A β-Ketoacyl-CoA Synthase encoded by DDP1 controls rice anther dehiscence and pollen fertility by maintaining lipid homeostasis in the tapetum

A β-Ketoacyl-CoA Synthase encoded by DDP1 controls rice anther dehiscence and pollen fertility by maintaining lipid homeostasis in the tapetum | Research Square window.SnipcartSettings = { analytics: { enabled: false } }; (function() { var accessVector = localStorage.getItem('access_vector') || ''; window.dataLayer = window.dataLayer || []; if (accessVector) { window.dataLayer.push({ user: { profile: { profileInfo: { snid: accessVector } } } }); } })(); (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],j=d.createElement(s),dl=l!='dataLayer'?'&l='+l:'';j.async=true;j.src='https://www.googletagmanager.com/gtm.js?id='+i+dl;f.parentNode.insertBefore(j,f);})(window,document,'script','dataLayer','GTM-K279D39R'); Browse Preprints In Review Journals COVID-19 Preprints AJE Video Bytes Research Tools Research Promotion AJE Professional Editing AJE Rubriq About Preprint Platform In Review Editorial Policies Our Team Help Center Sign In Submit a Preprint Cite Share Download PDF Research Article A β-Ketoacyl-CoA Synthase encoded by DDP1 controls rice anther dehiscence and pollen fertility by maintaining lipid homeostasis in the tapetum Yibo Xu, Shixu Zhou, Jingfei Tian, Wenfeng Zhao, Jianxin Wei, and 6 more This is a preprint; it has not been peer reviewed by a journal. https://doi.org/ 10.21203/rs.3.rs-4822227/v1 This work is licensed under a CC BY 4.0 License Status: Published Journal Publication published 03 Dec, 2024 Read the published version in Theoretical and Applied Genetics → Version 1 posted 5 You are reading this latest preprint version Abstract Anther dehiscence and pollen fertility are crucial for male fertility in rice. Here, we studied the function of Defective in Dehiscence and Pollen1 (DDP1), a novel member of the KCS family in rice, in regulating anther dehiscence and pollen fertility. DDP1 encodes an endoplasmic reticulum (ER)-localized protein and is ubiquitously expressed in various organs, predominately in the microspores and tapetum. The ddp1 mutant exhibited partial male sterility attributed to defective anther dehiscence and pollen fertility, which was notably distinct from those observed in Arabidopsis thaliana and rice mutants associated with lipid metabolism. Mutations of DDP1 altered the content and composition of wax on anther epidermis and pollen wall, causing abnormalities in their morphology. Moreover, genes implicated in lipid metabolism, pollen development and anther dehiscence exhibited significantly altered expression levels in the ddp1 mutant. These findings indicate that DDP1 controls anther dehiscence and pollen fertility to ensure normal male development by modulating lipid homeostasis in the tapetum, thereby enhancing our understanding of the mechanisms underlying rice anther dehiscence and pollen fertility. Figures Figure 1 Figure 2 Figure 3 Figure 4 Figure 5 Figure 6 Figure 7 Figure 8 Figure 9 Figure 10 Figure 11 Key Message DDP1 affects rice anther dehiscence and pollen fertility by maintaining lipid homeostasis in the tapetum. Introduction Rice ( Oryza sativa L.), one of the primary food crops globally, feeds approximately 50% of the global population. Increasing rice yields is essential for global food security, but low seed-setting rate impedes rice yield increase. Pollen fertility, which depends on the proper development of both pollen and anthers, significantly influences seed setting and rice yield. The pollen wall, a lipid-rich structure, contains the exine and intine (Shi et al. 2015 ). The anther wall is made up of four distinct layers, the outermost layer is the epidermis, followed in sequence by the endothecium and the middle layer, the innermost layer is tapetum (Zhang et al. 2011 ). The tapetum provides lipid precursors crucial for sporopollenin synthesis within the pollen wall and for wax and cutin formation in the anther epidermis. Aberrant tapetum development commonly leads to defective anthers and pollen. In addition to tapetum function, male fertility also depends on the timely release of mature pollen grains, which is strictly regulated by anther dehiscence. However, the precise mechanisms underlying anther dehiscence and pollen fertility remain unclear. Thus, elucidating the molecular mechanism behind these processes will not only enhance our knowledge of rice biology but also significantly propel the genetic improvement of rice fertility and yield traits. The main components of the anther epidermis and pollen wall include very long-chain fatty acids (VLCFAs) and related lipid derivatives.They provide critical protection against dehydration, environmental stresses and pathogen attacks (Buschhaus and Jetter 2011 ; Jenks et al. 1994 ). VLCFAs are initially de novo synthesized in the plastid and then elongated in ER, which is facilitated by the fatty acid elongation (FAE) complex (Ariizumi and Toriyama 2011 ; Shi et al. 2015 ). The FAE complex is made up of four distinct enzymes: β-ketoacyl-CoA synthase (KCS) for condensation, β-ketoacyl-CoA reductase (KCR) for reduction, 3-hydroxyacyl-CoA dehydratase (HCD) for dehydration, and trans-2,3-enoyl-CoA reductase (ECR) for secondary reduction. Together, they extend the carbon chain length of the substrate by incorporating two additional carbon atoms in each catalytic cycle (Lee and Suh 2013 ). Among the FAE enzymes, the KCS family exhibit strict substrate specificity, determining the chain lengths of the substrate (Blacklock and Jaworski 2006 ). KCS enzymes are also highly conserved across plants, with varying numbers of KCS genes from Arabidopsis thaliana , Zea mays , Oryza sativa , Arachis hypogaea and Gossypium hirsutum (Joubès et al. 2008 ; Yang et al. 2023 ; Campbell et al. 2019 ; Huai et al. 2020 ; Xiao et al. 2016 ). Notably, KCS6, characterized by its broad tissue distribution and potent catalytic activity, not only catalyzes the extension of C24 to C28 VLCFAs on its own but also synergizes with a CER2-like protein to promote the elongation of C30 to C34 VLCFAs (Haslam and Kunst 2013 ; Huang et al. 2022 ; Haslam et al. 2015 ). Abundant studies have explored the roles of KCS genes in Arabidopsis thaliana , where KCS mutations generally lead to the reduction in wax production and various deficiencies in vegetative development, such as KCS6 , KCS1 , KCS2/DAISY , KCS20, KCS9 , KCS16 , KCS4 , KCS5 (Millar et al. 1999 ; Fiebig et al. 2000 ; Todd et al. 1999 ; Lee et al. 2009 ; Franke et al. 2009 ; Lee et al. 2009 ; Kim et al. 2013 ; Hegebarth et al. 2017 ; Kim et al. 2021 ; Huang et al. 2022 ). In contrast, functional characterization of KCS enzymes in rice is limited. Mutations or overexpression of rice KCSs can result in diverse phenotypes by affecting wax deposition. For instance, wsl1 displays enhanced sensitivity to drought and low fertility (Yu et al. 2008 ), while sd38 mutation results in a semi-dwarf phenotype (Zhang et al. 2022 ); wsl4 exhibits reduced wax accumulation on leaves and its allelic mutant hms1 is characterized by decreased seed setting under low humidity condition (Gan et al. 2017 ; Chen et al. 2020 ). Additionally, oni1 and oni2 are seedling-lethal (Tsuda et al. 2013 ), and overexpression of OsCUT1 is closely associated with enhanced drought resistance (Gao et al. 2022 ). In conclusion, while KCS homologs share conserved biochemical function in wax deposition, their biological functions exhibit significant differentiation. However, the specific roles of KCS in contributing to male fertility are still unclear. In our research, we have conducted a functional characterization of DDP1 (Defective in Dehiscence and Pollen1), a novel member of the KCS family in rice. The ddp1 mutant showed a partial male sterile phenotype attributed to defective anther dehiscence and pollen fertility. This phenotype was notably distinct from those observed in Arabidopsis thaliana and rice mutants associated with lipid metabolism, underscoring the unique role of DDP1 in male fertility. Materials and methods Plant materials and growth conditions We generated knockout (KO) mutants ddp1-1 and ddp1-2 utilizing CRISPR/Cas9 technology. The target sequence within the DDP1 coding sequence was selected with the aid of designer software specifically tailored for CRISPR target prediction (Xie et al. 2017 ) (Fig. 1 a). Subsequently, the target sequence was synthesized and integrated into a CRISPR/Cas9 expression vector. Following its construction, the plasmid was transferred into the japonica rice cultivar Zhonghua 11. The plant materials analyzed in this research were cultivated in an experimental field at Nanning (Guangxi, China) under natural conditions and managed with standard agricultural practices. Characterization of mutant phenotypes A Nikon digital camera was utilized to photograph the phenotypes of whole plants and panicles after seed maturation. An sz61TR trinocular microscope (Olympus) was used to photograph the phenotypes of spikelets and anthers. Pollen fertility was examined by staining mature pollen grains using 1% I 2 -KI and photographed using an Axioscope 5 microscope (ZEISS). Yield traits were measured using the methods previously outlined by Qin et al ( 2021 ). Anther samples collected at various intervals during the flowering period were immersed in a 2.5% glutaraldehyde solution (v/v) to prepare them for subsequent examination via scanning electron microscopy (SEM) and transmission electron microscopy (TEM) following the previously described methods (Qin et al. 2013 ). In vitro and in vivo pollen germination assays In conducting the in vitro pollen germination assay, we harvested pollen grains at flowering stage and place them on a prepared germination medium containing 20% sucrose, 10% polyethylene glycol 4000, 40 mgL − 1 H 3 BO 3 , 3 mmolL − 1 Ca(NO 3 ) 2 , and 10 mgL − 1 vitamin B1(VBl) on slide glass. Following a 2 hours culture period at 35℃, pollen germination was observed using an Axioscope 5 microscope (ZEISS). To determine the germination rate, we measured the germination of 250 pollen grains from both ddp1 and WT anthers. For the in vivo assessment of pollen germination, pistils were harvested 3 hours after pollination and subsequently immersed in Carnoy solution (3:1 ethanol-to-glacial acetic acid mixture) for overnight. Following fixation, the pistils underwent three sequential washes using double-distilled water (ddH 2 O) and were then softened in 4M sodium hydroxide (NaOH) for 24 hours. After another three washes with ddH 2 O, the pistils were immersed in a 0.05% aniline blue solution for 12h in the dark. After staining, the pistils were carefully mounted onto glass slides for microscopic examination using an Axioscope 5 microscope (ZEISS). Examination of anther dehiscence The assessment of anther dehiscence was conducted in accordance with the previously published method (Zhang et al. 2004 ). The anthers were collected and observed with a stereoscopic microscope to assess dehiscence. The degree of anther dehiscence was categorized into five levels as follows: ●Level 5: Anthers were completely dehisced, releasing all pollen grains. ●Level 4: Anthers had large holes at the top and bottom, nearly releasing all pollen grains. ●Level 3: Anthers with small holes or a single chamber dehiscence released a portion of pollen grains. ●Level 2: Anthers with a small hole at the bottom released a minimal amount of pollen grains. ●Level 1: Anthers that were completely indehiscent did not release any pollen grain. The anther dehiscence phenotype was quantified using the dehiscence index, calculated as follows: Histochemical analysis For nuclear staining, the spikelets of ddp1-1 and WT were collected during stage 9 to 12 and then immersed in Carnoy solution for overnight. After being washed three times with 70% ethanol, anthers were dissected from the spikelets and carefully mounted onto a glass slide containing a small drop of 1 mgL − 1 DAPI solution. A cover slip was placed over the anthers to prevent evaporation and ensure even staining. After a 10 minutes incubation period, the stained anthers were observed under an Axioscope 5 microscope (ZEISS) to visualize nuclear morphology. For lipidic staining, the spikelets of ddp1-1 and WT at stage 12 were collected and then fixed in the 70% solution of formalin-acetic-alcohol (FAA) for 24 hour. Following fixation, the spikelets underwent dehydration using a sequential ethanol gradient, ranging from 100–30%. The dehydrated spikelets were then stained by Sudan Red 7B solution. The paraffin sections of anthers were prepared and processed by dewaxing, followed by hydration, and subsequently stained using Sudan Red 7B solution. After staining, the sections were washed three times using 1% sodium dodecyl sulfate (SDS) followed by double distilled H 2 O (ddH 2 O) to eliminate any surplus stain. The anthers, dissected from the spikelets, as well as paraffin sections and microspores, dissected from the anthers, were carefully mounted onto slides using a 50% (v/v) glycerol solution to prevent dehydration and distortion, and then observed under an Axioscope 5 microscope (ZEISS) for detailed examination. For the preparation of semi-thin sections, fresh panicles were initially fixed in Carnoy solution, followed by dehydration through an ascending series of ethanol concentrations. Following dehydration, the panicles were encased in EMbed812 resin (Hereaus Kulzer) and left to polymerize, ensuring a stable matrix for sectioning. The transverse sections of the embedded samples were cut to a thickness of 3µm using a Leica slicer (LEICA EMUC7FC7) and were stained in 0.1% (w/v) toluidine blue. The transverse sections were examined and captured with an Axioscope 5 microscope (ZEISS). For the observation of callose walls, paraffin sections underwent dehydration before being stained with a 0.1% (w/v) solution of aniline blue. Subsequently, they were mounted on slides using a 50% (v/v) glycerol medium and captured with an Axioscope 5 microscope (ZEISS). Wax components analysis Mature anthers from ddp1-1 and WT at stage 12 were collected with five biological replicates. Following vacuum drying, the dried anthers underwent rapid chloroform extraction to isolate wax components. Subsequently, the isolated components underwent a thorough analytical evaluation using gas chromatography-mass spectrometry (GC-MS), which was conducted at the SJTU-Metabolon Joint Metabolomics Lab in China following the previously described methods (Xu et al., 2017 ). Protein sequence analysis The full-length protein sequences of DDP1 homologs from various plant species were retrieved through a BLASTP search conducted on the NCBI database . The full-length protein sequences of DDP1 and its homologs across various plant species were aligned using MUSCLE version 3.6, a widely recognized software for multiple sequence alignment available at the EBI website. Following the alignment, the sequences were utilized to construct a phylogenetic tree, which was generated using the MEGA X software, a widely recognized tool for phylogenetic analysis. The neighbor-joining method was applied with default settings to infer the evolutionary relationships among the sequences. To ensure the reliability of the tree topology, 1000 bootstrap replications were performed, providing a statistical measure of the confidence in the branching order. To predict protein domains, the full-length protein sequences of DDP1 and ddp1-1/2 were analyzed using the SMART tool and the PSIPRED server . These resources are well-established for identifying protein domains and predicting secondary structures, respectively. For three-dimensional structure prediction, the same full-length protein sequences were deposited into the SWISS-MODEL platform, an online resource for protein modeling accessible at SWISS-MODEL . Quantitative real-time PCR and RNA in situ hybridization To determine DDP1 expression profiles, total RNA was extracted from multiple tissues of WT plant, such as roots, stems, leaves, and panicles at distinct stages as well as from panicles at different stages of ddp1 plant. The extraction was performed using a TRIzol kit (Invitrogen, USA). Both Reverse Transcription Polymerase Chain Reaction (RT-PCR) and Reverse Transcription Quantitative Polymerase Chain Reaction (RT-qPCR) were performed following established methods (Ma et al. 2021 ). OsActin was employed as the internal reference gene. Eample was assayed in triplicate to ensure biological reproducibility. The gene primers used for examination in our research were presented in Table S1 . RNA in situ hybridization was conducted following the established protocols detailed in previous studies (Xue et al. 2018 ). The DDP1 cDNA fragment was used as a template for probe labeling to generate the sense and antisense probes, which were amplified by specific primers (Table S1 ). The Axioscope 5 microscope (ZEISS) was used to capture the image of the assay result. Subcellular localization The complete cDNA sequences of DDP1 and ddp1-1 were replicated and subsequently inserted into the pCAMBIA2300 vector to produce the constructs 35S-GFP-DDP1 and 35S-GFP-ddp1-1. The ER marker was generated by fusing HDEL ER retention signal with mCherry (Caroli et al., 2011 ). The construct 35S-GFP-DDP1 and 35S-GFP-ddp1-1 was transiently co-introduced with the ER marker mCherry-HDEL into rice protoplasts, respectively. The transformation was performed using the polyethylene glycol (PEG)-mediated method, a widely used technique for introducing DNA into plant cells. A GFP reporter, serving as a control, was utilized to verify the success of the transformation process. The fluorescence signal, indicative of the localization of the GFP-tagged proteins and the ER marker, was detected and recorded through a confocal laser scanning microscope (Leica TCS SP8MP). Results ddp1 mutants exhibit partial pollen abortion The rice genome contains 22 KCS genes (Yang et al. 2023 ). To investigate the functions of these KCSs, we employed CRISPR/Cas9 technology to generate a series of knockout (KO) mutants targeting these genes (Table S1 ). Among all developed mutants, the knockout mutants of LOC_Os02g49920 exhibited a partial male sterility attributed to defective anther dehiscence and pollen fertility. Thus, the mutant of LOC_Os02g49920 was designated as ddp1 ( defective in dehiscence and pollen1 ). two alleles ddp1 namely ddp1 - 1 and ddp1 - 2 were identified in T 1 progeny. ddp1-1 and ddp1-2 carried 4-bp and 2-bp deletion in the sole exon of LOC_Os02g49920 , respectively (Fig. 1 b). These deletions caused reading-frame shifts, generating premature and delayed stop codon, respectively. Compared to WT, ddp1-1/2 mutants exhibited no significant differences in whole-plant morphology and the structure of flower organs such as spikelets and anthers (Fig. 1 c-f). However, at the mature stage, the seed-setting rates of ddp1 - 1 (41.533 ± 1.050%) and ddp1 - 2 (32.100 ± 1.400%) were significantly lower than that of WT (95.000 ± 0.816%) (Table 1 )(Fig. 1 g, k). To determine if the lower seed-setting rate in ddp1-1 / 2 mutants resulted from a male or female gametophyte impairment, we evaluated the pollen and female fertility. Notably, the fertile pollen rate was significantly lower in ddp1 - 1 (54.67% ± 3.68%) and ddp1 - 2 (49.17% ± 1.65%) compared to WT, which exhibited a fertile pollen rate of 95.13% ± 0.84% (Fig. 1 h-j, l). When ddp1 mutants were self-pollinated with its pollen, their seed setting rate was only 24.45% ± 2.53%. However, after pollination with WT pollen, the seed setting rate of ddp1 mutants reached 58.60% ± 5.88% (Fig. S1 ). The findings suggest that the reduced seed-setting rate observed in ddp1 mutants is due to abnormalities in pollen development, rather than any deficiency in the female gametophyte. Table 1 The agronomic traits of WT and ddp1 mutant. Agronomic traits WT Mean ± SD ddp1-1 Mean ± SD ddp1-2 Mean ± SD Plant height (cm) 86.333 ± 2.055 83.667 ± 1.247 88.000 ± 0.816 Panicle length (cm) 21.500 ± 0.408 23.533 ± 0.500 21.400 ± 0.638 1000-grain weight (g) 26.647 ± 0.509 27.406 ± 0.561 26.810 ± 0.752 Grain length (cm) 0.811 ± 0.009 0.797 ± 0.005 0.811 ± 0.009 Grain width (cm) 0.351 ± 0.002 0.354 ± 0.003 0.352 ± 0.002 Grain thickness (mm) 2.32 ± 0.037 2.303 ± 0.054 2.317 ± 0.049 Seed-setting Rate (%) 95.000 ± 0.816 41.533 ± 1.050** 32.100 ± 1.400* Number of tillers 10.333 ± 1.247 9.667 ± 1.247 9.667 ± 0923 Number of primary branches 10.000 ± 0.816 10.333 ± 1.247 10.000 ± 1.633 Number of secondary branches 27.667 ± 1.700 23.000 ± 2.60* 17.333 ± 1.700* Yield per plant (g) 16.000 ± 1.633 6.233 ± 1.481** 4.433 ± 0.419** *, ** significant at 5% and 1% levels of probability, respectively. In addition to partial pollen abortion, ddp1-1/2 mutants also exhibited significant differences in certain yield-related traits compared to WT. For instance, the number of secondary branches and yield per plant were significantly lower in ddp1-1 mutant (23.00 ± 2.16% and 6.23 ± 1.48%) compared to WT (27.67 ± 1.70% and 16.00 ± 1.62%) (Table 1 ). The ddp1 - 2 mutant showed similar trends to those observed in ddp1 - 1 (Table 1 ). Nevertheless, the comparison revealed no notable differences in plant height, number of tillers and primary branches, panicle length, 1000-grain weight, and grain dimensions (length, width, thickness) between ddp1-1/2 and WT (Table 1 ). To confirm whether LOC_Os02g49920 was the target gene responsible for the ddp1 mutants phenotype, a complementation test was performed by transforming a construct DPP1 pro : DPP1CDS - mCitrine containing a 2.5-kb DDP1 promoter region, 1.458-kb DDP1 coding region and 0.72-kb mCitrine coding region into Cas9-free ddp1-1 mutants (Table S1 ). As expected, the complementary transgenic lines exhibited a restoration of seed-setting rates and pollen fertility to WT levels (Fig. S2 ), thereby confirming that LOC_Os02g49920 is indeed the target gene whose knockout causes partial male sterility in ddp1 mutants. Anther dehiscence is defective in ddp1 mutants To determine whether partial male sterility of ddp1-1 / 2 mutants was associated with the defects in anther dehiscence, pollen germination, tube growth, and dehydration, we compared these critical reproductive processes in ddp1-1 / 2 mutants to those in WT. For anther dehiscence analysis, we examined the anther dehiscence phenotype in both ddp1-1/2 and WT. WT anthers typically undergo dehiscence, facilitating the dispersal of mature pollen (Fig. 2 a, f), while ddp1-1/2 mutants exhibited various defects in anther dehiscence and pollen grain release (Fig. 2 b-e, g-j). The anther dehiscence phenotype was quantified using the dehiscence index as reported previously (Zhang et al. 2004 ). A higher dehiscence index indicates that anthers have dehisced more completely. Our findings indicated that the anther dehiscence index was significantly lower in ddp1-1 (2.89) and ddp1-2 (2.73) compared to WT (4.09) (Table 2 ). This impaired anther dehiscence in ddp1-1/2 mutants may result in reduced adhesion and germination of fertile pollen grains on the stigmas. To validate this finding, we performed an in vivo pollen germination experiment to evaluate the pollen germination rates on the stigmas of ddp1-1/2 and WT. The assay demonstrated a markedly lower pollen germination rate on the stigmas in ddp1-1/2 mutants relative to WT (Fig. 2 n-r, u). Collectively, these results indicate that defective anther dehiscence in ddp1 - 1/2 mutants hinders the adhesion and subsequent germination of fertile pollen grains on the stigma, thereby reducing the seed-setting rate. Table 2 The anther dehiscence index of WT and ddp1 . Level of anther dehiscence Total number of anther Dehiscence index 5 4 3 2 1 WT 8 84 0 0 0 92 4.09 ddp1-1 10 34 26 18 24 112 2.89** ddp1-2 14 41 36 30 41 162 2.73** ** significant at 1% levels of probability. For pollen germination analysis, we compared pollen germination rate between ddp1-1/2 and WT using an in vitro pollen germination assay. Because ddp1-1/2 mutants contained sterile pollen grains which could not normally germinate (Fig. 2 k-m), the overall in vitro pollen germination rates were significantly lower in ddp1-1 (50.65 ± 1.86%) and ddp1-2 (42.23 ± 2.36%) compared to WT (89.4 ± 1.11%) (Fig. 2 s). However, when only considering the germination rate of fertile pollen grains, the comparison revealed no notable differences between ddp1-1/2 and WT (with 82.03 ± 0.82% of ddp1-1 and 81.37 ± 0.45% of ddp1-2 versus 84.90 ± 1.35% of WT) (Fig. 2 t). These findings suggest that the germination of fertile pollen in ddp1-1/2 mutants remains unaffected. For pollen tube growth analysis, we compared pollen tube growth within the pistil of ddp1-1/2 and WT using an in vivo pollen germination assay. In self-pollinated WT pistils, at 5 hours post-pollination, pollen tubes had successfully reached the ovule micropyle (Fig. 2 n). However, self-pollinated pistils of the ddp1-1/2 mutants showed a reduced germination rate of pollen grains, yet those that did germinate were able to extend their pollen tubes to the ovule micropyle (Fig. 2 o, q), suggesting normal pollen tube growth within ddp1-1/2 pistils. For pollen dehydration analysis, we compared the in vitro dehydration rate of fertile pollen between ddp1-1 and WT. However, no significant differences in the dehydration rate of fertile pollen were observed between ddp1-1 and WT from 0 second to 30 minutes (Fig. S3). Altogether, these findings suggest that while pollen germination, pollen tube growth and pollen dehydration are not compromised in ddp1-1/2 mutants, anther dehiscence is abnormal. Consequently, we conclude that the decrease in seed-setting rate of ddp1-1/2 mutants was attributed to the aborted pollen and aberrant anther dehiscence. Cytological comparison of anther development between ddp1 and WT To determine the morphological defect of ddp1-1/2 anthers, semi-thin sections of both ddp1-1/2 and WT anthers at different development stages were examined using light microscopy. Initial observations revealed that no significant differences were detected between ddp1-1/2 and WT anthers from stage 6 to 9 (Fig. 3 a-c, h-j, p-r). However, at stage 10, the epidermis and endothecium of ddp1-1 / 2 anthers appeared to exhibit a greater thickness compared to their counterparts in WT anthers, and microspores of ddp1-1/2 exhibited collapse and a defect in vacuolation (Fig. 3 k, s). At stage 11, the epidermis and endothecium of ddp1-1 / 2 anthers continued to show swelling, and tapetum degradation seemed to be delayed. Only a fraction of microspores formed falcate-shaped pollen grains filled with starch granules, while the rest developed into irregularly shaped pollen grains lacking starch accumulation (Fig. 3 l, t). At stage 12, the WT tapetum had completely degraded, allowing microspores to mature into pollen grains (Fig. 3 f). In contrast, in ddp1-1/2 anthers, the incompletely degraded tapetum residues were observed, with only some microspores maturing into fertile pollen grains, while others aborted (Fig. 3 m, u). At stage 14, WT anthers were able to dehisce normally as the connective tissue between anthers cracked (Fig. 3 g). However, in ddp1-1/2 , only a subset of anthers dehisced, while others remained closed (Fig. 3 n-o, v-w). These findings show that ddp1-1/2 mutations lead to developmental defects in anther and pollen from stage 10 to 14. To precisely characterize the differences between ddp1-1/2 and WT, SEM was employed to compare the anthers and pollen grains. The anthers of ddp1-1/2 and WT were comparable in size (Fig. 4 a, e, i). WT anthers exhibited an outer epidermis covered by spaghetti-like cuticle layers (Fig. 4 b) and an inner epidermis with Ubisch bodies (Fig. 4 c, d). In contrast, the cuticle layers of the outer epidermis and the Ubisch bodies of the inner epidermis in ddp1-1/2 anthers seemed to be denser (Fig. 4 f-h, g-l). In addition, WT pollen grains were spherical and smooth, uniformly coated by a layer of sporopollenin (Fig. 5 a, d). ddp1-1/2 mutants had two types of pollen grains, namely spherical pollen grains and shrunken pollen grains (Fig. 5 b-c, e-h). The spherical pollen grains in ddp1-1/2 mutants exhibited a slightly sparse sporopollenin layer (Fig. 5 j, l), while the sporopollenin on the shrunken pollen grains in ddp1-1/2 mutants appeared to be denser (Fig. 5 k, m). The increased accumulation of sporopollenin on the surfaces of shrunken ddp1-1/2 pollen may be attributed to the shrinkage of the pollen grain surface area. Given the similar phenotypes exhibited by ddp1-1 and ddp1-2 under identical growth conditions, the following analyses within this study were conducted solely on ddp1-1 . To further elucidate the cytological differences between ddp1 and WT, TEM was also employed to observe the ultrastructures of anthers and pollen grains. At stage 11, in accordance with our light microscopy results, the anther wall, particularly the tapetum of ddp1-1 mutant was thicker compared to that of WT (Fig. 6 a, e). At stage 13, the WT tapetum fully degraded while the incompletely degraded tapetum residue was still observed in ddp1-1 mutant (Fig. 6 i, m). At stage 11 and 13, the cuticle layer and the Ubisch body in ddp1-1 anthers were denser than those of WT (Fig. 6 f-g, n-o), aligning with SEM observations. Furthermore, the aborted ddp1 - 1 pollen grains exhibited a thicker exine and smaller bacula compared to WT (Fig. 6 h, p), indicating the alterations in the pollen wall ultrastructure. At stage 10, neither ddp1 - 1 nor WT microspores showed signs of starch accumulation and intine formation (Fig. 6 q, r). By stage 12, WT microspores had developed an intine and were filled with a substantial amount of starch granules (Fig. 6 s), whereas aborted pollen grains of ddp1 - 1 mutant lacked both features (Fig. 6 t). In summary, ddp1-1 mutant exhibited abnormalities in their anther cuticle layer, Ubisch bodies, tapetum degradation, anther dehiscence, pollen wall structure, and starch accumulation. Gametogenesis at stage 11 and 12 is defective in ddp1-1 anthers To determine whether gametogenesis was affected in ddp1 anthers, we performed the 4’,6-diamidino-2-phenylindole (DAPI) staining on microspores from both ddp1-1 and WT at different stages. At stage 9, WT microspores typically developed into uninucleate microspores. At stage 11, they underwent the first mitotic division, resulting in binucleate microspores. At stage 12, they underwent the second mitotic division, yielding trinucleate microspores with one vegetative nucleus and two generative nuclei. Accordingly, a portion of ddp1-1 microspores successfully developed into uninucleate, binucleate and trinucleate microspores at stage 9, 11 and 12, respectively, similar to WT (Fig. 7 a). However, other ddp1-1 microspores exhibited a brightly stained nucleus at stage 9 and 11 but failed to complete the first and second mitotic divisions to form binucleate and trinucleate microspores at stage 11 and 12 (Fig. 7 a). The DAPI staining analysis indicates that defective gametogenesis in the aborted ddp1 - 1 microspores begins at stage 11, which is roughly consistent with the semi-thin section observations that anther and pollen abnormalities occur at stage 10. Defective gametogenesis was often closely associated with abnormalities in callose biosynthesis and degradation. Callose biosynthesis initiated at stage 7, and its degradation at stage 9 facilitated the release of microspores from the tetrads. In order to investigate whether these processes were affected in ddp1-1 anthers, we performed aniline blue staining on anthers from both ddp1-1 and WT from stage 7 to 9. However, no obvious differences in the fluorescence signal surrounding microspores were observed between ddp1-1 and WT anthers (Fig. 7 b). This result suggests that the callose formation and degradation steps in ddp1-1 anthers from stage 7 to 9 are not impaired, consistent with the semi-thin section observations that anther and microspore development in ddp1-1 mutant appeared normal from stage 6 to 9. Altered wax content and composition of the anther epidermis and pollen wall in the ddp1 mutant DDP1 encodes a β-ketoacyl-CoA synthase with 485 amino acids residues, catalyzing cuticular wax synthesis. To elucidate the function of DDP1, a phylogenetic analysis was performed using DDP1 and other plant KCS proteins with both known and unknown biochemical and biological functions. Phylogenic analysis revealed that DDP1 shares high sequence similarity with its homologs (Fig. S4a). Domain homology analysis using SMART demonstrated that the DDP1 protein contains three conserved domains: an ACP_syn_III_C domain, a transmembrane region, and a FAE1_CUT1_RppA domain, similar to its counterparts in other plant species (Fig. S4b). The analysis suggests that DDP1 may play a conserved function in cuticular wax synthesis. Given that ddp1-1 mutant also showed structural abnormalities in the lipidic anther epidermis and pollen wall, we speculated that the wax content and composition of these structures in the ddp1-1 mutant might be altered. To test this speculation, we initially examined the lipidic compounds by staining anthers and pollen from ddp1-1 and WT at stage 12 with the lipophilic dye Sudan Red 7B. While the WT anther epidermis and pollen wall showed intense staining (Fig. 8a1-a3,), the ddp1 - 1 mutant displayed strong staining in anther epidermis and fertile pollen wall, and weak staining in the wall of aborted pollen grains (Fig. 8b1-b3). This suggests a reduction in lipidic compounds within the wall of ddp1 - 1 aborted pollen. Subsequently, we analyzed the phenolic compounds by comparing the fluorescence intensity emitted by phenolic compounds in pollen walls under ultraviolet radiation between ddp1-1 and WT. The fertile pollen grains of ddp1 - 1 emitted fluorescence similar in intensity to that of WT, whereas the aborted pollen grains exhibited significantly weaker fluorescence (Fig. 8b4), indicating a substantial decrease in phenolic compounds in the wall of ddp1 - 1 aborted pollen. In conclusion, these findings indicate that precursors to sporopollenin, including lipidic and phenolic compounds, are significantly reduced in the walls of ddp1 - 1 aborted pollen. To ascertain the chemical profiles of anther epidermis and pollen wall, we quantified wax constituents at stage 12 using gas GC-MS. This result indicated that the total wax content in ddp1 - 1 anthers increased by 34%±0.08% compared to WT (Fig. 8 c), primarily due to significant elevations in free fatty acids (C16:0, C18:2, C18:3, C18:0, C20:0, C22:0, C26:0,C28:0 and C30:0), alkenes (C25:0, C27:0, C33:1, C33:0, C35:0 and C35:1), and alcohols (C26:0 and C28:0), as well as sterols such as campersterol, stigmasterol and β-sitosterol (Fig. 8 d, e). In contrast, the levels of certain free fatty acid (C24:0), alkenes (C23:0 and C27:1) and inositol were dramatically decreased in ddp1-1 mutants, and other wax constituents remained largely unchanged (Fig. 8 e). The altered wax profile in ddp1-1 mutant indicated that DDP1 is essential for maintaining lipid metabolic homeostasis. The alteration in the content and composition of wax in the anther epidermis and pollen wall may underlies the structural abnormalities observed in the ddp1 - 1 anther epidermis and pollen wall. Expression pattern and subcellular location of DDP1 To determine DDP1 expression pattern, RT-qPCR was conducted to quantify its expression in various tissues of WT. The result suggested that DDP1 transcription was uniformly detected across all assessed tissues, with peak transcription observed in the leaves (Fig. 9 a). DDP1 expression was observed throughout the stages of anther development, peaking at stage 8 (Fig. 9 a). To further analyze the expression of DDP1 in anthers, RNA in situ hybridization was conducted on sections of WT anthers. The hybridization signal was first observed in tapetum and pollen mother cells (PMCs) at stage 7, then in tapetum and tetrads at stage 8, and in tapetum and microspores from stage 9 to 11 (Fig. 9 b). In control experiments, the sense probe failed to produce any detectable signal, confirming the specificity of the hybridization. These findings indicate that DDP1 is predominantly expressed in the tapetum, PMCs and microspores, which correlates with the phenotypes of delayed tapetum degradation and impaired microspore development in ddp1 mutants. To further elucidate the spatial distribution of DDP1 protein, we utilized confocal microscopy to observe the mCitrine signal in ddp1 -complementary transgenic plants expressing DDP1pro:DDP1cDNA-mCitrine . At stage 10, yellow mCitrine fluorescence was detected in the tapetum and microspores (Fig. 10 a-c). By stage 11, yellow mCitrine fluorescence was noted in the partially degraded tapetum residues and microspores (Fig. 10 d-f). At stage 12, with the tapetum fully degraded, mCitrine signal was exclusively detected in pollen grains (Fig. 10 g-i). These observations indicate that DDP1 expression aligns with DDP1 protein distribution in the tapetum, microspores, and pollen grains. Protein domain analysis using SMART revealed that the DDP1 protein featured a transmembrane domain at its N-terminus (Fig. S4b). Predictions of secondary structure and three-dimensional models using PSIPRED and SWISS-MODEL indicated that DDP1 possesses coil, helix, and strand domains (Fig. S5a). Mutations in the first helix domain of the ddp1-1/2 mutants led to noticeable alterations in the protein's three-dimensional structure (Fig. S5b, c). To confirm the localization of DDP1 and ddp1-1 in rice protoplasts, we produced DDP1-GFP and ddp1-1-GFP fusion constructs and introduced them into rice protoplasts alongside the ER marker mCherry-HDEL. DDP1-GFP fluorescence was found to almost completely overlap with the mCherry-HDEL fluorescence (Fig. 9 c), suggesting that DDP1 is specifically localized to the ER, as was expected. In contrast, the ddp1-1-GFP fluorescence signal only partially co-localized with the ER marker, with a significant portion of the green fluorescence observed in the cytoplasm (Fig. 9 c). The expression levels of known genes complicated in lipid metabolism, anther and pollen development, and anther dehiscence are significantly changed in ddp1 anthers Observations of delayed tapetum degradation, defective anther and pollen development, impaired lipid metabolism, and abnormal anther dehiscence in the ddp1-1 mutant have led us to hypothesize that DDP1 mutations may disrupt the expression of genes associated with these processes. To test this speculation, we performed a comparative analysis to evaluate the expression profiles of known genes associated with these processes between ddp1-1 and WT from stage 7 to 10. Compared to WT, the expression levels of six lipid metabolism genes ( OsABCG26 , OsPKS2 , OsNP1 , RMS2 , CYP703A3 and OsCER2 ), five genes complicated in the anther, pollen and tapetum development ( OsCP1 , GAMYB , OsSTRL2 , STS1 and DPW3 ), and two genes involved in anther dehiscence ( DAO and OsH1 ) were significantly decreased in the ddp1-1 mutant (Fig. 11 ). In contrast, the ddp1-1 mutant displayed a pronounced upregulation in the expression levels of two lipid metabolism genes (OsABCG3 and OsCER1), along with one tapetum development gene (OsAP25), specifically at stages 8 and 9 (Fig. 11 ). In addition, considering the close association of anther dehiscence with auxin and jasmonic acid (JA) signaling, we also conducted a comparative analysis of gene expression levels related to these signaling pathways between ddp1-1 and WT. Six genes ( OsETTIN1 , OsETTIN2 , OsETTIN3 , OsYUCCA1 , OsYUCCA4 and OsMP ) required for auxin synthesis and response and three JA signaling suppressor genes ( JAZ1 , JAZ6 and JAZ8 ) were prominently up-regulated expressed in the ddp1-1 mutant, while a significant downregulation of two JA synthesis genes ( LOX2 and AOS3 ) was detected in the ddp1-1 mutant at stage 9 and 10, respectively (Fig. 11 ). Together, these findings suggest that mutations in DDP1 alter the expression of known genes complicated in lipid metabolism, anther development and dehiscence, thus causing defective phenotypes associated with these processes. Discussion The anther epidermis contains cutin and wax, while the pollen exine is made up of sporopollenin, with their lipid precursors and derivatives being synthesized by the tapetum. Thus, the homeostasis of lipid metabolism in the tapetum is critical for the development of anther epidermis and pollen wall. This concept is supported by evidence that mutations in several genes associated with the accumulation of lipids in tapetum, including WDA1 (Jung et al. 2006 ), OsC6 (Zhang et al. 2010 ), CYP704B2 (Li et al. 2010 ), DPW (Shi et al. 2011 ), OsABCG15 (Wu et al. 2014 ), OsABCG26 (Chang et al. 2016 ) and CYP703A3 (Yang et al. 2018 ), cause defective tapetum, anther epidermis and pollen wall, ultimately leading to pollen sterility. In our research, we demonstrated that DDP1 , a novel member of the KCS family in rice, is essential for pollen fertility and lipid homeostasis in the tapetum. DDP1 was highly expressed in tapetum and microspore. DDP1 was localized in the ER, and distributed in tapetum, microspore and pollen. ddp1-1 mutant exhibited defects in the anther epidermis and pollen wall. Additionally, compared to WT, the wax content and composition in ddp1-1 were dramatically changed, and a significant shift in the expression levels of gene complicated in lipid metabolism, anther and pollen development was observed in the ddp1-1 anthers. These findings show that DDP1 , like many genes associated with lipid metabolism, affects rice pollen fertility by modulating lipid metabolic homeostasis: the knockout of DDP1 disrupts this homeostasis, resulting in partial pollen abortion. Although DDP1 is conserved across plant species, the phenotype of the ddp1 mutants was significantly distinct from those of its homologs from Arabidopsis and rice. The phenotypes of these homologs included reduced wax accumulation, defective growth of roots and pollen tubes, semi-dwarfism, seedling lethality, and increased drought resistance. However, ddp1 mutants showed no notable vegetative phenotypes, suggesting potential functional diversification between DDP1 and its homologs. HMS1, a DDP1 homolog, has also been implicated in male fertility. However, hms1 mutant exhibited a more severe complete male sterility compared to the partial male sterility of ddp1 mutants. The sterility of hms1 was due to reduced pollen adhesion and germination on stigmas, while sterility of ddp1 mutants arose from defects in the tapetum, anther epidermis, pollen wall, and anther dehiscence. These findings indicate a functional differentiation between DDP1 and HMS1 in the regulation of male fertility. Moreover, there was a difference in the expression patterns of DDP1 homologous genes. For examples, DDP1 , OsWSL1 , SD38 and OsWSL4 / OsHMS1 were expressed in all examined organs, including roots, stems, leaves and panicles, while OsCUT1 was found to has a higher level of transcription in young panicles and leaves. The transcription of ONI1 and ONI2 was confined to specific regions, notably the outer cell layer of the shoot apical meristem and the developmental stages of lateral organs. The significant differences in mutant phenotype and gene expression pattern between DDP1 and its homologs suggest that they may have different biological functions in plant development. Investigating the function of DDP1 will be instrumental in understanding the broader functions of KCS proteins within the plant kingdom. The ddp1 mutants exhibited a partial male sterile phenotype, suggesting a redundant function for DDP1 in controlling male fertility. The potential redundancy of DDP1 could be due to the widespread presence of VLCFA biosynthesis related genes and their homologs, in addition to the high expression levels of these genes in rice young inflorescences.VLCFA biosynthesis requires four key enzymes, including KCS, KCR, HCD and ECR. Loss of function of members from any of these enzyme families might impair VLCFAs formation, leading to male sterility. In addition, the rice genome contains 22 homologs of DDP1 (Yang et al., 2023 ). Analysis of gene expression patterns in the Bio-Analytic Resource for Plant Biology database revealed that eight DDP1 homologs with unknown functions, such as OsCUT8 , OsKCS16 , OsCUT6, OsKCS15 , OsKCS13 , OsKCS22, OsKCS2 , and OsKCS9 , are highly expressed in young inflorescences (Fig. S6). This suggests that these homologs may play crucial roles in VLCFA biosynthesis and male fertility, and DDP1 may interact directly or indirectly with other proteins to coordinately regulate rice male fertility. Despite attempts to screen for DDP1-interacting proteins in the rice anther cDNA library using yeast two-hybrid technology, no interacting protein was identified. Further research is necessary to elucidate the regulatory networks of DDP1 in male fertility by identifying its interacting proteins or upstream transcription factors. Mutations in certain genes associated with lipid metabolism result in reduced anther wax, as observed in KCS6 (Fiebig et al. 2000 ), WDA1 (Jung et al. 2006 ), WSL1 (Yu et al. 2008 ), OsGL1-2 (Islam et al. 2009 ), OsGL1-1 (Qin et al. 2011 ), OsGL1-6 (Zhou et al. 2013 ), ONI1 and ONI2 (Tsuda et al. 2013 ), OsGL1-3 (Zhou et al. 2015 ), WSL4/HMS1 (Gan et al. 2017 ; Chen et al. 2020 ), and KCS5 (Huang et al. 2022 ), SD38 (Zhang et al. 2022 ). In contrast, mutations of other genes associated with lipid metabolism cause a dramatical increase of anther wax, such as DPW2 (Xu et al. 2017 ), OsPKS2 (Zou et al. 2018 ), PEM1 (Song et al. 2022 ), Os12BGlu38 (Shim et al. 2022 ), KCS3 (Huang et al. 2023a ), and KCS12 (Huang et al. 2023b ). These findings suggest that changes in anther wax content may be an indirect consequence of mutations in genes related to lipid metabolism. In this study, the ddp1 mutants showed a denser anther cuticle. Consistent with this, elevated levels of free fatty acids, alkenes, alcohols and sterols were detected in the ddp1 mutants. Moreover, two lipid metabolism genes ( OsABCG3 and OsCER1 ) had up-regulated expression in the ddp1 mutants during stages 8 and 9. Given the role of DDP1 in lipid precursor formation, it is plausible to hypothesize that the knockout of DDP1 disrupts lipid metabolism homeostasis, potentially triggering a feedback mechanism that results in a thicker anther cuticle. In addition to the aforementioned defects in anthers and pollen, the ddp1 mutants also exhibited a distinct defect in anther dehiscence, a phenotype almost rarely observed in mutants associated with lipid metabolism. We speculate that the defect in ddp1 anther dehiscence may be due to the reduced mechanical pressure from aborted pollen grains or may be caused by defective endothecium lignification. Previous research has shown that anther dehiscence is closely related to auxin signaling, jasmonic acid (JA) biosynthesis and endothecium lignification. Excessive indole-3-acetic acid (IAA) accumulation generally leads to decreased JA content and abnormal endothecium lignification, thereby causing anther indehiscence (Cecchetti et al., 2013 ). Moreover, it is reported that cuticular wax is closely related to IAA and JA. Zhu et al ( 2014 ) reported that expression of EsWAX1 from Eutrema salsugineum was slightly increased by IAA treatment, thus promoting accumulation of cuticular wax. Recently, a study demonstrated that there was a negative relationship between total cuticular wax content and JA concentration in maize, the mutation of ZmGL8 , encoding a β-ketoacyl-CoA reductase, reduced wax accumulation and activated a JA-dependent pathway (Liu et al. 2024 ). These results reveal that IAA increases cuticular wax accumulation, thereby reducing JA levels and leading to anther indehiscence. Consistent with this, we observed that in the ddp1 mutants, the total wax content increased by 34%±0.08% compared to WT, a significant increase in expression was observed for six auxin signaling related genes and three JA signaling suppressor genes, whereas two genes critical for the production of JA showed a dramatic decrease in expression levels. These findings imply that DDP1 may regulate anther dehiscence by modulating auxin and JA signaling pathways. However, the exact mechanism by which DDP1 regulates these signaling pathways and endothecium lignification remains unclear. Therefore, additional research is required for fully elucidating the function of DDP1 in auxin signaling, JA biosynthesis and endothecium lignification. Declarations Author contribution statement B. Qin, L. Shang, X. He, and Y. Xu conceived and designed the experiments; Y. Xu, and S. Zhou performed most of the experiments and analyzed the data; J. He, W. Tan, J. Tian, W. Zhao, and J. Wei participated in the phenotype measurement and field experiments; B. Qin and Y. Xu wrote the manuscript; S. Zhou, J. Tian, W. Zhao, J. Wei, and R. Li revised the manuscript. All authors read and approved the final manuscript. Funding This work was supported by the National Natural Science Foundation of China (32372023 and 31971809), Centrally Guided Local Science and Technology Development Fund (ZY23055028), the Guangxi Natural Science Foundation (2019GXNSFDA185009 and 2024GXNSFGA010003), State Key Laboratory for Conservation and Utilization of Subtropical Agro-bioresources (SKLCUSA-b202306), Innovation Project of Guangxi Graduate Education (YCBZ2022016), the Project of Bama County for Talents in Science and Technology (No.20220009). Conflict of interest The authors declare that they have no conflict of interest. References Ariizumi T, Toriyama K (2011) Genetic regulation of sporopollenin synthesis and pollen exine development. Ann Rev Plant Biol 62:437–460. https://doi.org/10.1146/annurev-arplant-0 Blacklock B, Jaworski J (2006) Substrate specificity of Arabidopsis 3-ketoacyl-CoA synthases. 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PLoS ONE 8(5):e65139. https://doi.org/10.1371/journal.pone.0065139 Zhou X, Li X, Xiang J, Gao G, Xu F, Liu A, Zhang X, Peng Y, Chen X, Wan X (2015) OsGL1-3 is involved in cuticular wax biosynthesis and tolerance to water deficit in rice. PLoS ONE 10(1):e116676. https://doi.org/10.1371/journal.pone.0116676 Zou T, Liu M, Xiao Q, Wang T, Chen D, Luo T, Yuan G, Li Q, Zhu J, Liang Y, Deng Q, Wang S, Zheng A, Wang L, Li P, Li S (2018) OsPKS2 is required for rice male fertility by participating in pollen wall formation. Plant Cell Rep 37(5):759–773. https://doi.org/10.1007/s00299-018-2265-x Zhang Z, Lu Y, Feng J, Liu X, Zhang G (2004) Studies on the anther dehiscence in F 1 of hybrids between Taichung 65 and its F 1 pollen sterility near isogenic lines. J Trop Subtrop Bot 12(6):521–527. https://doi.org/10.3969/j.issn.1005-3395.2004.6.006 Zhu L, Guo J, Zhu J, Zhou C (2014) Enhanced expression of EsWAX1 improves drought tolerance with increased accumulation of cuticular wax and ascorbic acid in transgenic Arabidopsis . Plant Physiol Biochem 75:24–35. https://doi.org/10.1016/j.plaphy.2013.11.028 Supplementary Files AppendixA.docx supplementaryfigures.docx Cite Share Download PDF Status: Published Journal Publication published 03 Dec, 2024 Read the published version in Theoretical and Applied Genetics → Version 1 posted Editorial decision: Minor revisions 29 Sep, 2024 Reviewers agreed at journal 04 Aug, 2024 Reviewers invited by journal 03 Aug, 2024 Editor assigned by journal 30 Jul, 2024 First submitted to journal 29 Jul, 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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17:34:00","extension":"docx","order_by":6,"title":"","display":"","copyAsset":false,"role":"supplement","size":18555,"visible":true,"origin":"","legend":"","description":"","filename":"AppendixA.docx","url":"https://assets-eu.researchsquare.com/files/rs-4822227/v1/27bc6af1c682a603f4122736.docx"},{"id":63570953,"identity":"2d024d50-b34d-4b2f-8758-8355352641dc","added_by":"auto","created_at":"2024-08-29 17:33:59","extension":"docx","order_by":7,"title":"","display":"","copyAsset":false,"role":"supplement","size":1448605,"visible":true,"origin":"","legend":"","description":"","filename":"supplementaryfigures.docx","url":"https://assets-eu.researchsquare.com/files/rs-4822227/v1/67ddbc917aa79296fa1a6fc5.docx"}],"financialInterests":"","formattedTitle":"A β-Ketoacyl-CoA Synthase encoded by DDP1 controls rice anther dehiscence and pollen fertility by maintaining lipid homeostasis in the tapetum","fulltext":[{"header":"Key Message","content":"\u003cp\u003eDDP1 affects rice anther dehiscence and pollen fertility by maintaining lipid homeostasis in the tapetum.\u003c/p\u003e"},{"header":"Introduction","content":"\u003cp\u003eRice (\u003cem\u003eOryza sativa\u003c/em\u003e L.), one of the primary food crops globally, feeds approximately 50% of the global population. Increasing rice yields is essential for global food security, but low seed-setting rate impedes rice yield increase. Pollen fertility, which depends on the proper development of both pollen and anthers, significantly influences seed setting and rice yield. The pollen wall, a lipid-rich structure, contains the exine and intine (Shi et al. \u003cspan citationid=\"CR36\" class=\"CitationRef\"\u003e2015\u003c/span\u003e). The anther wall is made up of four distinct layers, the outermost layer is the epidermis, followed in sequence by the endothecium and the middle layer, the innermost layer is tapetum (Zhang et al. \u003cspan citationid=\"CR50\" class=\"CitationRef\"\u003e2011\u003c/span\u003e). The tapetum provides lipid precursors crucial for sporopollenin synthesis within the pollen wall and for wax and cutin formation in the anther epidermis. Aberrant tapetum development commonly leads to defective anthers and pollen. In addition to tapetum function, male fertility also depends on the timely release of mature pollen grains, which is strictly regulated by anther dehiscence. However, the precise mechanisms underlying anther dehiscence and pollen fertility remain unclear. Thus, elucidating the molecular mechanism behind these processes will not only enhance our knowledge of rice biology but also significantly propel the genetic improvement of rice fertility and yield traits.\u003c/p\u003e \u003cp\u003eThe main components of the anther epidermis and pollen wall include very long-chain fatty acids (VLCFAs) and related lipid derivatives.They provide critical protection against dehydration, environmental stresses and pathogen attacks (Buschhaus and Jetter \u003cspan citationid=\"CR3\" class=\"CitationRef\"\u003e2011\u003c/span\u003e; Jenks et al. \u003cspan citationid=\"CR21\" class=\"CitationRef\"\u003e1994\u003c/span\u003e). VLCFAs are initially \u003cem\u003ede novo\u003c/em\u003e synthesized in the plastid and then elongated in ER, which is facilitated by the fatty acid elongation (FAE) complex (Ariizumi and Toriyama \u003cspan citationid=\"CR1\" class=\"CitationRef\"\u003e2011\u003c/span\u003e; Shi et al. \u003cspan citationid=\"CR36\" class=\"CitationRef\"\u003e2015\u003c/span\u003e). The FAE complex is made up of four distinct enzymes: β-ketoacyl-CoA synthase (KCS) for condensation, β-ketoacyl-CoA reductase (KCR) for reduction, 3-hydroxyacyl-CoA dehydratase (HCD) for dehydration, and trans-2,3-enoyl-CoA reductase (ECR) for secondary reduction. Together, they extend the carbon chain length of the substrate by incorporating two additional carbon atoms in each catalytic cycle (Lee and Suh \u003cspan citationid=\"CR27\" class=\"CitationRef\"\u003e2013\u003c/span\u003e). Among the FAE enzymes, the KCS family exhibit strict substrate specificity, determining the chain lengths of the substrate (Blacklock and Jaworski \u003cspan citationid=\"CR2\" class=\"CitationRef\"\u003e2006\u003c/span\u003e). KCS enzymes are also highly conserved across plants, with varying numbers of KCS genes from \u003cem\u003eArabidopsis thaliana\u003c/em\u003e, \u003cem\u003eZea mays\u003c/em\u003e, \u003cem\u003eOryza sativa\u003c/em\u003e, \u003cem\u003eArachis hypogaea\u003c/em\u003e and \u003cem\u003eGossypium hirsutum\u003c/em\u003e (Joub\u0026egrave;s et al. \u003cspan citationid=\"CR22\" class=\"CitationRef\"\u003e2008\u003c/span\u003e; Yang et al. \u003cspan citationid=\"CR47\" class=\"CitationRef\"\u003e2023\u003c/span\u003e; Campbell et al. \u003cspan citationid=\"CR4\" class=\"CitationRef\"\u003e2019\u003c/span\u003e; Huai et al. \u003cspan citationid=\"CR16\" class=\"CitationRef\"\u003e2020\u003c/span\u003e; Xiao et al. \u003cspan citationid=\"CR42\" class=\"CitationRef\"\u003e2016\u003c/span\u003e). Notably, KCS6, characterized by its broad tissue distribution and potent catalytic activity, not only catalyzes the extension of C24 to C28 VLCFAs on its own but also synergizes with a CER2-like protein to promote the elongation of C30 to C34 VLCFAs (Haslam and Kunst \u003cspan citationid=\"CR13\" class=\"CitationRef\"\u003e2013\u003c/span\u003e; Huang et al. \u003cspan citationid=\"CR17\" class=\"CitationRef\"\u003e2022\u003c/span\u003e; Haslam et al. \u003cspan citationid=\"CR14\" class=\"CitationRef\"\u003e2015\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eAbundant studies have explored the roles of \u003cem\u003eKCS\u003c/em\u003e genes in \u003cem\u003eArabidopsis thaliana\u003c/em\u003e, where \u003cem\u003eKCS\u003c/em\u003e mutations generally lead to the reduction in wax production and various deficiencies in vegetative development, such as \u003cem\u003eKCS6\u003c/em\u003e, \u003cem\u003eKCS1\u003c/em\u003e, \u003cem\u003eKCS2/DAISY\u003c/em\u003e, KCS20, \u003cem\u003eKCS9\u003c/em\u003e, \u003cem\u003eKCS16\u003c/em\u003e, \u003cem\u003eKCS4\u003c/em\u003e, \u003cem\u003eKCS5\u003c/em\u003e (Millar et al. \u003cspan citationid=\"CR31\" class=\"CitationRef\"\u003e1999\u003c/span\u003e; Fiebig et al. \u003cspan citationid=\"CR9\" class=\"CitationRef\"\u003e2000\u003c/span\u003e; Todd et al. \u003cspan citationid=\"CR39\" class=\"CitationRef\"\u003e1999\u003c/span\u003e; Lee et al. \u003cspan citationid=\"CR26\" class=\"CitationRef\"\u003e2009\u003c/span\u003e; Franke et al. \u003cspan citationid=\"CR10\" class=\"CitationRef\"\u003e2009\u003c/span\u003e; Lee et al. \u003cspan citationid=\"CR26\" class=\"CitationRef\"\u003e2009\u003c/span\u003e; Kim et al. \u003cspan citationid=\"CR24\" class=\"CitationRef\"\u003e2013\u003c/span\u003e; Hegebarth et al. \u003cspan citationid=\"CR15\" class=\"CitationRef\"\u003e2017\u003c/span\u003e; Kim et al. \u003cspan citationid=\"CR25\" class=\"CitationRef\"\u003e2021\u003c/span\u003e; Huang et al. \u003cspan citationid=\"CR17\" class=\"CitationRef\"\u003e2022\u003c/span\u003e). In contrast, functional characterization of KCS enzymes in rice is limited. Mutations or overexpression of rice \u003cem\u003eKCSs\u003c/em\u003e can result in diverse phenotypes by affecting wax deposition. For instance, \u003cem\u003ewsl1\u003c/em\u003e displays enhanced sensitivity to drought and low fertility (Yu et al. \u003cspan citationid=\"CR48\" class=\"CitationRef\"\u003e2008\u003c/span\u003e), while \u003cem\u003esd38\u003c/em\u003e mutation results in a semi-dwarf phenotype (Zhang et al. \u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e2022\u003c/span\u003e); \u003cem\u003ewsl4\u003c/em\u003e exhibits reduced wax accumulation on leaves and its allelic mutant \u003cem\u003ehms1\u003c/em\u003e is characterized by decreased seed setting under low humidity condition (Gan et al. \u003cspan citationid=\"CR11\" class=\"CitationRef\"\u003e2017\u003c/span\u003e; Chen et al. \u003cspan citationid=\"CR8\" class=\"CitationRef\"\u003e2020\u003c/span\u003e). Additionally, \u003cem\u003eoni1\u003c/em\u003e and \u003cem\u003eoni2\u003c/em\u003e are seedling-lethal (Tsuda et al. \u003cspan citationid=\"CR40\" class=\"CitationRef\"\u003e2013\u003c/span\u003e), and overexpression of \u003cem\u003eOsCUT1\u003c/em\u003e is closely associated with enhanced drought resistance (Gao et al. \u003cspan citationid=\"CR12\" class=\"CitationRef\"\u003e2022\u003c/span\u003e). In conclusion, while KCS homologs share conserved biochemical function in wax deposition, their biological functions exhibit significant differentiation. However, the specific roles of KCS in contributing to male fertility are still unclear.\u003c/p\u003e \u003cp\u003eIn our research, we have conducted a functional characterization of DDP1 (Defective in Dehiscence and Pollen1), a novel member of the KCS family in rice. The \u003cem\u003eddp1\u003c/em\u003e mutant showed a partial male sterile phenotype attributed to defective anther dehiscence and pollen fertility. This phenotype was notably distinct from those observed in \u003cem\u003eArabidopsis thaliana\u003c/em\u003e and rice mutants associated with lipid metabolism, underscoring the unique role of DDP1 in male fertility.\u003c/p\u003e"},{"header":"Materials and methods","content":"\u003cdiv id=\"Sec3\" class=\"Section2\"\u003e \u003ch2\u003ePlant materials and growth conditions\u003c/h2\u003e \u003cp\u003eWe generated knockout (KO) mutants \u003cem\u003eddp1-1\u003c/em\u003e and \u003cem\u003eddp1-2\u003c/em\u003e utilizing CRISPR/Cas9 technology. The target sequence within the \u003cem\u003eDDP1\u003c/em\u003ecoding sequence was selected with the aid of designer software specifically tailored for CRISPR target prediction (Xie et al. \u003cspan citationid=\"CR43\" class=\"CitationRef\"\u003e2017\u003c/span\u003e) (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003ea). Subsequently, the target sequence was synthesized and integrated into a CRISPR/Cas9 expression vector. Following its construction, the plasmid was transferred into the \u003cem\u003ejaponica\u003c/em\u003e rice cultivar Zhonghua 11. The plant materials analyzed in this research were cultivated in an experimental field at Nanning (Guangxi, China) under natural conditions and managed with standard agricultural practices.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec4\" class=\"Section2\"\u003e \u003ch2\u003eCharacterization of mutant phenotypes\u003c/h2\u003e \u003cp\u003eA Nikon digital camera was utilized to photograph the phenotypes of whole plants and panicles after seed maturation. An sz61TR trinocular microscope (Olympus) was used to photograph the phenotypes of spikelets and anthers. Pollen fertility was examined by staining mature pollen grains using 1% I\u003csub\u003e2\u003c/sub\u003e-KI and photographed using an Axioscope 5 microscope (ZEISS). Yield traits were measured using the methods previously outlined by Qin et al (\u003cspan citationid=\"CR32\" class=\"CitationRef\"\u003e2021\u003c/span\u003e). Anther samples collected at various intervals during the flowering period were immersed in a 2.5% glutaraldehyde solution (v/v) to prepare them for subsequent examination via scanning electron microscopy (SEM) and transmission electron microscopy (TEM) following the previously described methods (Qin et al. \u003cspan citationid=\"CR34\" class=\"CitationRef\"\u003e2013\u003c/span\u003e).\u003c/p\u003e \u003cp\u003e \u003cb\u003eIn vitro\u003c/b\u003e \u003cb\u003eand\u003c/b\u003e \u003cb\u003ein vivo\u003c/b\u003e \u003cb\u003epollen germination assays\u003c/b\u003e\u003c/p\u003e \u003cp\u003eIn conducting the \u003cem\u003ein vitro\u003c/em\u003e pollen germination assay, we harvested pollen grains at flowering stage and place them on a prepared germination medium containing 20% sucrose, 10% polyethylene glycol 4000, 40 mgL\u003csup\u003e\u0026minus;\u0026thinsp;1\u003c/sup\u003e H\u003csub\u003e3\u003c/sub\u003eBO\u003csub\u003e3\u003c/sub\u003e, 3 mmolL\u003csup\u003e\u0026minus;\u0026thinsp;1\u003c/sup\u003e Ca(NO\u003csub\u003e3\u003c/sub\u003e)\u003csub\u003e2\u003c/sub\u003e, and 10 mgL\u003csup\u003e\u0026minus;\u0026thinsp;1\u003c/sup\u003e vitamin B1(VBl) on slide glass. Following a 2 hours culture period at 35℃, pollen germination was observed using an Axioscope 5 microscope (ZEISS). To determine the germination rate, we measured the germination of 250 pollen grains from both \u003cem\u003eddp1\u003c/em\u003e and WT anthers.\u003c/p\u003e \u003cp\u003eFor the \u003cem\u003ein vivo\u003c/em\u003e assessment of pollen germination, pistils were harvested 3 hours after pollination and subsequently immersed in Carnoy solution (3:1 ethanol-to-glacial acetic acid mixture) for overnight. Following fixation, the pistils underwent three sequential washes using double-distilled water (ddH\u003csub\u003e2\u003c/sub\u003eO) and were then softened in 4M sodium hydroxide (NaOH) for 24 hours. After another three washes with ddH\u003csub\u003e2\u003c/sub\u003eO, the pistils were immersed in a 0.05% aniline blue solution for 12h in the dark. After staining, the pistils were carefully mounted onto glass slides for microscopic examination using an Axioscope 5 microscope (ZEISS).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec5\" class=\"Section2\"\u003e \u003ch2\u003eExamination of anther dehiscence\u003c/h2\u003e \u003cp\u003eThe assessment of anther dehiscence was conducted in accordance with the previously published method (Zhang et al. \u003cspan citationid=\"CR55\" class=\"CitationRef\"\u003e2004\u003c/span\u003e). The anthers were collected and observed with a stereoscopic microscope to assess dehiscence. The degree of anther dehiscence was categorized into five levels as follows:\u003c/p\u003e \u003cp\u003e●Level 5: Anthers were completely dehisced, releasing all pollen grains.\u003c/p\u003e \u003cp\u003e●Level 4: Anthers had large holes at the top and bottom, nearly releasing all pollen grains.\u003c/p\u003e \u003cp\u003e●Level 3: Anthers with small holes or a single chamber dehiscence released a portion of pollen grains.\u003c/p\u003e \u003cp\u003e●Level 2: Anthers with a small hole at the bottom released a minimal amount of pollen grains.\u003c/p\u003e \u003cp\u003e●Level 1: Anthers that were completely indehiscent did not release any pollen grain.\u003c/p\u003e \u003cp\u003eThe anther dehiscence phenotype was quantified using the dehiscence index, calculated as follows:\u003c/p\u003e \u003cp\u003e \u003cspan class=\"InlineEquation\"\u003e \u003c/span\u003e \u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec6\" class=\"Section2\"\u003e \u003ch2\u003eHistochemical analysis\u003c/h2\u003e \u003cp\u003eFor nuclear staining, the spikelets of \u003cem\u003eddp1-1\u003c/em\u003e and WT were collected during stage 9 to 12 and then immersed in Carnoy solution for overnight. After being washed three times with 70% ethanol, anthers were dissected from the spikelets and carefully mounted onto a glass slide containing a small drop of 1 mgL\u003csup\u003e\u0026minus;\u0026thinsp;1\u003c/sup\u003e DAPI solution. A cover slip was placed over the anthers to prevent evaporation and ensure even staining. After a 10 minutes incubation period, the stained anthers were observed under an Axioscope 5 microscope (ZEISS) to visualize nuclear morphology.\u003c/p\u003e \u003cp\u003eFor lipidic staining, the spikelets of \u003cem\u003eddp1-1\u003c/em\u003e and WT at stage 12 were collected and then fixed in the 70% solution of formalin-acetic-alcohol (FAA) for 24 hour. Following fixation, the spikelets underwent dehydration using a sequential ethanol gradient, ranging from 100\u0026ndash;30%. The dehydrated spikelets were then stained by Sudan Red 7B solution. The paraffin sections of anthers were prepared and processed by dewaxing, followed by hydration, and subsequently stained using Sudan Red 7B solution. After staining, the sections were washed three times using 1% sodium dodecyl sulfate (SDS) followed by double distilled H\u003csub\u003e2\u003c/sub\u003eO (ddH\u003csub\u003e2\u003c/sub\u003eO) to eliminate any surplus stain. The anthers, dissected from the spikelets, as well as paraffin sections and microspores, dissected from the anthers, were carefully mounted onto slides using a 50% (v/v) glycerol solution to prevent dehydration and distortion, and then observed under an Axioscope 5 microscope (ZEISS) for detailed examination.\u003c/p\u003e \u003cp\u003eFor the preparation of semi-thin sections, fresh panicles were initially fixed in Carnoy solution, followed by dehydration through an ascending series of ethanol concentrations. Following dehydration, the panicles were encased in EMbed812 resin (Hereaus Kulzer) and left to polymerize, ensuring a stable matrix for sectioning. The transverse sections of the embedded samples were cut to a thickness of 3\u0026micro;m using a Leica slicer (LEICA EMUC7FC7) and were stained in 0.1% (w/v) toluidine blue. The transverse sections were examined and captured with an Axioscope 5 microscope (ZEISS).\u003c/p\u003e \u003cp\u003eFor the observation of callose walls, paraffin sections underwent dehydration before being stained with a 0.1% (w/v) solution of aniline blue. Subsequently, they were mounted on slides using a 50% (v/v) glycerol medium and captured with an Axioscope 5 microscope (ZEISS).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec7\" class=\"Section2\"\u003e \u003ch2\u003eWax components analysis\u003c/h2\u003e \u003cp\u003eMature anthers from \u003cem\u003eddp1-1\u003c/em\u003e and WT at stage 12 were collected with five biological replicates. Following vacuum drying, the dried anthers underwent rapid chloroform extraction to isolate wax components. Subsequently, the isolated components underwent a thorough analytical evaluation using gas chromatography-mass spectrometry (GC-MS), which was conducted at the SJTU-Metabolon Joint Metabolomics Lab in China following the previously described methods (Xu et al., \u003cspan citationid=\"CR44\" class=\"CitationRef\"\u003e2017\u003c/span\u003e).\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec8\" class=\"Section2\"\u003e \u003ch2\u003eProtein sequence analysis\u003c/h2\u003e \u003cp\u003eThe full-length protein sequences of DDP1 homologs from various plant species were retrieved through a BLASTP search conducted on the \u003cspan type=\"Underline\" class=\"Underline\" name=\"Emphasis\"\u003eNCBI database\u003c/span\u003e. The full-length protein sequences of DDP1 and its homologs across various plant species were aligned using MUSCLE version 3.6, a widely recognized software for multiple sequence alignment available at the EBI website. Following the alignment, the sequences were utilized to construct a phylogenetic tree, which was generated using the MEGA X software, a widely recognized tool for phylogenetic analysis. The neighbor-joining method was applied with default settings to infer the evolutionary relationships among the sequences. To ensure the reliability of the tree topology, 1000 bootstrap replications were performed, providing a statistical measure of the confidence in the branching order. To predict protein domains, the full-length protein sequences of DDP1 and ddp1-1/2 were analyzed using the \u003cspan type=\"Underline\" class=\"Underline\" name=\"Emphasis\"\u003eSMART tool\u003c/span\u003e and the \u003cspan type=\"Underline\" class=\"Underline\" name=\"Emphasis\"\u003ePSIPRED server\u003c/span\u003e. These resources are well-established for identifying protein domains and predicting secondary structures, respectively. For three-dimensional structure prediction, the same full-length protein sequences were deposited into the SWISS-MODEL platform, an online resource for protein modeling accessible at \u003cspan type=\"Underline\" class=\"Underline\" name=\"Emphasis\"\u003eSWISS-MODEL\u003c/span\u003e.\u003c/p\u003e \u003cp\u003e \u003cb\u003eQuantitative real-time PCR and RNA\u003c/b\u003e \u003cb\u003ein situ\u003c/b\u003e \u003cb\u003ehybridization\u003c/b\u003e\u003c/p\u003e \u003cp\u003eTo determine \u003cem\u003eDDP1\u003c/em\u003e expression profiles, total RNA was extracted from multiple tissues of WT plant, such as roots, stems, leaves, and panicles at distinct stages as well as from panicles at different stages of \u003cem\u003eddp1\u003c/em\u003e plant. The extraction was performed using a TRIzol kit (Invitrogen, USA). Both Reverse Transcription Polymerase Chain Reaction (RT-PCR) and Reverse Transcription Quantitative Polymerase Chain Reaction (RT-qPCR) were performed following established methods (Ma et al. \u003cspan citationid=\"CR30\" class=\"CitationRef\"\u003e2021\u003c/span\u003e). \u003cem\u003eOsActin\u003c/em\u003e was employed as the internal reference gene. Eample was assayed in triplicate to ensure biological reproducibility. The gene primers used for examination in our research were presented in Table \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003e.\u003c/p\u003e \u003cp\u003eRNA \u003cem\u003ein situ\u003c/em\u003e hybridization was conducted following the established protocols detailed in previous studies (Xue et al. \u003cspan citationid=\"CR45\" class=\"CitationRef\"\u003e2018\u003c/span\u003e). The \u003cem\u003eDDP1\u003c/em\u003e cDNA fragment was used as a template for probe labeling to generate the sense and antisense probes, which were amplified by specific primers (Table \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003e). The Axioscope 5 microscope (ZEISS) was used to capture the image of the assay result.\u003c/p\u003e \u003c/div\u003e \u003cdiv id=\"Sec9\" class=\"Section2\"\u003e \u003ch2\u003eSubcellular localization\u003c/h2\u003e \u003cp\u003eThe complete cDNA sequences of DDP1 and ddp1-1 were replicated and subsequently inserted into the pCAMBIA2300 vector to produce the constructs 35S-GFP-DDP1 and 35S-GFP-ddp1-1. The ER marker was generated by fusing HDEL ER retention signal with mCherry (Caroli et al., \u003cspan citationid=\"CR5\" class=\"CitationRef\"\u003e2011\u003c/span\u003e). The construct 35S-GFP-DDP1 and 35S-GFP-ddp1-1 was transiently co-introduced with the ER marker mCherry-HDEL into rice protoplasts, respectively. The transformation was performed using the polyethylene glycol (PEG)-mediated method, a widely used technique for introducing DNA into plant cells. A GFP reporter, serving as a control, was utilized to verify the success of the transformation process. The fluorescence signal, indicative of the localization of the GFP-tagged proteins and the ER marker, was detected and recorded through a confocal laser scanning microscope (Leica TCS SP8MP).\u003c/p\u003e \u003c/div\u003e"},{"header":"Results","content":"\u003cp\u003e \u003cb\u003eddp1\u003c/b\u003e \u003cb\u003emutants exhibit partial pollen abortion\u003c/b\u003e\u003c/p\u003e \u003cp\u003eThe rice genome contains 22 \u003cem\u003eKCS\u003c/em\u003e genes (Yang et al. \u003cspan citationid=\"CR47\" class=\"CitationRef\"\u003e2023\u003c/span\u003e). To investigate the functions of these KCSs, we employed CRISPR/Cas9 technology to generate a series of knockout (KO) mutants targeting these genes (Table \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003e). Among all developed mutants, the knockout mutants of \u003cem\u003eLOC_Os02g49920\u003c/em\u003e exhibited a partial male sterility attributed to defective anther dehiscence and pollen fertility. Thus, the mutant of \u003cem\u003eLOC_Os02g49920\u003c/em\u003e was designated as \u003cem\u003eddp1\u003c/em\u003e (\u003cem\u003edefective in dehiscence and pollen1\u003c/em\u003e). two alleles \u003cem\u003eddp1\u003c/em\u003e namely \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e and \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e2\u003c/em\u003e were identified in T\u003csub\u003e1\u003c/sub\u003e progeny. \u003cem\u003eddp1-1\u003c/em\u003e and \u003cem\u003eddp1-2\u003c/em\u003e carried 4-bp and 2-bp deletion in the sole exon of \u003cem\u003eLOC_Os02g49920\u003c/em\u003e, respectively (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eb). These deletions caused reading-frame shifts, generating premature and delayed stop codon, respectively.\u003c/p\u003e \u003cp\u003eCompared to WT, \u003cem\u003eddp1-1/2\u003c/em\u003e mutants exhibited no significant differences in whole-plant morphology and the structure of flower organs such as spikelets and anthers (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003ec-f). However, at the mature stage, the seed-setting rates of \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e (41.533\u0026thinsp;\u0026plusmn;\u0026thinsp;1.050%) and \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e2\u003c/em\u003e (32.100\u0026thinsp;\u0026plusmn;\u0026thinsp;1.400%) were significantly lower than that of WT (95.000\u0026thinsp;\u0026plusmn;\u0026thinsp;0.816%) (Table\u0026nbsp;\u003cspan refid=\"Tab1\" class=\"InternalRef\"\u003e1\u003c/span\u003e)(Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eg, k). To determine if the lower seed-setting rate in \u003cem\u003eddp1-1\u003c/em\u003e/\u003cem\u003e2\u003c/em\u003e mutants resulted from a male or female gametophyte impairment, we evaluated the pollen and female fertility. Notably, the fertile pollen rate was significantly lower in \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e (54.67% \u0026plusmn; 3.68%) and \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e2\u003c/em\u003e (49.17% \u0026plusmn; 1.65%) compared to WT, which exhibited a fertile pollen rate of 95.13% \u0026plusmn; 0.84% (Fig.\u0026nbsp;\u003cspan refid=\"Fig1\" class=\"InternalRef\"\u003e1\u003c/span\u003eh-j, l). When \u003cem\u003eddp1\u003c/em\u003e mutants were self-pollinated with its pollen, their seed setting rate was only 24.45% \u0026plusmn; 2.53%. However, after pollination with WT pollen, the seed setting rate of \u003cem\u003eddp1\u003c/em\u003e mutants reached 58.60% \u0026plusmn; 5.88% (Fig. \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003e). The findings suggest that the reduced seed-setting rate observed in \u003cem\u003eddp1\u003c/em\u003e mutants is due to abnormalities in pollen development, rather than any deficiency in the female gametophyte.\u003c/p\u003e \u003cp\u003e \u003cdiv class=\"gridtable\"\u003e\u003ctable float=\"Yes\" id=\"Tab1\" border=\"1\"\u003e \u003ccaption language=\"En\"\u003e \u003cdiv class=\"CaptionNumber\"\u003eTable 1\u003c/div\u003e \u003cdiv class=\"CaptionContent\"\u003e \u003cp\u003eThe agronomic traits of WT and \u003cem\u003eddp1\u003c/em\u003e mutant.\u003c/p\u003e \u003c/div\u003e \u003c/caption\u003e \u003ccolgroup cols=\"4\"\u003e \u003cdiv align=\"left\" class=\"colspec\" colname=\"c1\" colnum=\"1\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\"\u0026plusmn;\" class=\"colspec\" colname=\"c2\" colnum=\"2\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\"\u0026plusmn;\" class=\"colspec\" colname=\"c3\" colnum=\"3\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\"\u0026plusmn;\" class=\"colspec\" colname=\"c4\" colnum=\"4\"\u003e\u003c/div\u003e \u003cthead\u003e \u003ctr\u003e \u003cth align=\"left\" colname=\"c1\"\u003e \u003cp\u003eAgronomic traits\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c2\"\u003e \u003cp\u003eWT\u003c/p\u003e \u003cp\u003eMean\u0026thinsp;\u0026plusmn;\u0026thinsp;\u003cem\u003eSD\u003c/em\u003e\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c3\"\u003e \u003cp\u003e\u003cem\u003eddp1-1\u003c/em\u003e\u003c/p\u003e \u003cp\u003eMean\u0026thinsp;\u0026plusmn;\u0026thinsp;\u003cem\u003eSD\u003c/em\u003e\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c4\"\u003e \u003cp\u003e\u003cem\u003eddp1-2\u003c/em\u003e\u003c/p\u003e \u003cp\u003eMean\u0026thinsp;\u0026plusmn;\u0026thinsp;\u003cem\u003eSD\u003c/em\u003e\u003c/p\u003e \u003c/th\u003e \u003c/tr\u003e \u003c/thead\u003e \u003ctbody\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003ePlant height (cm)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e86.333\u0026thinsp;\u0026plusmn;\u0026thinsp;2.055\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e83.667\u0026thinsp;\u0026plusmn;\u0026thinsp;1.247\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e88.000\u0026thinsp;\u0026plusmn;\u0026thinsp;0.816\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003ePanicle length (cm)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e21.500\u0026thinsp;\u0026plusmn;\u0026thinsp;0.408\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e23.533\u0026thinsp;\u0026plusmn;\u0026thinsp;0.500\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e21.400\u0026thinsp;\u0026plusmn;\u0026thinsp;0.638\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e1000-grain weight (g)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e26.647\u0026thinsp;\u0026plusmn;\u0026thinsp;0.509\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e27.406\u0026thinsp;\u0026plusmn;\u0026thinsp;0.561\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e26.810\u0026thinsp;\u0026plusmn;\u0026thinsp;0.752\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eGrain length (cm)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e0.811\u0026thinsp;\u0026plusmn;\u0026thinsp;0.009\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e0.797\u0026thinsp;\u0026plusmn;\u0026thinsp;0.005\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e0.811\u0026thinsp;\u0026plusmn;\u0026thinsp;0.009\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eGrain width (cm)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e0.351\u0026thinsp;\u0026plusmn;\u0026thinsp;0.002\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e0.354\u0026thinsp;\u0026plusmn;\u0026thinsp;0.003\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e0.352\u0026thinsp;\u0026plusmn;\u0026thinsp;0.002\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eGrain thickness (mm)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e2.32\u0026thinsp;\u0026plusmn;\u0026thinsp;0.037\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e2.303\u0026thinsp;\u0026plusmn;\u0026thinsp;0.054\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e2.317\u0026thinsp;\u0026plusmn;\u0026thinsp;0.049\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eSeed-setting Rate (%)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e95.000\u0026thinsp;\u0026plusmn;\u0026thinsp;0.816\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e41.533\u0026thinsp;\u0026plusmn;\u0026thinsp;1.050**\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e32.100\u0026thinsp;\u0026plusmn;\u0026thinsp;1.400*\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eNumber of tillers\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e10.333\u0026thinsp;\u0026plusmn;\u0026thinsp;1.247\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e9.667\u0026thinsp;\u0026plusmn;\u0026thinsp;1.247\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e9.667\u0026thinsp;\u0026plusmn;\u0026thinsp;0923\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eNumber of primary\u003c/p\u003e \u003cp\u003ebranches\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e10.000\u0026thinsp;\u0026plusmn;\u0026thinsp;0.816\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e10.333\u0026thinsp;\u0026plusmn;\u0026thinsp;1.247\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e10.000\u0026thinsp;\u0026plusmn;\u0026thinsp;1.633\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eNumber of secondary\u003c/p\u003e \u003cp\u003ebranches\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e27.667\u0026thinsp;\u0026plusmn;\u0026thinsp;1.700\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e23.000\u0026thinsp;\u0026plusmn;\u0026thinsp;2.60*\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e17.333\u0026thinsp;\u0026plusmn;\u0026thinsp;1.700*\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eYield per plant (g)\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c2\"\u003e \u003cp\u003e16.000\u0026thinsp;\u0026plusmn;\u0026thinsp;1.633\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c3\"\u003e \u003cp\u003e6.233\u0026thinsp;\u0026plusmn;\u0026thinsp;1.481**\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\"\u0026plusmn;\" colname=\"c4\"\u003e \u003cp\u003e4.433\u0026thinsp;\u0026plusmn;\u0026thinsp;0.419**\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003c/tbody\u003e \u003c/colgroup\u003e \u003ctfoot\u003e \u003ctr\u003e\u003ctd colspan=\"4\"\u003e*, ** significant at 5% and 1% levels of probability, respectively.\u003c/td\u003e\u003c/tr\u003e \u003c/tfoot\u003e \u003c/table\u003e\u003c/div\u003e \u003c/p\u003e \u003cp\u003eIn addition to partial pollen abortion, \u003cem\u003eddp1-1/2\u003c/em\u003e mutants also exhibited significant differences in certain yield-related traits compared to WT. For instance, the number of secondary branches and yield per plant were significantly lower in \u003cem\u003eddp1-1\u003c/em\u003e mutant (23.00\u0026thinsp;\u0026plusmn;\u0026thinsp;2.16% and 6.23\u0026thinsp;\u0026plusmn;\u0026thinsp;1.48%) compared to WT (27.67\u0026thinsp;\u0026plusmn;\u0026thinsp;1.70% and 16.00\u0026thinsp;\u0026plusmn;\u0026thinsp;1.62%) (Table\u0026nbsp;\u003cspan refid=\"Tab1\" class=\"InternalRef\"\u003e1\u003c/span\u003e). The \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e2\u003c/em\u003e mutant showed similar trends to those observed in \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e (Table\u0026nbsp;\u003cspan refid=\"Tab1\" class=\"InternalRef\"\u003e1\u003c/span\u003e). Nevertheless, the comparison revealed no notable differences in plant height, number of tillers and primary branches, panicle length, 1000-grain weight, and grain dimensions (length, width, thickness) between \u003cem\u003eddp1-1/2\u003c/em\u003e and WT (Table\u0026nbsp;\u003cspan refid=\"Tab1\" class=\"InternalRef\"\u003e1\u003c/span\u003e).\u003c/p\u003e \u003cp\u003eTo confirm whether \u003cem\u003eLOC_Os02g49920\u003c/em\u003e was the target gene responsible for the \u003cem\u003eddp1\u003c/em\u003e mutants phenotype, a complementation test was performed by transforming a construct \u003cem\u003eDPP1\u003c/em\u003e\u003csub\u003e\u003cem\u003epro\u003c/em\u003e\u003c/sub\u003e:\u003cem\u003eDPP1CDS\u003c/em\u003e-\u003cem\u003emCitrine\u003c/em\u003e containing a 2.5-kb \u003cem\u003eDDP1\u003c/em\u003e promoter region, 1.458-kb \u003cem\u003eDDP1\u003c/em\u003e coding region and 0.72-kb mCitrine coding region into Cas9-free \u003cem\u003eddp1-1\u003c/em\u003e mutants (Table \u003cspan refid=\"MOESM1\" class=\"InternalRef\"\u003eS1\u003c/span\u003e). As expected, the complementary transgenic lines exhibited a restoration of seed-setting rates and pollen fertility to WT levels (Fig. \u003cspan refid=\"MOESM2\" class=\"InternalRef\"\u003eS2\u003c/span\u003e), thereby confirming that \u003cem\u003eLOC_Os02g49920\u003c/em\u003e is indeed the target gene whose knockout causes partial male sterility in \u003cem\u003eddp1\u003c/em\u003e mutants.\u003c/p\u003e \u003cp\u003e \u003cb\u003eAnther dehiscence is defective in\u003c/b\u003e \u003cb\u003eddp1\u003c/b\u003e \u003cb\u003emutants\u003c/b\u003e\u003c/p\u003e \u003cp\u003eTo determine whether partial male sterility of \u003cem\u003eddp1-1\u003c/em\u003e/\u003cem\u003e2\u003c/em\u003e mutants was associated with the defects in anther dehiscence, pollen germination, tube growth, and dehydration, we compared these critical reproductive processes in \u003cem\u003eddp1-1\u003c/em\u003e/\u003cem\u003e2\u003c/em\u003e mutants to those in WT. For anther dehiscence analysis, we examined the anther dehiscence phenotype in both \u003cem\u003eddp1-1/2\u003c/em\u003e and WT. WT anthers typically undergo dehiscence, facilitating the dispersal of mature pollen (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003ea, f), while \u003cem\u003eddp1-1/2\u003c/em\u003e mutants exhibited various defects in anther dehiscence and pollen grain release (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003eb-e, g-j). The anther dehiscence phenotype was quantified using the dehiscence index as reported previously (Zhang et al. \u003cspan citationid=\"CR55\" class=\"CitationRef\"\u003e2004\u003c/span\u003e). A higher dehiscence index indicates that anthers have dehisced more completely. Our findings indicated that the anther dehiscence index was significantly lower in \u003cem\u003eddp1-1\u003c/em\u003e (2.89) and \u003cem\u003eddp1-2\u003c/em\u003e (2.73) compared to WT (4.09) (Table\u0026nbsp;\u003cspan refid=\"Tab2\" class=\"InternalRef\"\u003e2\u003c/span\u003e). This impaired anther dehiscence in \u003cem\u003eddp1-1/2\u003c/em\u003e mutants may result in reduced adhesion and germination of fertile pollen grains on the stigmas. To validate this finding, we performed an \u003cem\u003ein vivo\u003c/em\u003e pollen germination experiment to evaluate the pollen germination rates on the stigmas of \u003cem\u003eddp1-1/2\u003c/em\u003e and WT. The assay demonstrated a markedly lower pollen germination rate on the stigmas in \u003cem\u003eddp1-1/2\u003c/em\u003e mutants relative to WT (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003en-r, u). Collectively, these results indicate that defective anther dehiscence in \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1/2\u003c/em\u003e mutants hinders the adhesion and subsequent germination of fertile pollen grains on the stigma, thereby reducing the seed-setting rate.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003e \u003cdiv class=\"gridtable\"\u003e\u003ctable float=\"Yes\" id=\"Tab2\" border=\"1\"\u003e \u003ccaption language=\"En\"\u003e \u003cdiv class=\"CaptionNumber\"\u003eTable 2\u003c/div\u003e \u003cdiv class=\"CaptionContent\"\u003e \u003cp\u003eThe anther dehiscence index of WT and \u003cem\u003eddp1\u003c/em\u003e.\u003c/p\u003e \u003c/div\u003e \u003c/caption\u003e \u003ccolgroup cols=\"8\"\u003e \u003cdiv align=\"left\" class=\"colspec\" colname=\"c1\" colnum=\"1\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c2\" colnum=\"2\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c3\" colnum=\"3\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c4\" colnum=\"4\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c5\" colnum=\"5\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c6\" colnum=\"6\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c7\" colnum=\"7\"\u003e\u003c/div\u003e \u003cdiv align=\"char\" char=\".\" class=\"colspec\" colname=\"c8\" colnum=\"8\"\u003e\u003c/div\u003e \u003cthead\u003e \u003ctr\u003e \u003cth align=\"left\" colname=\"c1\"\u003e\u0026nbsp;\u003c/th\u003e \u003cth align=\"left\" colspan=\"5\" nameend=\"c6\" namest=\"c2\"\u003e \u003cp\u003eLevel of anther dehiscence\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c7\" morerows=\"1\" rowspan=\"2\"\u003e \u003cp\u003eTotal number of anther\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c8\" morerows=\"1\" rowspan=\"2\"\u003e \u003cp\u003eDehiscence index\u003c/p\u003e \u003c/th\u003e \u003c/tr\u003e \u003ctr\u003e \u003cth align=\"left\" colname=\"c1\"\u003e\u0026nbsp;\u003c/th\u003e \u003cth align=\"left\" colname=\"c2\"\u003e \u003cp\u003e5\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c3\"\u003e \u003cp\u003e4\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c4\"\u003e \u003cp\u003e3\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c5\"\u003e \u003cp\u003e2\u003c/p\u003e \u003c/th\u003e \u003cth align=\"left\" colname=\"c6\"\u003e \u003cp\u003e1\u003c/p\u003e \u003c/th\u003e \u003c/tr\u003e \u003c/thead\u003e \u003ctbody\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003eWT\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e8\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c3\"\u003e \u003cp\u003e84\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c4\"\u003e \u003cp\u003e0\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c5\"\u003e \u003cp\u003e0\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c6\"\u003e \u003cp\u003e0\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c7\"\u003e \u003cp\u003e92\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c8\"\u003e \u003cp\u003e4.09\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e\u003cem\u003eddp1-1\u003c/em\u003e\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e10\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c3\"\u003e \u003cp\u003e34\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c4\"\u003e \u003cp\u003e26\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c5\"\u003e \u003cp\u003e18\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c6\"\u003e \u003cp\u003e24\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c7\"\u003e \u003cp\u003e112\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c8\"\u003e \u003cp\u003e2.89**\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003ctr\u003e \u003ctd align=\"left\" colname=\"c1\"\u003e \u003cp\u003e\u003cem\u003eddp1-2\u003c/em\u003e\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c2\"\u003e \u003cp\u003e14\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c3\"\u003e \u003cp\u003e41\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c4\"\u003e \u003cp\u003e36\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c5\"\u003e \u003cp\u003e30\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c6\"\u003e \u003cp\u003e41\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c7\"\u003e \u003cp\u003e162\u003c/p\u003e \u003c/td\u003e \u003ctd align=\"char\" char=\".\" colname=\"c8\"\u003e \u003cp\u003e2.73**\u003c/p\u003e \u003c/td\u003e \u003c/tr\u003e \u003c/tbody\u003e \u003c/colgroup\u003e \u003ctfoot\u003e \u003ctr\u003e\u003ctd colspan=\"8\"\u003e** significant at 1% levels of probability.\u003c/td\u003e\u003c/tr\u003e \u003c/tfoot\u003e \u003c/table\u003e\u003c/div\u003e \u003c/p\u003e \u003cp\u003eFor pollen germination analysis, we compared pollen germination rate between \u003cem\u003eddp1-1/2\u003c/em\u003e and WT using an \u003cem\u003ein vitro\u003c/em\u003e pollen germination assay. Because \u003cem\u003eddp1-1/2\u003c/em\u003e mutants contained sterile pollen grains which could not normally germinate (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003ek-m), the overall \u003cem\u003ein vitro\u003c/em\u003e pollen germination rates were significantly lower in \u003cem\u003eddp1-1\u003c/em\u003e (50.65\u0026thinsp;\u0026plusmn;\u0026thinsp;1.86%) and \u003cem\u003eddp1-2\u003c/em\u003e (42.23\u0026thinsp;\u0026plusmn;\u0026thinsp;2.36%) compared to WT (89.4\u0026thinsp;\u0026plusmn;\u0026thinsp;1.11%) (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003es). However, when only considering the germination rate of fertile pollen grains, the comparison revealed no notable differences between \u003cem\u003eddp1-1/2\u003c/em\u003e and WT (with 82.03\u0026thinsp;\u0026plusmn;\u0026thinsp;0.82% of \u003cem\u003eddp1-1\u003c/em\u003e and 81.37\u0026thinsp;\u0026plusmn;\u0026thinsp;0.45% of \u003cem\u003eddp1-2\u003c/em\u003e versus 84.90\u0026thinsp;\u0026plusmn;\u0026thinsp;1.35% of WT) (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003et). These findings suggest that the germination of fertile pollen in \u003cem\u003eddp1-1/2\u003c/em\u003e mutants remains unaffected.\u003c/p\u003e \u003cp\u003eFor pollen tube growth analysis, we compared pollen tube growth within the pistil of \u003cem\u003eddp1-1/2\u003c/em\u003e and WT using an \u003cem\u003ein vivo\u003c/em\u003e pollen germination assay. In self-pollinated WT pistils, at 5 hours post-pollination, pollen tubes had successfully reached the ovule micropyle (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003en). However, self-pollinated pistils of the \u003cem\u003eddp1-1/2\u003c/em\u003e mutants showed a reduced germination rate of pollen grains, yet those that did germinate were able to extend their pollen tubes to the ovule micropyle (Fig.\u0026nbsp;\u003cspan refid=\"Fig2\" class=\"InternalRef\"\u003e2\u003c/span\u003eo, q), suggesting normal pollen tube growth within \u003cem\u003eddp1-1/2\u003c/em\u003e pistils.\u003c/p\u003e \u003cp\u003eFor pollen dehydration analysis, we compared the \u003cem\u003ein vitro\u003c/em\u003e dehydration rate of fertile pollen between \u003cem\u003eddp1-1\u003c/em\u003e and WT. However, no significant differences in the dehydration rate of fertile pollen were observed between \u003cem\u003eddp1-1\u003c/em\u003e and WT from 0 second to 30 minutes (Fig. S3). Altogether, these findings suggest that while pollen germination, pollen tube growth and pollen dehydration are not compromised in \u003cem\u003eddp1-1/2\u003c/em\u003e mutants, anther dehiscence is abnormal. Consequently, we conclude that the decrease in seed-setting rate of \u003cem\u003eddp1-1/2\u003c/em\u003e mutants was attributed to the aborted pollen and aberrant anther dehiscence.\u003c/p\u003e \u003cp\u003e \u003cb\u003eCytological comparison of anther development between\u003c/b\u003e \u003cb\u003eddp1\u003c/b\u003e \u003cb\u003eand WT\u003c/b\u003e\u003c/p\u003e \u003cp\u003eTo determine the morphological defect of \u003cem\u003eddp1-1/2\u003c/em\u003e anthers, semi-thin sections of both \u003cem\u003eddp1-1/2\u003c/em\u003e and WT anthers at different development stages were examined using light microscopy. Initial observations revealed that no significant differences were detected between \u003cem\u003eddp1-1/2\u003c/em\u003e and WT anthers from stage 6 to 9 (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003ea-c, h-j, p-r). However, at stage 10, the epidermis and endothecium of \u003cem\u003eddp1-1\u003c/em\u003e/\u003cem\u003e2\u003c/em\u003e anthers appeared to exhibit a greater thickness compared to their counterparts in WT anthers, and microspores of \u003cem\u003eddp1-1/2\u003c/em\u003e exhibited collapse and a defect in vacuolation (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003ek, s). At stage 11, the epidermis and endothecium of \u003cem\u003eddp1-1\u003c/em\u003e/\u003cem\u003e2\u003c/em\u003e anthers continued to show swelling, and tapetum degradation seemed to be delayed. Only a fraction of microspores formed falcate-shaped pollen grains filled with starch granules, while the rest developed into irregularly shaped pollen grains lacking starch accumulation (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003el, t). At stage 12, the WT tapetum had completely degraded, allowing microspores to mature into pollen grains (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003ef). In contrast, in \u003cem\u003eddp1-1/2\u003c/em\u003e anthers, the incompletely degraded tapetum residues were observed, with only some microspores maturing into fertile pollen grains, while others aborted (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003em, u). At stage 14, WT anthers were able to dehisce normally as the connective tissue between anthers cracked (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003eg). However, in \u003cem\u003eddp1-1/2\u003c/em\u003e, only a subset of anthers dehisced, while others remained closed (Fig.\u0026nbsp;\u003cspan refid=\"Fig3\" class=\"InternalRef\"\u003e3\u003c/span\u003en-o, v-w). These findings show that \u003cem\u003eddp1-1/2\u003c/em\u003e mutations lead to developmental defects in anther and pollen from stage 10 to 14.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eTo precisely characterize the differences between \u003cem\u003eddp1-1/2\u003c/em\u003e and WT, SEM was employed to compare the anthers and pollen grains. The anthers of \u003cem\u003eddp1-1/2\u003c/em\u003e and WT were comparable in size (Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003ea, e, i). WT anthers exhibited an outer epidermis covered by spaghetti-like cuticle layers (Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003eb) and an inner epidermis with Ubisch bodies (Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003ec, d). In contrast, the cuticle layers of the outer epidermis and the Ubisch bodies of the inner epidermis in \u003cem\u003eddp1-1/2\u003c/em\u003e anthers seemed to be denser (Fig.\u0026nbsp;\u003cspan refid=\"Fig4\" class=\"InternalRef\"\u003e4\u003c/span\u003ef-h, g-l). In addition, WT pollen grains were spherical and smooth, uniformly coated by a layer of sporopollenin (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003ea, d). \u003cem\u003eddp1-1/2\u003c/em\u003e mutants had two types of pollen grains, namely spherical pollen grains and shrunken pollen grains (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003eb-c, e-h). The spherical pollen grains in \u003cem\u003eddp1-1/2\u003c/em\u003e mutants exhibited a slightly sparse sporopollenin layer (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003ej, l), while the sporopollenin on the shrunken pollen grains in \u003cem\u003eddp1-1/2\u003c/em\u003e mutants appeared to be denser (Fig.\u0026nbsp;\u003cspan refid=\"Fig5\" class=\"InternalRef\"\u003e5\u003c/span\u003ek, m). The increased accumulation of sporopollenin on the surfaces of shrunken \u003cem\u003eddp1-1/2\u003c/em\u003e pollen may be attributed to the shrinkage of the pollen grain surface area. Given the similar phenotypes exhibited by \u003cem\u003eddp1-1\u003c/em\u003e and \u003cem\u003eddp1-2\u003c/em\u003e under identical growth conditions, the following analyses within this study were conducted solely on \u003cem\u003eddp1-1\u003c/em\u003e.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eTo further elucidate the cytological differences between \u003cem\u003eddp1\u003c/em\u003e and WT, TEM was also employed to observe the ultrastructures of anthers and pollen grains. At stage 11, in accordance with our light microscopy results, the anther wall, particularly the tapetum of \u003cem\u003eddp1-1\u003c/em\u003e mutant was thicker compared to that of WT (Fig.\u0026nbsp;\u003cspan refid=\"Fig6\" class=\"InternalRef\"\u003e6\u003c/span\u003ea, e). At stage 13, the WT tapetum fully degraded while the incompletely degraded tapetum residue was still observed in \u003cem\u003eddp1-1\u003c/em\u003e mutant (Fig.\u0026nbsp;\u003cspan refid=\"Fig6\" class=\"InternalRef\"\u003e6\u003c/span\u003ei, m). At stage 11 and 13, the cuticle layer and the Ubisch body in \u003cem\u003eddp1-1\u003c/em\u003e anthers were denser than those of WT (Fig.\u0026nbsp;\u003cspan refid=\"Fig6\" class=\"InternalRef\"\u003e6\u003c/span\u003ef-g, n-o), aligning with SEM observations. Furthermore, the aborted \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e pollen grains exhibited a thicker exine and smaller bacula compared to WT (Fig.\u0026nbsp;\u003cspan refid=\"Fig6\" class=\"InternalRef\"\u003e6\u003c/span\u003eh, p), indicating the alterations in the pollen wall ultrastructure. At stage 10, neither \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e nor WT microspores showed signs of starch accumulation and intine formation (Fig.\u0026nbsp;\u003cspan refid=\"Fig6\" class=\"InternalRef\"\u003e6\u003c/span\u003eq, r). By stage 12, WT microspores had developed an intine and were filled with a substantial amount of starch granules (Fig.\u0026nbsp;\u003cspan refid=\"Fig6\" class=\"InternalRef\"\u003e6\u003c/span\u003es), whereas aborted pollen grains of \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e mutant lacked both features (Fig.\u0026nbsp;\u003cspan refid=\"Fig6\" class=\"InternalRef\"\u003e6\u003c/span\u003et). In summary, \u003cem\u003eddp1-1\u003c/em\u003e mutant exhibited abnormalities in their anther cuticle layer, Ubisch bodies, tapetum degradation, anther dehiscence, pollen wall structure, and starch accumulation.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003e \u003cb\u003eGametogenesis at stage 11 and 12 is defective in\u003c/b\u003e \u003cb\u003eddp1-1\u003c/b\u003e \u003cb\u003eanthers\u003c/b\u003e\u003c/p\u003e \u003cp\u003eTo determine whether gametogenesis was affected in \u003cem\u003eddp1\u003c/em\u003e anthers, we performed the 4\u0026rsquo;,6-diamidino-2-phenylindole (DAPI) staining on microspores from both \u003cem\u003eddp1-1\u003c/em\u003e and WT at different stages. At stage 9, WT microspores typically developed into uninucleate microspores. At stage 11, they underwent the first mitotic division, resulting in binucleate microspores. At stage 12, they underwent the second mitotic division, yielding trinucleate microspores with one vegetative nucleus and two generative nuclei. Accordingly, a portion of \u003cem\u003eddp1-1\u003c/em\u003e microspores successfully developed into uninucleate, binucleate and trinucleate microspores at stage 9, 11 and 12, respectively, similar to WT (Fig.\u0026nbsp;\u003cspan refid=\"Fig7\" class=\"InternalRef\"\u003e7\u003c/span\u003ea). However, other \u003cem\u003eddp1-1\u003c/em\u003e microspores exhibited a brightly stained nucleus at stage 9 and 11 but failed to complete the first and second mitotic divisions to form binucleate and trinucleate microspores at stage 11 and 12 (Fig.\u0026nbsp;\u003cspan refid=\"Fig7\" class=\"InternalRef\"\u003e7\u003c/span\u003ea). The DAPI staining analysis indicates that defective gametogenesis in the aborted \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e microspores begins at stage 11, which is roughly consistent with the semi-thin section observations that anther and pollen abnormalities occur at stage 10.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eDefective gametogenesis was often closely associated with abnormalities in callose biosynthesis and degradation. Callose biosynthesis initiated at stage 7, and its degradation at stage 9 facilitated the release of microspores from the tetrads. In order to investigate whether these processes were affected in \u003cem\u003eddp1-1\u003c/em\u003e anthers, we performed aniline blue staining on anthers from both \u003cem\u003eddp1-1\u003c/em\u003e and WT from stage 7 to 9. However, no obvious differences in the fluorescence signal surrounding microspores were observed between \u003cem\u003eddp1-1\u003c/em\u003e and WT anthers (Fig.\u0026nbsp;\u003cspan refid=\"Fig7\" class=\"InternalRef\"\u003e7\u003c/span\u003eb). This result suggests that the callose formation and degradation steps in \u003cem\u003eddp1-1\u003c/em\u003e anthers from stage 7 to 9 are not impaired, consistent with the semi-thin section observations that anther and microspore development in \u003cem\u003eddp1-1\u003c/em\u003e mutant appeared normal from stage 6 to 9.\u003c/p\u003e \u003cp\u003e \u003cb\u003eAltered wax content and composition of the anther epidermis and pollen wall in the\u003c/b\u003e \u003cb\u003eddp1\u003c/b\u003e \u003cb\u003emutant\u003c/b\u003e\u003c/p\u003e \u003cp\u003e \u003cem\u003eDDP1\u003c/em\u003e encodes a β-ketoacyl-CoA synthase with 485 amino acids residues, catalyzing cuticular wax synthesis. To elucidate the function of DDP1, a phylogenetic analysis was performed using DDP1 and other plant KCS proteins with both known and unknown biochemical and biological functions. Phylogenic analysis revealed that DDP1 shares high sequence similarity with its homologs (Fig. S4a). Domain homology analysis using SMART demonstrated that the DDP1 protein contains three conserved domains: an ACP_syn_III_C domain, a transmembrane region, and a FAE1_CUT1_RppA domain, similar to its counterparts in other plant species (Fig. S4b). The analysis suggests that DDP1 may play a conserved function in cuticular wax synthesis. Given that \u003cem\u003eddp1-1\u003c/em\u003e mutant also showed structural abnormalities in the lipidic anther epidermis and pollen wall, we speculated that the wax content and composition of these structures in the \u003cem\u003eddp1-1\u003c/em\u003e mutant might be altered. To test this speculation, we initially examined the lipidic compounds by staining anthers and pollen from \u003cem\u003eddp1-1\u003c/em\u003e and WT at stage 12 with the lipophilic dye Sudan Red 7B. While the WT anther epidermis and pollen wall showed intense staining (Fig.\u0026nbsp;8a1-a3,), the \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e mutant displayed strong staining in anther epidermis and fertile pollen wall, and weak staining in the wall of aborted pollen grains (Fig.\u0026nbsp;8b1-b3). This suggests a reduction in lipidic compounds within the wall of \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e aborted pollen. Subsequently, we analyzed the phenolic compounds by comparing the fluorescence intensity emitted by phenolic compounds in pollen walls under ultraviolet radiation between \u003cem\u003eddp1-1\u003c/em\u003e and WT. The fertile pollen grains of \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e emitted fluorescence similar in intensity to that of WT, whereas the aborted pollen grains exhibited significantly weaker fluorescence (Fig.\u0026nbsp;8b4), indicating a substantial decrease in phenolic compounds in the wall of \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e aborted pollen. In conclusion, these findings indicate that precursors to sporopollenin, including lipidic and phenolic compounds, are significantly reduced in the walls of \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e aborted pollen.\u003c/p\u003e \u003cp\u003eTo ascertain the chemical profiles of anther epidermis and pollen wall, we quantified wax constituents at stage 12 using gas GC-MS. This result indicated that the total wax content in \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e anthers increased by 34%\u0026plusmn;0.08% compared to WT (Fig.\u0026nbsp;\u003cspan refid=\"Fig8\" class=\"InternalRef\"\u003e8\u003c/span\u003ec), primarily due to significant elevations in free fatty acids (C16:0, C18:2, C18:3, C18:0, C20:0, C22:0, C26:0,C28:0 and C30:0), alkenes (C25:0, C27:0, C33:1, C33:0, C35:0 and C35:1), and alcohols (C26:0 and C28:0), as well as sterols such as campersterol, stigmasterol and β-sitosterol (Fig.\u0026nbsp;\u003cspan refid=\"Fig8\" class=\"InternalRef\"\u003e8\u003c/span\u003ed, e). In contrast, the levels of certain free fatty acid (C24:0), alkenes (C23:0 and C27:1) and inositol were dramatically decreased in \u003cem\u003eddp1-1\u003c/em\u003e mutants, and other wax constituents remained largely unchanged (Fig.\u0026nbsp;\u003cspan refid=\"Fig8\" class=\"InternalRef\"\u003e8\u003c/span\u003ee). The altered wax profile in \u003cem\u003eddp1-1\u003c/em\u003e mutant indicated that DDP1 is essential for maintaining lipid metabolic homeostasis. The alteration in the content and composition of wax in the anther epidermis and pollen wall may underlies the structural abnormalities observed in the \u003cem\u003eddp1\u003c/em\u003e-\u003cem\u003e1\u003c/em\u003e anther epidermis and pollen wall.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cdiv id=\"Sec11\" class=\"Section2\"\u003e \u003ch2\u003eExpression pattern and subcellular location of DDP1\u003c/h2\u003e \u003cp\u003eTo determine \u003cem\u003eDDP1\u003c/em\u003e expression pattern, RT-qPCR was conducted to quantify its expression in various tissues of WT. The result suggested that \u003cem\u003eDDP1\u003c/em\u003e transcription was uniformly detected across all assessed tissues, with peak transcription observed in the leaves (Fig.\u0026nbsp;\u003cspan refid=\"Fig9\" class=\"InternalRef\"\u003e9\u003c/span\u003ea). \u003cem\u003eDDP1\u003c/em\u003e expression was observed throughout the stages of anther development, peaking at stage 8 (Fig.\u0026nbsp;\u003cspan refid=\"Fig9\" class=\"InternalRef\"\u003e9\u003c/span\u003ea). To further analyze the expression of \u003cem\u003eDDP1\u003c/em\u003e in anthers, RNA \u003cem\u003ein situ\u003c/em\u003e hybridization was conducted on sections of WT anthers. The hybridization signal was first observed in tapetum and pollen mother cells (PMCs) at stage 7, then in tapetum and tetrads at stage 8, and in tapetum and microspores from stage 9 to 11 (Fig.\u0026nbsp;\u003cspan refid=\"Fig9\" class=\"InternalRef\"\u003e9\u003c/span\u003eb). In control experiments, the sense probe failed to produce any detectable signal, confirming the specificity of the hybridization. These findings indicate that \u003cem\u003eDDP1\u003c/em\u003e is predominantly expressed in the tapetum, PMCs and microspores, which correlates with the phenotypes of delayed tapetum degradation and impaired microspore development in \u003cem\u003eddp1\u003c/em\u003e mutants.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eTo further elucidate the spatial distribution of DDP1 protein, we utilized confocal microscopy to observe the \u003cem\u003emCitrine\u003c/em\u003e signal in \u003cem\u003eddp1\u003c/em\u003e-complementary transgenic plants expressing \u003cem\u003eDDP1pro:DDP1cDNA-mCitrine\u003c/em\u003e. At stage 10, yellow \u003cem\u003emCitrine\u003c/em\u003e fluorescence was detected in the tapetum and microspores (Fig.\u0026nbsp;\u003cspan refid=\"Fig10\" class=\"InternalRef\"\u003e10\u003c/span\u003ea-c). By stage 11, yellow \u003cem\u003emCitrine\u003c/em\u003e fluorescence was noted in the partially degraded tapetum residues and microspores (Fig.\u0026nbsp;\u003cspan refid=\"Fig10\" class=\"InternalRef\"\u003e10\u003c/span\u003ed-f). At stage 12, with the tapetum fully degraded, \u003cem\u003emCitrine\u003c/em\u003e signal was exclusively detected in pollen grains (Fig.\u0026nbsp;\u003cspan refid=\"Fig10\" class=\"InternalRef\"\u003e10\u003c/span\u003eg-i). These observations indicate that \u003cem\u003eDDP1\u003c/em\u003e expression aligns with DDP1 protein distribution in the tapetum, microspores, and pollen grains.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003cp\u003eProtein domain analysis using SMART revealed that the DDP1 protein featured a transmembrane domain at its N-terminus (Fig. S4b). Predictions of secondary structure and three-dimensional models using PSIPRED and SWISS-MODEL indicated that DDP1 possesses coil, helix, and strand domains (Fig. S5a). Mutations in the first helix domain of the \u003cem\u003eddp1-1/2\u003c/em\u003e mutants led to noticeable alterations in the protein's three-dimensional structure (Fig. S5b, c).\u003c/p\u003e \u003cp\u003eTo confirm the localization of DDP1 and ddp1-1 in rice protoplasts, we produced DDP1-GFP and ddp1-1-GFP fusion constructs and introduced them into rice protoplasts alongside the ER marker mCherry-HDEL. DDP1-GFP fluorescence was found to almost completely overlap with the mCherry-HDEL fluorescence (Fig.\u0026nbsp;\u003cspan refid=\"Fig9\" class=\"InternalRef\"\u003e9\u003c/span\u003ec), suggesting that DDP1 is specifically localized to the ER, as was expected. In contrast, the ddp1-1-GFP fluorescence signal only partially co-localized with the ER marker, with a significant portion of the green fluorescence observed in the cytoplasm (Fig.\u0026nbsp;\u003cspan refid=\"Fig9\" class=\"InternalRef\"\u003e9\u003c/span\u003ec).\u003c/p\u003e \u003cp\u003e \u003cb\u003eThe expression levels of known genes complicated in lipid metabolism, anther and pollen development, and anther dehiscence are significantly changed in\u003c/b\u003e \u003cb\u003eddp1\u003c/b\u003e \u003cb\u003eanthers\u003c/b\u003e\u003c/p\u003e \u003cp\u003eObservations of delayed tapetum degradation, defective anther and pollen development, impaired lipid metabolism, and abnormal anther dehiscence in the \u003cem\u003eddp1-1\u003c/em\u003e mutant have led us to hypothesize that \u003cem\u003eDDP1\u003c/em\u003e mutations may disrupt the expression of genes associated with these processes. To test this speculation, we performed a comparative analysis to evaluate the expression profiles of known genes associated with these processes between \u003cem\u003eddp1-1\u003c/em\u003e and WT from stage 7 to 10. Compared to WT, the expression levels of six lipid metabolism genes (\u003cem\u003eOsABCG26\u003c/em\u003e, \u003cem\u003eOsPKS2\u003c/em\u003e, \u003cem\u003eOsNP1\u003c/em\u003e, \u003cem\u003eRMS2\u003c/em\u003e, \u003cem\u003eCYP703A3\u003c/em\u003e and \u003cem\u003eOsCER2\u003c/em\u003e), five genes complicated in the anther, pollen and tapetum development (\u003cem\u003eOsCP1\u003c/em\u003e, \u003cem\u003eGAMYB\u003c/em\u003e, \u003cem\u003eOsSTRL2\u003c/em\u003e, \u003cem\u003eSTS1\u003c/em\u003e and \u003cem\u003eDPW3\u003c/em\u003e), and two genes involved in anther dehiscence (\u003cem\u003eDAO\u003c/em\u003e and \u003cem\u003eOsH1\u003c/em\u003e) were significantly decreased in the \u003cem\u003eddp1-1\u003c/em\u003e mutant (Fig.\u0026nbsp;\u003cspan refid=\"Fig11\" class=\"InternalRef\"\u003e11\u003c/span\u003e). In contrast, the \u003cem\u003eddp1-1\u003c/em\u003e mutant displayed a pronounced upregulation in the expression levels of two lipid metabolism genes (OsABCG3 and OsCER1), along with one tapetum development gene (OsAP25), specifically at stages 8 and 9 (Fig.\u0026nbsp;\u003cspan refid=\"Fig11\" class=\"InternalRef\"\u003e11\u003c/span\u003e). In addition, considering the close association of anther dehiscence with auxin and jasmonic acid (JA) signaling, we also conducted a comparative analysis of gene expression levels related to these signaling pathways between \u003cem\u003eddp1-1\u003c/em\u003e and WT. Six genes (\u003cem\u003eOsETTIN1\u003c/em\u003e, \u003cem\u003eOsETTIN2\u003c/em\u003e, \u003cem\u003eOsETTIN3\u003c/em\u003e, \u003cem\u003eOsYUCCA1\u003c/em\u003e, \u003cem\u003eOsYUCCA4\u003c/em\u003e and \u003cem\u003eOsMP\u003c/em\u003e) required for auxin synthesis and response and three JA signaling suppressor genes (\u003cem\u003eJAZ1\u003c/em\u003e, \u003cem\u003eJAZ6\u003c/em\u003e and \u003cem\u003eJAZ8\u003c/em\u003e) were prominently up-regulated expressed in the \u003cem\u003eddp1-1\u003c/em\u003e mutant, while a significant downregulation of two JA synthesis genes (\u003cem\u003eLOX2\u003c/em\u003e and \u003cem\u003eAOS3\u003c/em\u003e) was detected in the \u003cem\u003eddp1-1\u003c/em\u003e mutant at stage 9 and 10, respectively (Fig.\u0026nbsp;\u003cspan refid=\"Fig11\" class=\"InternalRef\"\u003e11\u003c/span\u003e). Together, these findings suggest that mutations in \u003cem\u003eDDP1\u003c/em\u003e alter the expression of known genes complicated in lipid metabolism, anther development and dehiscence, thus causing defective phenotypes associated with these processes.\u003c/p\u003e \u003cp\u003e \u003c/p\u003e \u003c/div\u003e"},{"header":"Discussion","content":"\u003cp\u003eThe anther epidermis contains cutin and wax, while the pollen exine is made up of sporopollenin, with their lipid precursors and derivatives being synthesized by the tapetum. Thus, the homeostasis of lipid metabolism in the tapetum is critical for the development of anther epidermis and pollen wall. This concept is supported by evidence that mutations in several genes associated with the accumulation of lipids in tapetum, including \u003cem\u003eWDA1\u003c/em\u003e (Jung et al. \u003cspan citationid=\"CR23\" class=\"CitationRef\"\u003e2006\u003c/span\u003e), \u003cem\u003eOsC6\u003c/em\u003e (Zhang et al. \u003cspan citationid=\"CR49\" class=\"CitationRef\"\u003e2010\u003c/span\u003e), \u003cem\u003eCYP704B2\u003c/em\u003e (Li et al. \u003cspan citationid=\"CR28\" class=\"CitationRef\"\u003e2010\u003c/span\u003e), \u003cem\u003eDPW\u003c/em\u003e (Shi et al. \u003cspan citationid=\"CR35\" class=\"CitationRef\"\u003e2011\u003c/span\u003e), \u003cem\u003eOsABCG15\u003c/em\u003e (Wu et al. \u003cspan citationid=\"CR41\" class=\"CitationRef\"\u003e2014\u003c/span\u003e), \u003cem\u003eOsABCG26\u003c/em\u003e (Chang et al. \u003cspan citationid=\"CR7\" class=\"CitationRef\"\u003e2016\u003c/span\u003e) and \u003cem\u003eCYP703A3\u003c/em\u003e (Yang et al. \u003cspan citationid=\"CR46\" class=\"CitationRef\"\u003e2018\u003c/span\u003e), cause defective tapetum, anther epidermis and pollen wall, ultimately leading to pollen sterility. In our research, we demonstrated that \u003cem\u003eDDP1\u003c/em\u003e, a novel member of the KCS family in rice, is essential for pollen fertility and lipid homeostasis in the tapetum. \u003cem\u003eDDP1\u003c/em\u003e was highly expressed in tapetum and microspore. DDP1 was localized in the ER, and distributed in tapetum, microspore and pollen. \u003cem\u003eddp1-1\u003c/em\u003e mutant exhibited defects in the anther epidermis and pollen wall. Additionally, compared to WT, the wax content and composition in \u003cem\u003eddp1-1\u003c/em\u003e were dramatically changed, and a significant shift in the expression levels of gene complicated in lipid metabolism, anther and pollen development was observed in the \u003cem\u003eddp1-1\u003c/em\u003e anthers. These findings show that \u003cem\u003eDDP1\u003c/em\u003e, like many genes associated with lipid metabolism, affects rice pollen fertility by modulating lipid metabolic homeostasis: the knockout of \u003cem\u003eDDP1\u003c/em\u003e disrupts this homeostasis, resulting in partial pollen abortion.\u003c/p\u003e \u003cp\u003eAlthough DDP1 is conserved across plant species, the phenotype of the \u003cem\u003eddp1\u003c/em\u003e mutants was significantly distinct from those of its homologs from \u003cem\u003eArabidopsis\u003c/em\u003e and rice. The phenotypes of these homologs included reduced wax accumulation, defective growth of roots and pollen tubes, semi-dwarfism, seedling lethality, and increased drought resistance. However, \u003cem\u003eddp1\u003c/em\u003e mutants showed no notable vegetative phenotypes, suggesting potential functional diversification between DDP1 and its homologs. HMS1, a DDP1 homolog, has also been implicated in male fertility. However, \u003cem\u003ehms1\u003c/em\u003e mutant exhibited a more severe complete male sterility compared to the partial male sterility of \u003cem\u003eddp1\u003c/em\u003e mutants. The sterility of \u003cem\u003ehms1\u003c/em\u003e was due to reduced pollen adhesion and germination on stigmas, while sterility of \u003cem\u003eddp1\u003c/em\u003e mutants arose from defects in the tapetum, anther epidermis, pollen wall, and anther dehiscence. These findings indicate a functional differentiation between DDP1 and HMS1 in the regulation of male fertility. Moreover, there was a difference in the expression patterns of \u003cem\u003eDDP1\u003c/em\u003e homologous genes. For examples, \u003cem\u003eDDP1\u003c/em\u003e, \u003cem\u003eOsWSL1\u003c/em\u003e, \u003cem\u003eSD38\u003c/em\u003e and \u003cem\u003eOsWSL4\u003c/em\u003e/\u003cem\u003eOsHMS1\u003c/em\u003e were expressed in all examined organs, including roots, stems, leaves and panicles, while \u003cem\u003eOsCUT1\u003c/em\u003e was found to has a higher level of transcription in young panicles and leaves. The transcription of \u003cem\u003eONI1\u003c/em\u003e and \u003cem\u003eONI2\u003c/em\u003e was confined to specific regions, notably the outer cell layer of the shoot apical meristem and the developmental stages of lateral organs. The significant differences in mutant phenotype and gene expression pattern between \u003cem\u003eDDP1\u003c/em\u003e and its homologs suggest that they may have different biological functions in plant development. Investigating the function of DDP1 will be instrumental in understanding the broader functions of KCS proteins within the plant kingdom.\u003c/p\u003e \u003cp\u003eThe \u003cem\u003eddp1\u003c/em\u003e mutants exhibited a partial male sterile phenotype, suggesting a redundant function for DDP1 in controlling male fertility. The potential redundancy of DDP1 could be due to the widespread presence of VLCFA biosynthesis related genes and their homologs, in addition to the high expression levels of these genes in rice young inflorescences.VLCFA biosynthesis requires four key enzymes, including KCS, KCR, HCD and ECR. Loss of function of members from any of these enzyme families might impair VLCFAs formation, leading to male sterility. In addition, the rice genome contains 22 homologs of \u003cem\u003eDDP1\u003c/em\u003e (Yang et al., \u003cspan citationid=\"CR47\" class=\"CitationRef\"\u003e2023\u003c/span\u003e). Analysis of gene expression patterns in the Bio-Analytic Resource for Plant Biology database revealed that eight \u003cem\u003eDDP1\u003c/em\u003e homologs with unknown functions, such as \u003cem\u003eOsCUT8\u003c/em\u003e, \u003cem\u003eOsKCS16\u003c/em\u003e, \u003cem\u003eOsCUT6, OsKCS15\u003c/em\u003e, \u003cem\u003eOsKCS13\u003c/em\u003e, \u003cem\u003eOsKCS22, OsKCS2\u003c/em\u003e, and \u003cem\u003eOsKCS9\u003c/em\u003e, are highly expressed in young inflorescences (Fig. S6). This suggests that these homologs may play crucial roles in VLCFA biosynthesis and male fertility, and DDP1 may interact directly or indirectly with other proteins to coordinately regulate rice male fertility. Despite attempts to screen for DDP1-interacting proteins in the rice anther cDNA library using yeast two-hybrid technology, no interacting protein was identified. Further research is necessary to elucidate the regulatory networks of DDP1 in male fertility by identifying its interacting proteins or upstream transcription factors.\u003c/p\u003e \u003cp\u003eMutations in certain genes associated with lipid metabolism result in reduced anther wax, as observed in \u003cem\u003eKCS6\u003c/em\u003e (Fiebig et al. \u003cspan citationid=\"CR9\" class=\"CitationRef\"\u003e2000\u003c/span\u003e), \u003cem\u003eWDA1\u003c/em\u003e (Jung et al. \u003cspan citationid=\"CR23\" class=\"CitationRef\"\u003e2006\u003c/span\u003e), \u003cem\u003eWSL1\u003c/em\u003e (Yu et al. \u003cspan citationid=\"CR48\" class=\"CitationRef\"\u003e2008\u003c/span\u003e), \u003cem\u003eOsGL1-2\u003c/em\u003e (Islam et al. \u003cspan citationid=\"CR20\" class=\"CitationRef\"\u003e2009\u003c/span\u003e), \u003cem\u003eOsGL1-1\u003c/em\u003e (Qin et al. \u003cspan citationid=\"CR33\" class=\"CitationRef\"\u003e2011\u003c/span\u003e), \u003cem\u003eOsGL1-6\u003c/em\u003e (Zhou et al. \u003cspan citationid=\"CR52\" class=\"CitationRef\"\u003e2013\u003c/span\u003e), \u003cem\u003eONI1\u003c/em\u003e and \u003cem\u003eONI2\u003c/em\u003e (Tsuda et al. \u003cspan citationid=\"CR40\" class=\"CitationRef\"\u003e2013\u003c/span\u003e), \u003cem\u003eOsGL1-3\u003c/em\u003e (Zhou et al. \u003cspan citationid=\"CR53\" class=\"CitationRef\"\u003e2015\u003c/span\u003e), \u003cem\u003eWSL4/HMS1\u003c/em\u003e (Gan et al. \u003cspan citationid=\"CR11\" class=\"CitationRef\"\u003e2017\u003c/span\u003e; Chen et al. \u003cspan citationid=\"CR8\" class=\"CitationRef\"\u003e2020\u003c/span\u003e), and \u003cem\u003eKCS5\u003c/em\u003e (Huang et al. \u003cspan citationid=\"CR17\" class=\"CitationRef\"\u003e2022\u003c/span\u003e), \u003cem\u003eSD38\u003c/em\u003e (Zhang et al. \u003cspan citationid=\"CR51\" class=\"CitationRef\"\u003e2022\u003c/span\u003e). In contrast, mutations of other genes associated with lipid metabolism cause a dramatical increase of anther wax, such as \u003cem\u003eDPW2\u003c/em\u003e (Xu et al. \u003cspan citationid=\"CR44\" class=\"CitationRef\"\u003e2017\u003c/span\u003e), \u003cem\u003eOsPKS2\u003c/em\u003e (Zou et al. \u003cspan citationid=\"CR54\" class=\"CitationRef\"\u003e2018\u003c/span\u003e), \u003cem\u003ePEM1\u003c/em\u003e (Song et al. \u003cspan citationid=\"CR38\" class=\"CitationRef\"\u003e2022\u003c/span\u003e), \u003cem\u003eOs12BGlu38\u003c/em\u003e (Shim et al. \u003cspan citationid=\"CR37\" class=\"CitationRef\"\u003e2022\u003c/span\u003e), \u003cem\u003eKCS3\u003c/em\u003e (Huang et al. \u003cspan citationid=\"CR18\" class=\"CitationRef\"\u003e2023a\u003c/span\u003e), and \u003cem\u003eKCS12\u003c/em\u003e (Huang et al. \u003cspan citationid=\"CR19\" class=\"CitationRef\"\u003e2023b\u003c/span\u003e). These findings suggest that changes in anther wax content may be an indirect consequence of mutations in genes related to lipid metabolism. In this study, the \u003cem\u003eddp1\u003c/em\u003e mutants showed a denser anther cuticle. Consistent with this, elevated levels of free fatty acids, alkenes, alcohols and sterols were detected in the \u003cem\u003eddp1\u003c/em\u003e mutants. Moreover, two lipid metabolism genes (\u003cem\u003eOsABCG3\u003c/em\u003e and \u003cem\u003eOsCER1\u003c/em\u003e) had up-regulated expression in the \u003cem\u003eddp1\u003c/em\u003e mutants during stages 8 and 9. Given the role of DDP1 in lipid precursor formation, it is plausible to hypothesize that the knockout of \u003cem\u003eDDP1\u003c/em\u003e disrupts lipid metabolism homeostasis, potentially triggering a feedback mechanism that results in a thicker anther cuticle.\u003c/p\u003e \u003cp\u003eIn addition to the aforementioned defects in anthers and pollen, the \u003cem\u003eddp1\u003c/em\u003e mutants also exhibited a distinct defect in anther dehiscence, a phenotype almost rarely observed in mutants associated with lipid metabolism. We speculate that the defect in \u003cem\u003eddp1\u003c/em\u003e anther dehiscence may be due to the reduced mechanical pressure from aborted pollen grains or may be caused by defective endothecium lignification. Previous research has shown that anther dehiscence is closely related to auxin signaling, jasmonic acid (JA) biosynthesis and endothecium lignification. Excessive indole-3-acetic acid (IAA) accumulation generally leads to decreased JA content and abnormal endothecium lignification, thereby causing anther indehiscence (Cecchetti et al., \u003cspan citationid=\"CR6\" class=\"CitationRef\"\u003e2013\u003c/span\u003e). Moreover, it is reported that cuticular wax is closely related to IAA and JA. Zhu et al (\u003cspan citationid=\"CR56\" class=\"CitationRef\"\u003e2014\u003c/span\u003e) reported that expression of \u003cem\u003eEsWAX1\u003c/em\u003e from \u003cem\u003eEutrema salsugineum\u003c/em\u003e was slightly increased by IAA treatment, thus promoting accumulation of cuticular wax. Recently, a study demonstrated that there was a negative relationship between total cuticular wax content and JA concentration in maize, the mutation of \u003cem\u003eZmGL8\u003c/em\u003e, encoding a β-ketoacyl-CoA reductase, reduced wax accumulation and activated a JA-dependent pathway (Liu et al. \u003cspan citationid=\"CR29\" class=\"CitationRef\"\u003e2024\u003c/span\u003e). These results reveal that IAA increases cuticular wax accumulation, thereby reducing JA levels and leading to anther indehiscence. Consistent with this, we observed that in the \u003cem\u003eddp1\u003c/em\u003e mutants, the total wax content increased by 34%\u0026plusmn;0.08% compared to WT, a significant increase in expression was observed for six auxin signaling related genes and three JA signaling suppressor genes, whereas two genes critical for the production of JA showed a dramatic decrease in expression levels. These findings imply that DDP1 may regulate anther dehiscence by modulating auxin and JA signaling pathways. However, the exact mechanism by which DDP1 regulates these signaling pathways and endothecium lignification remains unclear. Therefore, additional research is required for fully elucidating the function of DDP1 in auxin signaling, JA biosynthesis and endothecium lignification.\u003c/p\u003e "},{"header":"Declarations","content":"\u003cp\u003e\u003cstrong\u003eAuthor contribution statement\u0026nbsp;\u003c/strong\u003eB. Qin, L. Shang, X. He, and Y. Xu conceived and designed the experiments; Y. Xu, and S. Zhou performed most of the experiments and analyzed the data; J. He, W. Tan, J. Tian, W. Zhao, and J. Wei participated in the phenotype measurement and field experiments; B. Qin and Y. Xu wrote the manuscript; S. Zhou, J. Tian, W. Zhao, J. Wei, and R. Li revised the manuscript. All authors read and approved the final manuscript.\u003c/p\u003e\n\u003cp\u003e\u003cstrong\u003eFunding\u003c/strong\u003e This work was supported by the National Natural Science Foundation of China (32372023 and 31971809), Centrally Guided Local Science and Technology Development Fund (ZY23055028), the Guangxi Natural Science Foundation (2019GXNSFDA185009 and 2024GXNSFGA010003), State Key Laboratory for Conservation and Utilization of Subtropical Agro-bioresources (SKLCUSA-b202306), Innovation Project of Guangxi Graduate Education (YCBZ2022016), the Project of Bama County for Talents in Science and Technology (No.20220009).\u003c/p\u003e\n\u003cp\u003e\u003cstrong\u003eConflict of interest\u0026nbsp;\u003c/strong\u003eThe authors declare that they have no conflict of interest.\u003c/p\u003e"},{"header":"References","content":"\u003col\u003e\u003cli\u003e\u003cspan\u003eAriizumi T, Toriyama K (2011) Genetic regulation of sporopollenin synthesis and pollen exine development. 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Plant Physiol Biochem 75:24\u0026ndash;35. \u003cspan class=\"ExternalRef\"\u003e\u003cspan class=\"RefSource\"\u003ehttps://doi.org/10.1016/j.plaphy.2013.11.028\u003c/span\u003e\u003cspan address=\"10.1016/j.plaphy.2013.11.028\" targettype=\"DOI\" class=\"RefTarget\"\u003e\u003c/span\u003e\u003c/span\u003e\u003c/span\u003e\u003c/li\u003e\u003c/ol\u003e"}],"fulltextSource":"","fullText":"","funders":[],"hasAdminPriorityOnWorkflow":false,"hasManuscriptDocX":true,"hasOptedInToPreprint":true,"hasPassedJournalQc":"","hasAnyPriority":false,"hideJournal":false,"highlight":"","institution":"","isAcceptedByJournal":true,"isAuthorSuppliedPdf":false,"isDeskRejected":"","isHiddenFromSearch":false,"isInQc":false,"isInWorkflow":true,"isPdf":false,"isPdfUpToDate":true,"isWithdrawnOrRetracted":false,"journal":{"display":true,"email":"[email protected]","identity":"theoretical-and-applied-genetics","isNatureJournal":false,"hasQc":true,"allowDirectSubmit":false,"externalIdentity":"taag","sideBox":"Learn more about [Theoretical and Applied Genetics](https://www.springer.com/journal/122)","snPcode":"122","submissionUrl":"https://submission.nature.com/new-submission/122/3","title":"Theoretical and Applied Genetics","twitterHandle":"","acdcEnabled":true,"dfaEnabled":true,"editorialSystem":"em","reportingPortfolio":"Springer Hybrid","inReviewEnabled":true,"inReviewRevisionsEnabled":false},"keywords":"","lastPublishedDoi":"10.21203/rs.3.rs-4822227/v1","lastPublishedDoiUrl":"https://doi.org/10.21203/rs.3.rs-4822227/v1","license":{"name":"CC BY 4.0","url":"https://creativecommons.org/licenses/by/4.0/"},"manuscriptAbstract":"Anther dehiscence and pollen fertility are crucial for male fertility in rice. Here, we studied the function of Defective in Dehiscence and Pollen1 (DDP1), a novel member of the KCS family in rice, in regulating anther dehiscence and pollen fertility. DDP1 encodes an endoplasmic reticulum (ER)-localized protein and is ubiquitously expressed in various organs, predominately in the microspores and tapetum. The ddp1 mutant exhibited partial male sterility attributed to defective anther dehiscence and pollen fertility, which was notably distinct from those observed in Arabidopsis thaliana and rice mutants associated with lipid metabolism. Mutations of DDP1 altered the content and composition of wax on anther epidermis and pollen wall, causing abnormalities in their morphology. Moreover, genes implicated in lipid metabolism, pollen development and anther dehiscence exhibited significantly altered expression levels in the ddp1 mutant. These findings indicate that DDP1 controls anther dehiscence and pollen fertility to ensure normal male development by modulating lipid homeostasis in the tapetum, thereby enhancing our understanding of the mechanisms underlying rice anther dehiscence and pollen fertility.","manuscriptTitle":"A β-Ketoacyl-CoA Synthase encoded by DDP1 controls rice anther dehiscence and pollen fertility by maintaining lipid homeostasis in the tapetum","msid":"","msnumber":"","nonDraftVersions":[{"code":1,"date":"2024-08-29 17:33:54","doi":"10.21203/rs.3.rs-4822227/v1","editorialEvents":[{"type":"communityComments","content":0},{"type":"decision","content":"Minor revisions","date":"2024-09-29T19:05:38+00:00","index":"","fulltext":""},{"type":"reviewerAgreed","content":"","date":"2024-08-04T07:52:28+00:00","index":0,"fulltext":""},{"type":"reviewersInvited","content":"","date":"2024-08-04T01:34:11+00:00","index":"","fulltext":""},{"type":"editorAssigned","content":"","date":"2024-07-30T10:40:42+00:00","index":"","fulltext":""},{"type":"submitted","content":"Theoretical and Applied Genetics","date":"2024-07-29T09:03:41+00:00","index":"","fulltext":""}],"status":"published","journal":{"display":true,"email":"[email protected]","identity":"theoretical-and-applied-genetics","isNatureJournal":false,"hasQc":true,"allowDirectSubmit":false,"externalIdentity":"taag","sideBox":"Learn more about [Theoretical and Applied Genetics](https://www.springer.com/journal/122)","snPcode":"122","submissionUrl":"https://submission.nature.com/new-submission/122/3","title":"Theoretical and Applied Genetics","twitterHandle":"","acdcEnabled":true,"dfaEnabled":true,"editorialSystem":"em","reportingPortfolio":"Springer Hybrid","inReviewEnabled":true,"inReviewRevisionsEnabled":false}}],"origin":"","ownerIdentity":"43007970-2fb8-4a2f-ab65-a05ac85f5547","owner":[],"postedDate":"August 29th, 2024","published":true,"recentEditorialEvents":[],"rejectedJournal":[],"revision":"","amendment":"","status":"published-in-journal","subjectAreas":[],"tags":[],"updatedAt":"2024-12-09T16:07:01+00:00","versionOfRecord":{"articleIdentity":"rs-4822227","link":"https://doi.org/10.1007/s00122-024-04786-8","journal":{"identity":"theoretical-and-applied-genetics","isVorOnly":false,"title":"Theoretical and Applied Genetics"},"publishedOn":"2024-12-03 15:58:09","publishedOnDateReadable":"December 3rd, 2024"},"versionCreatedAt":"2024-08-29 17:33:54","video":"","vorDoi":"10.1007/s00122-024-04786-8","vorDoiUrl":"https://doi.org/10.1007/s00122-024-04786-8","workflowStages":[]},"version":"v1","identity":"rs-4822227","journalConfig":"researchsquare"},"__N_SSP":true},"page":"/article/[identity]/[[...version]]","query":{"redirect":"/article/rs-4822227","identity":"rs-4822227","version":["v1"]},"buildId":"zQwnuV7TCBrMSSSToR1PI","isFallback":false,"isExperimentalCompile":false,"dynamicIds":[84888],"gssp":true,"scriptLoader":[]}