Int J Biol Sci 2018; 14(3):294-305. doi:10.7150/ijbs.23898 This issue
1. College of Animal Science and Technology, Qingdao Agricultural University, Qingdao 266109, China;
2. Center for Reproductive Medicine, Qingdao Women's and Children's Hospital, Qingdao University, Qingdao 266034, China;
3. College of Life Sciences, Institute of Reproductive Sciences, Qingdao Agricultural University, Qingdao 266109, China;
4. College of Biological and Pharmaceutical Engineering, Wuhan Polytechnic University, Wuhan 430023, China
Zearalenone (ZEA), a metabolite of Fusarium fungi, is commonly found on moldy grains. Because it can competitively combine to estrogen receptor to disrupt estrogenic signaling, it has been reported to have serious adverse effects on animal reproduction systems. In order to explore the genotoxic effects of ZEA exposure on ovarian somatic cells, porcine granulosa cells were exposed to 10 μM and 30 μM ZEA for 24 or 72 h in vitro. The results showed that ZEA exposure for 24 h remarkably reduced the proliferation of porcine granulosa cells in a dose-dependent manner as determined by MTT analysis and flow cytometry. Furthermore, exposure to ZEA for 72 h induced apoptosis, and RNA sequence analysis also revealed that the expression of apoptosis related genes were altered. RT-qPCR, immunofluorescence and western blot analysis further confirmed the expression of DNA damage and repair related genes (γ-H2AX, BRCA1, RAD51 and PRKDC) were increased in ZEA exposed granulosa cells. When the estrogen antagonist, tamoxifen, was added with ZEA in the culture medium, the DNA damage and repairment by ZEA returned to normal level. Collectively, these results illustrate that ZEA disrupts genome stability and inhibits growth of porcine granulosa cells via the estrogen receptors which may promote granulosa cell apoptosis when the DNA repair system is not enough to rescue this serious damage.
Keywords: Zearalenone, Granulosa cells, Genomic stability, DNA damage
Mycotoxin that is mainly produced by Fusarium fungi and widely distributed in the temperate regions of the world . ZEA is generally found in contaminated corn, wheat, oatmeal and other livestock feeds [2, 3]. ZEA has structural similarity with 17β-estradiol (E2), and has been shown to competitively bind to estrogen receptors (ERs) and exert estrogenic effects in animals [4-8]. Moreover, ZEA has also been shown to be hepatotoxic, haematotoxic, immunotoxic and genotoxic.
Due to the estrogenic characteristic ZEA has been considered as a mammalian endocrine disrupter to produce adverse effects on the reproductive system [10, 11]. ZEA mainly has the effects on tissues, including the ovary, uterus, mammary glands and testes where the expression of ERs is high . ZEA exposure can lead to malignancies of the uterus, ovary and mammary gland in estrogen-dependent manner . Pre-pubertal Beagle bitches were exposed to low concentration of ZEA (75 μg/kg body weight (bw)) at 112 days, and the expression of β-ERs were affected in the ovary . Moreover, ZEA, alpha-zearalenol (α-ZOL) and bate-zearalenol (β-ZOL) can affect steroidogenesis in granulosa cells and increase progesterone (P4) level . ZEA and ethinyl estradiol accelerated the vaginal opening and increased uterine weight and antral follicle numbers in the ovary resulting from the increased expression of gonadotropin releasing hormone (GnRH) . Furthermore, ZEA and α-ZOL can also inhibit the synthesis and secretion of follicle stimulating hormone (FSH) in pigs through the non-classical estrogen membrane receptor GPR30 .
There are a number of examples to show that ZEA increases the oxidative stress in farm animals [9, 13, 18, 19]. Our previous studies have shown that ZEA increased the levels of reactive oxygen species (ROS) and repressed the activity and expression of anti-oxidative enzymes in porcine granulosa cells or oocytes at the concentrations from 15 μM to 60 μM [4, 5]. Moreover, in post weaned gilts serum alanine aminotransferase, aspartate aminotransferase, γ-glutamate transferase and alkaline phosphatase concentrations in liver and serum were increased linearly in a ZEA dose dependent manner but activities of glutathione peroxidase and superoxide dismutase and spleen weight were decreased as dietary ZEA increased . In the liver and spleen, it was observed that ZEA exposure induced different effects on oxidative stress and inflammation . When pregnant rats were fed with diets containing ZEA from gestation days (GD) 1 to 7 and then fed with ZEA-free diets until their offspring were weaned, interleukin-8 and glutathione peroxidase (GPx2) were altered in the gastrointestinal tract of offspring . Furthermore, ZEA exposure not only increased lipid peroxidation, but also induced oxidative DNA damage and inhibited DNA and protein syntheses [23-25]. It has been also reported that ROS may be the factor leading to decrease in mitochondrial membrane potential (MMP) and increase in DNA damage when exposed to ZEA . Several reports also suggested that oxidative damage seemed to be an important determinant of ZEA in vitro and in vivo [27, 28]. It was also found vitamin E could alleviate oxidative stress induced by ZEA and restore cell viability of Leydig cells but limit to restore other functions, showing that ROS production was not mainly caused by steroidogenic failure .
It is well known that maintenance of genomic stability is critical for the wellbeing of organisms . ZEA exposure can induce DNA double-strand breaks (DSBs) and upregulate the expression of ataxia telangiectasia mutated (ATM) and p53 family genes . The ATM pathway is responsible primarily for DNA-DSBs, ZEA exposure induced oxidative DNA-DSBs and the expression of ATM, and an increase in the concentration of ZEA further increased DNA damage [24, 31]. It has been found that ZEA can arrest the cell cycle at S and G2/M phases to block DNA replication in some somatic cells of the reproductive system . However, it is unknown the influence of ZEA on genomic stability of ovarian granulosa cells which played vital roles during oocytes growth and development. Therefore, the aim of this investigation was to explore ZEA genotoxicity in the ovarian granulosa cells and the underlying mechanisms.
The ovaries of adolescent sows were collected from the Pig Production Cooperation of Qingdao Wan Fu (Qingdao, Shandong, China). The ovaries were saved in saline, maintained at 37 °C, and transported to laboratory within around 2 h. The procedures of animal and tissue handling performed in this study were approved by the Ethics Committee of Qingdao Agricultural University.
Antral follicles with diameter more than 3 mm were used for porcine granulosa cells collected by a syringe (10 ml with 18-gauge needles). The collected granulosa cells were centrifuged at 1,500 rpm for 3 min as previously described . Washing out the blood cells with phosphate-buffered saline (PBS) followed by centrifugation at 1,500 rpm for 3 min. Finally, the granulosa cells were cultured in DMEM high glucose medium (HyClone, SH30022.01, Beijing, China), adding 10 % fetal bovine serum (FBS; Gibco, 10099-141, Australia), 1 % penicillin and streptomycin at 37 °C, 5 % CO2 .
ZEA (Sigma, Z2125, MO, USA) was dissolved in DMSO at 20 mM concentration and stored at - 20 ºC. Granulosa cells were cultured in 96-well plates or 6-well plates at a density of 5,000 cells or 1×10 5 cells per well, respectively. The cells were allowed to grow for 24 h, then the cells were incubated for 24 and 72 h with 10 μM or 30 μM ZEA. Control group was treated with DMSO at the same concentration in ZEA-treated groups.
MTT Detection Kit (Solarbio, M8180, Beijing, China) was utilized to detected cells growth. Briefly, after 24 or 72 h ZEA treatment, medium was removed and 50 μl/well MTT solution in blank medium was added to the 96-well plate and incubated for 4 h, and then 150 μl DMSO was added to each well and incubated at 37 ºC in the dark for 1 h. Finally, the plates were read at 570 and 630 nm using Microplate Reader (Bio-Rad, iMarkTM, USA).
Granulosa cells were treated with ZEA at 10 μM and 30 μM for 24 h and 72 h. Then they were collected and washed three times using PBS. Annexin V-FITC/PI kit (Tran, Fa101, Beijing, China) was used to detect apoptosis or necrosis of porcine granulosa cells by flow cytometry referring to the manufacturer's instruction.
According to the basis of DNA content, flow cytometry was used to analyze the cell-cycle distribution. After cultured for 24 and 72 h, granulosa cells were collected and washed two times using PBS. Then cells were fixed in 70 % ethanol for 2 h followed by centrifugation at 1,500 rpm for 3 min. And cells were stained by PI (BBI, E607306, Shanghai, China) and RNaseA (10 mg/ml, Beyotime, ST572, Nantong, China) for 10 min in the dark. All groups were collected 10,000 cells, respectively, for each analysis. The cell-cycle profile was analyzed with Flowjo 7.6 software.
Total RNA was extracted from granulosa cells using an RNAprep pure MicroKit (Aidlab, RN28, Beijing, China). Then total RNA was reverse transcribed into cDNA by cDNA Synthesis Kit (TransGen, AT311-03, Beijing, China). The reaction program was: 25 ºC for 10 min, 42 ºC for 15 min, 85 ºC 30 s, and 4 °C for cooling. Then the cDNA library was sequenced at Novogene Co. (Beijing, China). There were 3 independent samples sequenced. The sequencing data obtained with Illumina Hiseq 2000 sequencing system (San Diego, CA, USA) was aligned to reference genome by HISAT2 software. Next SAMTOOLS software were used to convert sam files to bam files and sort bam files. Then HTSeq software were used to count the amount of gene expression. Finally R Bioconductor/DESeq2 was applied for plotting differential and abundance expression results from HTSeq. The R Bioconductor/ clusterProfiler was applied for GO and KEGG enrich analysis. The bioinformatic analysis has been previously described [35-39].
RT-qPCR reaction was carried out on LC480 (Roche, Germany). A 20 μl reaction solution containing 0.8 μl of primers (20 μM), 2 μl cDNA, 10 μl of SYBR green, and 7.2 μl of nuclease-free water. The PCR reaction was 95 ºC for 10 min, 35 cycles at 95 ºC for 10 s, annealing at 60 ºC for 30 s. GAPGH was used as reference and the expression was analyzed by the formula 2 - (target gene CT value -reference gene CT. All the primers that used in this study were provided in Table S1.
After treatment, the granulosa cells were fixed in 4 % paraformaldehyde at 4 ºC for 1 h, and permeated with 1 % (V/V) Triton X- 100 for 20 min at 37 ºC. After washed with PBS, the samples were blocked with 10 % goat serum dissolved in PBST for 1 h, then incubated with anti-γ-H2AX (1:100 dilution, Bioworld, BS4760, Nanjing, China); anti-BRCA1 (BBI, 20321); anti-RAD51 (BBI, D262104) overnight at 4 ºC. After washed with 1 % BSA in PBS three times, the samples were labeled with CY3-conjugated goat anti-Rabbit IgG (H+I) (Beyotime, A0521) for 1 h at 37 ºC. Finally, it was stained for 5 min with Hoechst 33342, washed with PBS and examined under Olympus fluorescence microscope (BX51, Japan). Counting full positive cells of 5 different regions, then positive cells than in the total cells. Finally taking the average of 5 different regions.
Using the results of the immunofluorescent staining, defined a region of interest (ROI) by Image J software (v.1.47) to determine the average fluorescence intensity per unit area. We compared the average intensities between ZEA treated and control cells by using the average values of 5 different regions.
Western blotting analysis was followed the standard methods [40, 41]. The proteins were separated by SDS-PAGE and were transferred onto PVDF membranes. Then the membranes were blocked with 5 % BSA for 1 h, and then were incubated with primary antibodies: anti-GAPDH (ImmunoWay, YM3040, USA), anti-RAD51 (BBI, D262104), anti-XRCC4 (BBI, D151845), anti-TP53 (BBI, D120082), anti-RPA2 (BBI, D123054), anti-USP1 (BBI, D123511), anti-CCND1 (BBI, D220509), anti-ACTIN (Abcam, ab8226, USA) at the concentration of 1.0 μg/ml overnight at 4 °C. Then after washing three times in TBST (Tris-buffered saline, pH 7.4, containing 0.05 % Tween-20), the membranes were incubated at room temperature for 1 h with secondary antibodies (HRP - conjugated goat anti - rabbit lgG (H + L); BBI, D0216) or (HRP-conjugated goat anti-mouse lgG (H+L); Beyotime, A0216) at a dilution of 1:2000 in TBST. Actin/GAPDH was used as internal controls and the data were analyzed by using IPWIN software.
Each set of experiments were repeated at least three times, and data were represented as mean ±SD. Significance between groups was statistically analyzed via one-way analysis of variance (ANOVA) followed by the Tukey's test for multiple comparisons using Graph-Pad Prism analysis software. Results were considered statistically significant at P < 0.05 (*) and P < 0.01 (**).
To study the effect of ZEA on the growth of porcine granulosa cells, they were exposed to 10 μM or 30 μM ZEA and cultured in vitro for 24 h and 72 h (Figure 1A). MTT analysis showed that granulosa cell growth was significantly decreased following 30 μM ZEA exposure for 24 h and 72 h (P < 0.05 or P < 0.01), compared with that in the control group (Figure 1B). Cell cycles profiles of the granulosa cells were also changed following ZEA exposure for 24 h and 72 h, particularly for 72 h (Figure 1C).
Furthermore, the percentages of apoptotic granulosa cells was significantly increased following ZEA exposure for 72 h (10 μM, 12.29 % ± 0.01; 30 μM, 44.09 % ± 0.02) compared with the control group (6.38 % ± 0.01; Figure 2A-B). However, there was no significant difference between ZEA exposure and control group for 24 h.
To study the effects of ZEA on gene expression of granulosa cell and investigate the mechanism of granulosa cell apoptosis, RNA-seq was performed. With FDR-the False discovery rate at < 0.1, 11,825 genes were identified including 263 differentially expressed genes (DEGs) between the control group and 10 μM ZEA-treated group, 1,904 DEGs between the control group and 30 μM ZEA-treated group, and 1,839 DEGs between 30 μM and 10 μM ZEA-treated groups (Figure 3A), and a heat map was obtained for these DEGs (Figure 3B). After analyzing using principal components analysis (PCA), Figure 3C showed three repeats of different genes from RNA-seq data of control group and ZEA-treated group. Then the DEGs were analyzed by GO-enriched and the results showed that there were a great number of enriched genes in mitotic cell cycle checkpoint, cell cycle regulation, apoptosis process regulation, cell proliferation regulation and phosphorylation regulation (Figure 3D and Figure S2). Next, we chose the DEGs and its degree of difference were greater than 20 fold from the control vs ZEA-treated groups. The DEGs between the control and 30 μM ZEA-treated group were enriched in the nuclear factor-kappa B (NF-kB) pathway (Figure 3E).
Effect of ZEA on the proliferation of procine granulosa cells in vitro. The procine granulosa cells were cultured in vitro and treated with 0 μM, 10 μM and 30 μM of ZEA for 24 h or 72 h. (A) The morphology of porcine granulosa cells exposed to ZEA for 24 h or 72 h. (B) Cell viability was analyzed by the MTT assay that was used to measure the absorbance of porcine granulosa cells at 570 nm and 630 nm. The cell viability of porcine granulosa cells between the control group and ZEA-treatment groups was determined using the formula: A570-A630/A570 (treated with ZEA)/A570-A630/A570 (control). Control value was taken as 1. (C) Cell cycle of procine granulosa cells was determined by flow cytometer after propidium iodide (PI) staining. Compared to the control group, * indicates significant differences (P < 0.05), ** indicated extremely significant differences (P < 0.01). All experiments were repeated at least three times.
ZEA-induced apoptosis in porcine granulosa cells. (A) Porcine granulosa cells were cultured in the presence of ZEA (10 μM and 30 μM) for 24 h or 72 h and stained with Annexin V and Propidium. Cell apoptosis levels were determined using flow cytometry. (B) the apoptotic and necrotic percentages of porcine granulosa cells were analyzed acording to the results of flow cytometry. All experiments were repeated at least three times.
To further verify ZEA exposure disrupted the signaling pathways from GO-enriched analysis, 10 genes were selected and quantified by RT-qPCR. ZEA exposure significantly up-regulated the mRNA expression of DNA damage repair related genes, such as BRCA1, RAD51 and PRKDC, and strikingly decreased 53BP1, an apoptosis and cell cycle checkpoint related gene (P < 0.01; Figure 4). However, there was no significantly different expression of ATR, ATM, CHEK1, CHEK2, MRE11A and XRCC6. The result of the qRT-PCR was consistent with the date of the RNA-seq. Furthermore, the protein expression levels of XRCC4, TP53, USP1, RPA2 and CCND1 were significantly reduced, but RAD51 was significantly up-regulated, in the ZEA-treated groups compared with that in the control groups (P < 0.05 or P < 0.01; Figure 5).
To further determine whether ZEA exposure caused DNA damage, we analyzed the percentage of γ-H2AX positive cells following ZEA treatment for 24 h (Figure 6A). The percentage of γ-H2AX positive cells was significantly increased in the 10 μM (86.00 % ± 0.03) and 30 μM ZEA treated group (91.33 % ± 0.02) compared with that in the control group (43.33 % ± 0.06) (P < 0.05; Figure 6B). Moreover, the fluorescent intensity of γ-H2AX positive cells in 30 μM ZEA treatment was also remarkably increased by 1.44 fold compared with that in the control group (P < 0.05; Figure 6C).
The percentages of RAD51 positive cells was significantly increased in the 10 μM (54.25 % ± 0.09) and 30 μM ZEA treated group (59.63 % ± 0.02) compared with that in the control group (24.70 % ± 0.06) (P < 0.01; Figure 7A, 7B). Furthermore, the fluorescent intensity of RAD51 positive cells in 30 μM ZEA treatment was also significantly increased about 2.05 fold compared with that in the control group (P < 0.05) (Figure 7C).
Finally, there was a significant increase in the percentage of BRCA1 positive cells exposed to 10 μM or 30 μM ZEA for 24 h (P < 0.05 or P < 0.01; Figure 8A, 8B), and the fluorescent intensity of BRCA1positive cells was strikingly increased by 1.55 fold and 1.92 fold in 10 μM and 30 μM ZEA treated groups compared with that of the control group (P < 0.05 or P < 0.01; Figure 8C).
In order to explore the disruption in genomic stability in granulosa cells by ZEA via ER pathway, porcine granulosa cells were exposed to ZEA and ER antagonist tamoxifen for 72 h. There were no significant differences in the protein levels of DNA damage or repairment related genes RAD51, USP1, XRCC1 and RPA2 between the control group and the ZEA and tamoxifen groups (Figure 9).
RNA-seq analysis of granulosa cells in control and ZEA-treated groups. (A) Venn diagram demonstrating the different expression of genes between the control group and ZEA-treated groups. (B) Heatmap indicating the group differences of differentially expressed genes (DEGs) between the control group and the ZEA-treated groups, and the repeatability within each group. (C) principal components analysis (PCA) analysis. The 8 samples were shown in the 2D plane splanned by the first three principal components. (D) Scattergram of Gene Ontology (GO) enrich in biological process categories. (E) Different genes of the control group and the 30 μM ZEA-treated group enriched in the NF-kB pathway via Gene Set Enrichment Analysis (GSEA).
The mRNA expression of genes in granulosa cells in response to ZEA exposure (10 μM and 30 μM) in porcine granulosa cells for 24 h. The genes of ATM, ATR, CHEK1, CHEK2, P53, XRCC6, MRE11A, PRKDC, RAD51 and BRCA1 were measured using RT-qPCR. Compared to the control group, * indicated significant differences (P < 0.05) , ** indicated extremely significant differences (P < 0.01). All experiments were repeated 6 times.
Western blot analysis of the protein expression levels of DNA damage response (DDR) - related proteins in porcine granulosa cells treated with different concentrations of ZEA. GAPDH and ACTIN were used as protein loading controls. ZEA increased RAD51 protein levels while decreasing XRCC4, TP53, USP1, RPA2 and CCND protein levels. Compared to the control group, * indicated significant differences (P < 0.05), ** indicated extremely significant differences (P < 0.01). All experiments were repeated at least three times.
Immunostaining of γ-H2AX indicating DNA double strand breaks (DSBs) in porcine granulosa cells. (A) Porcine granulosa cells were treated with ZEA at 10 μM and 30 μM for 24 h and stained by indirect immunofluorescence. (B) The result of immunostaining of γ-H2AX was observed using fluorescence microscopy. The number of positive cells with CY3-γ-H2AX was displayed as a histogram. (C) The fluorescence intensity of γ-H2AX positive cells was analyzed using Image J. Compared to the control group, * indicated significant differences (P < 0.05). All experiments were repeated at least three times.
Immunostaining of RAD51 indicating DSBs in porcine granulosa cells. (A) Porcine granulosa cells were treated with ZEA at 10 μM and 30 μM for 24 h and stained by indirect immunofluorescence. (B) The result of immunostaining for RAD51 was observed using fluorescence microscopy. The number of positive cells with CY3- RAD51 was displayed as a histogram. (C) The fluorescence intensity of RAD51 positive cells was analyzed using Image J. Compared to the control group, * indicated significant differences (P < 0.05), ** indicated extremely significant differences (P < 0.01). All experiments were repeated at least three times.
Immunostaining of BRCA1 indicating DSBs in porcine granulosa cells. (A) Porcine granulosa cells were treated with ZEA at 10 μM and 30 μM for 24 h and stained by indirect immunofluorescence. (B) The result of immunostaining of BRCA1 was observed using fluorescence microscopy. The number of positive cells with CY3- BRCA1 was displayed as a histogram. (C) The fluorescence intensity of BRCA1 positive cells was analyzed using Image J. Compared to the control group, * indicated significant differences (P < 0.05), ** indicated extremely significant differences (P < 0.01). All experiments were repeated at least three times.
Effect of the estrogen recepter antagonist, Tamoxifen, on DDR in porcine granulosa cells treated with different concentrations of ZEA (10 μM and 30 μM) for 24 h. Western blot analysis of the expression levels of DDR-related proteins (RAD51, USP1, XRCC4 and RPA2). ACTIN was used as a protein loading control. All experiments were repeated at least three times.
ZEA is a toxic metabolite of Fusarium and commonly found in several food commodities worldwide. Previous studies found that ~50 % of the ZEA present in the plasma is present in the follicle fluid based on the linear regression between toxin compound concentrations in plasma and follicular fluid [15, 42]. A set of experiments demonstrated that ZEA produced several genotoxic effects, such as DNA fragmentation, micronuclei and chromosome aberrations including DNA strand breaks [30, 43-46]. Therefore, the genotoxic effects by ZEA in porcine granulosa cells might adversely affect the development of animal ovarian follicles.
Our results demonstrated that ZEA dramatically decreased the growth of porcine granulosa cells in a dose and time dependent manner, and caused a significant increase in apoptotic cells. It was of note that in a previous report from other groups, ZEA exposure led to apoptosis in porcine splenic lymphocytes, immortalized goat Leydig cells, and endometrial stromal cells [32, 47, 48]. Next, ZEA exposure considerably altered the mRNA expression of genes in the granulosa cells using an RNA-seq approach, and the DEGs were found to be involved in cellular processes, molecular functions, and biological processes that were closely associated with cell proliferation, cell cycle, apoptosis, and DNA damage repair. The results collectively suggested that ZEA was genotoxic for porcine granulosa cells in vitro.
In order to protect genomic stability from exogenous and endogenous DNA damaging agents , eukaryotic cells have evolved elaborated cell cycle checkpoints and DNA damage response (DDR) systems [49, 50]. When DNA damage, mutations or other abnormal conditions occur, the cell cycle checkpoint can timely block or delay cell cycle progression to repair the damaged DNA or regulate cell apoptosis [51, 52]. Cell cycle checkpoints can be divided into three types according to their different functions, such as DNA replication checkpoints, DNA damage checkpoints and spindle assembly checkpoints [53-55]. When cells are challenged with genotoxic stress, the ATM/ATR family of kinases can phosphorylate the histone H2AX. The phosphorylation of H2AX (γ-H2AX) is thought to recruit MRE11-RND51-NSB1 (MRN) directly to DNA-DSBs, and the γ-H2AX/MRN complex can recruit other DNA damage signals, such as MDC1 and BRCA1 . Furthermore, the MRN complex, 53BP1 and MDC1 can help ATM phosphorylate CHK2 to induce the cell cycle checkpoint . Also, ATR can directly phosphorylate CHK1 to impact the cell cycle process . RPA, as a heterotrimeric protein complex, specifically binds to single-stranded DNA assisting in DNA synthesis, and RPAs are required for DNA replication [59-62]. In this study, our results showed that ZEA exposure can increase the gene and protein expression of γ-H2AX, RAD51 and BRCA1, however significantly decrease p53 and RPA2 protein expression in granulosa cells (Figure 10).
A working model to inlustrate the role of DDR in ZEA-induced DSBs in porcine granulosa cells. DNA DSBs actived ATR or ATM protein. Subsequently, ATR or ATM induced cell cycle arrest of porcine granulosa allowing enought time to recruit DDR proteins (RAD51, BRCA1, PRKDC etc.) that then repair the damaged DNA.
It is well known that the DNA repairing pathway includes the non-homologous end joining (NHEJ, e.g. 53BP1, XRCC6 and RIF1) and the homologous recombination (HR, RAD51, BRCA1 and MRE11A) pathways [63, 64]. Some DDR proteins include ATM, ATR and DNA-dependent protein kinases . Some DDR proteins can not only repair DNA lesions but also manage cell cycle checkpoints. NHEJ is active throughout the cell cycle but favored in G1 cells, after DNA replication, HR is more prevalent, because there is an identical and available sister chromatid as a template for repairing . The balance between NHEJ and HR shifts during the cell cycle . The expression level of USP1, the deubiquitinating enzyme, through the APCCdh1 complex can determine which DNA repair pathway, HDR or NHEJ, will be used. When USP1 is degraded by APCCdh1, cells use the HR pathway of DNA repair, and conversely cells would use the NHEJ pathway . In this study, ZEA exposure reduced USP1 and XRCC4 protein levels in granulosa cells, which suggested that ZEA exposure caused DNA lesions and activated the DNA damage checkpoint in the S and G2/M phases ultimately inducing the HR pathway to repair the damaged DNA. ZEA exposure increased the transcriptional level of ATR and CHEK1 but not MRE11A, XRCC6, ATM and CHEK2, suggesting the impact of ZEA exposure on the cell cycle process or DNA repairing may be at the level of post- transcription and translation modification.
ZEA is a non-steroidal and can competitively bind to ERs affecting the development of ovary in pre-pubertal bitches , so we aimed to determine if ZEA exposure could negatively impact the genomic stability of cells through ERs, finally reducing the grow of cells or increasing cellular apoptosis. The results showed that there were not significantly change the expression level of RAD51, USP1, XRCC4 and RPA2 when added with 1 μM of the ER antagonist Tamoxifen to the medium in vitro.
In summary, our finding has shown that ZEA, as a DNA damaging agent, can cause DNA-DSBs and influence genome stability in porcine granulosa cells via the ER pathway, further leading to a reduced granulosa cell proliferation rate and arrest cell cycle in the S and G2/M phases. When the DNA repair system is not enough to rescue seriously damaged granulosa cells, it may promote granulosa cell apoptosis (Figure 10).
Supplementary figures and tables.
This work was supported by National Natural Science Foundation of China (31572225), National Key Research and Development Program of China (2016YFD0501207), and Natural Science Foundation of Hubei Province of China (2016CFC726). We would like to thank Prof. Paul W. Dyce (Auburn University) for his careful editing of the manuscript.
The authors have declared that no competing interest exists.
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Corresponding author: Dr. Lan Li E-mail: lilan9600com, Tel: 86-0532-88030246