The evolutionarily conserved PhLP3 is essential for sperm development inDrosophila melanogaster

The evolutionarily conserved PhLP3 is essential for sperm development in Drosophila melanogaster | bioRxiv /* */ /* */ <!-- <!-- /*! * yepnope1.5.4 * (c) WTFPL, GPLv2 */ (function(a,b,c){function d(a){return"[object Function]"==o.call(a)}function e(a){return"string"==typeof a}function f(){}function g(a){return!a||"loaded"==a||"complete"==a||"uninitialized"==a}function h(){var a=p.shift();q=1,a?a.t?m(function(){("c"==a.t?B.injectCss:B.injectJs)(a.s,0,a.a,a.x,a.e,1)},0):(a(),h()):q=0}function i(a,c,d,e,f,i,j){function k(b){if(!o&&g(l.readyState)&&(u.r=o=1,!q&&h(),l.onload=l.onreadystatechange=null,b)){"img"!=a&&m(function(){t.removeChild(l)},50);for(var d in y[c])y[c].hasOwnProperty(d)&&y[c][d].onload()}}var j=j||B.errorTimeout,l=b.createElement(a),o=0,r=0,u={t:d,s:c,e:f,a:i,x:j};1===y[c]&&(r=1,y[c]=[]),"object"==a?l.data=c:(l.src=c,l.type=a),l.width=l.height="0",l.onerror=l.onload=l.onreadystatechange=function(){k.call(this,r)},p.splice(e,0,u),"img"!=a&&(r||2===y[c]?(t.insertBefore(l,s?null:n),m(k,j)):y[c].push(l))}function j(a,b,c,d,f){return q=0,b=b||"j",e(a)?i("c"==b?v:u,a,b,this.i++,c,d,f):(p.splice(this.i++,0,a),1==p.length&&h()),this}function k(){var a=B;return a.loader={load:j,i:0},a}var l=b.documentElement,m=a.setTimeout,n=b.getElementsByTagName("script")[0],o={}.toString,p=[],q=0,r="MozAppearance"in l.style,s=r&&!!b.createRange().compareNode,t=s?l:n.parentNode,l=a.opera&&"[object Opera]"==o.call(a.opera),l=!!b.attachEvent&&!l,u=r?"object":l?"script":"img",v=l?"script":u,w=Array.isArray||function(a){return"[object Array]"==o.call(a)},x=[],y={},z={timeout:function(a,b){return b.length&&(a.timeout=b[0]),a}},A,B;B=function(a){function b(a){var a=a.split("!"),b=x.length,c=a.pop(),d=a.length,c={url:c,origUrl:c,prefixes:a},e,f,g;for(f=0;f<d;f++)g=a[f].split("="),(e=z[g.shift()])&&(c=e(c,g));for(f=0;f<b;f++)c=x[f](c);return c}function g(a,e,f,g,h){var i=b(a),j=i.autoCallback;i.url.split(".").pop().split("?").shift(),i.bypass||(e&&(e=d(e)?e:e[a]||e[g]||e[a.split("/").pop().split("?")[0]]),i.instead?i.instead(a,e,f,g,h):(y[i.url]?i.noexec=!0:y[i.url]=1,f.load(i.url,i.forceCSS||!i.forceJS&&"css"==i.url.split(".").pop().split("?").shift()?"c":c,i.noexec,i.attrs,i.timeout),(d(e)||d(j))&&f.load(function(){k(),e&&e(i.origUrl,h,g),j&&j(i.origUrl,h,g),y[i.url]=2})))}function h(a,b){function c(a,c){if(a){if(e(a))c||(j=function(){var a=[].slice.call(arguments);k.apply(this,a),l()}),g(a,j,b,0,h);else if(Object(a)===a)for(n in m=function(){var b=0,c;for(c in a)a.hasOwnProperty(c)&&b++;return b}(),a)a.hasOwnProperty(n)&&(!c&&!--m&&(d(j)?j=function(){var a=[].slice.call(arguments);k.apply(this,a),l()}:j[n]=function(a){return function(){var b=[].slice.call(arguments);a&&a.apply(this,b),l()}}(k[n])),g(a[n],j,b,n,h))}else!c&&l()}var h=!!a.test,i=a.load||a.both,j=a.callback||f,k=j,l=a.complete||f,m,n;c(h?a.yep:a.nope,!!i),i&&c(i)}var i,j,l=this.yepnope.loader;if(e(a))g(a,0,l,0);else if(w(a))for(i=0;i (function(w,d,s,l,i){w[l]=w[l]||[];w[l].push({'gtm.start':new Date().getTime(),event:'gtm.js'});var f=d.getElementsByTagName(s)[0];var j=d.createElement(s);var dl=l!='dataLayer'?'&l='+l:'';j.src='//www.googletagmanager.com/gtm.js?id='+i+dl;j.type='text/javascript';j.async=true;f.parentNode.insertBefore(j,f);})(window,document,'script','dataLayer','GTM-M677548'); Skip to main content Home About Submit ALERTS / RSS Search for this keyword Advanced Search New Results The evolutionarily conserved PhLP3 is essential for sperm development in Drosophila melanogaster Christopher Petit , Elizabeth Kojak , View ORCID Profile Samantha Webster , Michela Marra , View ORCID Profile Brendan Sweeney , Claire Chaikin , Jennifer C. Jemc , View ORCID Profile Stefan M. Kanzok doi: https://doi.org/10.1101/2024.06.24.600488 Christopher Petit 1 Department of Biology, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site Elizabeth Kojak 1 Department of Biology, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site Samantha Webster 1 Department of Biology, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Samantha Webster Michela Marra 3 Department of Microbiology and Immunology, Stritch School of Medicine, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site Brendan Sweeney 1 Department of Biology, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Brendan Sweeney Claire Chaikin 1 Department of Biology, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site Jennifer C. Jemc 1 Department of Biology, Loyola University Chicago , Chicago, Illinois, United States of America 2 Bioinformatics Program, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site For correspondence: skanzok{at}luc.edu jmierisch{at}luc.edu Stefan M. Kanzok 1 Department of Biology, Loyola University Chicago , Chicago, Illinois, United States of America 2 Bioinformatics Program, Loyola University Chicago , Chicago, Illinois, United States of America Find this author on Google Scholar Find this author on PubMed Search for this author on this site ORCID record for Stefan M. Kanzok For correspondence: skanzok{at}luc.edu jmierisch{at}luc.edu Abstract Full Text Info/History Metrics Preview PDF Abstract Phosducin-like proteins (PhLP) are thioredoxin domain-containing proteins that are highly-conserved across unicellular and multicellular organisms. PhLP family proteins are hypothesized to function as co-chaperones in the folding of cytoskeletal proteins. Here, we present the initial molecular, biochemical, and functional characterization of CG4511 as Drosophila melanogaster PhLP3 . We cloned the gene into a bacterial expression vector and produced enzymatically active recombinant PhLP3, which showed similar kinetics to previously characterized orthologues. A fly strain homozygous for a P-element insertion in the 5’ UTR of the PhLP3 gene exhibited significant downregulation of PhLP3 expression. We found these male flies to be sterile. Microscopic analysis revealed altered testes morphology and impairment of spermiogenesis, leading to a lack of mature sperm. Among the most significant observations was the lack of actin cones during sperm maturation. Excision of the P-element insertion in PhLP3 restored male fertility, spermiogenesis, and seminal vesicle size. Given the high level of conservation of PhLP3, our data suggests PhLP3 may be an important regulator of sperm development across species. Introduction The phosducin-like family of proteins (PhLP/PDCL/Plp) consists of small cytoplasmic proteins that are evolutionarily conserved among eukaryotes from yeast to humans [ 1 – 4 ] ( Fig 1A-B ). Their hypothesized cellular functions range from regulating trimeric G-proteins to regulating actin and tubulin-based cytoskeletal structures to chaperone-assisted protein folding [ 2 , 5 , 6 ]. The PhLP family is organized into three subgroups based primarily on sequence similarities and proposed cellular functions [ 7 ]. The PhLP1 group is involved in the folding, stabilizing, and regulating the beta-gamma dimers of trimeric G-proteins (reviewed in [ 8 ]). Members of the PhLP2 and PhLP3 groups are hypothesized to function as co-chaperones in conjunction with the Chaperonin-containing tailless complex polypeptide 1 (CCT), also referred to as the tailless complex polypeptide 1 ring complex (TRiC). The CCT is an essential molecular cytosolic chaperonin in eukaryotes responsible for folding cytosolic proteins, including α- and β-tubulin and actin [ 6 , 9 , 10 ]. Download figure Open in new tab Fig 1. Sequence and structure conservation of PhLP3 proteins. (A) Clustal Omega alignment of published sequences [ 11 ]. Similar amino acids are highlighted in gray. Secondary structure predictions using JPred4 [ 12 ] are shown above the sequences with alpha helices in red and beta strands in yellow. The blue box indicates the thioredoxin domain. The conserved putative redox-active cysteine is highlighted in yellow. At= Arabidopsis thaliana , Pb= Plasmodium berghei [ 4 ], Ce= Caenorhabditis elegans [ 2 ], Dm= Drosophila melanogaster (this paper, [ 2 ]), Dr= Danio rerio [ 13 ], Hs= Homo sapiens [ 4 , 6 ], Rn= Rattus norwegicus [ 14 ]. Similar amino acids are highlighted in gray. NCBI reference sequences: AtPLP3A AEE78732, PbPhLP3 SCO61590, CePhLP3 NP_498410, DmPhLP3 AAL28410, DrTXNDC9 AAI65424, HsTXNDC9 NP_005774, RnTXNDC9 NP_742051. (B) Phylogenetic tree of the aligned sequences. Alignment and phylogenetic tree were generated using Clustal Omega tools [ 11 ]. (C) Hypothetical structure of PhLP3 was generated using SWISS-MODEL and template PDB 7nvm: entity 11 [ 15 , 16 ]. The model is colored by secondary structure (alpha helices in red and beta strands in yellow); the putative redox-active cysteine 95 is indicated. Structure rendering was prepared using PyMOL (Pymol.org, The PyMOL Molecular Graphics System, Version 1.2r3pre, Schrödinger, LLC). PhLPs have been shown to be essential for unicellular organisms, including yeast Saccharomyces cerevisiase , the protozoan parasite Plasmodium berghei, and the amoeba Dictyostelium discoideum [ 4 , 7 , 10 ]. RNAi-mediated knockdown of PhLP in multicellular organisms, such as the nematode Caenorhabditis elegans, alters cytoskeletal-dependent mechanisms, including nuclear division and cytokinesis, and renders embryos unable to complete the first division [ 2 ]. Similar observations were reported in the plant Arabidopsis thaliana, where simultaneous knockdown of PLP3A and PLP3B disrupts microtubule-dependent oriented cell expansion in the meristem [ 17 ]. PhLP3 silencing or overexpression in Chinese Hamster Ovary (CHO) cells leads to disorganization of microtubules as well as actin-based cytoskeletal structures [ 18 ]. Several recent cryo-electron microscopy (CryoEM) studies on the yeast and human CCTs show that PhLP, together with tubulin or actin, localizes to the central chamber of the chaperonin ring complex [ 19 – 21 ]. Taken together, these data suggest that the function of PhLP3 is linked to the regulation and dynamics of the cytoskeleton. All PhLPs exhibiting molecular weights between 25 and 30 kD appear to share the same overall structural organization, consisting of an N-terminal helix domain, which ranges from 150 AA in PhLP1 to 59 AA in PhLP3, a central thioredoxin (Trx) domain comprised of 130 AA, and an unstructured C-terminal tail of varying length ( Fig 1 ) [ 1 ]. Within the structure, the Trx-domain exhibits the highest degree of sequence conservation [ 7 ]; for example, the protozoan organism P. berghei and its human homolog TXNDC9 share 49% AA sequence identity between their respective Trx-domains ( Fig 1 ) [ 4 ]. Furthermore, our group recently demonstrated that P. berghei PhLP3 and human TXNDC9 exhibit 1-cysteine-based redox activity [ 4 ]. These new insights into the molecular mechanism of this highly conserved protein could significantly advance our understanding of the biological role(s) of this conserved family of proteins. Here we utilized Drosophila melanogaster as a model system to further explore the function of PhLPs at a cellular and molecular level. Flybase currently lists three genes in the D. melanogaster genome as potentially belonging to the PhLP family, namely CG4511 , CG7650 , and viral inhibitor of apoptosis-associated factor ( viaf / CG18593 ) (S1 Fig) [ 22 ]. None of these genes have been experimentally characterized to date. Previous studies that included the D. melanogaster CG4511 gene in multiple sequence alignments show that it aligns with the PhLP3 group [ 2 , 7 ]. Therefore, we analyzed the conservation and predicted structure of the protein encoded by CG4511 as a potential PhLP3 family member in D. melanogaster . High-throughput expression data and single-cell RNA-sequencing (scRNA) data show high CG4511 expression in the testis, specifically in germline cells (S2 Fig) [ 23 – 25 ]. This prompted us to examine its cellular function in the context of spermatogenesis. Spermatogenesis in D. melanogaster is a stepwise process in which germline stem cells (GSCs) divide to give rise to differentiating daughter cells, known as gonialblasts. Gonialblasts undergo four rounds of mitosis followed by meiosis ( Fig 2 ; reviewed in [ 26 ]). During the post-meiotic stages of sperm development, known as spermiogenesis, spermatids extend axonemes, and nuclei begin to elongate, progressing through the leaf and canoe stages to a final needle-like morphology ( Fig 2 ; [ 27 ]). Microtubules are critical for axoneme formation and function, and for nuclear elongation, as components of the dense complex [ 27 ]. Actin has also been observed in the dense complexes, as well as the individualization complexes that promote sperm individualization [ 28 , 29 ]. During individualization, superfluous organelles and cytoplasm are stripped away, while each sperm cell is surrounded by its own plasma membrane [ 28 ]. Mature, individualized sperm coil and move into the seminal vesicle, where they are stored ( Fig 2 ; [ 30 ]). Download figure Open in new tab Fig 2. D. melanogaster sperm development. (A) Stages of D. melanogaster spermatogenesis. Germline stem cells (GSCs; light blue) and cyst stem cells (CySCs; light green) are regulated and maintained by hub cells (magenta) at the apical tip. GSCs and CySCs divide asymmetrically to give rise to differentiating daughter cells, known as gonialblasts (dark blue) and somatic cyst cells (dark green), respectively. Gonialblasts undergo four mitotic divisions with incomplete cytokinesis, yielding cysts of 16 interconnected spermatogonia. Following mitosis, spermatogonia mature into spermatocytes, which grow and proceed through meiosis with incomplete cytokinesis to form 64 interconnected, haploid, round spermatids encased within a syncytial cyst. The post-meiotic maturation of spermatids is referred to as spermiogenesis. During this stage, spermatids extend axonemes, elongate nuclei, and are individualized by actin-based individualization complexes, also known as actin cones or investment cones (yellow triangles). Mature sperm coil and move into the seminal vesicle [ 26 ]. (B) Stages of nuclear elongation during spermiogenesis. Following meiosis, spermatid nuclei are round and begin to elongate, passing through the leaf and canoe stage to the final needle-like stage [ 27 ]. N: nucleus, BB: basal body; ca: centriolar adjunct, and Ax: axoneme (axoneme not to scale). We have identified the D. melanogaster homolog of PhLP3 as the protein encoded by the previously uncharacterized CG4511 gene. Sequence alignment and structural modeling reveal a high level of conservation, which includes a critical cysteine in the active site of the thioredoxin domain. We demonstrated that D. melanogaster PhLP3 is redox-active, similar to other PhLP3 family members. Expression of PhLP3 in the testes led us to explore its role in sperm development. We have shown that PhLP3 is required for spermiogenesis in D. melanogaster. Males homozygous for a P-element insertion in the 5’ UTR of PhLP3 exhibited decreased PhLP3 expression and infertility. In PhLP3 mutants, spermatid nuclei were scattered throughout the syncytium and lacked actin-based individualization cones. Furthermore, needle-like nuclei indicative of mature sperm were absent, and seminal vesicle size was severely reduced. Germ-cell specific knockdown of PhLP3 yielded phenotypes similar to those observed in mutants. Given the importance of microtubules and actin at multiple stages of sperm development and the proposed role of PhLP3 family proteins in regulating the cytoskeleton, the testis is an ideal tissue to explore the cellular role of PhLP3 proteins in vivo . Results PhLP3 structure and redox activity are conserved across species The D. melanogaster PhLP3 protein is encoded by CG4511, a single copy gene located on the right arm of chromosome 3 in the D. melanogaster genome and spanning a region of 1,912 bp. The gene is organized into two coding exons flanking a 199 bp intron. A non-coding exon situated 111 bp upstream of the start codon, referred to as exon 2A and exon 2B, gives rise to the two PhLP3 splice variants CG4511-RA and CG4511-RB , which differ in their respective 5’ UTRs but not in their coding regions ( Fig 3 ). The PhLP3 coding sequence (CDS) spans 651 bp and codes for a 216 AA protein with an MW of 25.11 kD. We took advantage of the recently resolved structure of human PhLP2A [ 16 , 19 , 31 ] to generate a hypothetical model of D. melanogaster PhLP3 ( Fig 4 ). Our structural analysis shows the characteristic PhLP organization of an N-terminal helix domain, the central Trx-domain, and the unstructured N-terminal tail ( Fig 4 ; S1 Fig) [ 1 ]. The highly conserved globular Trx-domain exhibits three peripheral alpha helices surrounding a four-strand twisted beta-sheet in a structural organization characteristic of the thioredoxin fold [ 32 ]. D. melanogaster PhLP3 shares significant amino acid sequence identities with homologous proteins in a wide range of eukaryotic organisms. Most notably, it exhibits 69% and 63% AA sequence identity with the homologous TXNDC9 (thioredoxin-domain containing 9) proteins from zebrafish and human, respectively ( Fig 1 ). Download figure Open in new tab Fig 3. Organization of the PhLP3 gene. The gene is located on chromosome 3 in the D. melanogaster genome (10854501 – 10856412) (FlyBase: FB2023_06, released December 12, 2023). The transcription start sites (TSS) are indicated. Intron 1 is located in the 5’ UTR. Exon 2 contains a splice site resulting in two transcripts, RA and RB, containing exon 2A and exon 2B, respectively. The transcripts differ only in their 5’ UTR regions and translate into identical proteins. Green boxes indicate coding regions of exons, while light blue boxes indicate untranslated regions. Protein domains are indicated according to secondary structure prediction JPred [ 12 ] as well as structural alignment of human PhLP2A using SWISS-MODEL [ 15 ]. Primers used for RT-qPCR are indicated in purple and pink. Download figure Open in new tab Fig 4. Sequence alignment and structure superposition of D. melanogaster PhLP3 with human PhLP2A. (A) The PhLP3 structure is shown in red and yellow, and hPhLP2A (PDB 7nvm: entity 11; [ 16 ]) in blue. hPhLP2A was crystallized with actin trapped in the lumen of the chaperonin multicomplex CCT. The pairwise sequence alignment was generated using Clustal Omega [ 11 ]. Identical amino acids are shown in gray boxes, and the conserved cysteine is highlighted in yellow. The green box frames the Trx-domain. NCBI reference sequences: hPhLP2A NP_076970, DmPhLP3 AAL28410. (B) The superposition model was rotated by 90° to show the overlaid positions of the putative redox-active cysteines C95 (PhLP3) and C127 (hPhLP2A). The images were generated using PyMOL (Pymol.org, The PyMOL Molecular Graphics System, Version 1.2r3pre, Schrödinger, LLC). We previously demonstrated that human TXNDC9 and P. berghei PhLP3 exhibit redox activity with the thioredoxin system [ 4 ]. The sequence alignment and structure model show that the redox-active cysteine seems to be conserved in PhLP3 homologs across diverse species, including CYS93 in D. melanogaster PhLP3 ( Fig 1A , 4). To determine whether recombinant PhLP3 is redox-active, we cloned the CDS from D. melanogaste r cDNA into a bacterial expression vector. We purified recombinant PhLP3 using a Ni-NTA-based column approach under denaturing conditions as described previously [ 4 ] ( Fig 5A ). SDS gel electrophoresis showed a single band at ∼ 25 kD, the expected size of recombinant His-tagged PhLP3 (∼ 25 kD; Fig 5A ). Using this method, we routinely produced >10 mg of purified recombinant PhLP3 per liter of bacterial culture. Download figure Open in new tab Fig 5. Purification and enzyme activity of PhLP3. (A) SDS gel following protein purification of recombinant His-tagged PhLP3. Washes (W) and elutions with increasing imidazole concentrations are indicated. (B) Principal setup of an in vitro thioredoxin reduction assay. The oxidation of NADPH to NADP is monitored at 340 nm. Electrons flow from NADPH to Thioredoxin reductase (TrxR) to thioredoxin (Trx) and then to PhLP3, which will be reduced in the process. (C) Michaelis Menten diagram showing activity of PhLP3 with increasing thioredoxin concentrations. The indicated K m and V max values were determined using curve fitting. The values were verified by generating a Lineweaver Burk plot (inset). Based on our recent findings that P. berghei PhLP3 and human TXNDC9 exhibit redox activity and have a conserved cysteine at position 95 ( Fig 1A ), we hypothesized that D. melanogaster PhLP3 will also be redox-active. To test this, we conducted NADPH reduction assays as outlined in Fig 5B and as described previously [ 4 ]. Briefly, electron donor NADPH was added to a mix of recombinant P. berghei thioredoxin reductase (PbTrxR, PbANKA_0824700, [ 33 ]) and D. melanogaster thioredoxin (DmTrx1, CG4193, [ 34 ]). The resulting reduction reaction was allowed to come to completion before purified recombinant PhLP3 was added. We observed renewed oxidation of NADPH, indicating the flow of electrons from the Trx-system to PhLP3 and confirming that D. melanogaster PhLP3 is redox-active ( Fig 5B ). We determined that the reaction between Trx1 and PhLP3 follows Michaelis Menten kinetics, exhibiting a K m of 2.72 μM and a V max of 5.4 μM/min ( Fig 5C ). These values compare well with those of previously tested PhLP3 proteins, P. berghei PhLP3 and human TXNDC9, and support our hypothesis that redox activity is conserved in PhLPs between evolutionarily distant species and may be necessary for its biological function [ 4 ]. PhLP3 is required for male fertility The high expression of PhLP3 in the germ cells of D. melanogaster testes, as indicated by publicly available RNA-Seq and scRNA-Seq data, suggests a role for the gene in spermatogenesis (S2 Fig) [ 23 – 25 ]. To explore the expression of PhLP3 in reproductive tissue, we performed in situ hybridization combined with immunostaining on dissected testes. Our data indicate that the gene is expressed in germ cells from the spermatogonia stage until the early spermatid stage but is no longer observed in late stage spermatids in the distal end of the testis ( Fig 6A ). Download figure Open in new tab Fig 6. Expression of PhLP3 in the testes. (A-B) Fluorescent in situ hybridization for PhLP3. PhLP3 probe (cyan) and anti-Vasa to label germ cells (magenta). Scale bar is 100 µm. (A) PhLP3 +/+ testes exhibit expression in germ cells from spermatogonia through early spermatid stages (n=59). (B) RT-qPCR shows downregulation of PhLP3 expression in testes from males homozygous for the P-element insertion in the 5’ UTR of PhLP3 (-/-) , compared to wild-type (+/+) levels. Excision of the P-element (ΔP/ΔP) partially rescues PhLP3 expression. (C) PhLP3 -/- testes exhibit a loss of expression throughout the testis (n=36). Given the expression of PhLP3 in the germline until early spermatid stages, we next asked whether PhLP3 is required to produce mature sperm. We obtained a fly strain ( PhLP3 EY13373 ) carrying a P-element insertion in the 5’ UTR of Phlp3 , located 78 bp upstream of the start codon ( Fig 3 ) [ 35 ]. The location of the P-element in the 5’ UTR of PhLP3 was confirmed by inverse PCR and sequencing (S3 Fig). Homozygous PhLP3 EY13373/EY13373 male flies and control male flies ( w 1118 ) were mated to virgin female control flies ( w 1118 ). Surprisingly, each PhLP3 mutant cross failed to yield progeny over six independent crosses ( Fig 7 ). In contrast, the control crosses yielded an average of 108 progeny over six independent crosses ( Fig. 7 ). Based on these results, it appears that PhLP3 mutant male flies are sterile, which suggests that PhLP3 is required for male fertility. Download figure Open in new tab Fig 7. Fertility tests. Control males ( w 1118 ) , PhLP3 -/- ( PhLP3 EY13373/EY13373 ) males or P element excision males ( PhLP3 ΔP/ΔP ) were mated to w 1118 virgin females to assess fertility. The average number of progeny per cross was counted. Individual measurements for each cross are shown with the average and standard deviation indicated. **** indicates p<0.0001 and *** indicates p<0.001 based on ordinary one-way ANOVA; ns= not significant. We hypothesized that the P-element insertion in the 5’ UTR of PhLP3 causes downregulation of PhLP3 expression and links to the observed sterile phenotype. To test this, we performed real-time quantitative PCR (RT-qPCR) analysis on total RNA extracts from testes of PhLP3 mutant and control flies. In three independent experiments, we show that PhLP3 expression in mutant testes was downregulated by 94% when compared to control testes ( Fig 6B ). Similarly, fluorescent in situ hybridization of homozygous PhLP3 EY13373/EY13373 mutant testes exhibited only weak fluorescence for the PhLP3 probe, confirming our RT-qPCR results and the specificity of our probe ( Fig 6C ). Given the significant reduction in PhLP3 expression in this mutant strain, we will refer to these mutants as PhLP3 -/- for the remainder of the paper. These data strongly support our hypothesis that PhLP3 is required for male fertility in D. melanogaster . PhLP3 downregulation results in defects in sperm development Based on the infertility observed in PhLP3 -/- mutants, we determined whether mature sperm had been produced. We visually examined the testes and seminal vesicles of 1-3 day-old control and mutant male flies using DAPI staining and fluorescence microscopy ( Fig 8 and 9 ). In the control testes, we observed the characteristic DAPI clusters of elongating sperm nuclei aligned in a syncytium near the distal end of the testes, giving way to a large seminal vesicle filled with mature sperm ( Fig 8A-A ”; Fig 9A ). In contrast, PhLP3 -/- mutants lacked the aligned DAPI-stained nuclear clusters ( Fig 8B-B ’). Instead, the nuclei appeared scattered and failed to progress from the canoe stage to the needle-like nuclei, which would indicate maturing sperm ( Fig 9B ). Furthermore, compared to the controls, the size of the seminal vesicles in the mutant testes was diminished by 32%, and seminal vesicles lacked mature sperm ( Fig 8B ”, D). Download figure Open in new tab Fig 8. Mutation of PhLP3 causes arrest of spermiogenesis. (A-A’) Control PhLP3 +/+ testes have DAPI clusters and actin-based individualization complexes (n=40). Nuclei stained with DAPI (cyan) and actin-based individualization complexes stained with phalloidin (magenta). Arrows indicate DAPI clusters with individualization complexes. (A”) Seminal vesicles are large with mature sperm (n=21). Nuclei stained with DAPI. (B-B’) PhLP3 -/- testes have dispersed DAPI clusters, less elongated nuclei, and no actin-based individualization complexes (n=38). Nuclei stained with DAPI (cyan) and actin-based individualization complexes stained with phalloidin (magenta). (B”) Seminal vesicles are smaller and lack sperm (n=15). Nuclei stained with DAPI. (C) Excision of the P element in PhLP3 ( PhLP3 ΔP/ΔP ) rescues the mutant phenotype. (C-C’) Testis contain DAPI clusters and individualization complexes (n=23). Nuclei stained with DAPI (cyan) and actin-based individualization complexes stained with phalloidin (magenta). Arrows indicate DAPI clusters with individualization complexes. (C”) Seminal vesicles contain mature sperm (n=19). Nuclei stained with DAPI. (D) Cross section area of the seminal vesicle (n=10 for each genotype). Individual measurements are shown with the average and standard deviation indicated. **** indicates p<0.0001 and *** indicates p<0.001 based on ordinary one-way ANOVA; ns= not significant. Scale bars are 100 µM. Download figure Open in new tab Fig 9. Morphology of spermatids in PhLP3 mutants. (A) Control PhLP3 +/+ testes have clusters of spermatid nuclei undergoing multiple stages of spermiogenesis, as indicated by DAPI staining. (n=40). (B) PhLP3 -/- testes have dispersed spermatid nuclei at various stages of elongation but lack needle-like nuclei, based on DAPI staining (n=37). Arrowheads label round spermatids. Open arrows label leaf stage nuclei. Dashed arrows label canoe stage nuclei. Solid arrows label needle-like nuclei. Scale bars are 10 µM. Images are maximum intensity Z projections. Considering the absence of mature sperm in the seminal vesicles, we hypothesized that spermatids in PhLP3 -/- mutants are unable to initiate the process of individualization. Individualization of spermatids by actin-based sperm individualization complexes is an essential process that functions to remove excess organelles and cytoplasm and to encapsulate each spermatid with its own plasma membrane. To determine if individualization complexes could form, we used phalloidin staining to detect the presence of the characteristic actin cones. While control testes exhibited clusters of actin cones, typical of individualization complexes in the distal testes, PhLP3 -/- mutants completely lacked actin cones, suggesting that spermatids failed to assemble individualization complexes ( Fig 8A-A ’, B-B’). This data suggests that PhLP3 -/- mutant sperm development is arrested during the canoe stage of spermiogenesis, failing to reach the needle-like stage and progress through individualization. As a result, seminal vesicles are devoid of mature sperm and smaller in size. Excision of P-element in PhLP3 restores male fertility To confirm the specificity of the mutant phenotype observed in the P-element insertion in PhLP3 , we excised the P-element from the PhLP3 gene to reconstitute the 5’ UTR, restore PhLP3 expression, and rescue male fly fertility. We confirmed the successful and precise excision of the P-element by sequencing and refer to the resulting strain as PhLP3 ΔP / ΔP (S3 Fig). We first tested the fertility of PhLP3 ΔP / ΔP male flies by mating them to control virgin females. An average of 135 PhLP3 ΔP / ΔP progeny were produced over seven independent fertility crosses, compared to an average of 108 progeny for control crosses ( Fig 7 ). This data confirms that the P-element excision restored fertility to control levels and supports the hypothesis that PhLP3 is essential for male fertility. To determine whether gene expression was also restored, we performed RT-qPCR on total RNA from dissected PhLP3 ΔP / ΔP and control testes. Remarkably, our results from five independent experiments show that PhLP3 expression in the PhLP3 ΔP / ΔP was restored to only 33% of control expression levels ( Fig 6B ). This was surprising, given that fertility was completely restored. Furthermore, visual analysis of PhLP3 ΔP / ΔP testes revealed that sperm production was reestablished to levels comparable to control testes ( Fig 8C-C ”). DAPI-stained, aligned clusters of elongating spermatid nuclei in the PhLP3 ΔP / ΔP testes are evident, as are the actin cones of the individualization complexes ( Fig 8C-C ’). Seminal vesicles were filled with mature sperm, and the seminal vesicle area was 91.4% of the size of the control testes ( Fig 8C ”, D). Sperm maturation appeared to proceed normally in PhLP3 ΔP / ΔP testes despite only partially restored PhLP3 gene expression ( Fig 8C-C ”). Our results confirmed that the P-element insertion in the 5’ UTR of the PhLP3 gene prevents effective gene transcription. Despite fully restored fertility, the excision of the P-element only restores transcription activity levels to 33%, introducing the possibility that other factors may be involved in the observed phenotype. To affirm that the downregulation of PhLP3 specifically causes the male sterile phenotype, we utilized RNA interference (RNAi) as an alternative approach to reduce PhLP3 levels under the control of the Gal4/UAS system. We used bam- Gal4 to drive the expression of a UAS- PhLP3 -RNAi in the germline [ 36 , 37 ]. The efficacy of this RNAi approach was tested by RT-qPCR and showed a 77% knockdown in PhLP3 expression in bam -Gal4> PhLP3-RNAi testes compared to testes of the bam -Gal4 control ( Fig 10A ). We tested the fertility of these flies by mating bam -Gal4 control males or bam -Gal4> PhLP3-RNAi males to control virgin females. We scored the number of progeny and confirmed that the fertility was significantly reduced in PhLP3 -RNAi flies, with an average of 3 progeny eclosing per cross. Control crosses yielded an average of 135 progeny per cross, a similar number of progeny to control crosses described earlier ( Fig 10B ). Next, we examined the effect of PhLP3 RNAi knockdown on spermatogenesis by DAPI and phalloidin staining and confocal microscopy. The bam -Gal4 control testes exhibited spermatids that clustered, elongated, and individualized ( Fig 10C-C ”). In contrast, while bam -Gal4> PhLP3- RNAi testes possessed spermatids, they failed to elongate fully and appeared scattered throughout the syncytium they developed within, similar to our observation of the P-element containing PhLP -/- flies ( Fig 10D-D ”). Using phalloidin staining, we observed clustered and aligned actin cones in individualization complexes in bam -Gal4 control testes, but actin cones appeared scattered in PhLP3-RNAi testes ( Fig 10C-D ”). Consistent with the reduced fertility of PhLP3- RNAi flies compared to controls, seminal vesicles lack the mature sperm with needle-like nuclei observed in controls, demonstrating a failure to complete sperm maturation ( Fig 10C ’’’, 10D’’’). Our results provide strong evidence for the specificity of the phenotype to the PhLP3 -/- mutant and demonstrate an essential requirement for PhLP3 in D. melanogaster spermiogenesis and male fertility. Download figure Open in new tab Fig 10. Effects of PhLP3 RNAi on mature sperm production. (A) RT-qPCR demonstrates a 77% reduction in PhLP3 expression by RNA-interference (RNAi) in comparison to that of control ( bam-Gal4 ) samples. (B) Fertility cross data showing the number of progeny resulting from four virgin female w 1118 flies crossed with three male bam-Gal4 control flies or three male bam-Gal4>PhLP3-RNAi flies. Individual measurements for each cross are shown with the average and standard deviation indicated. **** indicates p<0.0001 based on Welch’s t-test. (C-C’’’) bam-Gal4 control testis (n=47). (C) Whole testis with nuclear DAPI stain. White arrows indicate clusters of elongating spermatid nuclei. (C’) Control testis stained with phalloidin to label actin cones, which are indicative of individualizing sperm. White arrows indicate actin-based individualization complexes. (C”) Clusters of aligned, elongating spermatid nuclei in a control testis. Arrows point out clusters. (C’”) Seminal vesicle of a control testis filled with mature sperm (n=24). (D-D’’’) bam-Gal4>PhLP3 - RNAi testis (n=29). (D) Whole testis with nuclear DAPI stain. There are few if any DAPI clusters compared to controls. (D’) bam-Gal4>PhLP3 - RNAi testis with the presence of a few deformed, scattered actin cones. White arrowheads indicate scattered actin-based individualization complexes. (D”) bam-Gal4>PhLP3 - RNAi testis have scattered, elongating spermatid nuclei. (D’’’) bam-Gal4>PhLP3 - RNAi seminal vesicles are reduced in size and lack mature sperm (n=19). Scale bar is 100 µM in C, C’, C’’’ and D, D’, D’’’. Scale bar is 50 µM in C’’ and D’’. Materials and Methods Ethics statement This study is exempted from institutional or national regulations on animal research, as it involves invertebrates that do not require such permission. Fly Strains The following fly strains were utilized in these studies: w 1118 ; Dr/TM6B, Tb, Hu, Deformed (Dfd)-Yellow Fluorescent Protein (YFP) [ 38 ]; PhLP3 EY13373/+ /TM3, Sb or PhLP3 EY13373/EY13373 (Bloomington Drosophila Stock Center (BDSC #21414; [ 35 ]); w*; Dr 1 /TMS, P{ry [+7.2] Δ2-3}99B (BDSC #1610); bam-Gal4 (BDSC #80579; [ 36 ]); and UAS-PhLP3-RNAi (Vienna Drosophila Stock Center #100784; [ 37 ]). Flies were raised at 25°C on standard Bloomington Drosophila cornmeal medium. The strain in which the P-element was precisely excised from the PhLP3 gene was generated as follows: virgin females of the genotype PhLP3 EY13373 /TM3, Sb were mated to males of the genotype w*; Dr 1 /TMS, P{ry [+7.2] Δ2-3}99B . Male progeny of the genotype PhLP3 EY13373 / TMS, P{ry [+7.2] Δ2-3}99B were collected and mated to Dr/TM6B, Tb, Hu, Dfd-YFP virgin females. Single white eyed progeny of the potential genotype PhLP3 ΔP / TM6B, Tb, Hu, Dfd-YFP were selected and mated to Dr/ TM6B, Tb, Hu, Dfd-YFP flies of the opposite sex to establish stocks. Stocks were screened by PCR and sequencing as described below. PCR and Sequencing To isolate genomic DNA for inverse PCR (iPCR) of the P element insertion, fifteen 1-3 day old PhLP3 EY1337/ EY13373 or control (w 1118 ) flies were collected and homogenized in 400 µl Buffer A (100mM Tris pH 7.5, 100 mM EDTA, 100 mM NaCl, 0.5% SDS), followed by a 30 min incubation at 65°C. 800 µl LiCl/KAc (2.28 M LiCl, 1.43 M KAc) was added and samples were incubated on ice for 10 min. Samples were spun for 15 min at 12,000 rpm at room temp. 1 mL of supernatant was transferred to a new tube and 600 µl of isopropanol was added, and tube was inverted to mix. Samples were spun for 20 min at 12,000 rpm at room temp. Supernatant was discarded and the samples were spun down quickly to remove additional supernatant. The pellet was washed with 500 µl cold 70% ethanol and spun down for 10 min at 12,000 rpm at room temp. Supernatant was discarded and the samples were spun down quickly to remove additional supernatant. Pellet was air dried and resuspended in 75 µl 1x TE (10mM Tris pH 7.5, 1 mM EDTA). Genomic DNA was then digested with HpaII at 37°C for 2.5 hours, followed by a 20 min heat inactivation at 65°C. NEB T4 DNA Ligase was then utilized in a ligation reaction to form a plasmid library from our genomic digest, and an inverse PCR was performed to amplify the 5’ and end of the P{EPgy2} P-element insertion, using the Plac1 and Pwht1 primers (S1 Table) [ 35 ]. Products were sequenced, using the 5.SUP.seq1 primer by Genewiz/Azenta. For sequencing across the genomic region of control ( w 1118 ) and P element excision flies, single flies were collected and homogenized using a pipette tip filled with 50 µl of Squishing Buffer (10 mM Tris-Cl pH 8.2, 1mM EDTA, 25 mM NaCl and 200 µg/mL Proteinase K)[ 39 ]. Samples were incubated for 20 min at 37°C. Proteinase K was heat inactivated for 2 min at 95°C and DNA was stored at 4°C. The genomic region around the site of the P element insertion was amplified by PCR using the CG4511-Fwd and CG4511-Rev primers and sequenced using the same primers by Genewiz/Azenta. Fertility crosses Four w 1118 virgin females were crossed to three male flies of genotype w 1118 , PhLP3 -/- , homozygous P-element excision ( PhLP3 ΔP/ΔP ), bam-Gal4, or bamGal4>PhLP3-RNAi. Flies were mated for 7 days. Parental flies were emptied from the bottle on day 7, and progeny were collected over a period of five days (days 10-15) and scored. Statistical analysis was carried out with GraphPad Prism. Immunohistochemistry Testes from 1-3 day old males were processed as described previously in the presence of 5% NGS [ 40 ]. Following antibody staining, samples were incubated with Phalloidin conjugated to Alexafluor 555 diluted 1:40 in 1x PBS for 10 minutes, washed for 5 minutes in 1x PBS, and mounted in DAPI Fluoromount-G (Southern Biotech). Images were acquired on a Zeiss LSM880 confocal microscope and processed using Fiji [ 41 ]. The cross-section area of seminal vesicles was measured in Fiji and statistical analysis of data was carried out in GraphPad Prism. RT-qPCR Testes from 1-3 day old w 1118 , PhLP3 -/- , or PhLP3 ΔP/ΔP males were dissected in RNase-free (DEPC-treated) PBS and incubated in 1 mL RNAzol at 4°C. Total RNA was extracted following manufacturer’s instructions. Isolated RNA was treated with DNAse I (Ambion) and subsequently quantified using a Qubit RNA Assay kit (Invitrogen). RNA samples were immediately used for cDNA synthesis employing a high-capacity RNA-to-cDNA kit (Applied Biosystems) with random hexamer primers. RT-qPCR was performed on a StepOnePlus machine (Applied Biosystems) using the PowerUp SYBR Green Master Mix (Applied Biosystems). Each sample was run in triplicate and yielded highly comparable Ct values (cycle threshold). No primer dimers were detected, and amplicons exhibited optimal efficiencies. Expression data was analyzed using the StepOne Software v2.2 (Applied Biosystems) and normalized against the expression of the endogenous glyceraldehyde 3-phosphate dehydrogenase ( gapdh ) enzyme, which is an established internal standard for expression analysis in D. melanogaster [ 42 ]. Ribosomal protein L32 ( RpL32 ) was used as an additional internal positive control [ 43 ]. Primers are listed in S1 Table. Cloning, expression, and purification of recombinant PhLP3 Gene-specific primers (S1 Table) for PhLP3 (Flybase CG4511 , NCBI NP_001163585) and Trx-1 ( CG4193 , [ 34 ]) were generated according to sequence information on Flybase and NCBI, respectively [ 22 ]. PCRs were performed using the following conditions: 35 cycles of 95 °C for 30 s, 54 °C for 1 min, and 72 °C for 45 s. Following sequence verification, the PhLP3 CDS was cloned into the bacterial pQE9 expression vector (Qiagen), which introduced an 6x HIS tag at the N-terminus of the recombinant protein. The PhLP3 expression plasmid was transformed into E. coli M15 expression cells (Qiagen). Protein expression was induced (1 mM IPTG), and bacteria were harvested after a 5-hour incubation period at 37 °C. Recombinant proteins were purified under denaturing conditions (8 M urea) using Ni-NTA resin (Thermo Scientific). The purity of the recombinant proteins was assessed via SDS-PAGE. Protein concentrations were determined using the Qubit fluorometer (Invitrogen) and Bradford assay. Enzyme assays All enzymatic assays were carried out in 1 ml volume at 25°C using a Genesys6 UV-Vis spectrophotometer (Thermo Fisher). The coupled enzymatic assays were conducted as previously described [ 4 ]. Briefly, the oxidation of NADPH was followed by an absorption decrease at 340 nm. All assays were performed at RT in assay buffer containing 100 mM KH 2 PO 4 , 2 mM EDTA, pH 7.4, 200 μM NADPH (ε340 nm = 6.22 mM -1 cm -1 ), and 20 μM D. melanogaster Trx-1. Each initial reaction was started with PbTrxR [ 4 ], and the decrease in absorption at 340 nm was monitored during the linear phase. Once the reaction was complete, purified recombinant D. melanogaster PhLP3 was added, and the initial velocities and kinetic values for each reaction were determined using the VISIONlite (Thermo Fisher) software. Enzyme kinetics were calculated using global curve fit in the Enzyme Kinetics Module of Sigma Plot 12.0. Comparative modeling The hypothetical models of D. melanogaster PhLP1, 2, and 3 were generated using SWISS-MODEL [ 15 ]. The crystal structure of the human PhLP2A (PDB ID: 7nvm Park 2023; [ 19 ]) was selected as the template from the RCSB Protein Data Bank ( http://www.rcsb.org/ ). The models were visualized using the PyMOL ( Pymol.org , The PyMOL Molecular Graphics System, Version 1.2r3pre, Schrödinger, LLC). In situ hybridization Testes from w 1118 (PhLP3 +/+ ) and PhLP3 -/- males were dissected and processed for fluorescent in situ hybridization combined with immunostaining as described previously [ 44 ]. Probes were prepared by Molecular Instruments and were conjugated to AlexaFluor 488. Samples were immunostained with rat anti-Vasa (1:50; Developmental Studies Hybridoma Bank; [ 45 ]) and goat anti-rat AlexaFluor 555 (1:500) to label germ cells. Samples were imaged on a Zeiss LSM880 confocal microscope and images processed using Fiji [ 41 ]. Discussion In this study, we identified the D. melanogaster homolog of the PhLP3 group of Phosducin-like proteins, as the protein encoded by the CG4511 gene. Phosducin-like proteins (PhLPs) are members of the thioredoxin (Trx) superfamily and have been identified in eukaryotes from yeast to humans [ 2 , 7 ]. They show surprisingly high sequence conservation across species and have been organized into three subgroups based on sequence similarities: PhLP1, PhLP2, and PhLP3 [ 7 ]. Three phosducin-like genes have been identified in the genome of D. melanogaster , namely CG4511 , CG7650 , and CG18593 (S1 Fig). BLAST analysis confirmed that the protein encoded by CG4511 readily aligns with members of the PhLP3 group, some of which have been implicated in the regulation of the cytoskeleton in S. cerevisiae, C. elegans , A. thaliana, and human cell lines [ 2 , 6 , 7 , 17 , 18 ]. Of the three genes, CG4511 ( PhLP3 ) exhibits high transcription levels in the testes and ovaries (S2 Fig) [ 23 , 24 ] and was thus chosen as our primary target. The CG7650 protein aligns most closely with PhLP1 group members, some of which are involved in trimeric G-protein folding and regulation [ 5 , 8 ]. A recent CyroEM study of the human CCT complex with PhLP1 bound gave a high-resolution insight that suggests that human PhLP1 assists in the folding, stabilizing, and releasing of the G-protein beta subunit from the cavity of the CCT complex, an essential step in forming the obligate G-protein beta-gamma dimer [ 46 ]. The CG18593 protein, annotated as Viral inhibitor of apoptosis-associated factor (Viaf) in Flybase, favorably aligns with the PhLP2 group (S1 Fig). In yeast, PhLP2 (Plp2) assists in the folding and assembly of actin and tubulin subunits, respectively [ 10 ]. Recent cyroEM studies show human PhLP2A (PDCL2)-actin and PhLP2A-tubulin complexes in the cavity of the CCT chaperonin complex, further supporting the hypothesis that PhLP family members are involved in the folding and regulation of cytoskeletal proteins [ 16 , 19 ]. Notably, two recent reports implicate the mouse PhLP2 (PDCL2) in the spermiogenesis of adult male mice [ 47 , 48 ]. The most recent data on PhLPs from all groups indicate interactions with the cellular protein folding machinery, specifically CCT and Heat shock proteins [ 49 ]. The precise mechanism of how PhLPs assist in this mechanism is not yet known. D. melanogaster PhLPs share the same structural organization as other PhLPs, consisting of a central thioredoxin domain flanked by an N-terminal helix domain and a short, variable, and mostly unstructured C-terminal tail [ 1 ]. The thioredoxin domain shows the highest degree of sequence and structure conservation between different organisms with D. melanogaster PhLP3 sharing 43% sequence identity with the protozoan organism P. berghei and even 65% identity with the human homolog TXNDC9. While the N-terminal sequences may differ significantly between species, they all form or are predicted to form two to three helices, depending on the PhLP group. The PhLP1 group with a longer N-terminus contains three helices, while members of the PhLP2 and PhLP3 group seem to only form two helices. Stirling et al. demonstrated that the helix domain as well as the C-tail are required for PhLP3 to interact with the CCT complex [ 6 ]. As the helix structure is being maintained, this may reflect species-specific sequence variations, while the highly conserved thioredoxin domain may possess an equally conserved functional mechanism involved in target protein folding or stabilization within the CCT complex. Many thioredoxins and thioredoxin-like proteins exhibit redox activity, often facilitated by a pair of cysteines in a characteristic CXXC active site motif [ 32 ]. The lack of this motif in PhLPs prompted the dismissal of potential redox activity for these proteins [ 7 ]. Yet, our group recently found that P. berghei PhLP3, as well as the human TXNDC9, exhibit redox activity with the thioredoxin system and that this redox activity is facilitated by a highly conserved cysteine residue exposed at the top of helix 2 in the thioredoxin domain ( Fig 1 , 4) [ 4 ]. This cysteine is conserved in D. melanogaster PhLP3 (CYS95), and it was therefore not surprising to find that the recombinant PhLP3 described in this paper also exhibits redox activity with thioredoxin. This is significant as the thioredoxin system plays an important role in the cellular redox homeostasis of D. melanogaster [ 50 , 51 ]. Interestingly, two germline-specific thioredoxins have recently been reported in D. melanogaster , Deadhead (Dhd) and Thioredoxin T (TrxT) [ 52 ]. Both are hypothesized to play important roles in redox homeostasis in the germline of D. melanogaster . Dhd is the thioredoxin used in this report to demonstrate electron transfer from the thioredoxin system to PhLP3. Considering the high abundance of Dhd in ovaries and TrxT in the testes it is possible that PhLP3 is a specific redox target. Whether TrxT can also transfer electrons to PhLP3 remains to be determined. While the kinetics data compares very well with that of previously characterized PhLP3s it also indicates that it probably does not function as an effective antioxidant scavenger, as the catalytic activity is too weak to justify a role in the defense against reactive oxygen species (ROS) as attributed to other thioredoxin and thioredoxin-like proteins [ 4 ]. Considering the recent structural insights into the interactions of PhLP3 and PhLP2A with the CCT complex and a potential role in folding actin and tubulin [ 6 , 19 ], it is feasible to hypothesize that the redox activity of PhLP3 plays a role in the mechanism that facilitates folding and/or release of target proteins in and from the CCT complex. Members of the thioredoxin superfamily are known to be involved in redox-assisted protein folding [ 32 ]. For example, protein disulfide isomerases utilize their redox activity to assist protein folding in the endoplasmic reticulum [ 53 ]. Supporting our hypothesis is the fact that the redox-active cysteine seems to be conserved in all PhLPs, notably between PhLP3 and human PhLP2A. We are currently investigating the role of the redox active cysteine in the cellular function and possible enzymatic mechanism of PhLP3. At the cellular level, the primary defects observed in PhLP3 mutants occur in the post-meiotic maturation stages, as spermatid nuclei elongate and spermatids undergo individualization. These processes are dependent on tubulin and actin. As PhLP3 proteins in other species have been demonstrated to regulate CCT function [ 6 ], mutation of PhLP3 could affect the folding of tubulin and actin subunits, leading to sperm maturation defects. Mutations in α- and β-tubulin subunits have been demonstrated to exhibit a variety of germ cell defects, ranging from defects in meiosis, nuclear elongation and alignment, and axoneme assembly [ 54 – 60 ]. While the function of only one α-tubulin, α1-tubulin (encoded by αTub84B), has been implicated in the post-mitotic germ cells, two β-tubulins have been identified to function post-mitotically in sperm development [ 60 , 61 ]. β1-tubulin (encoded by βTub56D) is present in testis through the spermatocyte stage when it is downregulated, with only low levels being detected in the spermatids heads, while β2-tubulin (encoded by βTub85D) begins to be detected in spermatocyte stages and through the remaining stages of sperm development [ 62 ]. Mutant alleles, resulting in an imbalance in α and β tubulin levels, lead to defects in spermatogenesis. For some mutant β-tubulin alleles, the resulting defects are similar to those we have observed in PhLP3 mutants, including defects in nuclear shaping and alignment [ 61 ]. Nuclear shaping and alignment appear to depend on the establishment of the microtubule organizing center post-meiotically during the round spermatid stage. In the testis, the centriole adjunct serves at the main microtubule organizing center, and the establishment of the centriole adjunct depends on the proper docking of the tubulin-based basal body at the nuclear envelope. The centriole adjunct nucleates the perinuclear microtubules of the dense complex (analogous to the nuclear manchette in mammals) and the tail microtubules (reviewed in [ 63 ]). In mutants for the γ-Tubulin Ring Complex subunits, grip75 and grip128 , the basal body fails to dock at the nuclear envelope, and the nuclei appear misshapen and are scattered throughout the syncytium, resulting in sterility, similar to the defects observed in our PhLP3 mutants [ 64 ]. Mutation of other genes encoding proteins believed to promote attachment of the basal body to the nuclear envelope, including sperm-associated antigen 4 (spag4) and y uri gagarin (y uri ), exhibit similar nuclear scattering defects, failed individualization, and male sterility [ 65 , 66 ]. Thus, failed docking of the tubulin-based basal body appears to result in nuclear shaping and alignment defects. Others have suggested these defects arise due a failure to nucleate the perinuclear microtubules of the dense complex. The dense complex begins to form in the round spermatids in the region where the nucleus is flattened and fenestrated near the basal body [ 27 ]. This region invaginates to form a concavity filled with microtubules during nuclear elongation, while a single layer of microtubules is observed around the convex region of the nucleus [ 27 ]. These microtubules are believed to provide support for the nucleus during elongation. More recent work suggests the presence of a second microtubule organizing center at the tip of the nucleus from which some perinuclear microtubules of the dense complex may emanate [ 67 ]. Interestingly, Sas-4 mutants lack basal bodies but still form dense complexes, suggesting this second microtubule organizing center could serve as a significant site of perinuclear microtubule nucleation [ 67 ]. Mutation of PhLP3 could lead to defects in basal body docking and/or formation of the microtubule-rich dense complex, which appear to be required for nuclear elongation and alignment. As PhLP3 proteins have also been demonstrated to regulate CCT-mediated folding of actin [ 6 ], sperm maturation defects in PhLP3 mutants could also result from reduced actin levels. Mutations in yuri result in a loss of actin accumulation in the dense complex, suggesting that defects in actin folding could affect dense complex quality and nuclear elongation [ 65 ]. Live imaging of syncytial cysts reveals that actin is first observed around the nucleus during the canoe stages and later accumulates at the base of the nucleus before moving down the elongated spermatids for the process of individualization [ 28 , 29 ]. If PhLP3 regulates folding of actin subunits as part of the CCT, a lack of available subunits would result in a failure to incorporate actin into dense complexes, which may contribute to the defects in nuclear elongation and alignment. In PhLP3 mutants, we do not observe the formation of actin-based individualization complexes, which could arise from reduced actin levels or a failure to reach the individualization stage of spermiogenesis. Interestingly, mutants for mulet , which encodes the Tubulin-binding cofactor E-like (TBCEL)), exhibit scattering of nuclei and defects in individualization; however, individualization complexes still form in these mutants and persist around scattered nuclei [ 68 – 70 ]. TBCEL appears to be required for microtubule disassembly to promote individualization. Other individualization mutants described in Fabrizio 1998 have disrupted individualization complexes or complexes that fail to migrate to the tail end of the cyst, but they do not appear to exhibit the degree of scattering observed in PhLP3 mutants [ 68 ]. Only mutants in the Clathrin heavy chain gene exhibit infrequent individualization complex formation and nuclear scattering, similar to our mutants [ 68 ]. While numerous genes have been identified to regulate individualization, including regulators of the actin and microtubule cytoskeleton (reviewed in [ 71 ]), the signal or event that initiates this process remains unknown. In mammals, proper localization of spermatids appears to be an important precursor step to the final steps of nuclear elongation and individualization. An adherens junction-like adhesion complex, known as the ectoplasmic specialization, forms between the Sertoli cell and the spermatid to promote the positioning of the spermatid as it continues sperm maturation (reviewed in [ 72 , 73 ]). Actin and some adherens junction components have been reported to accumulate at the tip of nucleus in D. melanogaster, suggesting a similar mechanism could function to align spermatids prior to the start of individualization [ 74 ]. However, the effect of reducing levels of these components in the germline and surrounding somatic cyst cells has not been examined. As PhLP3 mutants begin nuclear elongation, but do not complete the process and begin individualization, it is possible the arrest of spermatid maturation occurs as a result of the failure of spermatid nuclei to properly align. In this study, we have identified the D. melanogaster PhLP3 protein and demonstrated it has redox activity. We have shown that PhLP3 functions in the late stages of sperm development based on arrested spermatid maturation during the canoe stages in PhLP3 mutants. Nuclei fail to align and elongate and are scattered through the distal end of the testis. In addition, mutant seminal vesicles are smaller in size as compared to controls and lack mature sperm, resulting in male sterility ( Fig 11 ). PhLP3-RNAi results in slightly milder defects with some sperm still clustering, but still failing to complete elongation and to be transferred to the seminal vesicle. While our results demonstrate the requirement for PhLP3 in sperm maturation, the mechanism by which PhLP3 acts to promote sperm maturation remains unclear. While PhLP proteins have been demonstrated to interact with the CCT to regulate actin and tubulin folding in other species, it could play a different role in this context. Future studies exploring the localization of PhLP3 and its ability to interact with actin, tubulin and CCT will provide further insight into how PhLP3 acts to promote sperm maturation. Download figure Open in new tab Figure 11. Supporting Figure Captions S1 Fig. D. melanogaster possess three PhLPs. (A) Clustal Omega alignment of the three predicted PhLPs [ 11 , 22 ]. The conserved residues are indicated with gray boxes. The green boxes indicated the position of the thioredoxin domain with the putative redox-active cysteine highlighted in yellow. The percent identity between each sequence is shown in the box. (B) Comparison of the three PhLPs. Length and characteristic organization of the proteins are indicated. The blue bracket indicates the portion of each protein that was modeled. (C) Hypothetical models of the three predicted PhLP proteins in D. melanogaster . The models were generated using SWISS-MODEL template PDB 7nvm: entity 11, human PhLP2A The structures are colored by confidence level from high (blue) to low (red) [ 15 , 19 ]. S2 Fig. RNA-Seq data for PhLP3 in dissected tissues. (A) RNA-Seq expression data from select adult dissected tissues from the modENCODE project. Values listed are Reads per kilobase of transcript per Million reads (RPKM) [ 23 ]. (B) RNA-Seq expression data from select adult dissected tissues from the FlyAtlas2 project. Values listed are Reads per kilobase of transcript per Million reads (RPKM) [ 24 ]. We used FlyBase (FB2023_06, released December 12, 2023) to obtain the data presented in this figure. S3 Fig. Schematic of PhLP3 gene region and analysis of P element insertion site. (A) Schematic of the PhLP3 gene region. The location of the P element insertion P{EPgy2} EY13373 is indicated 78 bp upstream of the translation start site in the 5’ UTR. (B) Sequence around insertion site of P element. The following sequences and sequence data are represented: genomic sequence from Flybase (FBgn0037843), sequencing result of control strain ( w 1118 ), sequencing result of the PhLP3 ΔP/ΔP excision strain, inverse PCR (iPCR) sequencing result of the P element insertion strain ( PhLP3 EY13373 ), and the previously reported flanking sequence for the P element. Sites where HpaII would cut the sequence are indicated, as this enzyme was used for iPCR. The sequenced regions of the P element insertion strain that do not align with the consensus sequence correspond to sequence from the P element, P{EPgy2}, not the PhLP3 gene. Acknowledgements Thank you to the Bloomington Drosophila Stock Center and the Vienna Drosophila Resource Center for fly stocks. The rat anti-Vasa monoclonal antibody, developed by A. C. Spradling and D. Williams, was obtained from the Developmental Studies Hybridoma Bank, created by the NICHD of the NIH and maintained at The University of Iowa, Department of Biology, Iowa City, IA 52242. Thanks to E. O’Flaherty and Danielle Talbot for helpful discussions and comments on this project. This work was made possible by NSF MRI #1828164, which provided for the purchase of the Zeiss LSM880 confocal microscope. This work was supported by internal research awards to C. P., E. K., S. W., M. M., B. S., C. C., J. C. J., and S. M. K. from Loyola University Chicago. Footnotes ↵ ¶ JCJ and SMK are Joint Senior Authors References 1. ↵ Gaudet R , Bohm A , Sigler PB . Crystal structure at 2.4 angstroms resolution of the complex of transducin betagamma and its regulator, phosducin . Cell . 1996 ; 87 : 577 – 588 . doi: 10.1016/s0092-8674(00)81376-8 OpenUrl CrossRef PubMed Web of Science 2. ↵ Ogawa S , Matsubayashi Y , Nishida E . 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