:00:34","extension":"png","order_by":2,"title":"Figure 2","display":"","copyAsset":false,"role":"figure","size":354173,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cstrong\u003eLipidomic analysis of WT and N88S seipin-expressing cells.\u003c/strong\u003e Total levels of phospholipids \u003cstrong\u003e(A)\u003c/strong\u003e, lysophospholipids \u003cstrong\u003e(B)\u003c/strong\u003e, diacylglycerol/DG (\u003cstrong\u003eC\u003c/strong\u003e), phosphatidic acid/PA (\u003cstrong\u003eD\u003c/strong\u003e) and triacylglycerols/TG (\u003cstrong\u003eE\u003c/strong\u003e) in the N88S seipin mutant compared to WT cells grown to post-diauxic shift (PDS)phase in SC-glucose medium.\u003c/p\u003e","description":"","filename":"Figure2.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/79b6e809f9619662c3958be1.png"},{"id":66965311,"identity":"b568a9b3-012d-471b-978f-ebecb45c1b18","added_by":"auto","created_at":"2024-10-18 13:39:37","extension":"png","order_by":3,"title":"Figure 3","display":"","copyAsset":false,"role":"figure","size":296177,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cstrong\u003eInositol and phospholipid metabolism is impaired and contributes to the ER stress response in N88S seipin-expressing cells. (A) \u003c/strong\u003eOpi1p-controlled expression of\u003cstrong\u003e \u003c/strong\u003e\u003cem\u003eINO1\u003c/em\u003e promoter is increased in N88S-seipin expressing cells during lifespan. Cells of specified genotypes expressing \u003cem\u003eINO1\u003c/em\u003e-LacZ were grown in SC-glucose medium and allowed to reach exponential (EXP), post-diauxic shift (PDS) and stationary (STAT) phases. Specific β-galactosidase (β-Gal) activity was measured as described Material and Methods. Left side: comparison between phases within the same strain. Right side: comparison between phases (WT vs N88S). \u003cstrong\u003e(B) \u003c/strong\u003eWestern blot showing total Ino1p-HA protein levels at the indicated periods of growth. Pgk1p was used as loading control. WT (WT-VN WT-VC INO1-HA) and N88S seipin-expressing cells (N88S-VN N88S-VC INO1-HA) were grown in SC-glucose medium during growth and aliquots were collected at different stages as indicated. \u003cstrong\u003e(C) \u003c/strong\u003eOvernight precultures of cells expressing \u003cem\u003eINO1\u003c/em\u003e-LacZ grown in SC-glucose medium lacking inositol were diluted to OD600=0.2 and resuspended in fresh SC medium supplemented (or not) with inositol (1 mM) and incubated for 4 h. β-galactosidase activity was measured as in Fig. 3A. \u003cstrong\u003e(D)\u003c/strong\u003e Cells of specified genotypes expressing \u003cem\u003eUPRE-LacZ \u003c/em\u003ewere grown in SC medium and allowed to reach the exponential phase. Specific β-galactosidase (β-Gal) activity was determined as in Fig. 3A. \u003cstrong\u003e(E) \u003c/strong\u003eOvernight precultures of cells expressing \u003cem\u003eUPRE-LacZ \u003c/em\u003egrown in SC-glucose medium lacking inositol were diluted to OD600=0.2, resuspended in fresh SC medium lacking inositol and incubated for 4 h. Half of the culture was collected by centrifugation, while the remaining culture was incubated in SC-glucose medium supplemented with inositol (1 mM) for 2 h. Specific β-galactosidase (β-Gal) activity was assessed as in Fig. 3A. Results are mean±SD. * \u003cem\u003ep \u003c/em\u003e≤ 0.05; ** \u003cem\u003ep\u003c/em\u003e ≤ 0.01; *** \u003cem\u003ep\u003c/em\u003e ≤ 0.001; **** \u003cem\u003ep\u003c/em\u003e ≤ 0.0001; ns - non-significant.\u003c/p\u003e","description":"","filename":"Figure3.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/90e5f4acfaf90dcc05ec3c66.png"},{"id":66424648,"identity":"20f7c8a9-d6db-43f8-9d61-ac3d1043ed4d","added_by":"auto","created_at":"2024-10-11 16:52:34","extension":"png","order_by":4,"title":"Figure 4","display":"","copyAsset":false,"role":"figure","size":686639,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cstrong\u003eDysregulation of inositol and phospholipid biosynthetic pathways leads to ER stress and IB formation in cells with the N88S seipin mutation. (A-B) \u003c/strong\u003eCells with the indicating genotypes expressing \u003cem\u003eUPRE-LacZ \u003c/em\u003ewere precultured overnight in SC-glucose medium. Cells were centrifuged, washed twice with water, diluted to OD\u003csub\u003e600\u003c/sub\u003e=0.2 and resuspended in fresh SC medium lacking inositol and incubated for 4 h. Specific β-galactosidase (β-Gal) activity was assessed as in Fig. 3A. \u003cstrong\u003e(C) \u003c/strong\u003eCells of specified genotypes expressing \u003cem\u003eUPRE-LacZ\u003c/em\u003e were grown as in Fig. 4A. Tenfold dilution series were spotted onto SC-glucose plates lacking inositol, or supplemented with inositol (1 mM) when indicated. Plates were incubated at 26°C for 2 days. \u003cstrong\u003e(D) \u003c/strong\u003eFormation of IBs was monitored by fluorescence microscopy using the YFP/Venus channel (left panel) in cells grown to the exponential phase in SC-glucose medium. Quantification is defined as percentage of cells displaying IB foci (n\u0026gt;100 cells, right panel). Data were combined from 2 independent experiments. DIC: Differential interference contrast. Bar scale, 8 μm. \u003cstrong\u003e(E)\u003c/strong\u003e Formation of IBs was monitored by flow cytometry using the FL1 channel and quantification of the Venus fluorescence intensity, normalized to cell number, was determined in cells grown to stationary phase. Results are mean±SD. * \u003cem\u003ep \u003c/em\u003e≤ 0.05; ** \u003cem\u003ep\u003c/em\u003e ≤ 0.01; **** \u003cem\u003ep\u003c/em\u003e ≤ 0.0001; ns - non-significant.\u003c/p\u003e","description":"","filename":"Figure4.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/a9072ebdfdfb1d674a9d081e.png"},{"id":66424098,"identity":"bc57f724-b86b-40f5-91ce-b17837b04fbe","added_by":"auto","created_at":"2024-10-11 16:36:34","extension":"png","order_by":5,"title":"Figure 5","display":"","copyAsset":false,"role":"figure","size":408590,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cstrong\u003eAft1p-mediated transcriptional activity is diminished at the diauxic shift and under iron-depleted conditions in cells expressing the N88S seipin mutation.\u003c/strong\u003e \u003cstrong\u003e(A)\u003c/strong\u003e Total iron levels were quantified in WT and\u0026nbsp;N88S seipin-carrying cells grown to exponential (EXP) and post-diauxic shift (PDS) phases.\u003cstrong\u003e (B)\u003c/strong\u003e Cells with the indicated genotypes expressing YEplac181-\u003cem\u003eCTH2\u003c/em\u003e-LacZ were grown in SC-glucose medium and allowed to grow to the indicated phases. Specific β-galactosidase (β-Gal) activities were determined as in Fig. 3A. \u003cstrong\u003e(C) \u003c/strong\u003eCells\u003cstrong\u003e \u003c/strong\u003ecarrying YEplac181-\u003cem\u003eCTH2\u003c/em\u003e-LacZ were grown to the exponential phase and treated or not with bathophenanthrolinedisulfonate (BPS, 100 μM) for 4 h. When indicated, the medium also contained FeSO\u003csub\u003e4 \u003c/sub\u003e(II) at a final concentration of 5 mM, in order to repress the iron regulon. Specific β-galactosidase (β-Gal) activities were measured as in Fig. 3A. \u003cstrong\u003e(D) \u003c/strong\u003eOvernight precultures of cells grown in SC-glucose medium were diluted to OD\u003csub\u003e600\u003c/sub\u003e=0.15 in fresh medium. BPS was added at a final concentration of 100 μM and cells were allowed to grow for 48 h. The growth rate was monitored by optical density (OD) at 600 nm (OD\u003csub\u003e600, \u003c/sub\u003eleft panel). ROS levels were assessed with the same cells labeled with dihydroethidium (DHE) via flow cytometry using the FL3 channel (right panel). \u003cstrong\u003e(E)\u003c/strong\u003e Cells were grown as in Fig. 5D, except that BPS was added only 24 h (at PDS phase) after the dilution step. The growth rate and ROS levels were determined accordingly after a 24 h incubation period. \u003cstrong\u003e(F) \u003c/strong\u003eCells of indicated genotypes were grown in SC-glucose medium to the exponential phase and diluted to OD\u003csub\u003e600\u003c/sub\u003e = 0.1. Tenfold dilution series were spotted onto SC plates supplemented with tert-butyl hydroperoxide (t-BOOH, 50 mM) or hydrogen peroxide (H\u003csub\u003e2\u003c/sub\u003eO\u003csub\u003e2\u003c/sub\u003e, 250 mM) and supplemented (or not) with the iron chelator BPS at a final concentration of 30 mM. Plates were incubated at 26 °C for 2 days. ** \u003cem\u003ep\u003c/em\u003e ≤ 0.01; *** \u003cem\u003ep\u003c/em\u003e ≤ 0.001; **** \u003cem\u003ep\u003c/em\u003e ≤ 0.0001; ns - non-significant.\u003c/p\u003e","description":"","filename":"Figure5.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/573ae1ad3e7dc87530588482.png"},{"id":66424459,"identity":"9d7bdcca-2c4c-49bc-b04c-80a365af5a1e","added_by":"auto","created_at":"2024-10-11 16:44:34","extension":"png","order_by":6,"title":"Figure 6","display":"","copyAsset":false,"role":"figure","size":721454,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cstrong\u003eMAPK Hog1p contributes to iron accumulation and iron dyshomeostasis in cells carrying the N88S seipin mutation under Fe deficiency. (A) \u003c/strong\u003eCells with the specified genotypes expressing pMP253 (\u003cem\u003eCYC1prom‐(2xCRE\u003c/em\u003e\u003csub\u003e\u003cem\u003eENA1\u003c/em\u003e\u003c/sub\u003e\u003cem\u003e)‐LacZ\u003c/em\u003e) were grown to reach the exponential phase (EXP) and post-diauxic shift (PDS) phase. Specific β-galactosidase (β-Gal) activities were measured as in Fig. 3A. \u003cstrong\u003e(B) \u003c/strong\u003eWestern blot showing the phosphorylation and total Aft1p-HA protein levels at the indicated periods of growth. Pgk1p was used as loading control. WT and N88S seipin-expressing cells carrying pRS415-HA-AFT1 were grown in SC-glucose medium during growth and aliquots were collected at different phases as indicated. \u003cstrong\u003e(C) \u003c/strong\u003eCells expressing GFP-AFT1 were grown in SC medium to exponential phase supplemented with 300 mM FeSO\u003csub\u003e4 \u003c/sub\u003e(II). DAPI was used to stain nuclei. GFP-Aft1p localization and DAPI signal were monitored by fluorescence microscopy (left panel), and quantification of the number of cells with nuclear/cytosolic signal is defined (n\u0026gt;100 cells; right panel). Scale bar, 8 µm. DIC: Differential interference contrast; DAPI- 4′-6-diamidino-2-phenylindole. \u003cstrong\u003e(D) \u003c/strong\u003eTotal iron levels were measured in the specified cells grown to the specified phases, as described in Fig. 5A. \u003cstrong\u003e(E-F) \u003c/strong\u003eCells with the specified genotypes expressing YEplac181-\u003cem\u003eCTH2\u003c/em\u003e-LacZ were grown as described in Fig. 5B and 5C, respectively. \u003cem\u003eCTH2\u003c/em\u003e-LacZ associated β-galactosidase (β-Gal) activities were measured as in Fig. 3A. * \u003cem\u003ep \u003c/em\u003e≤ 0.05; ** \u003cem\u003ep\u003c/em\u003e ≤ 0.01; *** \u003cem\u003ep\u003c/em\u003e ≤ 0.001; **** \u003cem\u003ep\u003c/em\u003e ≤ 0.0001; ns - non-significant.\u003c/p\u003e","description":"","filename":"Figure6.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/86d8d4d586b9f8312b919ef3.png"},{"id":66424106,"identity":"e9986a03-cea2-4b05-a69f-9b2c23a53ffd","added_by":"auto","created_at":"2024-10-11 16:36:34","extension":"png","order_by":7,"title":"Figure 7","display":"","copyAsset":false,"role":"figure","size":295067,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cem\u003e\u003cstrong\u003eFET3 \u003c/strong\u003e\u003c/em\u003e\u003cstrong\u003eexpression is more induced at the diauxic shift and under iron deficiency in N88S seipin-expressing cells\u003c/strong\u003e. \u003cstrong\u003e(A)\u003c/strong\u003e Cells with the indicated genotypes expressing YEplac181-\u003cem\u003eFET3\u003c/em\u003e-LacZ were grown in SC-glucose medium and allowed to grow to reach the exponential phase (EXP) and post-diauxic shift (PDS) phase. Specific β-galactosidase (β-Gal) activities were measured as in Fig. 3A. \u003cstrong\u003e(B) \u003c/strong\u003eOvernight precultures of cells with the specified genotypes expressing YEplac181-\u003cem\u003eFET3\u003c/em\u003e-LacZ were grown in SC-glucose medium to the exponential phase. Cells were incubated with the iron chelator BPS (100 mM) for 4 h to limit iron availability. Specific β-galactosidase (β-Gal) activities were determined as in Fig. 3A. \u003cstrong\u003e(C) \u003c/strong\u003eSchematic representation of the \u003cem\u003eFET3\u003c/em\u003epromoter. Here, it is displayed the putative Aft1p binding site, the Ace1p-like sequence and the newly identified Msn2p/Msn4p binding sequence. \u003cstrong\u003e(D) \u003c/strong\u003eOvernight precultures of cells with the indicated genotypes (cells expressing \u003cem\u003eIZH2\u003c/em\u003eunder the native promoter, or overexpressing \u003cem\u003eIZH2 \u003c/em\u003eunder the constitutive GPD promoter) carrying YEplac181-\u003cem\u003eFET3\u003c/em\u003e-LacZ were grown in SC-glucose medium and allowed to grow to the indicated phases. Specific β-galactosidase (β-Gal) activity was measured as in Fig. 3A. \u003cstrong\u003e(E) \u003c/strong\u003eOvernight precultures of cells with the specified genotypes expressing pSTRE-LacZ were grown in SC-glucose medium to reach the EXP, PDS and stationary (STAT) phases. Specific β-galactosidase (β-Gal) activity was measured as in Fig. 3A.\u003cstrong\u003e (F) \u003c/strong\u003eAconitase activity was measured in PDS-grown cells in SC-glucose medium. Results are mean±SD. * \u003cem\u003ep \u003c/em\u003e≤ 0.05; ** \u003cem\u003ep\u003c/em\u003e ≤ 0.01; *** \u003cem\u003ep\u003c/em\u003e ≤ 0.001; **** \u003cem\u003ep\u003c/em\u003e ≤ 0.0001; ns - non-significant.\u003c/p\u003e","description":"","filename":"Figure7.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/955c8f9457be2e9753a321cd.png"},{"id":66424113,"identity":"6e466c97-c265-44ad-9ae3-1e848d31f027","added_by":"auto","created_at":"2024-10-11 16:36:34","extension":"png","order_by":8,"title":"Figure 8","display":"","copyAsset":false,"role":"figure","size":386428,"visible":true,"origin":"","legend":"\u003cp\u003e\u003cstrong\u003eUncovering iron imbalance and inositol metabolism disruption: insights from the yeast model of N88S seipinopathy. \u003c/strong\u003eIn this model system, there is an accumulation of PA associated with derepressed \u003cem\u003eINO1\u003c/em\u003eexpression, along with reduced protein levels of key enzymes in the phospholipid biosynthetic pathway. This dysregulation is accompanied by an increase in triglyceride (TG) levels in cells expressing the N88S mutation.\u003c/p\u003e\n\u003cp\u003eWhereas WT cells normally upregulate \u003cem\u003eCTH2\u003c/em\u003e and \u003cem\u003eFET3\u003c/em\u003e expression during the diauxic shift, responding to increased iron demand, cells expressing N88S seipin exhibit impaired Aft1p/Aft2p transcriptional activity, leading to reduced levels of iron transport and storage proteins such as Fit1p, Arn1p, Arn2p, and Hmx1p. This results in iron dyshomeostasis, particularly under iron-deficient conditions. The activation of the stress response via transcription factors Msn2p/Msn4p may provide an adaptive mechanism to better manage iron deficiency during the transition to the post-diauxic shift. This adaptation potentially allows cells to bypass the reduced function of Aft1p/Aft2p on the iron regulon, thereby enhancing iron assimilation through the reductive pathway. This pathway involves the reduction of ferric to ferrous ions and the protein complex formed by the Ftr1p transporter and the Fet3p ferroxidase. Moreover, we propose that \u003cem\u003eFET3\u003c/em\u003e expression is linked to potential disruptions in Fe-S cluster activity and/or assembly in cells carrying the N88S seipin mutation. This is supported by the observed reduction in aconitase activity, which relies on an intact [4Fe-4S] cluster for full functionality. Our findings indicate that human N88S seipinopathy might be both a proteinopathy and a lipidopathy, with disruption in inositol and lipid metabolism playing a significant role in triggering the ER stress response. Furthermore, the resulting iron imbalance may impair various cellular functions, including antioxidant mechanisms like catalase, and could contribute to the progression of neurodegenerative traits observed in human disease.\u003c/p\u003e\n\u003cp\u003eGreen and red indicates upregulated and downregulated, respectively. Dashed black line indicates gene expression, whereas solid line specifies protein levels.\u003c/p\u003e","description":"","filename":"8.png","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/f170f49b8fca7f6efc9dc47e.png"},{"id":73694757,"identity":"dd7b1f50-d57e-4586-a60f-06fdf9d01e4c","added_by":"auto","created_at":"2025-01-13 16:13:54","extension":"pdf","order_by":0,"title":"","display":"","copyAsset":false,"role":"manuscript-pdf","size":5295585,"visible":true,"origin":"","legend":"","description":"","filename":"manuscript.pdf","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/b12f7291-c871-4339-acb0-7812a950fa9b.pdf"},{"id":66424646,"identity":"32402d81-02d2-40b3-87f1-537a8e517c9b","added_by":"auto","created_at":"2024-10-11 16:52:34","extension":"docx","order_by":1,"title":"","display":"","copyAsset":false,"role":"supplement","size":60397,"visible":true,"origin":"","legend":"","description":"","filename":"TablesRibeiroetal2024.docx","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/13e70bb401ae2324de9034be.docx"},{"id":66424101,"identity":"dd5ff3ef-3c2a-42cc-8e97-0156597edcea","added_by":"auto","created_at":"2024-10-11 16:36:34","extension":"xls","order_by":2,"title":"","display":"","copyAsset":false,"role":"supplement","size":169818,"visible":true,"origin":"","legend":"","description":"","filename":"G2VSG1DownTableS3.xls","url":"https://assets-eu.researchsquare.com/files/rs-5224286/v1/2d64cb7dd7b5c8fd2ba556dd.xls"},{"id":66424110,"identity":"518c1604-ac9e-4247-851f-e76719064855","added_by":"auto","created_at":"2024-10-11 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Introduction","content":"\u003cp\u003eLipid droplets (LDs) are ubiquitous cellular organelles responsible for fat storage, consisting of a core of triacylglycerols (TG) and sterol esters (SE) surrounded by a protein-decorated phospholipid monolayer membrane (\u003cspan additionalcitationids=\"CR2\" citationid=\"CR1\" class=\"CitationRef\"\u003e1\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR3\" class=\"CitationRef\"\u003e3\u003c/span\u003e). LD dysfunction is linked to multiple diseases, making the study of LD biogenesis pivotal for understanding basic disease mechanisms.\u003c/p\u003e \u003cp\u003eLDs are formed in the Endoplasmic Reticulum (ER), where enzymes like DGAT1 and DGAT2 (diacylglycerol acyltransferases, Dga1p and Lro1p in yeast) and ACAT1 and ACAT2 (acyl-coenzyme A: cholesterol acyltransferases, Are1p and Are2p in yeast) convert excess cellular fatty acids and cholesterol into TG and SE (\u003cspan additionalcitationids=\"CR5\" citationid=\"CR4\" class=\"CitationRef\"\u003e4\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR6\" class=\"CitationRef\"\u003e6\u003c/span\u003e). These neutral lipids accumulate within the ER bilayer, coalescing to form an oil lens that grows and eventually buds off. Proteins such as fat storage-inducing transmembrane (FIT) proteins, perilipins, and the seipin complex (human BSCL2 and the Sei1p-Ldb16p complex in yeast) facilitate this process (\u003cspan additionalcitationids=\"CR5\" citationid=\"CR4\" class=\"CitationRef\"\u003e4\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR6\" class=\"CitationRef\"\u003e6\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eSeipin, which is expressed in motor neurons of the spinal cord and cortical neurons in the frontal lobe, hypothalamus, and brainstem (\u003cspan citationid=\"CR7\" class=\"CitationRef\"\u003e7\u003c/span\u003e), and is essential for excitatory synaptic transmission and neurotransmitter release (\u003cspan citationid=\"CR7\" class=\"CitationRef\"\u003e7\u003c/span\u003e). This protein functions as a membrane protein featuring two transmembrane domains, a conserved luminal loop, and cytosolic domains that assembles into an oligomeric ring-like complex, which is essential for TG binding and proper LD budding and growth (\u003cspan additionalcitationids=\"CR9 CR10 CR11 CR12\" citationid=\"CR8\" class=\"CitationRef\"\u003e8\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR13\" class=\"CitationRef\"\u003e13\u003c/span\u003e). For that reason, seipin plays a crucial role in the formation and maintenance of ER-LD contact sites. At these membrane junctions, seipin facilitates the transfer of neutral lipids from the ER to the forming LDs, ensuring efficient lipid storage and metabolism. In several organisms, deletion of seipin leads to severe cellular phenotypes, including the aberrant formation of LDs, which manifest as clustered or enlarged LDs (\u003cspan additionalcitationids=\"CR15\" citationid=\"CR14\" class=\"CitationRef\"\u003e14\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR16\" class=\"CitationRef\"\u003e16\u003c/span\u003e), and impaired lipid homeostasis associated with altered cellular lipid profile and metabolic dysfunctions (\u003cspan citationid=\"CR7\" class=\"CitationRef\"\u003e7\u003c/span\u003e, \u003cspan citationid=\"CR17\" class=\"CitationRef\"\u003e17\u003c/span\u003e), as observed in severe congenital generalized lipodystrophy and other metabolic diseases. On the other hand, gain-of-function mutations in seipin, including N88S and S90L, are associated with autosomal dominant motor neuron diseases (MNDs), such as hereditary spastic paraplegias (Silver syndrome), Charcot-Marie-Tooth disease type 2, and distal hereditary motor neuropathy type V (\u003cspan additionalcitationids=\"CR19 CR20\" citationid=\"CR18\" class=\"CitationRef\"\u003e18\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR21\" class=\"CitationRef\"\u003e21\u003c/span\u003e). This cohort of MNDs involve gradual involvement of both upper motor neurons (resulting in gait disturbances and pyramidal signs) and lower motor neurons (leading to amyotrophy of the peroneal muscles and small hand muscles), as well as \u003cem\u003epes cavus\u003c/em\u003e (\u003cspan citationid=\"CR22\" class=\"CitationRef\"\u003e22\u003c/span\u003e). By disrupting \u003cem\u003eN\u003c/em\u003e-glycosylation, these mutations stimulate protein aggregation, resulting in ER stress and cell death (\u003cspan citationid=\"CR7\" class=\"CitationRef\"\u003e7\u003c/span\u003e, \u003cspan citationid=\"CR23\" class=\"CitationRef\"\u003e23\u003c/span\u003e, \u003cspan citationid=\"CR24\" class=\"CitationRef\"\u003e24\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eThe molecular mechanisms underlying seipinopathy remain largely unresolved. Expression of dominant, unglycosylated N88L and S90L variants of seipin triggers a pronounced ER stress response by activating the unfolded protein response (UPR). This activation leads to the segregation of mutant seipin into inclusion bodies (IBs). The exact composition and characteristics of these IBs are still unclear. However, it is known that IBs do not colocalize with aggresomal markers such as pericentrin or vimentin (\u003cspan citationid=\"CR7\" class=\"CitationRef\"\u003e7\u003c/span\u003e). Despite these observations, the N88S seipin variant undergoes polyubiquitination and is subsequently targeted for degradation via the proteasome through the ER-associated degradation (ERAD) pathway (\u003cspan citationid=\"CR7\" class=\"CitationRef\"\u003e7\u003c/span\u003e, \u003cspan citationid=\"CR25\" class=\"CitationRef\"\u003e25\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eNeutral lipid metabolism, which drives LD biogenesis, is intricately linked to phospholipid biosynthesis pathways, as both processes are crucial for maintaining cellular lipid homeostasis and organellar membrane integrity (\u003cspan citationid=\"CR26\" class=\"CitationRef\"\u003e26\u003c/span\u003e). The synthesis of membrane phospholipids begins with the phospholipid phosphatidic acid (PA). In the \u003cem\u003ede novo\u003c/em\u003e pathways, membrane glycerophospholipids are synthesized from PA through the liponucleotide intermediate CDP-diacylglycerol (CDP-DAG). It can also be channelled towards the synthesis of phosphatidylglycerol (PG). Additionally, CDP-DAG serves as a precursor for the synthesis of TG stored in LDs (\u003cspan citationid=\"CR26\" class=\"CitationRef\"\u003e26\u003c/span\u003e). Phospholipid synthesis is tightly regulated by modulating both enzyme expression and activity. This regulation is influenced by various factors such as carbon source, nutrient availability, growth stage, pH, and temperature (\u003cspan citationid=\"CR26\" class=\"CitationRef\"\u003e26\u003c/span\u003e). Key to this control are \u003cem\u003ecis\u003c/em\u003e-acting elements like the inositol-responsive UAS\u003csub\u003e\u003cem\u003eINO\u003c/em\u003e\u003c/sub\u003e, and transcription factors including the Ino2p-Ino4p complex and the transcriptional repressor Opi1p, which orchestrate the transcriptional regulation of phospholipid biosynthetic genes (\u003cspan citationid=\"CR27\" class=\"CitationRef\"\u003e27\u003c/span\u003e, \u003cspan citationid=\"CR28\" class=\"CitationRef\"\u003e28\u003c/span\u003e). Genes involved in the CDP-DAG pathway (e.g., \u003cem\u003eCDS1, CHO1, PSD1, CHO2, OPI3\u003c/em\u003e), and in the synthesis of phosphatidylinositol (e.g., \u003cem\u003eINO1\u003c/em\u003e) are regulated by UAS\u003csub\u003eINO\u003c/sub\u003e elements in their promoters (\u003cspan citationid=\"CR29\" class=\"CitationRef\"\u003e29\u003c/span\u003e, \u003cspan citationid=\"CR30\" class=\"CitationRef\"\u003e30\u003c/span\u003e). This element binds the Ino2p-Ino4p heterodimer, which activates transcription when inositol levels drop. However, when Opi1p binds to Ino2p, which essentially occurs in response to an increase in inositol levels, this activation is repressed (\u003cspan citationid=\"CR30\" class=\"CitationRef\"\u003e30\u003c/span\u003e, \u003cspan citationid=\"CR31\" class=\"CitationRef\"\u003e31\u003c/span\u003e). It is known that Opi1p transcriptional repressor activity is influenced by its cellular localization. Although Opi1p lacks a membrane-spanning domain, it associates with the nuclear/ER membrane through interaction with the integral membrane protein Scs2p and PA via electrostatic interactions (\u003cspan citationid=\"CR32\" class=\"CitationRef\"\u003e32\u003c/span\u003e, \u003cspan citationid=\"CR33\" class=\"CitationRef\"\u003e33\u003c/span\u003e). When PA levels decrease (e.g., in response to an increase in inositol levels), Opi1p is no longer anchored to the ER and is translocated into the nucleus to repress transcription of \u003cem\u003eINO1\u003c/em\u003e and UAS\u003csub\u003eINO\u003c/sub\u003e-containing phospholipid synthesis genes (\u003cspan citationid=\"CR31\" class=\"CitationRef\"\u003e31\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eNeurological issues have also been linked to dysregulated iron (Fe) metabolism, which can promote oxidative stress and cellular damage. Iron (Fe) is essential for various biological processes, including cell respiration, neurotransmitter synthesis, metabolism, lipid biosynthesis, and oxygen delivery (\u003cspan citationid=\"CR34\" class=\"CitationRef\"\u003e34\u003c/span\u003e, \u003cspan citationid=\"CR35\" class=\"CitationRef\"\u003e35\u003c/span\u003e). However, excessive iron can generate ROS, leading to the oxidation of proteins, lipids, and nucleic acids, which is harmful (\u003cspan citationid=\"CR36\" class=\"CitationRef\"\u003e36\u003c/span\u003e, \u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e37\u003c/span\u003e). Dysregulated iron metabolism in the brain is associated with neurological issues, promoting oxidative stress and cellular damage. Thus, cells have developed complex mechanisms to regulate iron levels (\u003cspan citationid=\"CR36\" class=\"CitationRef\"\u003e36\u003c/span\u003e). In yeast, the transcription factors Aft1p and its paralog Aft2p manage the cellular response to iron deficiency by activating genes of the iron regulon (\u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e37\u003c/span\u003e, \u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e38\u003c/span\u003e). These factors are transported into the nucleus by karyopherin Pse1p, where they bind to target genes to initiate transcription (\u003cspan citationid=\"CR36\" class=\"CitationRef\"\u003e36\u003c/span\u003e, \u003cspan citationid=\"CR39\" class=\"CitationRef\"\u003e39\u003c/span\u003e). Under iron deficiency, \u003cem\u003eS. cerevisiae\u003c/em\u003e activates the Fe regulon to acquire iron from the environment via reductive and non-reductive pathways. In the reductive pathway, iron is reduced from the ferric (Fe\u003csup\u003e3+\u003c/sup\u003e) to the ferrous (Fe\u003csup\u003e2+\u003c/sup\u003e) state by Fre1-4p metalloreductases, and imported into the cytoplasm by a copper-dependent complex of Fet3p and Ftr1p. Copper activates Fet3p oxidase activity, aided by the copper chaperone Atx1p and the transporter Ccc2p (\u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e38\u003c/span\u003e, \u003cspan citationid=\"CR39\" class=\"CitationRef\"\u003e39\u003c/span\u003e). The non-reductive pathway imports siderophore-iron complexes retained by mannoproteins Fit1-3p and transported into the cell by Arn1-4p transporters (\u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e38\u003c/span\u003e, \u003cspan citationid=\"CR39\" class=\"CitationRef\"\u003e39\u003c/span\u003e). Iron homeostasis is also maintained by regulating iron-dependent metabolic processes. Non-essential pathways are downregulated, and iron is redirected to essential ones. Aft1p and Aft2p upregulate Cth2p, an mRNA-binding protein that restricts the expression of genes encoding iron-containing proteins or associated with iron-utilizing pathways (\u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e38\u003c/span\u003e, \u003cspan citationid=\"CR39\" class=\"CitationRef\"\u003e39\u003c/span\u003e). Cth2p also aids in prioritizing iron allocation towards specific pathways while stalling or inhibiting its mobilization in non-essential processes, including heme biosynthesis and mitochondrial respiration. The heme oxygenase Hmx1p degrades heme to free iron for essential pathways, helping cells survive under conditions of iron starvation (\u003cspan citationid=\"CR40\" class=\"CitationRef\"\u003e40\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eUnder iron-replete conditions, Aft1p is transported from the nucleus into the cytosol in a process facilitated by Msn5p. This export mechanism requires proper biosynthesis of mitochondrial Fe-S clusters and their subsequent export to the cytoplasm, ensuring inhibition of Aft1p activity when iron is readily available (\u003cspan citationid=\"CR41\" class=\"CitationRef\"\u003e41\u003c/span\u003e, \u003cspan citationid=\"CR42\" class=\"CitationRef\"\u003e42\u003c/span\u003e). Importantly, Aft1p phosphorylation is negatively regulated by Mitogen-Activated Protein Kinase (MAPK) Hog1p/p38 in iron-replete conditions (\u003cspan citationid=\"CR43\" class=\"CitationRef\"\u003e43\u003c/span\u003e), and Slt2p/Mpk1p is also involved in maintaining iron levels by directly regulating Aft1p activity (\u003cspan citationid=\"CR44\" class=\"CitationRef\"\u003e44\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eMore recently, we have developed a yeast model for N88S seipinopathy that recapitulates the cellular characteristics observed in human seipinopathy (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). This model exhibits increased ER stress levels with aging and the formation of IBs is also observed. Notably, cells expressing N88S homo-oligomers show reduced viability, increased oxidative damage from higher generation of reactive oxygen species (ROS), lipid peroxidation, and significantly decreased antioxidant activity (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). Using this system, we performed a multi mass spectrometry-based omics approach to investigate protein functions and delineate the signaling pathways involved in the pathological features of N88S seipinopathy. Altered cellular processes, as well as potential therapeutic targets and biomarkers, were identified and can be now explored in translational studies using human cell models.\u003c/p\u003e"},{"header":"2. Materials and Methods","content":"\u003cdiv id=\"Sec3\" class=\"Section2\"\u003e \u003ch2\u003e2.1. Yeast strains and plasmids\u003c/h2\u003e \u003cp\u003e \u003cem\u003eS. cerevisiae\u003c/em\u003e strains used in this study resulted from the W303α parental strain and are described in Table \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003e. Protein tagging and individual gene deletions were performed by standard PCR-based homologous recombination (\u003cspan citationid=\"CR46\" class=\"CitationRef\"\u003e46\u003c/span\u003e, \u003cspan citationid=\"CR47\" class=\"CitationRef\"\u003e47\u003c/span\u003e). Primers were designed using Primers-4-Yeast (\u003cspan citationid=\"CR48\" class=\"CitationRef\"\u003e48\u003c/span\u003e) for pFA6 and pYM plasmid sets (\u003cspan citationid=\"CR46\" class=\"CitationRef\"\u003e46\u003c/span\u003e, \u003cspan citationid=\"CR47\" class=\"CitationRef\"\u003e47\u003c/span\u003e). Plasmids used in this study are listed in Table \u003cspan refid=\"MOESM2\" class=\"InternalRef\"\u003eS2\u003c/span\u003e. For cloning of \u003cem\u003eCTH2-\u003c/em\u003eLacZ in the YEplac181 vector, pCM64-CTH2-FeRE-CYC1-LacZ plasmid (\u003cspan citationid=\"CR49\" class=\"CitationRef\"\u003e49\u003c/span\u003e) was digested with HindIII, and the insert was cloned into the HindIII restriction site of the YEplac181 vector. For cloning of ADH1pr-\u003cem\u003eCDS1\u003c/em\u003e-3HA into the pRS315-UPRE-LacZ vector (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e), the plasmid UG75-ADH-\u003cem\u003eCDS1\u003c/em\u003e-3HA (\u003cspan citationid=\"CR50\" class=\"CitationRef\"\u003e50\u003c/span\u003e) was digested with SacII, and the resulting insert was cloned into the SacII restriction site of the pRS315-UPRE-LacZ vector. Plasmid YEplac181-\u003cem\u003eFET3\u003c/em\u003e-LacZ was generated by digesting p\u003cem\u003eFET3\u003c/em\u003e-LacZ (\u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e51\u003c/span\u003e) with ScaI and performing ligation into the SmaI restriction site of YEplac181. To produce plasmid YEplac181-GFP-\u003cem\u003eAFT1\u003c/em\u003e, pRS426-GFP-\u003cem\u003eAFT1\u003c/em\u003e (\u003cspan citationid=\"CR52\" class=\"CitationRef\"\u003e52\u003c/span\u003e) was cut with SacI and KpnI and the resulting insert was ligated into the same restriction sites of YEplac181. All constructs were verified either by sequencing (plasmids) or PCR (mutant strains). Strains were transformed using the standard lithium acetate procedure (\u003cspan citationid=\"CR53\" class=\"CitationRef\"\u003e53\u003c/span\u003e).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec4\" class=\"Section2\"\u003e \u003ch2\u003e2.2. Culture media and growth conditions\u003c/h2\u003e \u003cp\u003eThe yeast cells were grown aerobically at 26 \u0026ordm;C in a gyratory shaker at 140 rpm using Erlenmeyer flasks. A 1:5 proportion of growth media to flask volume was used. The liquid growth media used for yeast grown were: Yeast peptone dextrose (YPD) [1% (wt/vol) yeast extract (Conda Pronadisa), 2% (wt/vol) bacto peptone (LabM) and 2% (wt/vol) glucose (Fisher Scientific)], and synthetic complete (SC) medium [2% (wt/vol) glucose (Fisher Scientific) and 0.67% (wt/vol) yeast nitrogen base (YNB) without amino acids (BD BioSciences), supplemented with appropriate amino acids and nucleotides: (0.008% (wt/vol) histidine (Sigma Aldrich), 0.008% (wt/vol) tryptophan (Sigma Aldrich), 0.04% (wt/vol) leucine (Sigma Aldrich), 0.008% (wt/vol) uracil (Sigma Aldrich) and 0.008% (wt/vol) adenine (Sigma Aldrich)]. When indicated, YNB without aa and inositol was used (FORMEDIUM, ref: CYN3701) to prepare SC-glucose medium without inositol. For solid medium, 1.5% (wt/vol) agar (Conda Pronadisa) was added, supplemented or not with 3 \u0026micro;M FeSO\u003csub\u003e4\u003c/sub\u003e (II). Where indicated, myo-inositol (Sigma Aldrich) was used at a final concentration of 1 mM. The iron chelator bathophenanthrolinedisulfonate (BPS, Sigma Aldrich) was added to a final concentration of 100 \u0026micro;M in liquid medium to create iron-starvation conditions. Cells were grown to exponential (OD\u003csub\u003e600\u003c/sub\u003e\u0026thinsp;\u0026asymp;\u0026thinsp;0,6), to the post-diauxic shift (PDS) phase (24 h after exponential phase) or to early stationary phase (48 h after exponential phase).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec5\" class=\"Section2\"\u003e \u003ch2\u003e2.3. Proteomics analysis\u003c/h2\u003e \u003cp\u003eFor proteome analysis, cells were grown to PDS phase in SC-glucose medium. Proteomics were performed by the company BGI on a commercial basis following standard protocols (\u003cspan citationid=\"CR54\" class=\"CitationRef\"\u003e54\u003c/span\u003e). The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE (\u003cspan citationid=\"CR55\" class=\"CitationRef\"\u003e55\u003c/span\u003e) partner repository with the dataset identifier PXD054826.\u003c/p\u003e \u003cp\u003e \u003col\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.3.1. Protein preparation for proteomic analysis\u003c/b\u003e. Proteins were extracted with Lysis buffer (7 M urea, 2 M thiourea, 20 mM tris-HCl, pH 8.0), containing 1X Cocktail and 10 mM dithiothreitol (DTT). The samples were then sonicated on ice and centrifuged at 4\u0026deg;C, 25,000 g for 15 min. The supernatant was mixed with ice-cold acetone (1:5, v/v) containing 20 mM DTT and incubated at -20\u0026deg;C overnight. After centrifugation at 4\u0026deg;C, 25,000 g for 15 min, the precipitate was collected, washed twice with ice-cold acetone containing 20 mM DTT, and then air-dried. To reduce disulfide bonds, the dried samples were re-dissolved in Lysis buffer (without SDS) containing 10 mM DTT (final concentration) and incubated at 56\u0026deg;C for 1 h. Subsequently, 55 mM iodoacetamide (IAM, final concentration) was added to block the cysteines and the samples were further incubated for 1 h in the darkroom. Following the incubation, the samples were then precipitated with ice-cold acetone, air-dried, and finally dissolved in 0.5 M TEAB (tetraethyl ammonium bromide) (Applied Biosystems, Milan, Italy), before being used for protein quantification and subsequent iTRAQ labeling.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.3.2. Peptide labeling\u003c/b\u003e. The protein (100 \u0026micro;g) was digested with Trypsin Gold (Promega, Madison, WI, USA) (30:1, protein: trypsin) at 37\u0026deg;C for 16 h. Digested samples were dried by vacuum centrifugation, reconstituted in 0.5 M TEAB and processed according to the manufacturer\u0026rsquo;s protocol for 6-plex iTRAQ reagent labeling (Applied Biosystems). The labeled peptide mixtures were then pooled and dried by vacuum centrifugation.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.3.3. Peptide Fractionation.\u003c/b\u003e The Shimadzu LC-20AB liquid phase system was used, and the separation column was a 5 \u0026micro;m, 4.6x250 mm Gemini C18 column for liquid phase separation of the sample. The dried peptide samples were reconstituted with mobile phase A (5% acetonitrile, ACN pH 9.8), injected and eluted at a flow rate of 1mL/min using the following gradients: 5% mobile phase B (95% ACN, pH 9.8) for 10 min. 5\u0026ndash;35% mobile phase B for 40 min, 35\u0026ndash;95% mobile phase B for 1-min, mobile phase B for 3 min, and 5% mobile phase B for 10 min. The elution peak was monitored at a wavelength of 214 nm, and one component was collected per min. The samples were combined according to the chromatographic elution peak map to obtain 20 fractions, which were then freeze-dried.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.3.4. LC-ESI-MS/MS analysis.\u003c/b\u003e The peptides were separated using a Thermo Easy nLC 1200 (Thermo Fisher Scientific, San Jose, CA) and loaded onto an analytical C18 column packed in-house (75 \u0026micro;m inner diameter, 1.8 \u0026micro;m column material particle size, 25 cm column length). The separation was carried out through the following effective gradient at a flow rate of 250 nL/min: 0\u0026thinsp;~\u0026thinsp;3 min, 5\u0026ndash;10% mobile phase B (80% ACN, 0.1% FA); 3\u0026thinsp;~\u0026thinsp;43 min, mobile phase B increased linearly from 10\u0026ndash;30%; 43\u0026thinsp;~\u0026thinsp;53 min, mobile phase B linearly increased from 35\u0026ndash;44%; 53\u0026thinsp;~\u0026thinsp;63 min, mobile phase B increased from 40\u0026ndash;100%; 63\u0026thinsp;~\u0026thinsp;70 min, 100% mobile phase B. The end of the nanoliter liquid phase separation was directly connected to the mass spectrometer.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.3.5. Mass Spectrometry Detection.\u003c/b\u003e The eluate was subjected to nanoelectrospray ionization and entered into the tandem mass spectrometer Orbitrap Eclipse (Thermo Fisher Scientific, San Jose, CA) for DDA (Data Dependent Acquisition) mode detection. Main parameter settings: the scanning range of the primary mass spectrometer was 350\u0026thinsp;~\u0026thinsp;1,600m/z; the resolution was set to 60,000; the initial m/z of the secondary mass spectrometer was fixed at 100; the resolution was 15,000. The precursor ion screening conditions for secondary fragmentation were: charge 2\u0026thinsp;+\u0026thinsp;to 7+, peak intensity over 25000, Data Dependent Mode set to Cycle Time, Time between Master Scans set to 2s. The ion fragmentation mode was HCD, the fragment ions were detected in Orbitrap, the fragmentation energy was 36, and the separation window was set to 0.7 m/z. The dynamic exclusion time was set to 45s. The AGC settings were: 1.2E6 for the first level and 5E4 for the second level.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.3.6. Bioinformatics analysis\u003c/b\u003e. Protein identification was performed using Mascot search engine (version 2.3.02; Matrix Science, London, UK) against the \u003cem\u003eSaccharomyces\u003c/em\u003e 811 (27719 sequences) database, after removal of redundant sequences). Search parameters were set as follows: monoisotopic mass; peptide mass tolerance at 10 ppm and fragment mass tolerance at 0.02 Da; trypsin as the enzyme; allowing one missed cleavage; +2 and +\u0026thinsp;3 as the peptide; oxidation (M), deamidated (NQ), Itraq8plex (Y) as the potential variable modifications, and carbamidomethyl (C), iTRAQ8plex (N-term), iTRAQ8plex (K) as fixed modifications.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.3.7. Protein Quantification.\u003c/b\u003e An automated software called IQuant (\u003cspan citationid=\"CR56\" class=\"CitationRef\"\u003e56\u003c/span\u003e) was used to quantitatively analyzing the labeled peptides with isobaric tags. It integrates Mascot Percolator, a well performing machine learning method for rescoring database search results, to provide reliable significant measures. To assess the confidence of peptides, the peptide-spectrum matches (PSMs) were pre-filtered at a PSM-level false discovery rate (FDR) of 1%. Then, based on the \"simple principle\" (The parsimony principle), identified peptide sequences were assembled into a set of confident proteins. In order to control the rate of false-positive at protein level, a protein FDR at 1%, which is based on Picked protein FDR strategy (\u003cspan citationid=\"CR57\" class=\"CitationRef\"\u003e57\u003c/span\u003e), was estimated after protein inference (Protein-level FDR\u0026thinsp;\u0026lt;\u0026thinsp;=\u0026thinsp;0.01). The protein quantification process included the following steps: Protein identification, Tag impurity correction, Data normalization, Missing value imputation, Protein ratio calculation, Statistical analysis, Results presentation. The main IQuant quantification parameters were: Quant peptide: Use all Unique peptide; Quant number: at least one unique spectra; Normalization: VSN; Protein Ratio: Weighted average; Statistical Analysis: Permutation Test. In total, there were 4543 proteins identified, among which 97 and 115 were up or down regulated, respectively. Functional annotations of the proteins were conducted using Blast2GO program against the non-redundant protein database (NCBInr). The KEGG database (\u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttp://www.genome.jp/kegg/\u003c/span\u003e\u003cspan address=\"http://www.genome.jp/kegg/\" targettype=\"URL\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e) and the COG database (\u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttp://www.ncbi.nlm.nih.gov/COG/\u003c/span\u003e\u003cspan address=\"http://www.ncbi.nlm.nih.gov/COG/\" targettype=\"URL\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e) were used to classify and group these proteins. To identify significantly enriched GO terms and KEGG pathways, enrichment analyses will be performed based on the hyper-geometric test (\u003cspan citationid=\"CR58\" class=\"CitationRef\"\u003e58\u003c/span\u003e).\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003c/ol\u003e \u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec6\" class=\"Section2\"\u003e \u003ch2\u003e2.4. Lipid quantification by mass spectrometric analysis\u003c/h2\u003e \u003cp\u003eFor lipidome analysis, cells were grown to PDS phase in SC-glucose medium. Lipidomics were performed by the company BGI on a commercial basis following standard protocols. Briefly, 20 mg cells were weighed and added into 2 mL thickened centrifuge tubes. Two steel balls and 800 \u0026micro;L of pre-chilled dichloromethane/methanol (3:1, v/v) precipitant were added into each sample, as well as 10 \u0026micro;L of the prepared internal standard. Samples were subjected to an ice bath ultrasound for 10 min and refrigerated overnight at -20\u0026deg;C. Samples were centrifuged at 25,000 \u0026times; g for 15 min at 4\u0026deg;C and 500 \u0026micro;L supernatant were taken and drained in a freezer dryer. 500 \u0026micro;L lipid reconstituted solution (in isopropanol: acetonitrile: water\u0026thinsp;=\u0026thinsp;2:1:1) was reconstituted and shaken for 30 sec. Then samples were implemented in ice bath ultrasound for 10 min and centrifuged at 25,000 \u0026times; g for 15 min at 4\u0026deg;C. 20 \u0026micro;L of each sample was used and mixed as QC samples.\u003c/p\u003e \u003cp\u003eFor UPLC-MS Analysis, waters 2777c UPLC (waters, USA) in series with Q exactive HF high resolution mass spectrometer (Thermo Fisher Scientific, USA) was used for the separation and detection of metabolites. Chromatographic separation was performed on CSH C18 column (1.7 \u0026micro;m, 2.1x100 mm, Waters, USA). In positive ion mode, solvent A was 60:40 \u003cem\u003ev\u003c/em\u003e/\u003cem\u003ev\u003c/em\u003e acetonitrile:water with 10 mM ammonium formate and 0.1% formic acid and solvent B was 90:10 \u003cem\u003ev\u003c/em\u003e/\u003cem\u003ev\u003c/em\u003e isopropanol:acetonitrile with 10 mM ammonium formate and 0.1% formic acid. In negative ion mode, solvent A was 60:40 \u003cem\u003ev\u003c/em\u003e/\u003cem\u003ev\u003c/em\u003e acetonitrile:water with 10 mM ammonium formate and solvent B was 90:10 \u003cem\u003ev\u003c/em\u003e/\u003cem\u003ev\u003c/em\u003e isopropanol:acetonitrile with 10 mM ammonium formate. The gradient conditions were as follows: 40% ~43% B over 0\u0026thinsp;~\u0026thinsp;2 min, 43%~50% B over 2\u0026thinsp;~\u0026thinsp;2.1 min, 50%~54% B over 2.1\u0026thinsp;~\u0026thinsp;7 min, 54% ~70% B over 7ཞ7.1 min, 70% ~99% B over 7.1\u0026thinsp;~\u0026thinsp;13 min, 99%~40% B over 13\u0026thinsp;~\u0026thinsp;13.1 min, held constant at 99%~40% B over 13.1\u0026thinsp;~\u0026thinsp;15 min and washed with 40% B over 13.1\u0026ndash;15 min. The flow rate was 0.4 mL/min and the injection volume was 5 \u0026micro;L.\u003c/p\u003e \u003cp\u003eThe instrument Q Exactive HF (Thermo Fisher Scientific, USA) was used for LC-MS analysis. The full scan range was 70\u0026ndash;1050 m/z with a resolution of 120,000, and the automatic gain control (AGC) target for MS acquisitions was set to 3e6 with a maximum ion injection time of 100 ms. Top 3 precursors were selected for subsequent MSMS fragmentation with a maximum ion injection time of 50 ms and resolution of 30000, the AGC was 1e5. The stepped normalized collision energy was set to 15, 30 and 45 eV. ESI parameters were setting as: sheath gas flow rate: 40; aux gas flow rate: 10; spray voltage in positive ion mode: 3.80 V; spray voltage in negative ion mode: 3.20 V; capillary temperature: 320\u0026deg;C; aux gas heater temp: 350\u0026deg;C. For compound identification, full-scan and MS/MS analyses were performed using Lipidsearch v.4.1 (Thermo Fisher Scientific, USA) software. Metabolite ion peak extraction and metabolite identification for lipidomics, data preprocessing using metaX (\u003cspan citationid=\"CR59\" class=\"CitationRef\"\u003e59\u003c/span\u003e) and data visualization were performed as described (\u003cspan citationid=\"CR60\" class=\"CitationRef\"\u003e60\u003c/span\u003e).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec7\" class=\"Section2\"\u003e \u003ch2\u003e2.5. Transcriptomics\u003c/h2\u003e \u003cp\u003eFor transcriptomics analysis, cells were grown to exponential phase in SC-glucose medium, and then BPS was added to a final concentration of 100 \u0026micro;M. Cells were then incubated for additional 4 h. RNA extraction, library construction, and sequencing were performed by the BGI company following internal procedures. The raw and processed RNA sequencing data are available from the NCBI GEO repository under the accession number GSE273946.\u003c/p\u003e \u003cp\u003e \u003col\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.5.1. RNA extraction\u003c/b\u003e. Cells were homogenized by mechanical disruption in 1.5 mL TRIzol lysis buffer. Samples were centrifuged at 12,000g for 5 min in 4\u0026ordm;C. The supernatant was transferred to new centrifuge tubes containing a chloroform/isoamyl alcohol (24:1) mix. After each shaking step, the samples were centrifuged at 12,000g for 8 min at 4\u0026ordm;C. Then, the supernatant was transferred to a new centrifuge tube containing isopropyl alcohol (2/3 vol/vol), gently shaken and cooled at -20\u0026ordm;C. Samples were then centrifuged for 25 min at 17,500 g (4\u0026ordm;C) and the supernatant was transferred to new microcentrifuge tubes, and combined twice with 75% (vol/vol) ethanol and mixed by pipetting. After centrifugation at 17,500 g for 3 min (4\u0026ordm;C), the supernatant was discarded, and the pellet was resuspended in 20\u0026ndash;200 \u0026micro;L DEPC-H\u003csub\u003e2\u003c/sub\u003eO or RNase-free water.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.5.2. Library construction methods.\u003c/b\u003e mRNA enrichment was performed on total RNA using oligo(dT)-attached magnetic beads. The enriched mRNA with poly(A) tails was fragmented using a fragmentation buffer, followed by reverse transcription using random N6 primers to synthesize cDNA double strands. The synthesized double-stranded DNA was then end-repaired and 5'-phosphorylated, with a protruding 'A' at the 3' end forming a blunt end, followed by ligation of a bubble-shaped adapter with a protruding 'T' at the 3' end. The ligation products were PCR amplified using specific primers. The PCR products were denatured to single strands, and then single-stranded circular DNA libraries were generated using a bridged primer. The constructed libraries were quality-checked and sequenced after passing the quality control.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.5.3. Data filtering.\u003c/b\u003e Sequencing was performed on a DNBSEQ platform with PE150 (read length). The sequencing data was filtered with SOAPnuke (\u003cspan citationid=\"CR61\" class=\"CitationRef\"\u003e61\u003c/span\u003e) by: (\u003cspan citationid=\"CR1\" class=\"CitationRef\"\u003e1\u003c/span\u003e) removing reads containing sequencing adapter; (\u003cspan citationid=\"CR2\" class=\"CitationRef\"\u003e2\u003c/span\u003e) removing reads whose low-quality base ratio (base quality less than or equal to 15) is more than 20%; (\u003cspan citationid=\"CR3\" class=\"CitationRef\"\u003e3\u003c/span\u003e) removing reads whose unknown base ('N' base) ratio is more than 5%, afterwards clean reads were obtained and stored in FASTQ format. The subsequent analysis and data mining were performed on Dr. Tom Multi-omics Data mining system (\u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttps://biosys.bgi.com\u003c/span\u003e\u003cspan address=\"https://biosys.bgi.com\" targettype=\"URL\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e).\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.5.4. Structure variation detection.\u003c/b\u003e Saccharomyces_cerevisiae_S288C_559292.NCBI.GCF_000146045.2_R64.v2201 was used a reference from NCBI. The clean reads were mapped to the reference genome using HISAT2 (\u003cspan citationid=\"CR62\" class=\"CitationRef\"\u003e62\u003c/span\u003e). After that, Ericscript (v0.5.5) (\u003cspan citationid=\"CR63\" class=\"CitationRef\"\u003e63\u003c/span\u003e) and rMATS (V3.2.5) (\u003cspan citationid=\"CR64\" class=\"CitationRef\"\u003e64\u003c/span\u003e) were used to detect fusion genes and differential splicing genes (DSGs), respectively.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.5.5. RNA identification\u003c/b\u003e. Bowtie2 (\u003cspan citationid=\"CR65\" class=\"CitationRef\"\u003e65\u003c/span\u003e) was applied to align the clean reads to the gene set, in which known and novel, coding and noncoding transcripts were included.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.5.6. Gene quantification differential expression analysis\u003c/b\u003e. Expression level of gene was calculated by RSEM (v1.3.1) (\u003cspan citationid=\"CR66\" class=\"CitationRef\"\u003e66\u003c/span\u003e). The heatmap was drawn by pheatmap (v1.0.8) according to the gene expression difference in different samples. Essentially, differential expression analysis was performed using the DESeq2 (v1.4.5) (\u003cspan citationid=\"CR67\" class=\"CitationRef\"\u003e67\u003c/span\u003e) [or DEGseq (68) or PoissonDis (\u003cspan citationid=\"CR69\" class=\"CitationRef\"\u003e69\u003c/span\u003e)] with Q value\u0026thinsp;\u0026le;\u0026thinsp;0.05 (or FDR\u0026thinsp;\u0026le;\u0026thinsp;0.001).\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003cspan\u003e \u003cli\u003e \u003cp\u003e \u003cb\u003e2.5.7. Gene annotation\u003c/b\u003e. To take insight to the change of phenotype, GO (\u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttp://www.geneontology.org/\u003c/span\u003e\u003cspan address=\"http://www.geneontology.org/\" targettype=\"URL\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e) and KEGG (\u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttps://www.kegg.jp/\u003c/span\u003e\u003cspan address=\"https://www.kegg.jp/\" targettype=\"URL\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e) enrichment analysis of annotated different expression gene was performed by Phyper (\u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttps://en.wikipedia.org/wiki/Hypergeometric_distribution\u003c/span\u003e\u003cspan address=\"https://en.wikipedia.org/wiki/Hypergeometric_distribution\" targettype=\"URL\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e) based on Hyper geometric test. The significant levels of terms and pathways were corrected by Q value with rigorous threshold (Q value\u0026thinsp;\u0026le;\u0026thinsp;0.05, \u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttp://github.com/jdstorey/qvalue\u003c/span\u003e\u003cspan address=\"http://github.com/jdstorey/qvalue\" targettype=\"URL\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e). Genes meeting this criterion were considered significantly enriched in the candidate gene set.\u003c/p\u003e \u003c/li\u003e \u003c/span\u003e \u003c/ol\u003e \u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec8\" class=\"Section2\"\u003e \u003ch2\u003e2.6. β-Galactosidase (β-Gal) activity assay\u003c/h2\u003e \u003cp\u003eCells harboring LacZ-reporter fusion plasmids were grown in SC-glucose medium. Cells were harvested by centrifugation, resuspended in breaking buffer (100 mM Tris, 1 mM DTT, 10% (vol/vol) glycerol) and protease inhibitors (Complete mini EDTA-free Protease cocktail inhibitor tablets) and mechanically lysed with zirconium beads for 5 min. Debris were pelleted at 12,044 g for 15 min at 4 \u0026ordm;C and the supernatant was collected for protein quantification. Total protein levels were quantified by the Lowry method using a bovine serum albumin standard curve. Volumes corresponding to 15\u0026ndash;100 \u0026micro;g of total extract protein were diluted up to 800 \u0026micro;L with β-Gal buffer (60 mM Na\u003csub\u003e2\u003c/sub\u003eHPO\u003csub\u003e4\u003c/sub\u003e, 40 mM NaH\u003csub\u003e2\u003c/sub\u003ePO\u003csub\u003e4\u003c/sub\u003e, 10 mM KCl, 1 mM MgSO\u003csub\u003e4\u003c/sub\u003e, 50 mM β-mercaptoethanol). β-Galactosidase (β-Gal) activity was measured at 30\u0026deg;C using the substrate \u003cem\u003eo\u003c/em\u003e-nitrophenyl-β-D-galactopyranoside (ONPG; Merck, Kenilworth, NJ, USA), as described previously (\u003cspan citationid=\"CR70\" class=\"CitationRef\"\u003e70\u003c/span\u003e).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec9\" class=\"Section2\"\u003e \u003ch2\u003e2.7. Western blotting analysis\u003c/h2\u003e \u003cp\u003eFor assessment of total protein levels of Ino1p, strains WT-VN WT-VC INO1-HA and N88S-VN N88S-VC INO1-HA were grown to exponential or PDS phases in SC-glucose medium. To evaluate the phosphorylation status and total protein levels of Aft1p, strains expressing pRS415-HA-AFT1 were grown to PDS phase in SC-glucose medium at 26 \u0026ordm;C. The cells were washed and harvested by centrifugation for 4 min at 4000 rpm (4 \u0026ordm;C). Proteins were extracted by alkaline lysis, and prepared in Laemmli sample buffer. Proteins were separated by SDS-PAGE, using 10% (Ino1p-3HA/HA-Aft1p total levels) and 6% (HA-Aft1p phosphorylation) polyacrylamide gels, and transferred to nitrocellulose membranes (Hybond-ECL GE Healthcare) in a semi-dry system for 1 h. Membranes were blocked with 5% (wt/vol) nonfat dry milk in TTBS (20 mM Tris, 140 mM NaCl, 0.05% (vol/vol), Tween-20 pH 7.6) for 1 h. Next, membranes were incubated with primary antibodies: mouse anti-HA tag antibody F-7 (1:1000, sc-7392 Santa Cruz Biotechnology) or mouse anti-Pgk1 (1:50,000, Molecular Probes). After washing with TTBS, membranes were incubated with the secondary antibody mouse IgG-peroxidase. Immunodetection was performed by chemiluminescence using WesternBright ECL reagent (Advansta) and exposing the membranes to LucentBlue X-ray films (Advansta). Band intensities were analyzed using the GS-900 Calibrated Densitometer (Bio-Rad).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec10\" class=\"Section2\"\u003e \u003ch2\u003e2.8. Fluorescence microscopy\u003c/h2\u003e \u003cp\u003eTo examine the intracellular localization of IBs using the Venus signal upon reconstitution of the VN and VC fragments, cells were grown to exponential phase in SC-glucose medium. To evaluate the localization of GFP-Aft1p, cells transformed with YEplac181-GFP-\u003cem\u003eAFT1\u003c/em\u003e were grown to the exponential phase in SC-glucose medium supplemented with 300 \u0026micro;M FeSO\u003csub\u003e4\u003c/sub\u003e (II). For nuclear staining, cells were incubated with 4 \u0026micro;g/mL of 4\u0026prime;-6-diamidino-2-phenylindole (DAPI, Molecular Probes, Invitrogen) for 15 min at room temperature, and protected from light. Cells were washed twice with PBS and observed by fluorescence microscopy (Zeiss Axio Imager Z1 Apotome or Leica TCS SP8). Z-stacks were acquired for DIC, DAPI and GFP/Venus channels. The output final images and colocalization analysis were performed using ImageJ 1.51k software. When applicable, all quantifications were performed from two independent experiments, and more than 100 cells per condition were scored. Values were recorded in Excel (Microsoft) and analyzed in Prism 8.0 (GraphPad Software). Brightness and contrast were adjusted using Inkscape (The Inkscape Project).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec11\" class=\"Section2\"\u003e \u003ch2\u003e2.9. Iron Levels\u003c/h2\u003e \u003cp\u003eTotal iron levels were quantified in yeast cells (3\u0026ndash;7 \u0026times; 10\u003csup\u003e7\u003c/sup\u003e cells mL\u003csup\u003e\u0026minus;\u0026thinsp;1\u003c/sup\u003e) grown in SC glucose medium to late exponential (OD\u003csub\u003e600\u003c/sub\u003e\u0026thinsp;\u0026asymp;\u0026thinsp;2) and PDS (OD\u003csub\u003e600\u003c/sub\u003e\u0026thinsp;\u0026asymp;\u0026thinsp;6-7.5) phases, using a colorimetric assay as described (\u003cspan citationid=\"CR43\" class=\"CitationRef\"\u003e43\u003c/span\u003e).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec12\" class=\"Section2\"\u003e \u003ch2\u003e2.10. ROS staining and IB formation\u003c/h2\u003e \u003cp\u003eTo assess ROS, cells grown in SC-glucose medium at specified phases were incubated with 5 \u0026micro;g/mL dihydroethidium (DHE, Molecular Probes) for 10 min at room temperature in the dark. The quantification of Venus fluorescence intensity, normalized to the number of cells, was used as a means to monitor IB formation (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). Then, cells were centrifuged, washed twice and resuspended in PBS (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). Flow cytometry analysis was performed using the FL1 (533/30) for IB monitoring, and FL3 (670 LP) channels (BD Accuri C6 Flow cytometer) for ROS quantification via DHE. Data were evaluated with FlowJow software (v. 10.6.1).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec13\" class=\"Section2\"\u003e \u003ch2\u003e2.11. Yeast Spotting Assay\u003c/h2\u003e \u003cp\u003eThe oxidative stress agents \u003cem\u003etert\u003c/em\u003e-Butyl hydroperoxide (\u003cem\u003et\u003c/em\u003e-BOOH, Sigma Aldrich) and hydrogen peroxide (H\u003csub\u003e2\u003c/sub\u003eO\u003csub\u003e2\u003c/sub\u003e, Merck) were added at a final concentration of 50 \u0026micro;M and 250 \u0026micro;M to iron-supplemented SC-glucose plates. The iron chelator BPS was added to a final concentration of 30 \u0026micro;M. Growth assays were performed by spotting 1:10 serial dilutions of exponentially grown cell cultures onto SC-glucose plates and containing the specified compounds. The growth was observed and recorded after a 2-day incubation period at 26\u0026deg;C.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec14\" class=\"Section2\"\u003e \u003ch2\u003e2.12. Bioinformatics Analysis\u003c/h2\u003e \u003cp\u003e \u003cem\u003eIn-silico\u003c/em\u003e analysis of transcriptional regulation of the \u003cem\u003eFET3\u003c/em\u003e promoter was carried out using the Yeast Search for Transcriptional Regulators and Consensus Tracking (YEASTRACT+) database (\u003cspan citationid=\"CR71\" class=\"CitationRef\"\u003e71\u003c/span\u003e). The search was performed to define unbiased regulatory associations between transcription factors (TFs) and the promoter region, either document or potential associations (based on TF binding sites). YEASTRACT\u0026thinsp;+\u0026thinsp;was also used to find genes encoding proteins found to be elevated in the mutant strain and regulated by Msn2/Msn4p. For that, documented associations between genes and transcription factors Msn2p and Msn4p were searched using the following parameters: 1) Simultaneous DNA binding and expression evidence and 2) Transcription factor acting as activator.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec15\" class=\"Section2\"\u003e \u003ch2\u003e2.13. Aconitase activity assay\u003c/h2\u003e \u003cp\u003eThe measurement of aconitase activity was performed as described (\u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e51\u003c/span\u003e, \u003cspan citationid=\"CR72\" class=\"CitationRef\"\u003e72\u003c/span\u003e, \u003cspan citationid=\"CR73\" class=\"CitationRef\"\u003e73\u003c/span\u003e), with minor modifications. Briefly, cells were grown to PDS phase in SC-glucose medium and harvested by centrifugation for 5 min at 4000 rpm (4 \u0026ordm;C). Cells were resuspended in aconitase buffer (100 mM Tris-HCl pH 7.4 and 0.6 M sorbitol) containing protease inhibitors (Complete, EDTA-free Protease Inhibitor Cocktail, Roche). The protein extracts were obtained by vortexing in the presence of glass beads for 10 min. Cell debris was removed by centrifugation at 3000 rpm for 15 min at 4 \u0026ordm;C, and protein concentration was determined by the method of Lowry, using bovine serum albumin as a standard. Cell lysates were assayed at 25\u0026deg;C in aconitase reaction buffer containing 100 mM Tris-HCl (pH 7.4), 1.2 mM \u003cem\u003ecis\u003c/em\u003e-aconitate (Sigma-Aldrich) and 45 \u0026micro;L of protein sample. The lysis and enzymatic activity measurement steps were performed under an anaerobic atmosphere using buffers flushed with nitrogen gas. The decrease in absorbance at 240 nm was measured as a function of time (normalized to protein concentration), and an extinction coefficient of 3.6 (mM.cm)\u003csup\u003e\u0026minus;1\u003c/sup\u003e was used to calculate the specific activity of aconitase. 1 unit of aconitase activity is defined as 1 nmol of \u003cem\u003ecis\u003c/em\u003e-aconitate converted per minute and per mg of protein.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec16\" class=\"Section2\"\u003e \u003ch2\u003e2.14. Statistical analysis\u003c/h2\u003e \u003cp\u003eUnless specified otherwise, the results were derived from a minimum of three independent experiments. The images shown are representative of these findings. Quantitative data are presented as the mean\u0026thinsp;\u0026plusmn;\u0026thinsp;standard deviation (SD). Statistical comparisons were made using unpaired, two-tailed Student's t-tests or two-way ANOVA, conducted with Prism 8.0 software (GraphPad Software). \u003cem\u003eP\u003c/em\u003e-values\u0026thinsp;\u0026lt;\u0026thinsp;0.05 were considered significant: * \u003cem\u003ep\u003c/em\u003e\u0026thinsp;\u0026le;\u0026thinsp;0.05; ** \u003cem\u003ep\u003c/em\u003e\u0026thinsp;\u0026le;\u0026thinsp;0.01; *** \u003cem\u003ep\u003c/em\u003e\u0026thinsp;\u0026le;\u0026thinsp;0.001; **** \u003cem\u003ep\u003c/em\u003e\u0026thinsp;\u0026le;\u0026thinsp;0.0001.\u003c/p\u003e \u003c/div\u003e"},{"header":"3. Results","content":"\u003cdiv id=\"Sec18\" class=\"Section2\"\u003e \u003ch2\u003e3.1. Lipid metabolism is altered in N88S seipin-expressing cells\u003c/h2\u003e \u003cp\u003eIn this study, we employed comparative unbiased quantitative mass spectrometric proteomic analysis to examine changes in protein abundance and profile between the WT-VN WT-VC and N88S-VN N88S-VC strain at the post-diauxic shift (PDS) phase, when cells shifted from a fermentative (exponential phase) to aerobic utilization of non-glycolytic substrates (e.g. ethanol) by mitochondria. The goal was to define a set of differentially expressed proteins (DEPs - either up- or down-regulated) and sort into functional networks to highlight perturbed protein functions and signalling pathways contributing to disease-related phenotypes. We were able to identify 115 proteins with reduced abundance and 97 proteins with increased abundance in N88S seipin-expressing cells (Fig.\u0026nbsp;1A and Fig. \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003eA, Tables S3 and S4). A volcano plot (Fig.\u0026nbsp;1B) is shown to highlight the differences in protein levels. Using YEASTRACT+ (\u003cspan citationid=\"CR74\" class=\"CitationRef\"\u003e74\u003c/span\u003e), a Gene Ontology (GO) analysis and KEEG pathway analysis for DEPs in biological processes revealed an enrichment in proteins related to ion transport (GO:0006811; \u003cem\u003ep\u003c/em\u003e-value\u0026thinsp;=\u0026thinsp;0.001380), phospholipid biosynthetic process (GO:0008654; \u003cem\u003ep\u003c/em\u003e-value\u0026thinsp;=\u0026thinsp;2.920 \u0026times; 10\u003csup\u003e\u0026minus;\u0026thinsp;9\u003c/sup\u003e) and lipid metabolic process (GO:0006629; \u003cem\u003ep\u003c/em\u003e-value\u0026thinsp;=\u0026thinsp;1.562 \u0026times; 10\u003csup\u003e\u0026minus;\u0026thinsp;6\u003c/sup\u003e) (Fig. \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003eB-C and Fig.\u0026nbsp;1C).\u003c/p\u003e \u003cp\u003eNotably, among the protein identified, eight showed reduced abundance, including seven key players in the phospholipid biosynthetic pathway: Cho1p, Cho2p, Opi1p, Opi3p, Psd1p, Cpt1p and Cds1p (Table \u003cspan refid=\"MOESM3\" class=\"InternalRef\"\u003eS3\u003c/span\u003e and Fig.\u0026nbsp;1D). This suggests potential alterations in the lipid profile, particularly in phospholipid and neutral lipids content. To investigate these changes, we conducted a quantitative lipidomic analysis at the same growth phase (PDS phase) to measure the levels of major phospholipids and their derivatives, inositol phosphates, and neutral lipids along with their corresponding precursors. We observed a decrease in 46 lipid metabolites, while 41 lipid molecules levels were increased (Fig. \u003cspan refid=\"MOESM2\" class=\"InternalRef\"\u003eS2\u003c/span\u003eA-B). The levels of fatty acids (Fig. \u003cspan refid=\"MOESM2\" class=\"InternalRef\"\u003eS2\u003c/span\u003eC) and of major phospholipids (PC, PE, PS and PI) remained essentially unaltered (Fig.\u0026nbsp;2A), however the levels of PG, which is derived from CDP-DAG, were decreased (Fig.\u0026nbsp;2A). The amount of ceramide (Fig. \u003cspan refid=\"MOESM2\" class=\"InternalRef\"\u003eS2\u003c/span\u003eD) and lysophospholipids (Fig.\u0026nbsp;2B) was increased, suggesting that the activity of lysophospholipid acyltransferases may be impaired in the mutant. Despite the fact of DG abundance was unchanged (Fig.\u0026nbsp;2C), the levels of PA and TG are increased (Fig.\u0026nbsp;2D-E), suggesting that PA and lipid precursors are being redirected towards neutral lipid synthesis.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec19\" class=\"Section2\"\u003e \u003ch2\u003e3.2. Inositol metabolism is deregulated in cells expressing the mutant seipin\u003c/h2\u003e \u003cp\u003eGenes encoding enzymes in both the CDP-DAG (\u003cem\u003eCDS1, CHO1, PSD1, CHO2, OPI3\u003c/em\u003e) and Kennedy (\u003cem\u003eCPT1\u003c/em\u003e) pathways contain a UAS\u003csub\u003eINO\u003c/sub\u003e element in their promoters whose expression is transcriptionally repressed by Opi1p (\u003cspan citationid=\"CR31\" class=\"CitationRef\"\u003e31\u003c/span\u003e, \u003cspan citationid=\"CR75\" class=\"CitationRef\"\u003e75\u003c/span\u003e). To evaluate if their lower protein abundance in N88S seipin-expressing cells correlates with reduced transcription, we measured the transcription of Opi1p-dependent genes in WT and mutant cells, using an \u003cem\u003eINO1\u003c/em\u003e-LacZ transcriptional reporter during lifespan. We observed that \u003cem\u003eINO1\u003c/em\u003e expression remains unchanged in the WT, however there is a\u0026thinsp;~\u0026thinsp;4-fold increase in N88S seipin-expressing cells at PDS and stationary phases (Fig.\u0026nbsp;3A). It was previously demonstrated that the accumulation of PA acts as the metabolic signal that triggers the derepression of \u003cem\u003eINO1\u003c/em\u003e (\u003cspan citationid=\"CR29\" class=\"CitationRef\"\u003e29\u003c/span\u003e, \u003cspan citationid=\"CR76\" class=\"CitationRef\"\u003e76\u003c/span\u003e, \u003cspan citationid=\"CR77\" class=\"CitationRef\"\u003e77\u003c/span\u003e). Therefore, a plausible explanation for lower Opi1p repressor activity is the retention of Opi1p in the ER potentiated by accumulation of PA as observed by lipidomic analysis (Fig.\u0026nbsp;2D), allowing the Ino2p-Ino4p heteromeric complex to stimulate the transcription of \u003cem\u003eINO1\u003c/em\u003e. We then conclude that post-transcriptional mechanisms may operate to control the steady protein levels of these phospholipid biosynthetic enzymes in response to changes in the lipid profile observed in the mutant strain (Fig.\u0026nbsp;1D). More recently, it was shown that the levels of PA (34:1) is correlated with optimal expression of \u003cem\u003eINO1\u003c/em\u003e irrespective of total PA content (\u003cspan citationid=\"CR78\" class=\"CitationRef\"\u003e78\u003c/span\u003e). We observed that the amount of the PA (34:1) is increased by ~\u0026thinsp;7-fold at PDS phase in mutant cells, which coincides with the increase in \u003cem\u003eINO1\u003c/em\u003e expression at the same phase (Fig. \u003cspan refid=\"MOESM2\" class=\"InternalRef\"\u003eS2\u003c/span\u003eE).\u003c/p\u003e \u003cp\u003eNext, we decided to evaluate if higher \u003cem\u003eINO1\u003c/em\u003e expression was correlated with changes in Ino1p protein levels during lifespan. For that, we analyzed Ino1p-HA levels at the exponential and PDS phases by Western Blotting. We observed increased protein levels starting at the exponential phase, which remained elevated during the PDS phase (Fig.\u0026nbsp;3B), where \u003cem\u003eINO1\u003c/em\u003e expression is largely derepressed in mutant cells (Fig.\u0026nbsp;3A). Ino1p is essential for the \u003cem\u003ede novo\u003c/em\u003e biosynthesis of inositol, which is incorporated into phosphatidylinositol (PI) for the synthesis of phosphatidylinositol phosphates (PIP). In N88S seipin-expressing cells, we also observed changes in PI-derived lipids, including decreased levels of phosphoinositides (PIP and PIP\u003csub\u003e3\u003c/sub\u003e). This indicates that PI metabolism is also deregulated (Fig. \u003cspan refid=\"MOESM2\" class=\"InternalRef\"\u003eS2\u003c/span\u003eF).\u003c/p\u003e \u003cp\u003eWe next tested whether cells expressing the seipin N88S mutation are responsive to changes in inositol levels. For that, cells expressing the \u003cem\u003eINO1\u003c/em\u003e-LacZ reporter fusion were grown to exponential phase in the absence of inositol and then shifted to medium containing inositol. While WT cells adapted to inositol by reducing \u003cem\u003eINO1\u003c/em\u003e expression, the mutant was unable to adapt and failed to repress \u003cem\u003eINO1\u003c/em\u003e expression (Fig.\u0026nbsp;3C). Importantly, in the absence of inositol, \u003cem\u003eINO1\u003c/em\u003e expression was lower in the mutant compared to WT cells which is reminiscent of the behavior displayed by the mutant Opi1\u003csup\u003eFFAT\u003c/sup\u003e, in which the Opi1p-Scs2p interaction motif two phenylalanines (\u003cspan type=\"Underline\" class=\"Underline\" name=\"Emphasis\"\u003eFF\u003c/span\u003e) in an \u003cspan type=\"Underline\" class=\"Underline\" name=\"Emphasis\"\u003ea\u003c/span\u003ecidic \u003cspan type=\"Underline\" class=\"Underline\" name=\"Emphasis\"\u003et\u003c/span\u003eract (FFAT) is absent, and the activity of Opi1p is mainly driven by the electrostatic interaction with PA is absent, and the activity of Opi1p is mainly driven by the electrostatic interaction with PA (\u003cspan citationid=\"CR79\" class=\"CitationRef\"\u003e79\u003c/span\u003e). Overall, we provide strong evidence that inositol and lipid metabolism is highly deregulated in the mutant.\u003c/p\u003e \u003cp\u003eIn summary, the results suggest that increased PA levels may be linked to decreased flux of lipid precursors into phospholipid biosynthesis, due to lower protein levels of key enzymes in this pathway. Consequently, accumulation of PA levels causes Opi1p to be retained in the ER, allowing the transcription of \u003cem\u003eINO1\u003c/em\u003e to be derepressed, thus leading to elevated Ino1p protein levels. Additionally, PA may be redirected towards the synthesis of neutral lipids, thus explaining the higher amount of TG exhibited by the mutant.\u003c/p\u003e \u003cp\u003e \u003cb\u003e3.3. PA and impaired inositol metabolism contribute to ER stress independently of protein misfolding in mutant cells\u003c/b\u003e \u003c/p\u003e \u003cp\u003eER stress and UPR activation can influence cellular processes beyond ER protein folding, playing critical roles in lipid metabolism, as it constitutes a key site for lipid synthesis and storage (\u003cspan citationid=\"CR80\" class=\"CitationRef\"\u003e80\u003c/span\u003e). Previous studies showed that inositol depletion can trigger ER stress without causing a noticeable accumulation of unfolded proteins in the ER lumen (\u003cspan additionalcitationids=\"CR82\" citationid=\"CR81\" class=\"CitationRef\"\u003e81\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR83\" class=\"CitationRef\"\u003e83\u003c/span\u003e). Instead, this stress response appears to activate the UPR via a membrane-based mechanism that functions independently of unfolded proteins (\u003cspan citationid=\"CR84\" class=\"CitationRef\"\u003e84\u003c/span\u003e). This offers an ideal framework to investigate whether deregulated lipid metabolism contributes to ER stress observed in the yeast model of N88S seipinopathy. We then evaluated how \u003cem\u003eINO1\u003c/em\u003e deficiency affects the activity of the UPRE-LacZ ER stress reporter. As previously described, N88S seipin-expressing cells displayed higher levels of ER stress (Fig.\u0026nbsp;3D) associated with elevated expression of the reporter fusion (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). Importantly, β-galactosidase activity further increased in mutant cells upon deletion of \u003cem\u003eINO1\u003c/em\u003e, although to lower extent, indicating that misregulation of \u003cem\u003eINO1\u003c/em\u003e expression and impaired inositol metabolism also contribute to ER stress.\u003c/p\u003e \u003cp\u003eNotably, \u003cem\u003eINO1\u003c/em\u003e deletion is associated with reduced PI levels and accumulation of lipid precursors, including PA and CDP-DAG (\u003cspan citationid=\"CR31\" class=\"CitationRef\"\u003e31\u003c/span\u003e). This led us to investigate whether accumulation of PA is associated with higher induction of the UPR. When WT cells are grown in inositol-depleted conditions, PI levels remain low, leading to PA buildup (\u003cspan citationid=\"CR31\" class=\"CitationRef\"\u003e31\u003c/span\u003e). Importantly, under these conditions, N88S seipin-expressing cells exhibited higher UPR levels when grown in the absence of inositol in a \u003cem\u003eINO1\u003c/em\u003e-dependent manner (Fig.\u0026nbsp;3E). In the presence of exogenous inositol, where PA is consumed as a precursor to support PI biosynthesis, the β-galactosidase activity of the ER stress reporter remained unchanged in WT cells regardless of inositol levels, but decreased in the mutant (Fig.\u0026nbsp;3E). This reinforces the hypothesis that the response to changing PA levels involves the induction of the UPR in cells expressing N88S mutant seipin.\u003c/p\u003e \u003cp\u003eNext, we tested how the overexpression of \u003cem\u003eCDS1\u003c/em\u003e affects the ER stress response. Cds1p is responsible for the synthesis of CDP-DAG from PA. Cds1p consumes the PA pools and channels the CDP-DAG pool towards PI biosynthesis under conditions of inositol surplus (\u003cspan citationid=\"CR85\" class=\"CitationRef\"\u003e85\u003c/span\u003e). However, in the absence of inositol, where PI biosynthesis is essentially halted, CDP-DAG derived from PA is channeled into the phospholipid biosynthetic pathway. Under inositol starvation, we observed that the UPR is significantly increased in WT cells, and even more induced in N88S seipin-expressing cells upon overexpression of \u003cem\u003eCDS1\u003c/em\u003e (Fig.\u0026nbsp;4A). Higher UPR induction in the mutant might be linked to reduced enzymatic capacity to promote phospholipid biosynthesis under these conditions, as the overall phospholipid biosynthesis rate is likely reduced due to decreased protein levels of key enzymes involved in the pathway (Fig.\u0026nbsp;1D). So, we tested whether stimulation of phospholipid biosynthesis by overexpressing \u003cem\u003eCHO1\u003c/em\u003e in WT and N88S mutant cells induces ER stress under the same conditions (in the absence of inositol). In this case, we observed no changes in the induction of the LacZ reporter fusion for all strains tested (Fig.\u0026nbsp;4B). Notably, overexpression of \u003cem\u003eCDS1\u003c/em\u003e, in contrast with \u003cem\u003eCHO1\u003c/em\u003e counterparts, leads to inositol auxotrophy and significant viability loss in the absence of inositol (Fig.\u0026nbsp;4C). Overall, the data support a model in which the accumulation of PA, whether due to a reduced rate of phospholipid biosynthesis or in response to changes in lipid flux upon inositol availability (Fig.\u0026nbsp;1D, 3C-E, and 4A-B), is a key feature of the ER stress response in N88S seipin mutant cells. This is particularly significant, as it demonstrates that lipid imbalance also contributes to the ER stress response beyond protein misfolding of seipin caused by the N88S mutation. In agreement with this idea, we found that \u003cem\u003eINO1\u003c/em\u003e deletion actually reduced IB formation by ~\u0026thinsp;50% in N88S seipin-expressing cells, as monitored by fluorescence microscopy and flow cytometry (Fig.\u0026nbsp;4D-E), despite the earlier observation that the UPR is more strongly induced in cells grown under the same conditions (Fig.\u0026nbsp;3D).\u003c/p\u003e \u003cp\u003eFinally, we tested the relationship between impaired lipid metabolism and ROS production in the mutant strain. For this purpose, cells were grown to stationary phase, and ROS levels were detected using the DHE probe. The results showed that \u003cem\u003eINO1\u003c/em\u003e deficiency reduced ROS levels by ~\u0026thinsp;30% in WT cells, but did not affect ROS levels in mutant cells (Fig. \u003cspan refid=\"MOESM3\" class=\"InternalRef\"\u003eS3\u003c/span\u003eA). This indicates that oxidative damage is not directly linked to defects in membrane lipid metabolism in N88S seipin-expressing cells.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec20\" class=\"Section2\"\u003e \u003ch2\u003e3.4. N88S seipin expressing cells are sensitive to iron deficiency conditions\u003c/h2\u003e \u003cp\u003eThe proteomic analysis revealed that proteins involved in iron ion homeostasis, including Fit1p, Arn1p, Arn2p and Hmx1p, were present at lower levels in N88S seipin expressing cells (Fig.\u0026nbsp;1C and Table \u003cspan refid=\"MOESM3\" class=\"InternalRef\"\u003eS3\u003c/span\u003e). This prompted us to investigate whether there were alterations in cellular iron levels during lifespan imparted by the N88S seipin mutation. The results revealed that cells expressing the N88S seipin mutant accumulated iron (Fe) at the exponential phase (Fig.\u0026nbsp;5A). Nevertheless, there was a significant decrease in Fe levels from the exponential to PDS phase in the mutant, suggesting that cells experience iron deficiency. It is known that the demand for iron increases during the diauxic shift, and Aft1p is responsible for the regulation of proteins involved in capturing, internalizing, and mobilizing Fe to meet the needs of mitochondria, DNA repair, and other cellular processes (\u003cspan additionalcitationids=\"CR87\" citationid=\"CR86\" class=\"CitationRef\"\u003e86\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR88\" class=\"CitationRef\"\u003e88\u003c/span\u003e). Using a LacZ reporter where the Aft1p binding sequence from the \u003cem\u003eCTH2\u003c/em\u003e promoter is fused to the LacZ gene, we found that Aft1p transcriptional activity boosted\u0026thinsp;~\u0026thinsp;15-fold in WT cells grown from exponential phase to PDS phase. In contrast, in N88S seipin-expressing cells, the increase was approximately 7-fold, about half of the one observed in WT cells (Fig.\u0026nbsp;5B). This is in agreement with decreased protein levels of Fit1p, Arn1p, Arn2p and Hmx1p observed in these cells at PDS phase as identified by proteomic analysis (Table \u003cspan refid=\"MOESM3\" class=\"InternalRef\"\u003eS3\u003c/span\u003e), which collectively correspond to proteins whose genes are transcriptionally activated by Aft1p/Aft2p in response to iron deficiency (\u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e37\u003c/span\u003e). To test if this effect is related to impaired ability to activate the iron regulon, cells were grown to the exponential phase and treated with the iron chelator bathophenanthrolinedisulfonate (BPS), which limits iron availability and causes an iron deprivation condition. As expected, β-galactosidase activity was significantly increased in WT cells as an adaptive response to BPS-induced iron depletion, but the induction was lower by 50\u0026ndash;60% in the mutant strain compared to WT cells (Fig.\u0026nbsp;5C). To further address how Aft1p deregulation affects the iron deficiency response in cells expressing mutant seipin, WT and N88S seipin-expressing cells were subjected to transcriptomic analysis under BPS-induced iron deprivation (Fig. \u003cspan refid=\"MOESM4\" class=\"InternalRef\"\u003eS4\u003c/span\u003eA-D). As expected, bioinformatic analysis revealed that GO functional categories were enriched among differentially expressed genes (DEGs) involved in iron-regulated processes and mitochondrial-related functions, namely tricarboxylic acid cycle and mitochondrial electron transport chain, iron-sulfur cluster assembly, sterol biosynthetic process and aminoacid metabolism (Fig. \u003cspan refid=\"MOESM4\" class=\"InternalRef\"\u003eS4\u003c/span\u003eA-D). The results revealed that 197 and 250 genes had lower and higher expression in the mutant respectively, when compared to WT cells (Tables S5 and S6). We thus focused our attention on transcripts that are transcriptionally regulated by Aft1p/Aft2p upon BPS treatment, as defined in a previous study (\u003cspan citationid=\"CR49\" class=\"CitationRef\"\u003e49\u003c/span\u003e). Of the DEGs, 10 out of 28 genes previously reported to be upregulated during Fe starvation in WT cells (\u003cspan citationid=\"CR49\" class=\"CitationRef\"\u003e49\u003c/span\u003e) are downregulated in N88S seipin-expressing cells, including members of the Fe regulon: \u003cem\u003eCCC2, ARN1, FIT1\u003c/em\u003e, \u003cem\u003eFTH1\u003c/em\u003e, \u003cem\u003eOLE1\u003c/em\u003e, \u003cem\u003eFIT3, FET4\u003c/em\u003e, \u003cem\u003eATX1, SIT1\u003c/em\u003e and \u003cem\u003eFTR1\u003c/em\u003e (Fig. \u003cspan refid=\"MOESM4\" class=\"InternalRef\"\u003eS4\u003c/span\u003eE and Table \u003cspan refid=\"MOESM6\" class=\"InternalRef\"\u003eS6\u003c/span\u003e). Conversely, 13 (\u003cem\u003eISA1, COR1, PYC2, LEU1, RNR4, BIO2, CYC1, HAP4, NFU1, CCP1, CYT1, QCR2 and RIP1\u003c/em\u003e) out of 34 genes with reduced expression in WT cells under similar conditions (\u003cspan citationid=\"CR49\" class=\"CitationRef\"\u003e49\u003c/span\u003e) are increased in the mutant strain (Fig. \u003cspan refid=\"MOESM4\" class=\"InternalRef\"\u003eS4\u003c/span\u003eE and Table \u003cspan refid=\"MOESM5\" class=\"InternalRef\"\u003eS5\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eOverall, these results suggest that the N88S mutation renders cells unable to effectively activate Aft1p-mediated transcription of the iron regulon in response to changes in iron levels during lifespan and in response to iron deficiency. We then propose that this defective response may contribute to the increased ROS generation and oxidative damage previously reported for the mutant strain (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). To test this, cells were incubated with BPS at different growth phases and then allowed to grow in medium for 48 hours. When treated with the iron chelator at the exponential phase, where iron accumulation was observed in mutant cells (Fig.\u0026nbsp;5A), both WT and N88S seipin-expressing cells exhibited an acute growth defect (Fig.\u0026nbsp;5D). Although an increase in ROS content was noted in BPS-treated WT cells, the mutant displayed similar levels of ROS regardless of the presence of BPS in the medium (Fig.\u0026nbsp;5D). When cells were incubated with BPS at the diauxic shift, we observed no changes in growth and ROS content in WT and mutant cells (Fig.\u0026nbsp;5E). Next, we evaluated the sensitivity of WT and mutant cells to the oxidants \u003cem\u003et\u003c/em\u003e-BOOH and H\u003csub\u003e2\u003c/sub\u003eO\u003csub\u003e2\u003c/sub\u003e, and determined if this was altered by the addition of BPS to the medium (Fig.\u0026nbsp;5F). We observed that N88S seipin-expressing cells were slightly more sensitive to the tested oxidants than WT cells, but their sensitivity was not significantly altered by BPS when compared to WT cells (Fig.\u0026nbsp;5F). In the absence of any oxidative stress but in the presence of BPS, N88S seipin-expressing cells also displayed a mild growth defect as previously reported for \u003cem\u003ecth2\u003c/em\u003eΔ cells (\u003cspan citationid=\"CR89\" class=\"CitationRef\"\u003e89\u003c/span\u003e), which is in agreement with lower Aft1p transcriptional activity and impaired response to iron deficiency (Fig.\u0026nbsp;5F). Overall, the data suggest that disruption of iron homeostasis is not the primary cause of oxidative damage in the yeast model of N88S seipinopathy.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec21\" class=\"Section2\"\u003e \u003ch2\u003e3.5. The MAPK Hog1p/p38 contributes to impaired iron metabolism in cells carrying the seipin N88S mutation\u003c/h2\u003e \u003cp\u003eThe regulation of Aft1p phosphorylation by the MAPK kinases Hog1p and Slt2p has been implicated in the control of iron homeostasis and associated stress response pathways (\u003cspan citationid=\"CR43\" class=\"CitationRef\"\u003e43\u003c/span\u003e, \u003cspan citationid=\"CR44\" class=\"CitationRef\"\u003e44\u003c/span\u003e). In particular, Hog1p negatively regulates Aft1p transcriptional activity, which allows its export from the nucleus to the cytosol under iron sufficient conditions (\u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e37\u003c/span\u003e, \u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e38\u003c/span\u003e, \u003cspan citationid=\"CR43\" class=\"CitationRef\"\u003e43\u003c/span\u003e, \u003cspan citationid=\"CR90\" class=\"CitationRef\"\u003e90\u003c/span\u003e). Based on this, we posit that reduced activation of the iron regulation by Aft1p might be associated with changes in Hog1p activation and/or Aft1p phosphorylation. Detailed proteomic analysis revealed increased levels of Sko1p (Table \u003cspan refid=\"MOESM4\" class=\"InternalRef\"\u003eS4\u003c/span\u003e). Sko1p is a key transcription factor regulating osmostress-induced gene expression under the direct control of the Hog1p (\u003cspan citationid=\"CR91\" class=\"CitationRef\"\u003e91\u003c/span\u003e). Sko1p binds to cAMP-responsive element (CRE) sequences, and the expression analysis of CRE-driven reporter genes is used as a reporter of osmostress-activated expression, which depends solely on Sko1p and Hog1p proteins (\u003cspan additionalcitationids=\"CR93\" citationid=\"CR92\" class=\"CitationRef\"\u003e92\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR94\" class=\"CitationRef\"\u003e94\u003c/span\u003e). Using a 2xCRE-LacZ reporter, we evaluated changes in Hog1p activation during lifespan. At the exponential phase, we observed no significant changes, however a higher activation of the reporter fusion was observed in N88S seipin-expressing cells at PDS phase, indicating higher Hog1p activation (Fig.\u0026nbsp;6A). This coincided with reduced Aft1p transcriptional activity at this phase (Fig.\u0026nbsp;5B). To evaluate changes in Aft1p phosphorylation, we analyzed the migration pattern of HA-tagged Aft1p using Western blotting at PDS phase (Fig.\u0026nbsp;6B). Although total Aft1p levels are slightly higher (but not statistically significant), no noticeable alterations in the phosphorylation mobility pattern of Aft1p were observed in the mutant compared to WT cells (Fig.\u0026nbsp;6B). As a result, we conclude that the Aft1p phosphorylation status is not a primary cause for defective activation of the iron regulon at PDS phase (Fig.\u0026nbsp;5B).\u003c/p\u003e \u003cp\u003eThe transcriptional activity of Aft1p is governed by its localization in the nucleus, which is controlled by several regulatory mechanisms involving a range of proteins. These interactions can result in alterations in the activation of the iron regulon. We thus investigated the localization of GFP-Aft1p in WT and mutant cells using fluorescence microscopy. Under iron-rich conditions, around 40% of wild-type cells displayed nuclear Aft1p, whereas only 21% of cells expressing the N88S seipin variant showed nuclear localization of the transcription factor (Fig.\u0026nbsp;6C). These data suggest increased export of Aft1p to the cytosol, which could explain why full activation of the iron regulon is hampered in the yeast model of N88S seipinopathy.\u003c/p\u003e \u003cp\u003eWe decided to extend our analysis of the contribution of Hog1p to the loss of iron homeostasis imparted by the N88S seipin mutation. Firstly, we measured iron levels during lifespan, and the results revealed that deletion of \u003cem\u003eHOG1\u003c/em\u003e in WT cells increased iron levels at the exponential phase, consistent with its role as a negative regulator of the iron regulon (Fig.\u0026nbsp;6D). Importantly, the absence of Hog1p suppressed the iron accumulation phenotype of the mutant, and restored its ability to maintain proper iron levels as observed in WT cells (Fig.\u0026nbsp;6D). Next, we analyzed the Aft1p transcriptional activity during lifespan and upon BPS treatment in cells expressing p\u003cem\u003eCTH2\u003c/em\u003e-LacZ. At PDS phase, we observed that deletion of \u003cem\u003eHOG1\u003c/em\u003e had no significant alterations in the β-galactosidase reporter activity in both WT and N88S seipin-expressing cells (Fig.\u0026nbsp;6E). This indicates that during lifespan, the activation of the iron regulon by Aft1p/Aft2p is mediated by other signal transduction pathways in addition to Hog1p regulation (\u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e37\u003c/span\u003e, \u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e38\u003c/span\u003e). However, under iron deprivation, \u003cem\u003eCTH2\u003c/em\u003e-LacZ expression was induced in WT cells and reached higher levels in the corresponding \u003cem\u003ehog1\u003c/em\u003eΔ mutant (Fig.\u0026nbsp;6F). Notably, the transcriptional activity of Aft1p in cells expressing the N88S mutation was restored to WT levels (Fig.\u0026nbsp;6F) in the absence of the MAPK, supporting the idea that Hog1p controls iron levels and the adaptive response to iron deficiency in the yeast model of N88S seipinopathy.\u003c/p\u003e \u003cp\u003eWe also decided to investigate whether Hog1p signalling also modulates IB formation in the mutant. For that, we followed intracellular localization of IBs using the Venus signal (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). We observed a reduction of number of cells displaying IBs upon deletion of either \u003cem\u003eHOG1\u003c/em\u003e or \u003cem\u003eSKO1\u003c/em\u003e (Fig. \u003cspan refid=\"MOESM5\" class=\"InternalRef\"\u003eS5\u003c/span\u003eA-B), indicating that Hog1p/p38 also promotes IB generation beyond iron imbalance in cells expressing mutant seipin.\u003c/p\u003e \u003cp\u003eFinally, we decided to investigate if regulation of ER stress response is linked to loss of iron homeostasis observed in the mutant. To test this hypothesis, we analyzed \u003cem\u003eCTH2\u003c/em\u003e-LacZ reporter activity in cells shifted to SC-glucose medium with or without inositol, supplemented or not with BPS. In WT cells, shifting to inositol-containing medium did not result in measurable changes in the β-galactosidase activity. Notably, \u003cem\u003eCTH2\u003c/em\u003e-LacZ expression was induced only in the presence of BPS, with no significant changes due to inositol alone in these cells (Fig. \u003cspan refid=\"MOESM5\" class=\"InternalRef\"\u003eS5\u003c/span\u003eC). However, in N88S seipin-expressing cells, there was a subtle but consistent increase in Aft1p transcriptional activity when grown in inositol-containing medium supplemented with BPS, compared to cells grown without inositol plus BPS (Fig. \u003cspan refid=\"MOESM5\" class=\"InternalRef\"\u003eS5\u003c/span\u003eC). This finding is particularly important as it reveals a previously unexplored functional relationship between inositol and iron metabolism. It indicates that under conditions where PA is consumed and the ER stress response is attenuated in the mutant (Fig.\u0026nbsp;3E), there is higher activation of the iron regulon by Aft1p/Aft2p in the yeast model of N88S seipinopathy.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec22\" class=\"Section2\"\u003e \u003ch2\u003e3.6. \u003cem\u003eFET3\u003c/em\u003e expression is altered in cells carrying the seipin N88S mutation\u003c/h2\u003e \u003cp\u003eThe expression of \u003cem\u003eFET3\u003c/em\u003e, a gene involved in iron uptake, is also regulated by the transcription factor Aft1p (\u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e37\u003c/span\u003e, \u003cspan citationid=\"CR95\" class=\"CitationRef\"\u003e95\u003c/span\u003e, \u003cspan citationid=\"CR96\" class=\"CitationRef\"\u003e96\u003c/span\u003e). To evaluate if Aft1p inhibition in N88S seipin-expressing cells also affects \u003cem\u003eFET3\u003c/em\u003e expression, we used a construct containing the \u003cem\u003eFET3\u003c/em\u003e promoter (-863 bp to +\u0026thinsp;1) fused to the LacZ reporter gene (YEplac181-\u003cem\u003eFET3\u003c/em\u003e-LacZ) (\u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e51\u003c/span\u003e). In this construct, there is an identified functional Aft1p consensus site (\u003cspan citationid=\"CR96\" class=\"CitationRef\"\u003e96\u003c/span\u003e) located \u0026minus;\u0026thinsp;254 bp upstream of the ATG translation initiation codon, and a predicted Aft1p-binding site at position \u0026minus;\u0026thinsp;670 bp (GGCACCC) in the \u003cem\u003eFET3\u003c/em\u003e promoter (\u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e51\u003c/span\u003e). The impact of N88S seipin mutation on \u003cem\u003eFET3\u003c/em\u003e-LacZ expression was firstly assessed by measuring the β-galactosidase activity of the reporter during lifespan (Fig.\u0026nbsp;7A). The results showed no differences in the reporter gene expression in WT and N88S seipin-expressing cells at the exponential phase. We observed an increase in \u003cem\u003eFET3\u003c/em\u003e expression in WT cells at PDS phase, but the induction was higher in the mutant (Fig.\u0026nbsp;7A), which contrasts with reduced Aft1p-controlled \u003cem\u003eCTH2\u003c/em\u003e expression observed at the same phase (Fig.\u0026nbsp;5B). This suggests that in mutant cells, Aft1p regulates \u003cem\u003eFET3\u003c/em\u003e expression differently compared to other Aft1p-regulated genes.\u003c/p\u003e \u003cp\u003eWe also tested if this effect is also observed under BPS-induced iron deficient conditions. As expected, BPS treatment induced \u003cem\u003eFET3\u003c/em\u003e expression in WT cells, but the reporter fusion activity was even higher in N88S seipin expressing cells (Fig.\u0026nbsp;7B). Overall, the results indicate that \u003cem\u003eCTH2\u003c/em\u003e expression was reduced, whereas \u003cem\u003eFET3\u003c/em\u003e expression is increased at PDS phase and under iron-deficient conditions in cells expressing N88S mutant seipin.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec23\" class=\"Section2\"\u003e \u003ch2\u003e3.7. \u003cem\u003eIn-silico\u003c/em\u003e analysis revealed the presence of a potential Msn2p/Msn4p binding site in the FET3 promoter\u003c/h2\u003e \u003cp\u003eIt was previously shown that \u003cem\u003eFET3\u003c/em\u003e expression is not entirely dependent on Aft1p, and that the transcription factor Ace1p regulates the response to copper overload by limiting the expression of \u003cem\u003eFET3\u003c/em\u003e (\u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e51\u003c/span\u003e). To delineate potential promoter regions responsible for Aft1p-independent activation of \u003cem\u003eFET3\u003c/em\u003e, we performed an unbiased bioinformatic analysis of the \u003cem\u003eFET3\u003c/em\u003e promoter (-863 bp to +\u0026thinsp;1) to search for potential transcription factor binding sites using YEASTRACT+ (\u003cspan citationid=\"CR74\" class=\"CitationRef\"\u003e74\u003c/span\u003e). The results revealed more than 50 transcription factors that could potentially bind to the \u003cem\u003eFET3\u003c/em\u003e promoter (Table \u003cspan refid=\"MOESM7\" class=\"InternalRef\"\u003eS7\u003c/span\u003e). The results identified the putative Aft1p/Aft2p binding sequence (-670 bp), the predicted Ace1p-like binding site (-783 bp) (\u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e51\u003c/span\u003e), and importantly a Msn2p binding sequence located upstream (-813 bp) on the \u003cem\u003eFET3\u003c/em\u003e promoter was now uncovered (Fig.\u0026nbsp;7C).\u003c/p\u003e \u003cp\u003eIn \u003cem\u003eS. cerevisiae\u003c/em\u003e, the stress response involves a sophisticated network of sensing and signal transduction mechanisms, prominently featuring the transcriptional regulation of various genes. In yeast, the zinc-finger transcription factors Msn2p and Msn4p, which share 66% sequence homology, are key regulators of stress-responsive gene expression (\u003cspan additionalcitationids=\"CR98 CR99 CR100 CR101\" citationid=\"CR97\" class=\"CitationRef\"\u003e97\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR102\" class=\"CitationRef\"\u003e102\u003c/span\u003e). They bind specifically to the stress response element (STRE) sequences 5\u0026prime;-AGGGG or 5\u0026prime;-GGGGA. Msn2p and Msn4p control the expression of over 90% of genes activated in response to heat stress, osmotic stress, and carbon starvation, and are essential for regulating chronological lifespan (\u003cspan additionalcitationids=\"CR98 CR99 CR100 CR101\" citationid=\"CR97\" class=\"CitationRef\"\u003e97\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR102\" class=\"CitationRef\"\u003e102\u003c/span\u003e). Importantly, it was reported that overexpression of the plasma membrane receptor \u003cem\u003eIZH2\u003c/em\u003e inhibits \u003cem\u003eFET3\u003c/em\u003e expression via negative regulation of Msn2p/Msn4p transcriptional activation without requiring Aft1p-dependent induction of the iron-responsive element FeRE (\u003cspan citationid=\"CR103\" class=\"CitationRef\"\u003e103\u003c/span\u003e). Based on this study, we posit that overexpression of \u003cem\u003eIZH2\u003c/em\u003e should decrease the \u003cem\u003eFET3-\u003c/em\u003eLacZ reporter gene expression if the latter relies on Msn2p/Msn4p activation. At the exponential phase, no significant differences were observed in all strains tested, but upon transition to PDS phase, we observed higher β-galactosidase activity of the \u003cem\u003eFET3\u003c/em\u003e-LacZ reporter in cells expressing mutant seipin cells, which was reduced to WT levels upon overexpression of \u003cem\u003eIZH2\u003c/em\u003e (Fig.\u0026nbsp;7D). Importantly, we observed a reduction in \u003cem\u003eFET3\u003c/em\u003e expression in WT cells when \u003cem\u003eIZH2\u003c/em\u003e was overexpressed (Fig.\u0026nbsp;7D), which is consistent with a negative regulation of \u003cem\u003eFET3\u003c/em\u003e expression by Izh2p.\u003c/p\u003e \u003cp\u003eIn keeping with a role for Msn2p/Msn4p in the regulation of \u003cem\u003eFET3\u003c/em\u003e expression, we further tested the expression of the pSTRE-LacZ reporter gene, which contains the STRE sequences from the \u003cem\u003eCTT1\u003c/em\u003e promoter regulated by these transcription factors (\u003cspan citationid=\"CR104\" class=\"CitationRef\"\u003e104\u003c/span\u003e). Here, we transformed both strains with the reporter, and β-galactosidase activity was measured during lifespan. We found that higher \u003cem\u003eFET3\u003c/em\u003e expression (Fig.\u0026nbsp;7A) paralleled the increased activation of Msn2p/Msn4p transcriptional activity at PDS phase in N88S seipin-expressing cells (Fig.\u0026nbsp;7E). In addition, a bioinformatic search for target genes with documented regulation by Msn2p/Msn4p identified genes encoding proteins whose levels were found to be higher at PDS phase by proteomic analysis (Table \u003cspan refid=\"MOESM4\" class=\"InternalRef\"\u003eS4\u003c/span\u003e), including \u003cem\u003eGRX2\u003c/em\u003e, \u003cem\u003ePUT3\u003c/em\u003e, \u003cem\u003eHXT1\u003c/em\u003e, \u003cem\u003eHXT7\u003c/em\u003e, \u003cem\u003eRAS2\u003c/em\u003e, \u003cem\u003eDIP5\u003c/em\u003e, \u003cem\u003eARO10\u003c/em\u003e, \u003cem\u003eMAL12\u003c/em\u003e and \u003cem\u003eARO9\u003c/em\u003e (Table \u003cspan refid=\"MOESM8\" class=\"InternalRef\"\u003eS8\u003c/span\u003e). Altogether, the data strongly suggest that stress responsive Msn2p/Msn4p transcription factors are activated and may positively regulate \u003cem\u003eFET3\u003c/em\u003e expression at PDS phase, thus compensating for the reduced Aft1p transcriptional activity (as observed for \u003cem\u003eCTH2\u003c/em\u003e-LacZ reporter) in N88S seipin-expressing cells (Fig.\u0026nbsp;5B). It is possible that \u003cem\u003eFET3\u003c/em\u003e expression acts as an adaptive response to partially counteract the reduced Aft1p-controlled \u003cem\u003eCTH2\u003c/em\u003e expression and lower protein levels of Fit1p, Arn1p, Arn2p, and Hmx1p. It is important to note that analysis of the \u003cem\u003eCTH2\u003c/em\u003e promoter used in the \u003cem\u003eCTH2\u003c/em\u003e-LacZ reporter fusion (\u003cspan citationid=\"CR49\" class=\"CitationRef\"\u003e49\u003c/span\u003e) did not reveal any binding sites for Msn2p/Msn4p using YEASTRACT+ (data not shown).\u003c/p\u003e \u003cp\u003e \u003cb\u003e3.8. The induction of\u003c/b\u003e \u003cb\u003eFET3\u003c/b\u003e \u003cb\u003eexpression is associated with a reduction in aconitase activity in cells expressing N88S mutant seipin\u003c/b\u003e\u003c/p\u003e \u003cp\u003eCells respond to defective Fe-S cluster synthesis by accumulating iron both within the mitochondria and in the cell. It is known that reducing intracellular iron pool results in decreased activity of the Fe-S cluster enzyme aconitase and subsequently triggers \u003cem\u003eFET3\u003c/em\u003e expression (\u003cspan citationid=\"CR105\" class=\"CitationRef\"\u003e105\u003c/span\u003e, \u003cspan citationid=\"CR106\" class=\"CitationRef\"\u003e106\u003c/span\u003e). Based on this, we measured aconitase activity of WT and N88S seipin-expressing cells grown to PDS phase, when \u003cem\u003eFET3\u003c/em\u003e expression was increased for the mutant. Aconitase activity was decreased by ~\u0026thinsp;40% in the mutant (Fig.\u0026nbsp;7F), suggesting that mitochondrial Fe-S cluster synthesis/assembly may signal the upregulation of \u003cem\u003eFET3\u003c/em\u003e expression at PDS phase, while compensating for the reduced activation of the iron regulon by Aft1p, in an attempt to reestablish homeostatic intracellular iron levels. In agreement with this hypothesis, we observed that many genes involved in Fe-S cluster assembly were among the most affected DEGs in cells expressing the N88S seipin mutation under conditions of Fe deprivation (Fig. \u003cspan refid=\"MOESM4\" class=\"InternalRef\"\u003eS4\u003c/span\u003eD).\u003c/p\u003e \u003c/div\u003e"},{"header":"4. Discussion","content":"\u003cp\u003eIn this project, we provide evidence that inositol and neutral lipid metabolism and cellular iron homeostasis are compromised in the yeast model of N88S seipinopathy (Fig.\u0026nbsp;8). Importantly, our results are consistent with a reduced rate of phospholipid biosynthesis and increased TG content coupled with PA accumulation. As a result, the activity of the Opi1p transcriptional repressor is impaired, leading to derepression of \u003cem\u003eINO1\u003c/em\u003e expression and increased levels of Ino1p. Nevertheless, we did not observe altered levels of major phospholipids, including PC, PE, PS or PI. It has been previously reported that about 10% of the WT level of activity of the phospholipid biosynthetic enzymes is sufficient to maintain normal growth and almost normal lipid composition (\u003cspan citationid=\"CR31\" class=\"CitationRef\"\u003e31\u003c/span\u003e, \u003cspan citationid=\"CR85\" class=\"CitationRef\"\u003e85\u003c/span\u003e, \u003cspan citationid=\"CR107\" class=\"CitationRef\"\u003e107\u003c/span\u003e). However, a decrease in the protein levels of these enzymes is expected to significantly influence the flux of lipid precursor at the PA metabolic branch point, where PA can be channeled towards TG synthesis at the expense of a reduced rate of \u003cem\u003ede novo\u003c/em\u003e synthesis of phospholipids (Fig.\u0026nbsp;8). Curiously, PG levels which is derived from CDP-DAG, were reduced. One possibility is impaired synthesis of CDP-DAG, resulting from decreased activity of Tam41p, thereby reducing the substrate availability for PG production. Additionally, dysfunction of enzymes responsible for the biosynthesis of PG could also contribute to lower PG levels (\u003cspan citationid=\"CR108\" class=\"CitationRef\"\u003e108\u003c/span\u003e).\u003c/p\u003e \u003cp\u003ePA increases membrane order in the ER, and its accumulation has been associated with the induction of the ER stress response and apoptosis under various conditions (\u003cspan citationid=\"CR109\" class=\"CitationRef\"\u003e109\u003c/span\u003e, \u003cspan citationid=\"CR110\" class=\"CitationRef\"\u003e110\u003c/span\u003e). It would then be interesting to further explore whether changes in ER ultrastructure could also contribute to ER stress beyond IB formation associated with seipin misfolding. In addition, we observed increased levels of the pro-apoptotic ceramide, indicating a degree of pathological convergence of ceramide accumulation observed in different MNDs (\u003cspan citationid=\"CR111\" class=\"CitationRef\"\u003e111\u003c/span\u003e, \u003cspan citationid=\"CR112\" class=\"CitationRef\"\u003e112\u003c/span\u003e). Interestingly, we observed increased levels of lysophospholipids, indicating that lysophospholipid:acyl-CoA acyltransferases (LPLATs) Slc1p and Ale1p activities are impaired. Of particular interest, dysfunction in LPA signaling has been associated with several neurological conditions, including Alzheimer\u0026rsquo;s disease and Parkinson\u0026rsquo;s disease, and other disorders (\u003cspan additionalcitationids=\"CR114\" citationid=\"CR113\" class=\"CitationRef\"\u003e113\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR115\" class=\"CitationRef\"\u003e115\u003c/span\u003e). Moreover, LPC has been shown to contribute to pericyte loss, disruption of the vascular barrier, demyelination, and motor function impairments (\u003cspan additionalcitationids=\"CR117\" citationid=\"CR116\" class=\"CitationRef\"\u003e116\u003c/span\u003e\u0026ndash;\u003cspan citationid=\"CR118\" class=\"CitationRef\"\u003e118\u003c/span\u003e). Additionally, LPC exacerbates the neurotoxicity of amyloid β1\u0026ndash;42 peptide oligomer formation and promotes neurotoxic protein aggregation, highlighting its potential as a therapeutic target for neurodegenerative diseases (\u003cspan citationid=\"CR119\" class=\"CitationRef\"\u003e119\u003c/span\u003e, \u003cspan citationid=\"CR120\" class=\"CitationRef\"\u003e120\u003c/span\u003e). Notably, one study found that patients with repetitive mild traumatic brain injury exhibited significantly elevated LPC levels (\u003cspan citationid=\"CR121\" class=\"CitationRef\"\u003e121\u003c/span\u003e). Unfortunately, search for diagnostic and prognostic biomarkers in seipinopathy and related MNDs is scarce, and there are currently no definitive molecular biomarkers associated with such disorders. Here, we propose that PA and lysophospholipids could serve as potential candidates for biomarkers of this cohort of diseases.\u003c/p\u003e \u003cp\u003eOverall, we provide strong evidence that N88S seipinopathy is also a lipidopathy. In fact, deletion of \u003cem\u003eINO1\u003c/em\u003e increased basal levels of the ER stress response, however this was associated with reduced IB formation in N88S seipin-expressing cells. It should be noted that \u003cem\u003eINO1\u003c/em\u003e deletion did not affect ROS levels in mutant cells, suggesting that oxidative stress is not directly linked to lipid metabolism defects. In line with abnormal lipid profile observed in cells expressing N88S seipin, which influences the activation of the ER stress response, we posit that an imbalance in cellular lipid homeostasis is a potential major driver of the neurotoxic process in human seipinopathy, with N88S seipin misfolding acting as the initiating trigger. This aligns with seipin\u0026acute;s crucial role in phospholipid and neutral lipid metabolism. However, we cannot exclude the possibility that seipinopathy and related human MNDs may be defined as both proteinopathies and lipidopathies. A vicious cycle of dysregulation in protein folding and lipid metabolism might be initiated by early and subtle changes in either lipid or protein handling as previously proposed (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eAnother interesting finding of this work was the loss of iron homeostasis in the yeast model of N88S seipinopathy (Fig.\u0026nbsp;8). Our proteomic analysis revealed that levels of iron homeostasis-associated proteins, including Fit1p, Arn1p, Arn2p, and Hmx1p, were reduced in cells expressing the N88S seipin mutation. The expression of these proteins is regulated by the major iron-sensing transcription factor Aft1p, a key transcription factor that manages the cellular response to iron deficiency. In this study, it was shown that Aft1p transcriptional activity is deregulated during lifespan and upon iron depletion, which likely contributes to a defective adaptive response, particularly under conditions of iron deficiency. We provide strong evidence that Aft1p localization was impaired under excess iron conditions, and importantly MAPK Hog1p/p38 was involved in the regulation of \u003cem\u003eCTH2\u003c/em\u003e expression in response to iron starvation, but not throughout lifespan. This indicates that other major signaling effectors (e.g., Snf1p/AMPK or PKA) might control the transcription of genes belonging to the iron regulon via regulation of Aft1p activation and its transcriptional activity (\u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e37\u003c/span\u003e, \u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e38\u003c/span\u003e). Yet, we found that the expression of the ferroxidase Fet3p, which is required for high affinity iron transport and also regulated by Aft1p, was increased. While both Cth1p and Cth2p are transcriptionally induced by Aft1p/Aft2p, \u003cem\u003eFET3\u003c/em\u003e expression appears to be adaptively regulated by multiple transcription factors in response to changes in iron and other ion levels, including Ace1p, Aft1p and Msn2p. Importantly, Cth1/2p functions post-transcriptionally by targeting and degrading RNA transcripts of nonessential proteins that require large amounts of iron (\u003cspan citationid=\"CR49\" class=\"CitationRef\"\u003e49\u003c/span\u003e). In contrast, Fet3p operates upstream by capturing iron to fulfil cellular iron needs, with its expression being more closely associated with the iron-sulfur (Fe-S) biogenesis machinery (\u003cspan citationid=\"CR105\" class=\"CitationRef\"\u003e105\u003c/span\u003e, \u003cspan citationid=\"CR106\" class=\"CitationRef\"\u003e106\u003c/span\u003e). Notably, defects in the assembly of cytosolic Fe-S cluster-containing proteins do not trigger activation of the iron regulon. Instead, alterations in mitochondrial iron-sulfur cluster assembly are important for signaling iron bioavailability to Aft1p or Aft2p (\u003cspan citationid=\"CR122\" class=\"CitationRef\"\u003e122\u003c/span\u003e, \u003cspan citationid=\"CR123\" class=\"CitationRef\"\u003e123\u003c/span\u003e). The activity of the mitochondrial Fe-S enzyme aconitase was inversely correlated with the expression of \u003cem\u003eFET3\u003c/em\u003e in the mutant, in agreement with previous findings (\u003cspan citationid=\"CR106\" class=\"CitationRef\"\u003e106\u003c/span\u003e). We currently envision a model where coupling transcription of the high affinity iron transport system Ftr1p/Fet3p to the Fe-S cluster activity may provide a potential link that might explain why \u003cem\u003eFET3\u003c/em\u003e expression increased via activation of stress responsive transcription factors Msn2p/Msn4p (Fig.\u0026nbsp;8), despite reduced Aft1p transcriptional activity and iron imbalance. Moreover, it is known that Fe-S clusters are primary targets of ROS, so impaired Fe-S metabolism, as suggested by partial loss of aconitase activity, could potentially contribute to ROS buildup and oxidative damage exhibited by the N88S mutant strain (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). Loss of aconitase activity may therefore reflect increased levels of cellular dysfunction due to oxidative damage or possibly changes in other cellular processes, as recently proposed for Parkinson\u0026acute;s disease (\u003cspan citationid=\"CR124\" class=\"CitationRef\"\u003e124\u003c/span\u003e). This could be relevant to human N88S seipinopathy pathogenesis as a biomarker candidate to improve diagnostics/disease progression. Whether mitochondrial mobilization of iron coupled with the synthesis of Fe-S clusters is altered in N88S seipin-expressing cells is currently undefined, and should be explored in future studies.\u003c/p\u003e"},{"header":"5. Conclusions","content":"\u003cp\u003eThis study presents compelling evidence that human N88S seipinopathy may also be a lipidopathy linked to the disruption of iron homeostasis. The accumulation of PA and TG, combined with a decreased rate of phospholipid synthesis, plays a crucial role in inducing ER stress. This underscores the potential therapeutic strategy of targeting phospholipid and neutral lipid metabolism to manage ER stress and cell death arising from disruption of inositol metabolism. Such an approach could benefit patients with seipinopathy and other MNDs.\u003c/p\u003e \u003cp\u003eAlthough many neurodegenerative and neuromotor syndromes are mostly related to iron overload with its deleterious effects in proteotoxicity and oxidative damage, there is increasing evidence that response to both iron overload and iron deficiency affects signalling pathways contributing to neuronal death. For instance, patients carrying biallelic mutations in \u003cem\u003eIREB2\u003c/em\u003e (Iron Responsive Element Binding Protein 2) display neurological and haematological defects associated with iron deficiency, impaired transcriptional regulation of iron metabolism and mitochondrial dysfunction (\u003cspan citationid=\"CR125\" class=\"CitationRef\"\u003e125\u003c/span\u003e), which are neuropathological cellular phenotypes reminiscent of seipinopathy (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e). More recently, the analysis of primary fibroblasts from a patient with a loss-of-function mutation in L-ferritin revealed reduced cellular iron levels, lower catalase activity, ROS accumulation and increased levels of oxidized proteins (\u003cspan citationid=\"CR126\" class=\"CitationRef\"\u003e126\u003c/span\u003e). We have also previously reported a loss of catalase activity associated with ROS generation in the yeast model of seipinopathy (\u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e45\u003c/span\u003e), indicating that in both cases, impaired response to iron deficiency is likely associated with the oxidative stress response. Whether these phenotypes are closely related to the development of neuromotor defects observed in patients with seipinopathy remains to be investigated, but emerges as a novel and exciting avenue for therapeutic intervention in this cohort of MNDs.\u003c/p\u003e \u003cp\u003eTo the best of our knowledge, this study represents the first detailed description of protein and lipid alterations in N88S seipinopathy using systems biology.\u003c/p\u003e"},{"header":"Abbreviations","content":"\u003cp\u003eACAT - Acyl-coenzyme A: cholesterol acyltransferase; AGPAT - Acylglycerolphosphate Acyltransferase; BiFC - Biomolecular Fluorescence Complementation; BPS - Bathophenanthrolinesulfonate; BSCL2 - Berardinelli-Seip congenital lipodystrophy type 2; CDP-DAG - Cytidine Diphosphate-Diacylglycerol; CYC1t - CYC1 terminator; DEG - Differentially Expressed Genes; DEP - Differentially Expressed Protein; DG - Diacylglycerol; DGAT - Acyl-CoA Diacylglycerol Acyltransferase; DNA - Deoxyribonucleic Acid; ER - Endoplasmic Reticulum; ERAD - ER-Associated Degradation; EXP - Exponential Phase; Fe-S - Iron-Sulfur; FIT - Fat storage-inducing transmembrane; GO - Gene Ontology; GPAT - Glycerol-3 Phosphate Acyltransferase; GPDpr - GPD promoter; IB - Inclusion body; IREB2 - Iron Responsive Element Binding Protein 2; LA - Lithium Acetate; LD - Lipid Droplet; LPA - Lysophosphatidic Acid; LPC - Lysophosphatidylcholine; LPLAT - Lysophospholipid:acyl-CoA acyltransferases; MAPK - Mitogen-Activated Protein Kinase; MNDs - Motor Neuron Diseases; MS - Mass Spectrometry; ONPG - O-nitrophenylgalactopyranosyde; PA - Phosphatidic Acid; PC - Phosphatidylcholine; PE - Phosphatidylethanolamine; PG - Phosphatidylglycerol; PI - Phosphatidylinositol; PS - Phosphatidylserine; PDS - Post-diauxic shift; PEG - Polyethylene glycol; ROS - Reactive Oxygen Species; SC - Synthetic Complete; SE - Sterol Esters; STRE - Stress Response Element; TFs - Transcription Factors; TG - Triacylglycerol; UPR - Unfolded Protein Response; VC - Venus C-terminal fragment; VN - Venus N-terminal fragment; WT - Wild-type; YNB - Yeast Nitrogen Base; YPD - Yeast Peptone Dextrose.\u003c/p\u003e"},{"header":"Declarations","content":"\u003cp\u003e \u003ch2\u003e \u003cb\u003eCompeting interests\u003c/b\u003e:\u003c/h2\u003e \u003cp\u003eThe authors declare that they have no known competing financial interests or personal relationships that could have appeared to influence the work reported in this paper. The funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript, or in the decision to publish the results.\u003c/p\u003e \u003c/p\u003e\u003ch2\u003eFunding:\u003c/h2\u003e \u003cp\u003eThis work was funded by national funds through Foundation for Science and Technology (FCT), under the project 2022.02305.PTDC, CEECIND/00724/2017 and CEECIND/00724/2017/CP1386/CT0006, and EMBO Scientific Exchange Grant 9890.\u003c/p\u003e\u003ch2\u003eAuthor Contribution\u003c/h2\u003e\u003cp\u003eV. T. and V. C. conceived and supervised the project. V. T. and V. C. designed the experiments and analyzed most of the data. M. R., M. O. and V. N. performed most of the experiments. V. T. wrote the manuscript with input from all authors.\u003c/p\u003e\u003ch2\u003eAcknowledgement\u003c/h2\u003e\u003cp\u003eWe would like to thank the YSN Group for productive discussions and the i3S Scientific Platforms and BGI commercial services for their technical assistance with bioinformatic analysis, flow cytometry, fluorescence microscopy, and omics approaches used in this study.\u003c/p\u003e"},{"header":"References","content":"\u003col\u003e\u003cli\u003e\u003cspan\u003eZadoorian A, Du X, Yang H. Lipid droplet biogenesis and functions in health and disease. Nat Rev Endocrinol. 2023;19(8):443\u0026ndash;59.\u003c/span\u003e\u003c/li\u003e \u003cli\u003e\u003cspan\u003eRakotonirina-Ricquebourg R, Costa V, Teixeira V. Hello from the other side: Membrane contact of lipid droplets with other organelles and subsequent functional implications. Prog Lipid Res. 2022;85:101141.\u003c/span\u003e\u003c/li\u003e \u003cli\u003e\u003cspan\u003eHenne W. The Molecular Era of Lipid Droplets. 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J Exp Med. 2013;210(9):1779\u0026ndash;91.\u003c/span\u003e\u003c/li\u003e\u003c/ol\u003e"}],"fulltextSource":"","fullText":"","funders":[],"hasAdminPriorityOnWorkflow":false,"hasManuscriptDocX":true,"hasOptedInToPreprint":true,"hasPassedJournalQc":"","hasAnyPriority":true,"hideJournal":false,"highlight":"","institution":"","isAcceptedByJournal":true,"isAuthorSuppliedPdf":false,"isDeskRejected":"","isHiddenFromSearch":false,"isInQc":false,"isInWorkflow":false,"isPdf":false,"isPdfUpToDate":true,"isWithdrawnOrRetracted":false,"journal":{"display":true,"email":"[email protected]","identity":"cell-communication-and-signaling","isNatureJournal":false,"hasQc":true,"allowDirectSubmit":false,"externalIdentity":"ccas","sideBox":"Learn more about [Cell Communication and Signaling](http://biosignaling.biomedcentral.com/)","snPcode":"12964","submissionUrl":"https://submission.nature.com/new-submission/12964/3","title":"Cell Communication and Signaling","twitterHandle":"@bmc","acdcEnabled":true,"dfaEnabled":true,"editorialSystem":"em","reportingPortfolio":"BMC/SO AJ","inReviewEnabled":true,"inReviewRevisionsEnabled":true},"keywords":"lipid droplet, seipin, misfolding, seipinopathy, lipidopathy, proteinopathy, inositol, iron","lastPublishedDoi":"10.21203/rs.3.rs-5224286/v1","lastPublishedDoiUrl":"https://doi.org/10.21203/rs.3.rs-5224286/v1","license":{"name":"CC BY 4.0","url":"https://creativecommons.org/licenses/by/4.0/"},"manuscriptAbstract":"\u003ch2\u003eBackground\u003c/h2\u003e \u003cp\u003eSeipin is a protein encoded by the \u003cem\u003eBSCL2\u003c/em\u003e gene in humans and \u003cem\u003eSEI1\u003c/em\u003e gene in yeast, forming an Endoplasmic Reticulum (ER)-bound homo-oligomer. This oligomer is crucial in targeting ER-lipid droplet (LD) contact sites, facilitating the delivery of triacylglycerol (TG) to nascent LDs. Mutations in BSCL2, particularly N88S and S90L, lead to seipinopathies, which correspond to a cohort of motor neuron diseases (MNDs) characterized by the accumulation of misfolded N88S seipin into inclusion bodies (IBs) and cellular dysfunctions.\u003c/p\u003e\u003ch2\u003eMethods\u003c/h2\u003e \u003cp\u003eQuantitative untargeted mass spectrometric proteomic and lipidomic analyses were conducted to examine changes in protein and lipid abundance in wild-type (WT) versus N88S seipin-expressing mutant cells. Differentially expressed proteins were categorized into functional networks to highlight altered protein functions and signaling pathways. Statistical comparisons were made using unpaired, two-tailed Student's t-tests or two-way ANOVA. \u003cem\u003eP\u003c/em\u003e-values\u0026thinsp;\u0026lt;\u0026thinsp;0.05 are considered significant.\u003c/p\u003e\u003ch2\u003eResults\u003c/h2\u003e \u003cp\u003eIn a well-established yeast model of N88S seipinopathy, misfolded N88S seipin forms IBs and exhibits higher levels of ER stress, leading to decreased cell viability due to increased reactive oxygen species (ROS), oxidative damage, lipid peroxidation, and reduced antioxidant activity. Proteomic and lipidomic analyses revealed alterations in phosphatidic acid (PA) levels, associated with disrupted inositol metabolism and decreased flux towards phospholipid biosynthesis. Importantly, deregulation of lipid metabolism contributed to ER stress beyond N88S seipin misfolding and IB formation. Additionally, the model exhibited deregulated iron (Fe) homeostasis during lifespan. N88S seipin-expressing cells showed impaired ability to cope with iron deficiency. This was linked to changes in the expression of Aft1p-controlled iron regulon genes, including the mRNA-binding protein \u003cem\u003eCTH2\u003c/em\u003e and the high-affinity iron transport system member \u003cem\u003eFET3\u003c/em\u003e, in a p38/Hog1p- and Msn2p/Msn4p-dependent manner. Importantly, we unraveled a novel link between inositol metabolism and activation of the iron regulon in cells expressing the N88S seipin mutation. Despite iron accumulation, this was not associated with oxidative stress.\u003c/p\u003e\u003ch2\u003eConclusions\u003c/h2\u003e \u003cp\u003eThe study highlights that the effects of N88S seipin mutation extend beyond protein misfolding, with significant disruptions in lipid metabolism and iron homeostasis. This research marks a significant advance in understanding and defining the roles of proteins and signaling pathways that contribute to human seipinopathy. Altered cellular processes, as well as potential therapeutic targets and biomarkers, were identified and can be explored in translational studies using human cell models.\u003c/p\u003e","manuscriptTitle":"N88S seipin-related seipinopathy is a lipidopathy associated with loss of iron homeostasis","msid":"","msnumber":"","nonDraftVersions":[{"code":1,"date":"2024-10-11 16:36:29","doi":"10.21203/rs.3.rs-5224286/v1","editorialEvents":[{"type":"communityComments","content":0},{"type":"decision","content":"Revision requested","date":"2024-11-23T17:22:48+00:00","index":"","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2024-11-18T10:32:25+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2024-11-18T04:47:14+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2024-11-17T21:02:59+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2024-11-13T13:49:16+00:00","index":"hide","fulltext":""},{"type":"editorInvitedReview","content":"","date":"2024-11-06T11:16:53+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"16106929599101213775018951641405885238","date":"2024-11-05T12:03:29+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"314356520498019761608683121891811521234","date":"2024-11-04T21:04:10+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"288788703514248582256572396248327063508","date":"2024-11-04T06:51:48+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"1224179446606670691548673238870230877","date":"2024-11-03T09:32:11+00:00","index":"hide","fulltext":""},{"type":"reviewerAgreed","content":"201261992771981498204112334197237706422","date":"2024-10-16T07:28:14+00:00","index":"hide","fulltext":""},{"type":"reviewersInvited","content":"","date":"2024-10-14T11:52:27+00:00","index":"","fulltext":""},{"type":"editorAssigned","content":"","date":"2024-10-09T13:04:08+00:00","index":"","fulltext":""},{"type":"checksComplete","content":"","date":"2024-10-09T13:01:06+00:00","index":"","fulltext":""},{"type":"submitted","content":"Cell Communication and Signaling","date":"2024-10-08T09:58:12+00:00","index":"","fulltext":""}],"status":"published","journal":{"display":true,"email":"[email protected]","identity":"cell-communication-and-signaling","isNatureJournal":false,"hasQc":true,"allowDirectSubmit":false,"externalIdentity":"ccas","sideBox":"Learn more about [Cell Communication and Signaling](http://biosignaling.biomedcentral.com/)","snPcode":"12964","submissionUrl":"https://submission.nature.com/new-submission/12964/3","title":"Cell Communication and Signaling","twitterHandle":"@bmc","acdcEnabled":true,"dfaEnabled":true,"editorialSystem":"em","reportingPortfolio":"BMC/SO AJ","inReviewEnabled":true,"inReviewRevisionsEnabled":true}}],"origin":"","ownerIdentity":"c649e33e-3db2-4f33-94ad-4f3aeb561647","owner":[],"postedDate":"October 11th, 2024","published":true,"recentEditorialEvents":[],"rejectedJournal":[],"revision":"","amendment":"","status":"published-in-journal","subjectAreas":[],"tags":[],"updatedAt":"2025-01-13T16:10:12+00:00","versionOfRecord":{"articleIdentity":"rs-5224286","link":"https://doi.org/10.1186/s12964-024-02007-9","journal":{"identity":"cell-communication-and-signaling","isVorOnly":false,"title":"Cell Communication and Signaling"},"publishedOn":"2025-01-07 15:57:50","publishedOnDateReadable":"January 7th, 2025"},"versionCreatedAt":"2024-10-11 16:36:29","video":"","vorDoi":"10.1186/s12964-024-02007-9","vorDoiUrl":"https://doi.org/10.1186/s12964-024-02007-9","workflowStages":[]},"version":"v1","identity":"rs-5224286","journalConfig":"researchsquare"},"__N_SSP":true},"page":"/article/[identity]/[[...version]]","query":{"redirect":"/article/rs-5224286","identity":"rs-5224286","version":["v1"]},"buildId":"8U1c8b4HqxoKbykW_rLl7","isFallback":false,"isExperimentalCompile":false,"dynamicIds":[84888],"gssp":true,"scriptLoader":[]}