- Research Article
- Open Access
Binding and entry of peste des petits ruminants virus into caprine endometrial epithelial cells profoundly affect early cellular gene expression
Veterinary Researchvolume 49, Article number: 8 (2018)
Peste des petits ruminants virus (PPRV), the etiological agent of peste des petits ruminants (PPR), causes an acute or subacute disease in small ruminants. Although abortion is observed in an unusually large proportion of pregnant goats during outbreaks of PPR, the pathogenic mechanism underlying remains unclear. Here, the gene expression profile of caprine endometrial epithelial cells (EECs) infected with PPRV Nigeria 75/1 was determined by DNA microarray to investigate the cellular response immediately after viral entry. The microarray analysis revealed that a total of 146 genes were significantly dysregulated by PPRV internalization within 1 h post-infection (hpi). Of these, 85 genes were upregulated and 61 genes were downregulated. Most of these genes, including NFKB1A, JUNB, and IL1A, have not previously been reported in association with PPRV infection in goats. Following viral replication (24 hpi), the expression of 307 genes were significantly upregulated and that of 261 genes were downregulated. The data for the genes differentially expressed in EECs were subjected to a time sequence profile analysis, gene network analysis and pathway analysis. The gene network analysis showed that 13 genes (EIF2AK3, IL10, TLR4, ZO3, NFKBIB, RAC1, HSP90AA1, SMAD7, ARG2, JUNB, ZFP36, APP, and IL1A) were located in the core of the network. We clearly demonstrate that PPRV infection upregulates the expression of nectin-4 after 1 hpi, which peaked at 24 hpi in EECs. In conclusion, this study demonstrates the early cellular gene expression in the caprine endometrial epithelial cells after the binding and entry of PPRV.
Peste des petits ruminants virus (PPRV) is a Morbillivirus of the family Paramyxoviridae, which causes an acute, highly contagious, and fatal disease that primarily affects goats and sheep. In general, goats are more severely affected than sheep [1,2,3]. It is noteworthy that PPRV infection often causes fetal mummification, abortions late in pregnancy, or the birth of dead or weak lambs that die within a couple of days [4, 5]. Although a number of studies for PPRV infection in vitro based on Vero cells, which are currently considered highly permissive cells for the isolation and propagation of various viruses [6,7,8], little is known about the characteristics of the PPRV-infected reproductive system in goats.
Like all morbilliviruses, PPRV has a well-established lymphatic and epithelial tissue tropism [9, 10]. Similar to Measles virus (MV), PPRV has three cellular receptors: CD46, the protein signaling lymphocyte activation molecule (SLAM or CD150), and the poliovirus receptor-like protein 4 (also known as PVRL4 or nectin-4). Ovine nectin-4 was identified as the epithelial receptor for PPRV. It is predominantly expressed in epithelial tissues and is encoded by multiple haplotypes in sheep breeds around the world . Cell lines expressing nectin-4 have previously been used to propagate MV, Canine distemper virus (CDV), and PPRV [11,12,13,14,15,16].
Although the pathogenesis of PPRV infection has been relatively well described in experimental animals, only a few studies have shed light on the molecular events following PPRV infection in goats [17, 18]. Therefore, it is important to determine the responses of individual caprine cell types to PPRV infection. The epithelial cells that are in contact with the virus may be responsible for generating the immune response required for the initiation of inflammation. Lingual and buccal mucosae and lung epithelial tissue infected by PPRV show significant inducible nitric oxide synthase (iNOS), interferon γ (IFN-γ), and tumor necrosis factor α (TNF-α) expression, which may play important roles in the initiation and regulation of the cytokine responses . There has been little close study of the progression or causes of the PPRV-associated pathology, except for a recent thorough histological investigation of the distribution of the virus during the early stages of infection , which showed that the virus spreads in a similar way to MV in humans [20, 21]. Interestingly, apoptosis was also observed in UV-inactivated MV-treated peripheral blood mononuclear cells (PBMCs), suggesting that MV replication is not necessary for virus-induced gene expression in the host cells .
The aim of this study was to determine the gene expression profile of caprine endometrial epithelial cells (EECs) in response to the PPRV vaccine virus, using the DNA microarray technology, and to thus clarify the virus–host interactions. We first determined the gene expression profile of EECs 1 h after in vitro exposure to PPRV and compared it with that of mock-exposed cells. We also distinguished between the responses induced by virion binding or entry and the responses that require viral gene expression.
Materials and methods
Cells and viruses
The caprine EECs were kindly provided by Prof. Yaping Jin (Northwest A&F University Yangling, Shaanxi, China), and we confirmed that their secretory function was consistent with that of primary endometrial epithelial cells [23, 24]. The cells were immortalized by transfection with human telomerase reverse transcriptase (hTERT), as previously reported , and cultured in Dulbecco’s minimal essential medium/nutrient mixture F-12 Ham’s medium (DMEM/F12) supplemented with 10% fetal bovine serum (FBS), penicillin (100 IU/mL), and streptomycin (10 μg/mL) at 37 °C under 5% CO2.
The PPRV vaccine strain, Nigeria 75/1, was obtained from the Lanzhou Veterinary Research Institute, Chinese Academy of Agricultural Sciences (Lanzhou, China). The viral stock was prepared by collecting the infected cell supernatant when a cytopathic effect (CPE) was apparent in about 80% of the cells. The cells were freeze–thawed three times and stored as aliquots at −80 °C. The viral titers were estimated with the method of Reed and Muench, and expressed as 50% tissue culture infective doses (TCID50)/mL.
Kinetics of viral internalization
EECs grown in 12-well plates (3 × 105 cells/well) were infected with PPRV at a multiplicity of infection (MOI) of 2, and incubated at 37 °C. To separate the adsorption and internalization processes, the EECs were pretreated with PPRV at 4 °C for 1 h and then shifted to 37 °C. Proteinase K treatment significantly affected the number of virions attached to the cell surface, suggesting that proteinase K removes the viruses attached to cells . At different time points, the cells were washed with phosphate-buffered saline (PBS) and treated with proteinase K (2 mg/mL) (Solarbio, China) for 45 min at 4 °C to remove the adsorbed but not internalized virus. The proteinase K was then inactivated with 2 mM phenylmethylsulfonyl fluoride in PBS with 5% bovine serum albumin (BSA), and the cells were washed with PBS–0.5% BSA with low-speed centrifugation. Finally, the cell pellet was resuspended in DMEM/F12 and serial tenfold dilutions of the cell suspension were plated. EEC monolayers were grown in 96-well plates containing DMEM with 2% FBS. Eight replicates were established for each dilution, and 100 μL of virus diluent was added to each well. The cells were incubated at 37 °C under 5% CO2 for about 5–7 days, and the numbers of wells with or without CPE were counted. TCID50 was calculated with the Reed–Muench method and used to calculate the infectivity of the viral stocks: infectivity (plaque-forming units/mL) = 0.69 × TCID50. Each test was performed in triplicate. To determine the rate of virus internalization, a parallel set of cultures was processed under the same conditions, except that proteinase K was replaced with PBS.
Western blotting analysis
To examine viral growth and receptor expression in EECs, PPRV at an MOI of 2 was adsorbed onto the cells at 4 °C for 1 h. After adsorption, the inoculum was discarded, and any unbound virus was removed by rinsing the plates with cold PBS. The infection was allowed to proceed at 37 °C with the addition of maintenance medium containing 2% serum. At the indicated time points, cell lysates were generated by adding 5 × sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) sample buffer to the cells. The samples were boiled for 10 min and fractionated with SDS-PAGE. The resulting proteins were transferred onto 0.22 µm polyvinylidene difluoride membranes (Millipore, Billerica, MA, USA). The membranes were blocked with 5% nonfat milk and incubated with primary antibodies, and then with horseradish-peroxidase-conjugated secondary antibodies (Santa Cruz Biotechnology, CA, USA). The following antibodies were used: anti-PPRV-N monoclonal antibody provided by the China Animal Health and Epidemiology Center (Qingdao, China), anti-nectin-4 (Abcam, Cambridge, MA, USA), and anti-β-actin (Santa Cruz Biotechnology, CA, USA). The bound antibodies were detected with western chemiluminescent HRP substrate (Millipore, MA, USA). The data are expressed as the means ± standard deviations (SD) of three independent experiments.
Sample selection and DNA microarray
PPRV was adsorbed onto the cells at an MOI of 2 at 4 °C for 1 h. After full adsorption, the cells were incubated at 37 °C for 1 h (PPRV 1 hpi, N = 3) or 24 h (PPRV 24 hpi, N = 2). To determine the rate of viral internalization, a parallel set of cultures was processed under the same conditions, except that PPRV was replaced with culture medium (control, N = 3). RNAiso Plus (1 mL; Takara, Tokyo, Japan) was added to each group of samples. The RNA quantity and quality were measured spectrophotometrically with a NanoDrop ND-1000 spectrophotometer (Thermo Fisher Scientific, Waltham, MA, USA; Additional file 1). The integrity of the RNA was assessed with standard denaturing agarose gel electrophoresis.
Because no genomic reference sequence for Capra hircus is available, the Sheep Gene Expression Microarray, 8 × 15 K was used (Agilent Technologies, CA, USA), which contains >15 000 sheep genes and transcripts, all with public domain annotations.
RNA labeling and array hybridization
Sample labeling and array hybridization were performed according to the Agilent One-Color Microarray-Based Gene Expression Analysis protocol (Agilent Technologies). Briefly, the total RNA from each sample was linearly amplified and labeled with Cy3-UTP. The labeled complementary RNAs (cRNAs) were purified with the RNeasy Mini Kit (Qiagen, Düsseldorf, Germany), and the concentrations and specific activities of the labeled cRNAs (pmol Cy3/μg cRNA) were measured with a NanoDrop ND-1000 spectrophotometer. Each labeled cRNA (1 μg) was fragmented by the addition of 11 μL of 10 × Blocking Agent and 2.2 μL of 25 × Fragmentation Buffer, with heating at 60 °C for 30 min. Then 55 μL of 2 × GE Hybridization Buffer was added to dilute the labeled cRNAs. Hybridization solution (100 μL) was dispensed into the gasket slide of the array, which was then attached to the gene expression microarray slide. The slides were incubated for 17 h at 65 °C in an Agilent Hybridization Oven. The hybridized arrays were washed, fixed, and scanned with an Agilent DNA Microarray Scanner (Part Number G2505C).
The Agilent Feature Extraction software (version 126.96.36.199) was used to extract the array images. Quantile normalization and subsequent data processing were performed with the GeneSpring GX v11.5.1 software package (Agilent Technologies). After quantile normalization of the raw data, the genes that that were flagged in Detected (“All Targets Value”) in at least two of eight samples were selected for further analysis. Genes that were statistically significantly differentially expressed in the two groups were identified with Volcano Plot filtering. The hclust function (R package stats) was used to perform hierarchical clustering (Ward’s method) . Heatmaps were produced with the heatmap.2 function (R package gplots) .
The datasets for the microarray analysis of the whole transcriptome, based on eight samples, were deposited in the Gene Expression Omnibus (GEO) database under accession number GSE85204.
Analyses of differentially expressed genes (DEGs)
Time sequence profile analysis of gene expression
We selected a set of distinct and representative temporal expression profiles. These model profiles corresponded to the possible profiles of the changes in the expression of the genes over time. Each gene was assigned to the model profile that most closely matched its expression profile, which was determined with a correlation coefficient. Because the model profiles were selected independently of the data, an algorithm could determine which profiles had a statistically significantly higher number of genes assigned to them using a permutation test. It then used standard hypothesis testing to determine which model profiles had significantly more genes assigned under the true ordering of time points compared with the average number assigned to the model profile in the permutation runs. The significant model profiles could then be either analyzed further independently, or grouped together based on their similarity to form clusters of significant profiles.
Construction of the gene coexpression network
A gene coexpression network of all the DEGs identified in the comparative and temporal analyses was generated using the interactions available in the BioGRID Database , and the genes were found to be densely interconnected. In the network, cycle nodes represent genes, and the edges between two nodes represent the interactions between genes. Because network elements represent the ways in which genes may regulate other genes, we selected genes from the four most significant profiles (profiles 2, 7, 8, and 13) to construct a coexpression network. The network edges were specified to feature correlation coefficients of >0.9 to ensure strong gene coexpression relationships. The genes labeled with different colors represent different degrees of connectedness. The network of genes was analyzed with the SPSS software and visualized with the Cytoscape 2.8.3 software .
We performed a pathway analysis of the DEGs based on the latest Kyoto Encyclopedia of Genes and Genomes (KEGG) Database . The P values denote the significance of the pathways (cutoff is 0.05).
Validation with qRT–PCR
To validate the microarray data, the expression of the genes upregulated at 1 hpi (vs. the control), such as TNF, NFKB1A, JUNB, IL1A, TGFB3, and CXCL1, were determined with the qRT–PCR analysis of three independent biological replicates. When we compared their expression at 24 and 1 hpi, the TLR4 gene was upregulated and genes TNF, JUNB, NFKB1A, NFKB1B, IL1A, HSP90AA1, and SMAD7 were downregulated. The primer sequences used are listed in Table 1. To validate the assay, the purified products were sequenced to confirm that the correct target was amplified. We calculated the relative expression level of each gene with the formula 2−△△CT , where CT is the threshold cycle, normalized to the goat housekeeping gene glyceraldehyde-3-phosphate-dehydrogenase (GAPDH), and represented it as the fold change relative to the mean of the samples. The standard deviations were calculated using the relative expression ratios of three replicates for each gene analyzed.
All data obtained in this study were analyzed with an independent-samples t test and expressed as the means ± standard deviations (SD) of at least three independent samples. P values of less than 0.05 were considered significant, and P < 0.01 was considered extremely significant.
Kinetics and rate of PPRV internalization
To accurately define the conditions of the viral internalization assay required to monitor PPRV entry during different treatments, we first determined the kinetics and rate of virus penetration into the EECs by measuring the productive internalized viral particles. As shown in Figure 1, significant PPRV particles were detached from the cells by proteinase K at 30 min postinoculation compared with the control cells (P < 0.01). After incubation for 60 min, most of viruses were resistant to proteinase K treatment compared with the control treatment, indicating the successful internalization of the infectious virions. Therefore, in the subsequent DNA microarray experiments, 1 h after PPRV infection was considered the optimal time point to measure viral entry.
Receptor nectin-4 expression in EECs inoculated with PPRV
To accurately define the conditions of the viral replication cycle in the host cells, PPRV strain Nigeria 75/1 was used to infect EECs. As shown in Figure 2A, experimental infection of the EECs with PPRV resulted in large syncytia, which formed at 72–120 hpi. The refractivity of the infected cells was also significantly enhanced. In contrast, no syncytia or visible CPE were observed within 24 hpi. Similar expression of nectin-4 and PPRV-N in the EECs exposed to the Nigeria 75/1 strain was detected with a western blotting assay. The viral protein was detected as early as 12 hpi and its levels increased until 48 hpi, followed by a slight decline (Figures 2B and C). The overall changes in the receptor nectin-4 levels expressed in the PPRV-infected cells were consistent with the changes in the PPRV-N expression detected, except that the receptor protein was first detected at 3 hpi and peaked at 24 hpi in the EECs (Figures 2B and C). Therefore, in the subsequent DNA microarray experiments, 24 h after PPRV infection was considered the optimal time point to determine early viral replication and the highest expression of the receptor before CPE occurred.
DNA microarray data analysis
We used the Agilent one-color Sheep Gene Expression Microarray, 8 × 15 K (Catalogue No. 019921) to monitor the cellular gene expression after viral adsorption and internalization by the cells. A minimum fold-change cutoff value of 2.0 was set to filter the data. A cluster analysis showed distinct trends in the expression of genomic transcripts in the cells at 1 and 24 h after in vitro exposure to PPRV compared with that in the mock-exposed control cells (Figure 3A). Of the >15 000 genes analyzed, 146 were significantly more strongly expressed in the PPRV-infected EECs at 1 hpi than in the mock-infected cells (P < 0.05). Of these genes, 85 were upregulated and 61 were downregulated (Additional file 2). A proportion of the DEGs, which were associated with viral infection or inflammatory cytokines, such as IRF1, JUNB, TNF, CXCL1, IL1, and TGFB3, were shown in a heatmap (Figure 3B), and the 25 most strongly DEGs (Fold change > 2, P < 0.01) are shown in Table 2. We also compared the expression of DEGs at 1 and 24 hpi. The expression of 307 genes were significantly upregulated and that of 261 genes were downregulated in the cells at 24 hpi relative to their expression at 1 hpi (Additional file 3). A proportion of the DEGs, which were associated with antiviral processes and immunity, such as TLR4, HSP90AA1, FOS, and RAC1, were shown in a heatmap (Figure 3C), and the 30 most strongly DEGs (Fold change > 3, P < 0.01) are listed in Table 3. Moreover, we compared the expression of DEGs at 24 hpi and mock-infected cells. The expression of 319 genes were significantly upregulated and that of 276 genes were downregulated in the PPRV-infected EECs at 24 hpi than in the mock-infected cells (Additional file 4), which has a great consistency with the data of comparision between 24 and 1 hpi. A proportion of the DEGs, which were associated with antiviral processes and immunity, such as CASP3, SMAD7, IL10 and DDX3X, were shown in a heatmap (Figure 3D), and the 30 most strongly DEGs (Fold change > 3, P < 0.01) are listed in Table 4.
Model profile and gene coexpression analysis
We detected 146 DEGs at PPRV 1 hpi (vs. the control) and 568 DEGs at PPRV 24 hpi (vs. the 1 hpi), but 110 common genes were differentially expressed at both time points, so the total number of DEGs was 604. To further examine the most significant target genes among these 604 DEGs, we used 16 model profiles to summarize the expression patterns of the genes. As shown in Figure 4, among the 16 patterns, we identified six patterns of genes that showed significant P values of < 0.05 (colored boxes). Among these patterns, the four most significant patterns were profiles Nos 2, 7, 8, and 13. Whereas profiles No. 8 and No. 13 contained 318 genes whose expression increased slightly before 1 hpi but markedly after PPRV infection, profiles No. 2 and No. 7 contained 222 downregulated genes whose expression decreased markedly after 1 hpi (Figure 5).
The genes in profiles Nos 2, 7, 8, and 13 were then analyzed and identified with a gene coexpression network to determine which gene or genes play/s a pivotal role in the early stage of PPRV infection. The gene network was constructed from functional gene associations. In a network, the cycle nodes represent genes and the edges between two nodes represent the interactions between the genes, which are quantified by their degree of interaction. The size and color of the cycle node represent the degree of interaction within the network, which describes the number of single genes that are regulated by the gene. The higher the degree, the more central the gene is within the network. This analysis produced the set of interactions illustrated in Figure 6. The genes with highest degree (degree ≥ 10) in our results were considered to have core status within the large-scale gene network made up of 13 DEGs. Most of these genes were involved in translation initiation, protein synthesis, transcellular transport, cellular stress adaptation, immunoregulation, or inflammation. In this network, genes encoding transmembrane proteins, such as toll-like receptor 4 (TLR4), were highly connected, interacting with MYF5, INSL3, TAC1, etc. Interleukin 10 (IL-10) is a cytokine with multiple, pleiotropic effects in immunoregulation and inflammation, and its gene was found to be connected to ZO3, EIF2AK3, UCP2, TRYPTASE-1, etc. HSP90AA1 was connected to RAC1, SMAD7, PLAU, NFKBIB, etc. APP, which encodes a precursor of the β-amyloid protein, known for its proinflammatory activity, was downregulated and connected to IL1A, AGR2, ZFP36, JUNB, etc.
Pathway overrepresentation analysis of gene expression
To systematically identify the biological associations of the DEGs and the pathways associated with PPRV infection, we performed a pathway overrepresentation analysis (ORA) with the KEGG Database. At 1 hpi, this analysis identified 38 KEGG pathways closely associated with the upregulated gene functions that were statistically enriched relative to their expression in mock-infected cells (P < 0.05). The top 10 pathways of upregulated genes were directly related to proinflammatory signaling pathways (Table 5). Many of the genes identified as central nodes in the gene coexpression analysis (IL1A, JUNB, NFKBIA, etc.) also occupied central positions in the signaling pathways identified. No pathway was enriched with any gene downregulated at 1 hpi. We also compared the datasets established for the PPRV-infected cells at 24 and 1 h. Twenty-three pathways were closely related to the upregulated genes and the top 10 differentially regulated pathways are shown in Table 5. In contrast, the differentially upregulated signaling responses among the top 10 pathways at 24 hpi were strongly associated with the anti-inflammatory, cell-cycle, and steroid hormone regulation signaling pathways. Many genes that occupy central positions in these signaling pathways also were identified at central nodes in the gene coexpression analysis (IL10 and TLR4). Interestingly, downregulated genes were associated with 64 pathways at 24 hpi. The top 10 pathways associated with immune regulation were identified (Table 5). In addition, when we compared the datasets established for PPRV-infected cells at 24 h and mock-infected cells, the differentially signaling pathways are consistent with the data of comparision between 24 and 1 hpi as shown in Table 5. When we compared the differentially regulated pathway (ORA) datasets in 1 h PPRV-infected cells and mock-infected cells, and in PPRV-infected cells at 24 and 1 h, the regulatory pathways identified showed opposite trends (Figure 7). Whereas PPRV insult caused the upregulation of genes largely related to the TNF, TLR, T cell receptor, RIG1, chemokine, and NF-κB signaling pathways (Figure 7A), most these genes were significantly downregulated in the cells at 24 hpi relative to their expression at 1 hpi (Figure 7B).
qRT–PCR verification of the microarray data
To verify the DNA microarray data, qRT–PCR was used to analyze the same RNA samples as were used in the original microarray experiment for 10 selected genes. At 1 hpi, the trends in expression of the genes analyzed with qRT–PCR, including TNF, NFKB1A, CXCL1, JUNB, IL1A, and TGFB3, were consistent with the trends observed with the DNA microarray analysis (Figure 8A). However, the increase in the expression of TLR4 at 24 hpi was significantly greater when detected with PCR than when detected with the microarray analysis (Figure 8A). The expression levels of genes TNF, JUNB, NFKB1A, NFKB1B, IL1A, HSP90AA1, and SMAD7 did not differ markedly between the microarray data and the qRT–PCR data (Figure 8B).
Several strains of MV and PPRV infect epithelial cells using nectin-4 as the receptor . Previous studies have shown that wild-type MV infection upregulates nectin-4 expression in human and murine brain endothelial cells . The present study confirms the same trends in the changes in PPRV-N and nectin-4 expression in PPRV-exposed goat-derived epithelial cells, which implies that PPRV replication has a role in regulating the expression of the receptor nectin-4. Conversely, the viral receptors expressed on cells may regulate viral binding, internalization, and replication [34, 35]. In the present study, we first demonstrated that PPRV uptake occurs within 1 h of exposure in goat-derived EECs and that viral replication occurs after internalization. The proliferation of PPRV in EECs observed in this study suggests that the clinical phenomenon of abortion in PPRV-infected goats is partly attributable to the replication of PPRV in the uterus. Furthermore, the interaction between the virus and its receptor on EECs implies that this cell line can be used to investigate the role of PPRV infection in the pathogenesis of the reproductive system in goats.
To our knowledge, this is the first broad analysis of the initial transcriptional responses to PPRV in caprine endometrial epithelial cells [11, 18, 33]. To ensure the accurate identification of the cellular genes that respond significantly to virion exposure, the DNA microarray data were scrutinized and stringently filtered with statistical techniques. The expression levels of the selected genes were also experimentally verified with real-time qPCR. Using these methods for statistical verification and experimental confirmation, our study identified a large number of genes not previously implicated in the early cellular responses to PPRV infection. The detected changes in gene expression occurred within the first hours after caprine EECs were exposed to PPR virions in vitro. The upregulation of pathways related to cytokine/chemokine signaling events suggests that specific innate immune responses are mounted during that acute phase of PPRV insult. With a multiple-pathway ORA, we identified broad cellular functional networks that are modulated during the early course of PPRV infection, and importantly, correlated these with specific cell signaling pathways. The identities of the individual signaling pathways modulated by PPRV infection provide critical information regarding disease pathogenesis and information required for the development of novel antiviral therapeutics.
PPRV infection in goats induces a classic inflammatory response, characterized by the enhanced expression of cytokines such as IFN-β, IFN-γ, IL-4, IL-1β, IL-8, IL-10, IL-6, and IL-12 [18, 19]. Consistent with this, our study detected inflammatory factors induced by early PPRV infection. This not only confirms the accuracy of the microarray expression analysis, but also suggests that the stimulation of inflammatory cytokines occurs in the early stages of PPRV infection, during its binding and entry into caprine epithelial cells. The innate immune defense is achieved by activating the NF-κB and type I IFN (IFN-α/β) responses. It has been demonstrated that PPRV antagonizes the production of type I IFN and suppresses the host cell antiviral responses by blocking IFN signaling by interacting with STAT1/2 [36, 37]. The present study detected no changes in IFN expression in EECs exposed to PPRV for either 1 or 24 h. Furthermore, the upregulation of TNF-α expression and the activation of a TNF-α-related signaling pathway in the PPRV-infected EECs at 1 hpi may be attributable to the activation of the NF-κB signaling pathway. It is interesting to note that although some genes that have already been implicated in the pathogenesis of PPRV infection in goats, such as IL1A, IL1B, and TNFA, were induced in the EECs at 1 hpi, they were significantly downregulated at 24 hpi in this study. These results contradict observations made in vivo, which indicated that the cytokine expression is upregulated for extended periods of time [18, 19, 38, 39]. It is plausible that the early cytokine peak observed after high-MOI infection in vitro is only achieved at a later time during infection in vivo. Another possible explanation for this discrepancy is the difference in the duration of stimulation and therefore, the duration of the response. For instance, in vivo, progeny virions are continuously produced by PPRV-infected cells and will therefore bind to and enter additional target cells, resulting in continuous stimulation, which may maintain cytokine production and facilitate prolonged activation . Therefore, our in vitro approach probably yielded results that are indicative of the phenomenon that occurs continuously in vivo. Interestingly, the TNF (FOS, JUNB, MAP2K1, NFκBIα, SELE, and TNF), NF-κB (NFκBIα, PLAU, and TNF), and PI3K–AKT (HSP90AA1, MAP2K1, MCL1, MYC, RAC1, and VEGFA) signaling pathways were suppressed at 24 hpi. Previous studies have shown that the MV V protein binds to p65 (RELA) to suppress NF-κB activity . NF-κB, receptor tyrosine kinase, and phosphatidylinositol 3-kinase (PI3K) are important signaling pathways required for efficient viral propagation and have attracted attention as suitable targets for antiviral interventions [41,42,43,44]. Previous microarray analyses have indicated that during the infection and replication of various viruses, the genes induced in the antiviral responses include those that are involved in the activation of NF-κB [45, 46] and IRF-3 [47, 48]. Overall, NF-κB plays an essential role in PPRV replication.
The cellular genes whose expression levels were altered after exposure to PPR virions belonged to different functional categories (Table 5), and encoded proteins such as inflammatory cytokines, molecules that regulate B-cell receptor signaling, chemokines, pattern recognition receptors, and proteins involved in steroid-related regulation, cell-cycle arrest, and cell adhesion. Our pathway ORA also identified similar functional categories of differentially regulated signaling pathways after PPRV infection. The opposite directions of the changes in immune-related gene expression in response to the binding/entry (1 hpi) and replication (24 hpi) of PPRV raise the questions: is viral replication involved in PPRV infection and what is its role in the suppression of the host immune system, especially its innate immunity? In the genus Paramyxovirus, nonstructural proteins V and C both play important roles in inhibiting the cellular antiviral state [37, 49,50,51]. Recent studies have demonstrated that the PPRV V protein influences IFN signal transduction by interacting with STAT1/2 . Although we did not determine the expression levels of the PPRV V and C proteins, the replication of PPRV is critical for its inhibition of the innate-immune-related responses in goat epithelial cells. Recently, an analysis of RNA-sequencing data, followed by a functional analysis, identified the key dysregulated genes in goat PBMCs infected with the PPR vaccine virus for 120 h, which were involved in immune-system-regulating pathways, spliceosomal pathways, and apoptotic pathways . Further studies are required to establish whether there are fundamentally different cellular responses to PPRV binding and entry in goat PBMCs.
Our gene coexpression network represents the most significantly expressed genes profiles at 1 and 24 hpi, with correlation coefficients of >0.9. The expression of genes involved in inflammatory activity (such as IL10, APP, IL1A, and TLR4), immune regulation (NFKBIB, HSP90AA1, SMAD7, and JUNB), autophagy activity (EIF2AK3), and cell-cycle progression (RAC1, ZFP36, and ZO3) correlated closely in goat-derived EECs in response to PPR virion exposure. Eukaryotic translation initiation factor 2-alpha kinase 3 is an enzyme encoded in humans by the EIF2AK3 gene [53, 54]. The protein encoded by this gene phosphorylates the alpha subunit of eukaryotic translation-initiation factor 2 (EIF2), leading to its inactivation, and thus to a rapid reduction in the translational initiation and repression of global protein synthesis. With our gene coexpression network analysis, we identified the central role of EIF2AK3 within the PPRV-infected gene network. TLR4 plays a critical role in bacterial infections by recognizing lipopolysaccharide. However, there is accumulating evidence that TLR4 is also involved in viral infections and contributes to the immune escape of MV and other viruses [55, 56]. Importantly, there are significant changes in the cytokines of the MV signaling pathway, which upregulates the expression of cytokines such as TLR4 and downregulates cytokines such as IL1α, NFκBIα, and NFκBIβ. Our study is the first to suggest that PPRV replication is closely associated with TLR4. The changes in TNF, IL1A, NFKB1A, and NFKB1B expression also indicate that the RIG1 signaling pathway and apoptosis are regulated by PPRV. HSP90AA1 was also identified as a core gene in our gene coexpression analysis. HSP90AA1, a pathogen receptor, induces autophagy via an AKT–MTOR-dependent pathway during early infection . MV infection regulates HSP90 expression and is closely related to the immune response . Further studies should determine the role of HSP90 in regulating the intracellular signaling pathways after PPRV infection. Interestingly, our analysis identified APP, a gene involved in proinflammatory activity, as playing a central role in the gene network of PPRV-infected EECs. It is important to remember that in a previous study that characterized the response of goat-derived PBMCs to PPRV infection, APP expression was downregulated in cells after exposure to the virus for 120 h . However, in the present study, APP was downregulated at 1 hpi but upregulated at 24 hpi. This prompts the fundamentally interesting question of whether PPRV induces different cellular responses in a cell-type specific or incubation-time-dependent manner.
In conclusion, our data indicate that the immediate responses of early cellular PPRV targets in EECs to virion binding and entry do not require viral gene expression. The expression of some cellular genes, such as TNF, IL1A, and NFKB1A, was elevated in PPRV-infected EECs at 1 hpi, but downregulated at 24 hpi, which indicates that the downregulation of these genes must be regulated by factors other than viral binding or entry. In this context, it is important to note that PPRV infection regulates the TNF, NF-κB, and TLR signaling pathways in EECs to resist the cellular antiviral response.
peste des petits ruminants virus
caprine endometrial epithelial cells
quantitative real-time PCR
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The authors declare that they have no competing interests.
BY performed the majority of experiments. ZC, SC, QX, PJ, TW participated part of the experiments. JW and XQ conceived the study, participate in its design and coordination. XQ prepared and revised the manuscript. All authors read and approved the final manuscript.
This work was supported by grants from the National Science Foundation of China (Grant No. 31602035). We are grateful to Yaping Jin (Northwest A & F University Yangling, Shaanxi, China) for the caprine endometrial epithelial cells. We thank Chinese Academy of Agricultural Sciences (Lanzhou, China) and China Animal Health and Epidemiology Center (Qingdao, China) for virus and antibody in these studies. We thank Janine Miller, Ph. D, from Liwen Bianji, Edanz Editing China, for editing the English text of a draft of this manuscript.
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