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Article

The Loss-Function of the Male Sterile Gene ZmMs33/ZmGPAT6 Results in Severely Oxidative Stress and Metabolic Disorder in Maize Anthers

by
Ziwen Li
1,†,
Shuangshuang Liu
1,2,†,
Taotao Zhu
1,†,
Xueli An
1,2,
Xun Wei
1,
Juan Zhang
1,
Suowei Wu
1,2,
Zhenying Dong
1,
Yan Long
1,* and
Xiangyuan Wan
1,2,*
1
Shunde Graduate School, Zhongzhi International Institute of Agricultural Biosciences, Research Center of Biology and Agriculture, University of Science and Technology Beijing, Beijing 100024, China
2
Beijing Engineering Laboratory of Main Crop Bio-Tech Breeding, Beijing International Science and Technology Cooperation Base of Bio-Tech Breeding, Beijing Solidwill Sci-Tech Co., Ltd., Beijing 100192, China
*
Authors to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Cells 2022, 11(15), 2318; https://doi.org/10.3390/cells11152318
Submission received: 22 June 2022 / Revised: 23 July 2022 / Accepted: 25 July 2022 / Published: 27 July 2022
(This article belongs to the Special Issue Pollen Development)
Browse Figures
Versions Notes

Abstract

:
In plants, oxidative stress and metabolic reprogramming frequently induce male sterility, however our knowledge of the underlying molecular mechanism is far from complete. Here, a maize genic male-sterility (GMS) mutant (ms33-6038) with a loss-of-function of the ZmMs33 gene encoding glycerol-3-phosphate acyltransferase 6 (GPAT6) displayed severe deficiencies in the development of a four-layer anther wall and microspores and excessive reactive oxygen species (ROS) content in anthers. In ms33-6038 anthers, transcriptome analysis identified thousands of differentially expressed genes that were functionally enriched in stress response and primary metabolism pathways. Further investigation revealed that 64 genes involved in ROS production, scavenging, and signaling were specifically changed in expression levels in ms33-6038 anthers compared to the other five investigated GMS lines. The severe oxidative stress triggered premature tapetal autophagy and metabolic reprogramming mediated mainly by the activated SnRK1-bZIP pathway, as well as the TOR and PP2AC pathways, proven by transcriptome analysis. Furthermore, 20 reported maize GMS genes were altered in expression levels in ms33-6038 anthers. The excessive oxidative stress and the metabolic reprogramming resulted in severe phenotypic deficiencies in ms33-6038 anthers. These findings enrich our understanding of the molecular mechanisms by which ROS and metabolic homeostasis impair anther and pollen development in plants.

1. Introduction

Genic male sterility (GMS) is a common phenomenon existing in different crops, such as maize [1], rice [2], wheat [3], and so on. It is now widely used in hybrid production and heterosis research [1,4]. Male sterility is closely related to anther development and pollen formation. In general, the anther wall in higher plants consists of four layers: epidermis, endothecium (En), middle layer, and tapetum from outer to inner. Their formation and functions are precisely regulated during anther development to ensure mature pollen formation [5,6]. So far, hundreds of GMS mutants have been identified in plants [7]. Until now, 39 GMS genes have been identified in maize [1,8,9,10,11], including 21 genes encoding transcriptional factors (TFs), such as ZmMS7 [12,13], ZmOCL4 [14], and ZmMS23 [15]; 13 lipid metabolic genes, such as ZmMs26 [16,17], ZmMs30 [18], and ZmMs33 [19,20,21]; 2 sugar metabolic genes, ZmMs8 [22] and ZmMs39 [23]; and 3 genes with other functions. Although the molecular mechanisms of some GMS genes have been well investigated, the physiological and metabolic mechanisms of these genes in regulating male fertility are largely unknown.
Reactive oxygen species (ROS) represent one class of oxygen-containing substances, such as singlet oxygen (1O2), superoxide anions (O2−), hydroxyl radicals (•OH), hydrogen peroxide (H2O2), and nitric oxide (NO) [24]. It is well-known that ROS is an essential regulator of many metabolic pathways, and it plays a critical role in signal transduction [25,26]. During plant anther development, dynamic ROS levels are related to the initiation and progression of tapetal programmed cell death (PCD) [2,27]. For example, in rice, DEFECTIVE TAPETUM CELL DEATH 1 (DTC1) regulates male reproduction through tapetal PCD by modulating ROS-scavenging activity [28]. Besides the DTC1 gene, many other genes, such as ARGONAUTE 2 (AGO2) [25], HEXOKINASE1 (HXK1) [25], and a MADS-box transcription factor gene (MADS3) [26], are found to regulate male sterility through modulating the ROS accumulation in anthers. In Arabidopsis, the stage-specific expressed NADPH oxidase gene (RBOH) can affect the timing of tapetal PCD [29]. Although these findings suggest that ROS is involved in anther development and pollen formation, some problems remain, e.g., how ROS homeostasis is maintained during anther development and how ROS status leads to male sterility.
Autophagy is another important physiological process related to metabolic reprogramming, and it plays a critical role in many biological processes, including plant male reproduction [20]. In rice, the autophagy defective mutants, Osatg7-1 and Osatg9, show sporophytic male sterility and fail to undergo anther dehiscence under normal growth conditions [30]. In Picea abies, autophagy is necessary for the vacuolar cell death of the embryo suspensor [31]. However, how the autophagy and metabolic reprogramming affect anther development and pollen formation is rarely investigated.
Our previous studies showed that the ZmMs33 gene is preferentially expressed at anther stages S5 and S6, and it encodes a glycerol-3-phosphate acyltransferase (GPAT) enzyme that catalyzes the first step of glycerophospholipid biosynthesis. Its loss-function mutants exhibited severe male-sterility phenotypes [19,20,32]. While there are still some questions to be answered, i.e., why the mutant anthers showed the severe male-sterility phenotypes and why the appeared stages of mutational phenotypes greatly lagged in time behind the expression stages of the causal mutation gene. Here, a comparative transcriptome analysis combined with cytological and physiological experiments were used to investigate these problems. Excessive ROS content and severely oxidative stress as well as transcriptional alterations of a lot of genes involved in metabolic reprogramming and male reproduction were identified in ms33-6038 anthers, which may result in the severe phenotypic defects of ms33-6038 anthers. Furthermore, the comparative transcriptome analysis revealed specific functions of the ZmMs33 gene in impairing the expression of ROS-related genes. These findings deepen our understanding of molecular mechanisms underlying that ROS and metabolic homeostasis impair anther development in plants.

2. Materials and Methods

2.1. Plant Materials, Growth Condition, and Phenotypic Characterization

The ms33-6038 (No. 228I) mutant was initially obtained from the Maize Genetics Cooperation Stock Center (http://maizecoop.cropsci.uiuc.edu, accessed on 20 July 2014). All plant materials were grown at the experimental station of USTB in Beijing. Photos of WT and ms33-6038 tassels were taken by a Canon EOS 700D camera (Canon, Tokyo, Japan). Fresh anthers of WT and ms33-6038 at stages S8b and S9 were photographed using an SZX2-ILLB stereomicroscope (Olympus, Tokyo, Japan). Pollen grains were stained with 1% I2-KI and photographed using a BX-53F microscope (Olympus, Japan).

2.2. Cytological Observation and Microscopy

For transverse section and scanning electron microscope (SEM) analyses, fresh anthers of WT and ms33-6038 at different developmental stages were fixed in an FAA solution (SL16220, Coolaber, Beijing, China). The subsequent procedures were performed as previously described [33,34]. The semi-thin sections were observed and photographed using a BX-53F microscope (Olympus, Japan). The gold-coated anthers were observed and photographed using a HITACHI S-3400N scanning electron microscope (Hitachi, Tokyo, Japan). The transmission electron microscope (TEM) analysis was performed as previously described [34] in which the fresh anthers were prefixed using a 3% glutaraldehyde solution (G5882, Sigma-Aldrich, City of Saint Louis, MO, USA). The ultrathin sections were observed and photographed using a HITACHI H-7500 transmission electron microscope (Hitachi, Japan).

2.3. Transcriptomic Analysis

Transcriptomic data were analyzed as previously described [35]. Specifically, TopHat2 was used to map the clean reads to the maize B73_AGPv4 reference genome with default parameters [36]. Expression levels of coding genes were estimated by the Rsubread package [37]. Anther transcriptomes of ocl4, mac1, ms23, ms30-6028, and p5126-ZmMs7 were reanalyzed by the same method (Table S1). Differentially expressed genes (DEGs) were identified by the edgeR package [38], with a false discovery rate <0.05 and a fold change >3 for each gene. GO enrichment analysis was performed using agriGO [39]. Pathway enrichment analysis was conducted using data from the KEGG database (https://www.kegg.jp/, accessed on 25 March 2019).

2.4. Measurement of ROS and •OH

For ROS measurement, H2DCF-DA (D6883, Sigma-Aldrich, USA) was dissolved in DMSO (D2650, Sigma-Aldrich, USA) to prepare a 10 mM stock solution. Then, it was diluted to 5 μM as a working solution in 1× HHBS Buffer (MS3510, Maokang Bio-Technology, Shanghai, China). For •OH measurement, HPF (MX4805, Maokang Bio-Technology, China) was dissolved in DMF (227056, Sigma-Aldrich, USA) to prepare a 5 mM stock solution. Then, it was diluted to 10 μM as a working solution in 1× HHBS Buffer (MS3510, Maokang Bio-Technology, China). In the ROS and •OH measurement assays, fresh anthers of WT and ms33-6038 at different developmental stages were immersed in a 2 mL centrifuge tube, which contained 1 mL of 1× HHBS. After washing the anthers, the supernatant was discarded, a 1 mL working solution (1 mL of H2DCF-DA for ROS measurement or 1 mL of HPF working solution for •OH measurement) and 0.5 μL of Silwet L-77 (SL77080596, GE, Boston, MA, USA) was added; it was vacuumed for 15 min and then shaken at 25 °C in darkness (80–100 rmp) for 3 h. After discarding the dye solution, anthers were washed once with 1× HHBS, then 1 mL of 1× HHBS was added into the centrifuge tube [40,41]. The green fluorescence signals were detected by a Leica TCS SP8 confocal microscope (Leica, Wetzlar, Germany). The relative levels of ROS and •OH were quantified by the ImageJ software (http://rsbweb.nih.gov/ij/, accessed on 25 September 2020). Data in a histogram were represented by the average value and the standard deviation of three anthers from a representative of three independent analyses.

2.5. Quantitative Real-Time PCR Analysis

Total RNA was isolated from anthers using TRIzol reagent (15596026, Invitrogen, Carlsbad, CA, USA). The concentration and purity of the isolated RNA were measured by a NanoDrop ND-1000 Spectrophotometer (Thermo Fisher, Waltham, MA, USA). After removing genomic DNA with Dnase I (M6101, Promega, Madison, WI, USA), cDNA was synthesized using 5× All-In-One RT MasterMix (G592, abm, Vancouver, BC, Canada). The quantitative real-time PCR (qPCR) analysis was conducted with the corresponding primer set (Table S2) on a QuantStudio 5 Real-Time PCR system (ABI, Waltham, MA, USA), using TB Green Premix EX Tag (RR420A, Takara, Osaka, Japan); ZmActin1 was used as the internal control. Each sample had 3 biological replicates with 3 technical replicates, the amplification data were analyzed by the 2−△△Ct method, and the quantitative results were given as means ± standard deviations.

3. Results

3.1. Transcriptomic Analysis of Wild Type and ms33-6038 Mutant Anthers with Severe Male-sterility Phenotypes Induced by Loss-Function of ZmMs33 Gene

The causal mutation gene (ZmMs33/ZmGPAT6) has been identified for the ms33-6038 mutant that exhibits severe male-sterility phenotypes previously comprehensively characterized [19,20,21]. Specifically, compared with wild type (WT) anthers, loss of the ZmMs33 function disrupted anther elongation since stage S9 (Figure 1A). For anther wall layers, unlike the WT anthers that possessed a reticulated accumulation of wax and cutin on the epidermal outer surface at stage S13, invisible starch granules in En chloroplasts at stage S10, and degraded and thin tapetal layers at stages S10 and S11, the ms33-6038 anthers displayed a smooth outer surface of the epidermis, an excessive starch accumulation in En chloroplasts, and enlarged tapetal cells at the corresponding stages, respectively (Figure 1B). Inside the anthers, the WT pollen possessed typical exine layers, obviously swelled at stage 10, and exhibited round shapes filled with starch granules at stage 13. While, the ms33-6038 pollen displayed smaller sizes with obviously thin exine layers and failed to develop to mature pollen grains at the corresponding stages, respectively (Figure 1C). These results indicate that loss of the ZmMs33 function induces severe phenotypic deficiencies of both anther wall layers and pollen grains, at least from stages S9 to S13.
To investigate possible mechanisms underlying the severe effects of ZmMs33 deficiency on anther development, we performed a transcriptome analysis. Considering the ZmMs33 gene is highly expressed in anthers at stages S5 and S6 [20] and the phenotypic changes obviously appeared since stage S9, the ms33-6038 and WT anthers of six stages from S5 to S9 were included in RNA-sequencing (RNA-seq) analysis. It is worth mentioning that the developmental stages of anther samples were not only estimated by the anther lengths but also determined by the cytological evidence from the semi-thin transverse section analysis of maize anthers from the same spikelet of sampled anthers (Figure 2A,B). Three biological replicates were conducted in both WT and ms33-6038 anthers at each of the six stages. The results of similarity analysis suggested a high repeatability among 3 biological replicates (Figure 2C and Figure S1), indicating that the transcriptomes have a good representation of transcriptional changes in both WT and ms33-6038 anthers from stages S5 to S9.
Principal component analysis (PCA) of RNA-seq data revealed that ms33-6038 or WT anther samples at the same stages were clustered together and the anther samples were successively arranged with the developmental stages identified by the cytological evidence, emphasizing that the transcriptomes are usable (Figure 3A). Hierarchical clustering analysis of the transcriptomes showed that samples from stages S5 to S7 were clustered by the three developmental stages, while samples from stages S8a to 9 were clustered according to the genotypes of WT or ms33-6038 (Figure 3B). Moreover, the numbers of DEGs between ms33-6038 and WT anthers at stages S5, S6, and S7 do not exceed the numbers of DEGs between stages S6 and S5, stages S7 and S6, and stages S8a and S7, respectively (Figure 3C). In contrast, the numbers of DEGs between ms33-6038 and WT anthers from stages S8a to S9 obviously exceeded those between the adjacent stages in WT anthers (Figure 3C). These results indicate that ZmMs33 deficiency has a relatively small effect on the anther transcriptomes before microsporocyte meiosis (stages S5, S6, and S7), while dramatic changes occur at anther meiotic (stages S8a and S8b) and postmeiotic (stage S9) processes. Gene ontology (GO) analysis suggested that the DEGs between ms33-6038 and WT anthers from stages S5 to S7 were functionally enriched in dispersed biological processes, including fatty acid (FA) and phenylpropanoid metabolisms and stimulus responses at stage S5, carbohydrate metabolism at stage S6, and cellular amino acid derivate metabolism at stage S7 (Figure 3D). However, the DEGs from stages S8a to S9 were significantly enriched in consistent biological processes, including photosynthesis and stress responses (Figure 3D). Specifically, from stages S8a to S9, the upregulated DEGs were annotated to be involved in stress responses and the downregulated DEGs were functionally enriched in photosynthesis and electron transport chain related to carbon and energy metabolisms (Figure 3E). Taken together, the ZmMs33 deficiency leads to abnormally activated stress responses and reprogrammed metabolisms at the transcriptional level, which may result in severe phenotypic defects in anther development.

3.2. ZmMs33 Deficiency Caused Severe Oxidative Stress in Maize Anthers

To reveal which type of stress is mainly induced in ms33-6038 anthers, we conducted KEGG pathway enrichment analysis and found that genes involved in plant MAPK signaling pathway and plant hormone signal transduction were activated in ms33-6038 anthers, while the downregulated genes mainly functioned in the primary metabolic pathways (Figure 4A). The MAPK signaling pathway was reported to respond to various environmental stresses, such as hyperosmolarity, extreme pH, temperature changes, and ROS as one type of plant defense signal [42]. ROS homeostasis is of great importance for the development of germ cells and tapetal cells in plant anthers [29,43]. Since ms33-6038 anthers were not stimulated through external stresses, it can be speculated that the severe phenotypic deficiencies in ms33-6038 anthers may be endogenously induced by oxidative stress. To test it, we investigated the expression changes of genes included in the GO term of the response to the oxygen-contained compound (GO term ID: 1901700) and found that 194 related genes were obviously upregulated in ms33-6038 anthers mainly from stages S8a to S9 (Figure 4B and Table S3). Furthermore, the levels of •OH, an important ROS type formed non-enzymatically by the Fenton reaction between H2O2 and Fe2+, were significantly higher in ms33-6038 anthers from stage S8a to S13 compared with those of WT anthers (Figure 4C). Besides, the total ROS levels in ms33-6038 anthers were significantly higher than those of WT anthers from stages S10 to S13 (Figure 4D). These findings suggest ZmMs33 deficiency induces the excessive ROS levels in anthers and activates a large number of genes in response to oxidative stress.
To further reveal the molecular mechanism underlying the excessive ROS accumulation in ms33-6038 anthers, we comprehensively investigated expression changes of 64 genes involved in ROS generation (4 pathways), scavenging (5 pathways), and signaling (the MAPK pathway), according to previous studies (Figure 5A and Table S4). In ms33-6038 anther transcriptomes, 2 genes encoding NADPH oxidases, 6 genes involved in FA β-oxidation, and 13 genes in branched-chain amino acid (BCAA) catabolism pathway were upregulated mainly from stages S8a to S9, while 2 genes encoding mitochondria-located HXKs were downregulated, which could promote ROS generation (Figure 5A). In addition, 11 genes involved in the peroxiredoxin cycle and 3 in water–water cycle were downregulated mainly from stages S8a to S9, contributing to a reduced ability of ROS scavenging in ms33-6038 anthers (Figure 5A). However, 10 genes participated in ascorbate glutathione and glutathione peroxidase cycles, 2 catalase genes, 8 peroxidase genes, 2 blue copper protein genes, and 1 metallothionein gene, were upregulated in ms33-6038 anthers (Figure 5A), which may be induced by the high ROS levels. Furthermore, four genes involved in the MAPK signaling pathway were transcriptionally activated in ms33-6038 anthers (Figure 5A). The expression patterns of 15 representative genes were confirmed by qPCR analysis (Figure 5B). These results indicate that the excessive ROS content in ms33-6038 anthers is produced most probably via the comprehensive activation of ROS generation pathways yet the repression of ROS scavenging pathways, which together induce the extreme oxidative stress and activate oxidative stress responses by the MAPK signaling pathway.

3.3. The Uniqueness of ZmMs33 Deficiency-Induced Excessive Oxidative Stress among Maize GMS Mutants

The excessive oxidative stress can impact the differentiation of sporogenous cells and the degeneration of tapetal cells in anther development [25,29,43]. The ocl4, mac1, and ms23 GMS lines displayed abnormal differentiations of anther wall layers and sporogenous cells [14,44,45] (Figure S2). Both ZmMs30 deficiency (ms30-6028) and ZmMs7 overexpression (p5126-ZmMs7) anthers exhibited abnormal tapetum development [13,18]. All of these five GMS lines exhibit oxidative stress-induced phenotypic deficiencies during anther development. To examine whether ms33-6038 and other GMS lines share a similar mechanism underlying the abnormal ROS content that impair anther development and male fertility, we performed a comparative transcriptome analysis on the 64 genes related to ROS metabolism and oxidative stress responses between ms33-6038 and each of the 5 GMS lines (ms30-6028, p5126-ZmMs7, ocl4, mac1, and ms23). Unlike ms33-6038 anthers displaying a comprehensive transcriptional reprograming of the 64 maker genes, only a few of these genes in the 5 investigated GMS lines have changed expression patterns similar with those of ms33-6038 anthers (Figure 6). Specifically, the p5126-ZmMs7, mac1, and ms23 anthers possessed fewer genes (10/64, 7/64, and 6/64, respectively), with similar expression changes to those of ms33-6038 anthers, and these genes were separately distributed in several pathways. In the MAPK signaling pathway, only one maker gene was upregulated in ocl4 anthers. These results revealed that the comprehensive transcriptional changes of ROS metabolic and signaling genes in ms33-6038 anthers were not observed in the five investigated GMS lines, indicating that the excessive oxidative stress and the expression alterations of anti-oxidative genes were specific in ms33-6038 anthers.

3.4. ZmMs33 Deficiency-Induced Oxidative Stress Activated Premature Autophagy and Metabolic Reprogramming in Tapetum, Leading to Transcriptional Changes of Other GMS Genes

Tapetum degeneration and autophagy usually occur at anther developmental stage S10 in maize, which is triggered by a transient oxidative burst in tapetum [20] and is closely associated with cellular vacuolations [46]. Here, we found the tapetal cells of ms33-6038 anthers experienced severe vacuolations and even lost their nuclear structure compared with those of WT anthers at stage S9 by TEM analysis (Figure 7A). The premature and excessive vacuolation have been demonstrated to be mediated by the activated SnRK1-bZIP signaling and the downstream genes (ASN1 and DIN10) [47], which induced metabolic reprogramming by activating catabolism and repressing anabolism in ms33-6038 anthers [20]. Specifically, in ms33-6038 anther transcriptomes, the metabolic reprogramming was proven by the transcriptional alterations of genes involved in primary metabolic pathways from stages S8a to S9 (Figures S3–S5). To further uncover molecular mechanisms underlying the excessive autophagy and metabolic reprogramming besides the active SnRK1-mediated sugar signaling pathway previously reported in ms33-6038 anthers [20], we investigated the expression changes of genes in controlling metabolic homeostasis, including the TOR signaling pathway, PYL-PP2CA pathway, and SnRK2-mediated stress response pathway (Table S5). In ms33-6038 anthers, we found the repressed TOR (an energy and nutrient sensor) reflected by the downregulated expression of S6K gene involved in protein synthesis [48,49] (Figure 7B). In addition, four PP2CA genes, encoding core regulators negatively controlling plant photosynthesis and starch degeneration through abscisic acid (ABA) signaling, were upregulated in ms33-6038 anthers, consistent with the downregulated expression of two PYL genes, encoding ABA receptors those inhibit the phosphorylation activities of PP2CA proteins [50,51,52] (Figure 7B). Meanwhile, three SnRK2 homologous genes responsible for abiotic stress responses were upregulated in ms33-6038 anthers (Figure 7B). The qPCR results confirmed the expression changes of four representative genes (Figure 7C).
Collectively, the excessive ROS accumulation and oxidative stress in ms33-6038 anthers induce severe autophagy and metabolic reprogramming and the activated SnRK1-bZIP signaling pathway that can repress starch and FA syntheses, following interrupted protein synthesis by inhibiting TOR activity, repressed photosynthesis and starch degeneration by the activated PP2AC pathway and additionally activated SnRK2-mediated stress response (Figure 7D), finally result in severe phenotypic deficiencies of anther wall layers and pollen grains.
To investigate whether ZmMs33 deficiency alters the expression patterns of other GMS genes and to further reveal the underlying molecular mechanism of the severe phenotypic defects, we investigated transcriptional changes of all reported maize GMS genes in the ms33-6038 anther transcriptomes. Among the 38 reported maize GMS genes except ZmMs33 (Table S6), 20 of them (11 TF genes, 8 lipid metabolic genes, and 1 sugar metabolic gene) were significantly altered in expression levels in the ms33-6038 anther transcriptomes (Figure 8A) from stages S5 to S9, 10 of which were confirmed by qPCR analysis (Figure 8B). These results suggest loss of the ZmMs33 function severely impairs the expression of half of the reported maize GMS genes. ZmMs33 was highly expressed at stages S5 and S6 [20]. The expression peaks of the 20 GMS genes in the anther transcriptomes of 3 maize lines have consistent patterns ranging from stages S5 to S13 (Figure 8C), suggesting that ZmMs33 deficiency induces a long-term effect on the transcriptional changes of GMS genes that are expressed after ZmMs33 gene expression. Half of the 20 GMS genes were downregulated in expression levels in ms33-6038 anthers during stages S5 to S9, 6 genes were upregulated, and the remaining 4 genes displayed up- or down-regulated expressions at separated stages, indicating a complex effect of ZmMs33 deficiency on the expressions of other GMS genes. Taken together, loss of the ZmMs33 function induces a severe, long-term, and complex transcriptional reprogramming of a large number of the reported maize GMS genes, which may contribute to the excessive phenotypic alterations in ms33-6038 anthers.
Collectively, based on results previously reported and obtained in this study, we proposed a working model underlying the excessive phenotypic deficiencies in ms33-6038 anthers (Figure 9). Specifically, loss of the ZmMs33 function directly disrupts glycerophospholipid metabolism [20], leading to reduced lipid accumulation and transport related to the smooth outer surface of anthers, disabled En chloroplasts, and abnormally thin pollen exine. The specific and excessive ROS accumulation and oxidative stress responses in ms33-6038 anthers induce the premature and severe tapetal autophagy and metabolic reprogramming associated with the activated SnRK1 [20], PYL-PP2CA and SnRK2 signaling pathways, as well as the inhibited TOR pathway; meanwhile, the expression of many GMS genes that further excessively impaired the development of a four-layer anther wall and microspores were disturbed (Figure 9).

4. Discussion

4.1. Severe ROS Accumulation and Oxidative Stress in ZmMs33-Deficient Anthers among Maize GMS Lines

ZmMs33 encodes a GPAT enzyme involved in glycerophospholipid biosynthesis [19,32]. The ZmMs33-deficient anthers produce the reduced contents of membrane lipid components, which impair the function of En chloroplasts [20]. Energy-generating processes including photosynthesis produce ROS as by-products [53]. The abnormal membrane structure of En chloroplasts results in the leakage of electron transport chains in the photosynthesis process, increasing the cellular ROS content that in turn impairs the photosynthetic activity [54]. In addition, loss of the ZmMs33 function leads to enhanced FA degradation or β-oxidation in anthers suffering metabolic reprogramming [20], which is another source of excess ROS content. In ms33-6038 anthers, a large number of genes involved in four ROS production pathways and five ROS scavenging processes are changed in expression levels, breaking the critical balance of ROS dynamics and inducing excessive ROS content. The high ROS concentration can induce oxidative stress, causing cellular damage of DNA strand breaks, lipid peroxidation, membrane leakage, and cell lysis [55]. It has been proven that the number of germ cells in anthers is determined by their surrounding oxidizing status [43] and that a transient oxidative burst is closely related to tapetal degeneration [27], indicating the redox environment— represented mainly by the ROS content—is a critical determinant in plant anther development and male reproduction. A lot of genes in controlling the ROS dynamics during anther development have been characterized, and their functional deficiencies frequently cause abnormal PCD and degeneration of tapetum [26,28,29]. Similarly, excessive ROS content triggers premature and severe vacuolations in ms33-6038 tapetal cells, leading to premature tapetal degeneration and abnormal pollen exine, as well as the lack of a cutin and wax layer [20,32]. Unlike ms33-6038 anthers, the majority of marker genes involved in ROS production and scavenging were normally expressed in the other five investigated GMS lines during anther development. The result that the ROS content seriously exceeds the homeostatic level in ms33-6038 anthers may reflect the specific role of this GPAT gene in maintaining cellular ROS homeostasis by regulating the production of membrane lipids and impairing the homeostasis of FA metabolism among the reported maize GMS genes in controlling anther development and pollen formation.

4.2. The Phenotypic Alterations Lag behind the Preferentially Expressed Stages of ZmMs33 during Maize Anther Development

The phenotypic changes of GMS lines usually appear at or closely behind the stages when the investigated GMS gene is preferentially expressed [1,8]. The ZmMs33 gene is preferentially expressed at stages S5 and S6 before microspore meiosis, while obvious morphologic alteration was not observed in ms33-6038 anthers at the two stages. The phenotypic differences in ms33-6038 compared with WT anthers appeared mainly after stage S8a, including the enhanced •OH and ROS levels and premature tapetal vacuolations observed in this study, as well as the arrested anther length and En chloroplast development, the increased H2O2 level, the metabolic reprogramming, and the abnormal results in transverse section analysis revealed in previous studies [20,21,32]. The phenotypic lagging is reflected by the numbers and functions of DEGs in the ms33-6038 anther transcriptomes from stages S5 to S9. The numbers of DEGs between ms33-6038 and WT anthers at stages S5 and S6 are greatly less than the numbers of DEGs required by the normal development of WT anthers from stages S5 to S7, indicating the transcriptional changes in ms33-6038 anthers at stages S5 and S6 are insufficient to switch the normal development trend of anthers to an abnormal route. However, along with the development of ms33-6038 anthers, more genes are differentially expressed since stage S8a, exceeding the number of DEGs during normal anther development, which start to induce obvious phenotypic alterations in ms33-6038 anthers. In addition, the DEGs from stages S5 to S7 are functionally enriched in the biological processes not related to anther development. In contrast, the DEGs from stages S8a to S9 are enriched in the functions of metabolic reprogramming, plant hormone signal transduction, and those stress responses that fundamentally impair anther development [20,56,57]. Besides the lagging of transcriptional changes, metabolic reprogramming can generate energy and carbon supply endogenously to keep anther alive before the microspore meiosis in ms33-6038 anthers [20]. When microspores undergo meiosis, the consumption of internal substances is insufficient to support the survival of ms33-6038 anthers in which severe phenotypic alterations appear. Thus, both the transcriptional and metabolic alterations contribute to the lagging of severe phenotypic changes in ms33-6038 anthers, leading to the specificity of phenotypic lagging in ms33-6038 anthers among the reported GMS lines.

4.3. The Severe Transcriptional Reprogramming Induced by ZmMs33 Deficiency during Maize Anther Development

Though ZmMs33 encodes an enzyme, its deficiency results in thousands of DEGs in anther transcriptomes from stages S8a to S9. Interestingly, the number of DEGs in ms33-6038 anthers is equivalent to those in the GMS lines with functionally defective TF-encoding genes, such as ZmMs23 and ZmMs7 [13,15,58]. Besides the comprehensive regulatory roles of TFs on target genes, genome-wide transcriptional reprogramming can be triggered by cellular stresses, including oxidative stress [59,60]. By the transcriptional reprogramming, plants can maintain metabolic and physiological homeostasis under adverse growth environments [59]. Thus, the transcriptional reprogramming in ms33-6038 anthers may be partially triggered by the excessive oxidative stress induced by loss of the ZmMs33 function. This inference is confirmed by the results of GO and KEGG enrichment analyses in which the functions of DEGs are closely related to abiotic stress responses. Moreover, 11 reported maize GMS genes encoding TFs, including the key regulator genes modulating tapetal development (ZmbHLH122, ZmbHLH51, and ZmMs84) [10,61,62] are changed in transcription levels in ms33-6038 anthers, which strengthen transcriptional reprogramming by directly impairing the expression of target genes. Thus, ZmMs33 deficiency disturbs the expression of genes involved in both the stress response and the regulatory network of male reproduction, which brings about genome-wide transcriptional reprogramming. Furthermore, under transcriptional reprogramming, the severe oxidative stress induced by ZmMs33 deficiency finally causes complete male sterility, prompting us to think about the possible crosstalk between stress response and male sterility during plant anther development in a further study.

5. Conclusions

In conclusion, this study shows that loss of the ZmMs33 function can lead to ROS accumulation and severe oxidative stress in maize anthers, which are mediated by specific underlying mechanisms among the investigated maize GMS lines. Additionally, due to loss of the ZmMs33 function, anthers suffered metabolic reprogramming mediated by several key regulators (i.e., TOR, PP2CA, and SnRK2) in controlling metabolic homeostasis and the stress response. Excessive oxidative stress and metabolic reprogramming may induce the transcriptional reprograming of tens of reported maize GMS genes, which could explain the severe phenotypic changes in ZmMs33-deficient anthers. The interplay among lipid metabolism, ROS metabolism, and plant male sterility are worthy of further study.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/cells11152318/s1, Table S1: A summary of the transcriptomic data used in this study; Table S2: Primers used in this study; Table S3: A list of 194 genes related to the response to oxygen-containing components; Table S4: A list of 64 genes involved in ROS production, ROS scavenging, and oxidative stress responses; Table S5: A list of 32 genes involved in metabolic reprogramming; Table S6: A list of 39 reported maize GMS genes; Figure S1: Similarities of anther transcriptomic data in WT and ms33-6038 mutant from stages S5 to S9; Figure S2: Phenotypes of anthers and pollen grains of ms33-6038 and the other five maize GMS lines (ms30-6028, p5126-ZmMs7, ocl4, ms23, and mac1); Figures S3–S5: Expression changes of genes involved in primary metabolism pathways in the ms33-6038 anther transcriptomes at stages S5 and S6 (Figure S3), stages S7 and S8a (Figure S4), and stages S8b and S9 (Figure S5).

Author Contributions

Conceptualization, X.W. (Xiangyuan Wan) and Z.L.; methodology, Z.L., S.L. and T.Z.; software, Z.L.; formal analysis, Z.L., S.L. and T.Z.; investigation, S.L., T.Z., X.A., X.W. (Xun Wei), J.Z., S.W. and Z.D.; data curation, Z.L., S.L. and T.Z.; writing—original draft preparation, Z.L., Y.L., T.Z. and S.L.; writing—review and editing, X.W. (Xiangyuan Wan), Z.L., Y.L., T.Z. and S.L.; visualization, Z.L., S.L. and T.Z.; supervision, X.W. (Xiangyuan Wan) and Y.L.; project administration, X.W. (Xiangyuan Wan) and Y.L.; funding acquisition, Z.L., Y.L. and X.W. (Xiangyuan Wan). All authors have read and agreed to the published version of the manuscript.

Funding

This research was funded by the National Key Research and Development Program of China (2021YFF1000302), Fundamental Research Funds for the Central Universities of China (06500136), the Interdisciplinary Research Project for Young Teachers of USTB (Fundamental Research Funds for the Central Universities) (FRF-IDRY-20-038), and the National Natural Science Foundation of China (32172057).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

All data included in this study are available upon request by contacting the corresponding author.

Acknowledgments

We are indebted to the three anonymous referees for their valuable suggestions.

Conflicts of Interest

The authors declare no conflict of interest. Beijing Solidwill Sci-Tech Co., Ltd. has the Beijing Engineering Laboratory and the Beijing International Science and Technology Cooperation Base, which provided the research platform, instruments, and funds for this study, so the company is one of the signed units of this paper.

References

  1. Wan, X.; Wu, S.; Li, Z.; Dong, Z.; An, X.; Ma, B.; Tian, Y.; Li, J. Maize genic male-sterility genes and their applications in hybrid breeding: Progress and perspectives. Mol. Plant 2019, 12, 321–342. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  2. Zhang, D.; Yang, L. Specification of tapetum and microsporocyte cells within the anther. Curr. Opin. Plant Biol. 2014, 17, 49–55. [Google Scholar] [CrossRef] [PubMed]
  3. Gupta, P.K.; Balyan, H.S.; Gahlaut, V.; Saripalli, G.; Pal, B.; Basnet, B.R.; Joshi, A.K. Hybrid wheat: Past, present and future. Theor. Appl. Genet. 2019, 132, 2463–2483. [Google Scholar] [CrossRef] [PubMed]
  4. Wan, X.; Wu, S.; Li, X. Breeding with dominant genic male-sterility genes to boost crop grain yield in the post-heterosis utilization era. Mol. Plant 2021, 14, 531–534. [Google Scholar] [CrossRef]
  5. Wilson, Z.A.; Zhang, D.B. From Arabidopsis to rice: Pathways in pollen development. J. Exp. Bot. 2009, 60, 1479–1492. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  6. Wilson, Z.A.; Song, J.; Taylor, B.; Yang, C. The final split: The regulation of anther dehiscence. J. Exp. Bot. 2011, 62, 1633–1649. [Google Scholar] [CrossRef] [Green Version]
  7. Timofejeva, L.; Skibbe, D.S.; Lee, S.; Golubovskaya, I.; Wang, R.; Harper, L.; Walbot, V.; Cande, W.Z. Cytological characterization and allelism testing of anther developmental mutants identified in a screen of maize male sterile lines. G3 2013, 3, 231–249. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  8. Wan, X.; Wu, S.; Li, Z.; An, X.; Tian, Y. Lipid metabolism: Critical roles in male fertility and other aspects of reproductive development in plants. Mol. Plant 2020, 13, 955–983. [Google Scholar] [CrossRef]
  9. Liu, S.; Li, Z.; Wu, S.; Wan, X. The essential roles of sugar metabolism for pollen development and male fertility in plants. Crop J. 2021, 9, 1223–1236. [Google Scholar] [CrossRef]
  10. Jiang, Y.; An, X.; Li, Z.; Yan, T.; Zhu, T.; Xie, K.; Liu, S.; Hou, Q.; Zhao, L.; Wu, S.; et al. CRISPR/Cas9-based discovery of maize transcription factors regulating male sterility and their functional conservation in plants. Plant Biotechnol. J. 2021, 19, 1769–1784. [Google Scholar] [CrossRef]
  11. Liu, X.; Zhang, S.; Jiang, Y.; Yan, T.; Fang, C.; Hou, Q.; Wu, S.; Xie, K.; An, X.; Wan, X. Use of CRISPR/Cas9-based gene editing to simultaneously mutate multiple homologous genes required for pollen development and male fertility in Maize. Cells 2022, 11, 439. [Google Scholar] [CrossRef] [PubMed]
  12. Zhang, D.; Wu, S.; An, X.; Xie, K.; Dong, Z.; Zhou, Y.; Xu, L.; Fang, W.; Liu, S.; Liu, S.; et al. Construction of a multicontrol sterility system for a maize male-sterile line and hybrid seed production based on the ZmMs7 gene encoding a PHD-finger transcription factor. Plant Biotechnol. J. 2018, 16, 459–471. [Google Scholar] [CrossRef] [Green Version]
  13. An, X.; Ma, B.; Duan, M.; Dong, Z.; Liu, R.; Yuan, D.; Hou, Q.; Wu, S.; Zhang, D.; Liu, D.; et al. Molecular regulation of ZmMs7 required for maize male fertility and development of a dominant male-sterility system in multiple species. Proc. Natl. Acad. Sci. USA 2020, 117, 23499–23509. [Google Scholar] [CrossRef]
  14. Vernoud, V.; Laigle, G.; Rozier, F.; Meeley, R.B.; Perez, P.; Rogowsky, P.M. The HD-ZIP IV transcription factor OCL4 is necessary for trichome patterning and anther development in maize. Plant J. 2009, 59, 883–894. [Google Scholar] [CrossRef]
  15. Nan, G.L.; Zhai, J.; Arikit, S.; Morrow, D.; Fernandes, J.; Mai, L.; Nguyen, N.; Meyers, B.C.; Walbot, V. MS23, a master basic helix-loop-helix factor, regulates the specification and development of the tapetum in maize. Development 2017, 144, 163–172. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  16. Djukanovic, V.; Smith, J.; Lowe, K.; Yang, M.; Gao, H.; Jones, S.; Nicholson, M.G.; West, A.; Lape, J.; Bidney, D.; et al. Male-sterile maize plants produced by targeted mutagenesis of the cytochrome P450-like gene (MS26) using a re-designed I-CreI homing endonuclease. Plant J. 2013, 76, 888–899. [Google Scholar] [CrossRef]
  17. Cigan, A.M.; Singh, M.; Benn, G.; Feigenbutz, L.; Kumar, M.; Cho, M.J.; Svitashev, S.; Young, J. Targeted mutagenesis of a conserved anther-expressed P450 gene confers male sterility in monocots. Plant Biotechnol. J. 2017, 15, 379–389. [Google Scholar] [CrossRef]
  18. An, X.; Dong, Z.; Tian, Y.; Xie, K.; Wu, S.; Zhu, T.; Zhang, D.; Zhou, Y.; Niu, C.; Ma, B.; et al. ZmMs30 encoding a novel GDSL lipase is essential for male fertility and valuable for hybrid breeding in maize. Mol. Plant 2019, 12, 343–359. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  19. Xie, K.; Wu, S.; Li, Z.; Zhou, Y.; Zhang, D.; Dong, Z.; An, X.; Zhu, T.; Zhang, S.; Liu, S.; et al. Map-based cloning and characterization of Zea mays male sterility33 (ZmMs33) gene, encoding a glycerol-3-phosphate acyltransferase. Theor. Appl. Genet. 2018, 131, 1363–1378. [Google Scholar] [CrossRef] [Green Version]
  20. Zhu, T.; Li, Z.; An, X.; Long, Y.; Xue, X.; Xie, K.; Ma, B.; Zhang, D.; Guan, Y.; Niu, C.; et al. Normal structure and function of endothecium chloroplasts maintained by ZmMs33-mediated lipid biosynthesis in tapetal cells are critical for anther development in maize. Mol. Plant 2020, 13, 1624–1643. [Google Scholar] [CrossRef]
  21. Zhang, L.; Luo, H.; Zhao, Y.; Chen, X.; Huang, Y.; Yan, S.; Li, S.; Liu, M.; Huang, W.; Zhang, X.; et al. Maize male sterile 33 encodes a putative glycerol-3-phosphate acyltransferase that mediates anther cuticle formation and microspore development. BMC Plant Biol. 2018, 18, 318. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Wang, D.; Oses-Prieto, J.A.; Li, K.H.; Fernandes, J.F.; Burlingame, A.L.; Walbot, V. The male sterile 8 mutation of maize disrupts the temporal progression of the transcriptome and results in the mis-regulation of metabolic functions. Plant J. 2010, 63, 939–951. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Zhu, Y.; Shi, Z.; Li, S.; Liu, H.; Liu, F.; Niu, Q.; Li, C.; Wang, J.; Rong, T.; Yi, H.; et al. Fine mapping of the novel male-sterile mutant gene ms39 in maize originated from outer space flight. Mol. Breed. 2018, 38, 125. [Google Scholar] [CrossRef]
  24. Mittler, R. Oxidative stress, antioxidants and stress tolerance. Trends Plant Sci. 2002, 7, 405–410. [Google Scholar] [CrossRef]
  25. Zheng, S.; Li, J.; Ma, L.; Wang, H.; Zhou, H.; Ni, E.; Jiang, D.; Liu, Z.; Zhuang, C. OsAGO2 controls ROS production and the initiation of tapetal PCD by epigenetically regulating OsHXK1 expression in rice anthers. Proc. Natl. Acad. Sci. USA 2019, 116, 7549–7558. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  26. Hu, L.; Liang, W.; Yin, C.; Cui, X.; Zong, J.; Wang, X.; Hu, J.; Zhang, D. Rice MADS3 regulates ROS homeostasis during late anther development. Plant Cell 2011, 23, 515–533. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  27. Yu, S.X.; Feng, Q.N.; Xie, H.T.; Li, S.; Zhang, Y. Reactive oxygen species mediate tapetal programmed cell death in tobacco and tomato. BMC Plant Biol. 2017, 17, 76. [Google Scholar] [CrossRef] [Green Version]
  28. Yi, J.; Moon, S.; Lee, Y.S.; Zhu, L.; Liang, W.; Zhang, D.; Jung, K.H.; An, G. Defective Tapetum Cell Death 1 (DTC1) regulates ROS levels by binding to metallothionein during tapetum degeneration. Plant Physiol. 2016, 170, 1611–1623. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  29. Xie, H.T.; Wan, Z.Y.; Li, S.; Zhang, Y. Spatiotemporal production of reactive oxygen species by NADPH oxidase is critical for tapetal programmed cell death and pollen development in Arabidopsis. Plant Cell 2014, 26, 2007–2023. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  30. Kurusu, T.; Koyano, T.; Hanamata, S.; Kubo, T.; Noguchi, Y.; Yagi, C.; Nagata, N.; Yamamoto, T.; Ohnishi, T.; Okazaki, Y.; et al. OsATG7 is required for autophagy-dependent lipid metabolism in rice postmeiotic anther development. Autophagy 2014, 10, 878–888. [Google Scholar] [CrossRef]
  31. Minina, E.A.; Filonova, L.H.; Fukada, K.; Savenkov, E.I.; Gogvadze, V.; Clapham, D.; Sanchez-Vera, V.; Suarez, M.F.; Zhivotovsky, B.; Daniel, G.; et al. Autophagy and metacaspase determine the mode of cell death in plants. J. Cell Biol. 2013, 203, 917–927. [Google Scholar] [CrossRef] [Green Version]
  32. Zhu, T.; Wu, S.; Zhang, D.; Li, Z.; Xie, K.; An, X.; Ma, B.; Hou, Q.; Dong, Z.; Tian, Y.; et al. Genome-wide analysis of maize GPAT gene family and cytological characterization and breeding application of ZmMs33/ZmGPAT6 gene. Theor. Appl. Genet. 2019, 132, 2137–2154. [Google Scholar] [CrossRef] [PubMed]
  33. Somaratne, Y.; Tian, Y.; Zhang, H.; Wang, M.; Huo, Y.; Cao, F.; Zhao, L.; Chen, H. ABNORMAL POLLEN VACUOLATION1 (APV1) is required for male fertility by contributing to anther cuticle and pollen exine formation in maize. Plant J. 2017, 90, 96–110. [Google Scholar] [CrossRef]
  34. Chen, X.; Zhang, H.; Sun, H.; Luo, H.; Zhao, L.; Dong, Z.; Yan, S.; Zhao, C.; Liu, R.; Xu, C.; et al. IRREGULAR POLLEN EXINE1 is a novel factor in anther cuticle and pollen exine formation. Plant Physiol. 2017, 173, 307–325. [Google Scholar] [CrossRef] [Green Version]
  35. Li, Z.; An, X.; Zhu, T.; Yan, T.; Wu, S.; Tian, Y.; Li, J.; Wan, X. Discovering and constructing ceRNA-miRNA-target gene regulatory networks during anther development in maize. Int. J. Mol. Sci. 2019, 20, 3480. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  36. Trapnell, C.; Pachter, L.; Salzberg, S.L. TopHat: Discovering splice junctions with RNA-Seq. Bioinformatics 2009, 25, 1105–1111. [Google Scholar]
  37. Liao, Y.; Smyth, G.K.; Shi, W. The R package Rsubread is easier, faster, cheaper and better for alignment and quantification of RNA sequencing reads. Nucleic Acids Res. 2019, 47, e47. [Google Scholar] [CrossRef] [Green Version]
  38. Robinson, M.D.; McCarthy, D.J.; Smyth, G.K. edgeR: A Bioconductor package for differential expression analysis of digital gene expression data. Bioinformatics 2010, 26, 139–140. [Google Scholar]
  39. Tian, T.; Liu, Y.; Yan, H.; You, Q.; Yi, X.; Du, Z.; Xu, W.; Su, Z. agriGO v2.0: A GO analysis toolkit for the agricultural community, 2017 update. Nucleic Acids Res. 2017, 45, W122–W129. [Google Scholar] [CrossRef] [Green Version]
  40. Duan, Q.; Kita, D.; Johnson, E.A.; Aggarwal, M.; Gates, L.; Wu, H.M.; Cheung, A.Y. Reactive oxygen species mediate pollen tube rupture to release sperm for fertilization in Arabidopsis. Nat. Commun. 2014, 5, 3129. [Google Scholar]
  41. Zhang, L.; Huang, J.; Su, S.; Wei, X.; Yang, L.; Zhao, H.; Yu, J.; Wang, J.; Hui, J.; Hao, S.; et al. FERONIA receptor kinase-regulated reactive oxygen species mediate self-incompatibility in Brassica rapa. Curr. Biol. 2021, 31, 3004–3016. [Google Scholar] [CrossRef] [PubMed]
  42. Morris, P.C. MAP kinase signal transduction pathways in plants. New Phytol. 2001, 151, 67–89. [Google Scholar] [CrossRef]
  43. Kelliher, T.; Walbot, V. Hypoxia triggers meiotic fate acquisition in maize. Science 2012, 337, 345–348. [Google Scholar] [CrossRef] [Green Version]
  44. Chaubal, R.; Zanella, C.; Trimnell, M.R.; Fox, T.W.; Albertsen, M.C.; Bedinger, P. Two male-sterile mutants of Zea mays (Poaceae) with an extra cell division in the anther wall. Am. J. Bot. 2000, 87, 1193–1201. [Google Scholar] [CrossRef]
  45. Wang, C.J.; Nan, G.L.; Kelliher, T.; Timofejeva, L.; Vernoud, V.; Golubovskaya, I.N.; Harper, L.; Egger, R.; Walbot, V.; Cande, W.Z. Maize multiple archesporial cells 1 (mac1), an ortholog of rice TDL1A, modulates cell proliferation and identity in early anther development. Development 2012, 139, 2594–2603. [Google Scholar] [CrossRef] [Green Version]
  46. Vizcay-Barrena, G.; Wilson, Z.A. Altered tapetal PCD and pollen wall development in the Arabidopsis ms1 mutant. J. Exp. Bot. 2006, 57, 2709–2717. [Google Scholar] [CrossRef] [PubMed]
  47. Mair, A.; Pedrotti, L.; Wurzinger, B.; Anrather, D.; Simeunovic, A.; Weiste, C.; Valerio, C.; Dietrich, K.; Kirchler, T.; Nagele, T.; et al. SnRK1-triggered switch of bZIP63 dimerization mediates the low-energy response in plants. Elife 2015, 4, e05828. [Google Scholar] [CrossRef]
  48. Smeekens, S.; Ma, J.; Hanson, J.; Rolland, F. Sugar signals and molecular networks controlling plant growth. Curr. Opin. Plant Biol. 2010, 13, 274–279. [Google Scholar] [CrossRef]
  49. Garrocho-Villegas, V.; de Jimenez, E.S. TOR pathway activation in Zea mays L. tissues: Conserved function between animal and plant kingdoms. Plant Signal. Behav. 2012, 7, 675–677. [Google Scholar] [CrossRef] [Green Version]
  50. Rodrigues, A.; Adamo, M.; Crozet, P.; Margalha, L.; Confraria, A.; Martinho, C.; Elias, A.; Rabissi, A.; Lumbreras, V.; Gonzalez-Guzman, M.; et al. ABI1 and PP2CA phosphatases are negative regulators of Snf1-related protein kinase1 signaling in Arabidopsis. Plant Cell 2013, 25, 3871–3884. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  51. Ramon, M.; Rolland, F.; Thevelein, J.M.; Van Dijck, P.; Leyman, B. ABI4 mediates the effects of exogenous trehalose on Arabidopsis growth and starch breakdown. Plant Mol. Biol. 2007, 63, 195–206. [Google Scholar] [CrossRef]
  52. Penfield, S.; Li, Y.; Gilday, A.D.; Graham, S.; Graham, I.A. Arabidopsis ABA INSENSITIVE4 regulates lipid mobilization in the embryo and reveals repression of seed germination by the endosperm. Plant Cell 2006, 18, 1887–1899. [Google Scholar] [CrossRef] [Green Version]
  53. Mittler, R.; Vanderauwera, S.; Gollery, M.; Van Breusegem, F. Reactive oxygen gene network of plants. Trends Plant Sci. 2004, 9, 490–498. [Google Scholar] [CrossRef]
  54. Farooq, M.A.; Niazi, A.K.; Akhtar, J.; Saifullah; Farooq, M.; Souri, Z.; Karimi, N.; Rengel, Z. Acquiring control: The evolution of ROS-induced oxidative stress and redox signaling pathways in plant stress responses. Plant Physiol. Biochem. 2019, 141, 353–369. [Google Scholar] [CrossRef]
  55. Van Breusegem, F.; Dat, J.F. Reactive oxygen species in plant cell death. Plant Physiol. 2006, 141, 384–390. [Google Scholar] [CrossRef] [Green Version]
  56. Zhang, Z.; Hu, M.; Xu, W.; Wang, Y.; Huang, K.; Zhang, C.; Wen, J. Understanding the molecular mechanism of anther development under abiotic stresses. Plant Mol. Biol. 2021, 105, 1–10. [Google Scholar] [CrossRef] [PubMed]
  57. Zheng, Y.; Wang, D.; Ye, S.; Chen, W.; Li, G.; Xu, Z.; Bai, S.; Zhao, F. Auxin guides germ-cell specification in Arabidopsis anthers. Proc. Natl. Acad. Sci. USA 2021, 118, e2101492118. [Google Scholar] [CrossRef]
  58. Li, Z.; Zhu, T.; Liu, S.; Jiang, Y.; Liu, H.; Zhang, Y.; Xie, K.; Li, J.; An, X.; Wan, X. Genome-wide analyses on transcription factors and their potential microRNA regulators involved in maize male fertility. Crop J. 2021, 9, 1248–1262. [Google Scholar] [CrossRef]
  59. Himanen, S.V.; Sistonen, L. New insights into transcriptional reprogramming during cellular stress. J. Cell Sci. 2019, 132, jcs238402. [Google Scholar] [CrossRef] [PubMed]
  60. Vihervaara, A.; Duarte, F.M.; Lis, J.T. Molecular mechanisms driving transcriptional stress responses. Nat. Rev. Genet. 2018, 19, 385–397. [Google Scholar] [CrossRef]
  61. Nan, G.L.; Teng, C.; Fernandes, J.; O’Connor, L.; Meyers, B.C.; Walbot, V. A cascade of bHLH-regulated pathways programs maize anther development. Plant Cell 2022, 34, 1207–1225. [Google Scholar] [CrossRef] [PubMed]
  62. Liu, X.; Yue, Y.; Gu, Z.; Huang, Q.; Pan, Z.; Zhao, Z.; Zheng, M.; Zhang, Z.; Li, C.; Yi, H.; et al. The characterization and candidate gene isolation for a novel male-sterile mutant ms40 in maize. Plant Cell Rep. 2021, 40, 1957–1970. [Google Scholar]
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Figure 1. Phenotypic comparisons of anthers, anther wall layers, and pollen grains between WT and ms33-6038 mutant. (A) Phenotypic comparison of WT and ms33-6038 anthers at stages S8b and S9. (B) Phenotypic comparisons of epidermis (Ep), endothecium (En), and tapetum (Ta) layers in WT and ms33-6038 anthers. (C) Phenotypic comparison of WT and ms33-6038 pollen grains.
Figure 1. Phenotypic comparisons of anthers, anther wall layers, and pollen grains between WT and ms33-6038 mutant. (A) Phenotypic comparison of WT and ms33-6038 anthers at stages S8b and S9. (B) Phenotypic comparisons of epidermis (Ep), endothecium (En), and tapetum (Ta) layers in WT and ms33-6038 anthers. (C) Phenotypic comparison of WT and ms33-6038 pollen grains.
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Figure 2. Sampling and the quality of RNA-seq data of WT and ms33-6038 anther transcriptomes. (A) Semi-thin transverse section analysis of WT and ms33-6038 anthers from stages S5 to S9. Dy, dyad; E, epidermis; En, endothecium; MC, meiocyte; ML, middle layer; MMC, microspore mother cell; Msp, microspore; Sp, sporogenous cell; T, tapetum; Tds, tetrads. Scale bars, 50 μm. (B) SEM analysis of WT and ms33-6038 anthers from stages 5 to 9. Scale bars, 0.5 mm (C) Comparisons of the transcriptomic data of WT (left) and ms33-6038 (right) anthers at six stages. The similarity between two samples was estimated by Pearson’s correlation coefficient.
Figure 2. Sampling and the quality of RNA-seq data of WT and ms33-6038 anther transcriptomes. (A) Semi-thin transverse section analysis of WT and ms33-6038 anthers from stages S5 to S9. Dy, dyad; E, epidermis; En, endothecium; MC, meiocyte; ML, middle layer; MMC, microspore mother cell; Msp, microspore; Sp, sporogenous cell; T, tapetum; Tds, tetrads. Scale bars, 50 μm. (B) SEM analysis of WT and ms33-6038 anthers from stages 5 to 9. Scale bars, 0.5 mm (C) Comparisons of the transcriptomic data of WT (left) and ms33-6038 (right) anthers at six stages. The similarity between two samples was estimated by Pearson’s correlation coefficient.
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Figure 3. Transcriptome analysis of RNA-seq data of WT and ms33-6038 anthers. (A) Principal component analysis of WT and ms33-6038 anther transcriptomes from stages S5 to S9. (B) Hierarchical clustering of WT and ms33-6038 anther transcriptomes from stages S5 to S9. (C) The number of DEGs between WT and ms33-6038 anther transcriptomes and between adjacent developmental stages from stages S5 to S9. (D) GO enrichment analysis of DEGs between WT and ms33-6038 anther transcriptomes at each of six stages. (E) GO enrichment analysis of up- or down-regulated DEGs in ms33-6038 anther transcriptome compared to WT from stages S8a to S9.
Figure 3. Transcriptome analysis of RNA-seq data of WT and ms33-6038 anthers. (A) Principal component analysis of WT and ms33-6038 anther transcriptomes from stages S5 to S9. (B) Hierarchical clustering of WT and ms33-6038 anther transcriptomes from stages S5 to S9. (C) The number of DEGs between WT and ms33-6038 anther transcriptomes and between adjacent developmental stages from stages S5 to S9. (D) GO enrichment analysis of DEGs between WT and ms33-6038 anther transcriptomes at each of six stages. (E) GO enrichment analysis of up- or down-regulated DEGs in ms33-6038 anther transcriptome compared to WT from stages S8a to S9.
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Figure 4. Active oxidative stress responses and increased ROS accumulation in ms33-6038 anthers. (A) KEGG pathway enrichment analysis of 712 upregulated and 462 downregulated genes between ms33-6038 and WT anthers from stages S8a to S9. (B) Expression changes of 194 genes related to the response to oxygen-containing component between ms33-6038 and WT anthers from stages S5 to S9. The 194 genes were functionally grouped into 7 types including ROS response (Table S3). FC, fold change. (C,D) Fluorescence imaging and relative quantification of the •OH contents (C) and the total ROS levels (D) in WT and ms33-6038 anthers from stages S6 to S13. * p < 0.05, ** p < 0.01, *** p < 0.001, Student’s t-test.
Figure 4. Active oxidative stress responses and increased ROS accumulation in ms33-6038 anthers. (A) KEGG pathway enrichment analysis of 712 upregulated and 462 downregulated genes between ms33-6038 and WT anthers from stages S8a to S9. (B) Expression changes of 194 genes related to the response to oxygen-containing component between ms33-6038 and WT anthers from stages S5 to S9. The 194 genes were functionally grouped into 7 types including ROS response (Table S3). FC, fold change. (C,D) Fluorescence imaging and relative quantification of the •OH contents (C) and the total ROS levels (D) in WT and ms33-6038 anthers from stages S6 to S13. * p < 0.05, ** p < 0.01, *** p < 0.001, Student’s t-test.
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Figure 5. Transcriptional changes of genes related to ROS metabolism and oxidative stress responses in ms33-6038 anthers. (A) Expression changes of 64 genes involved in ROS production, ROS scavenging, and oxidative stress responses. (B) Validation of expression change patterns of 15 representative genes related to ROS metabolism and oxidative stress response by qPCR analysis. * p < 0.05, ** p < 0.01, Student’s t-test.
Figure 5. Transcriptional changes of genes related to ROS metabolism and oxidative stress responses in ms33-6038 anthers. (A) Expression changes of 64 genes involved in ROS production, ROS scavenging, and oxidative stress responses. (B) Validation of expression change patterns of 15 representative genes related to ROS metabolism and oxidative stress response by qPCR analysis. * p < 0.05, ** p < 0.01, Student’s t-test.
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Figure 6. Transcriptome analysis of ROS and oxidative stress-related genes between ms33-6038 and each of the other five GMS lines. (A) The expression heatmap of ROS and oxidative stress-related genes in ms33-6038 and the other five GMS lines (ms30-6028, p5126-ZmMs7, ocl4, mac1, and ms23). Arrow indicates a gene with a similar expression change to that in ms33-6038 anthers. (B) A summary of the numbers and percentages of ROS and oxidative stress-related genes with similar expression changes to ms33-6038 in each GMS line.
Figure 6. Transcriptome analysis of ROS and oxidative stress-related genes between ms33-6038 and each of the other five GMS lines. (A) The expression heatmap of ROS and oxidative stress-related genes in ms33-6038 and the other five GMS lines (ms30-6028, p5126-ZmMs7, ocl4, mac1, and ms23). Arrow indicates a gene with a similar expression change to that in ms33-6038 anthers. (B) A summary of the numbers and percentages of ROS and oxidative stress-related genes with similar expression changes to ms33-6038 in each GMS line.
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Figure 7. Premature and excessive tapetal autophagy and the underlying mechanism of metabolic reprogramming in ms33-6038 anthers. (A) Premature and excessive tapetal autophagy in ms33-6038 anthers. (B) Expressions changes of genes involved in metabolic reprogramming related to SnRK1, TOR, PP2CA pathways, and oxidative stress responses in the ms33-6038 anther transcriptomes. (C) Validation of expression change patterns of four representative genes related to metabolic reprogramming by qPCR analysis. * p < 0.05, ** p < 0.01, *** p < 0.001, Student’s t-test. (D) The potential molecular mechanism of metabolic reprogramming in ms33-6038 anthers.
Figure 7. Premature and excessive tapetal autophagy and the underlying mechanism of metabolic reprogramming in ms33-6038 anthers. (A) Premature and excessive tapetal autophagy in ms33-6038 anthers. (B) Expressions changes of genes involved in metabolic reprogramming related to SnRK1, TOR, PP2CA pathways, and oxidative stress responses in the ms33-6038 anther transcriptomes. (C) Validation of expression change patterns of four representative genes related to metabolic reprogramming by qPCR analysis. * p < 0.05, ** p < 0.01, *** p < 0.001, Student’s t-test. (D) The potential molecular mechanism of metabolic reprogramming in ms33-6038 anthers.
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Figure 8. Expression changes of all reported maize GMS genes in ms33-6038 anthers. (A) Expression changes of all 38 reported maize GMS genes in ms33-6038 anther transcriptomes. (B) Validation of the expression change patterns of 10 differentially expressed GMS genes by qPCR analysis. * p < 0.05, ** p < 0.01, *** p < 0.001, Student’s t-test. (C) Expression patterns of ZmMs33 and 20 differentially expressed GMS genes in anther transcriptomes of 3 maize lines. (D) Numbers of upregulated and downregulated genes among the 20 differentially expressed GMS genes.
Figure 8. Expression changes of all reported maize GMS genes in ms33-6038 anthers. (A) Expression changes of all 38 reported maize GMS genes in ms33-6038 anther transcriptomes. (B) Validation of the expression change patterns of 10 differentially expressed GMS genes by qPCR analysis. * p < 0.05, ** p < 0.01, *** p < 0.001, Student’s t-test. (C) Expression patterns of ZmMs33 and 20 differentially expressed GMS genes in anther transcriptomes of 3 maize lines. (D) Numbers of upregulated and downregulated genes among the 20 differentially expressed GMS genes.
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Figure 9. A reconstructed working mode underlying excessive phenotypic deficiencies in ms33-6038 anthers. ZmMs33 deficiency induces an excessive ROS accumulation and metabolic reprogramming in tapetum, further impairs the expression and function of many other GMS genes, and finally leads to severe phenotypic deficiencies in the development of an anther wall and pollen grains.
Figure 9. A reconstructed working mode underlying excessive phenotypic deficiencies in ms33-6038 anthers. ZmMs33 deficiency induces an excessive ROS accumulation and metabolic reprogramming in tapetum, further impairs the expression and function of many other GMS genes, and finally leads to severe phenotypic deficiencies in the development of an anther wall and pollen grains.
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Li, Z.; Liu, S.; Zhu, T.; An, X.; Wei, X.; Zhang, J.; Wu, S.; Dong, Z.; Long, Y.; Wan, X. The Loss-Function of the Male Sterile Gene ZmMs33/ZmGPAT6 Results in Severely Oxidative Stress and Metabolic Disorder in Maize Anthers. Cells 2022, 11, 2318. https://doi.org/10.3390/cells11152318

AMA Style

Li Z, Liu S, Zhu T, An X, Wei X, Zhang J, Wu S, Dong Z, Long Y, Wan X. The Loss-Function of the Male Sterile Gene ZmMs33/ZmGPAT6 Results in Severely Oxidative Stress and Metabolic Disorder in Maize Anthers. Cells. 2022; 11(15):2318. https://doi.org/10.3390/cells11152318

Chicago/Turabian Style

Li, Ziwen, Shuangshuang Liu, Taotao Zhu, Xueli An, Xun Wei, Juan Zhang, Suowei Wu, Zhenying Dong, Yan Long, and Xiangyuan Wan. 2022. "The Loss-Function of the Male Sterile Gene ZmMs33/ZmGPAT6 Results in Severely Oxidative Stress and Metabolic Disorder in Maize Anthers" Cells 11, no. 15: 2318. https://doi.org/10.3390/cells11152318

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