Influenza viruses cause severe respiratory infections in humans and birds, triggering global health concerns and economic burden. Influenza infection is a dynamic process involving complex biological host responses. The objective of this study was to illustrate global biological processes in ileum and cecal tonsils at early time points after chickens were infected with low pathogenic avian influenza virus (LPAIV) H9N2 through transcriptome analysis. Total RNA isolated from ileum and cecal tonsils of non-infected and infected layers at 12-, 24- and 72-h post-infection (hpi) was used for mRNA sequencing analyses to characterize differentially expressed genes and overrepresented pathways. Statistical analysis highlighted transcriptomic signatures significantly occurring 24 and 72 hpi, but not earlier at 12 hpi. Interferon (IFN)-inducible and IFN-stimulated gene (ISG) expression was increased, followed by continued expression of various heat-shock proteins (HSP), including HSP60, HSP70, HSP90 and HSP110. Some upregulated genes involved in innate antiviral responses included DDX60, MX1, RSAD2 and CMPK2. The ISG15 antiviral mechanism pathway was highly enriched in ileum and cecal tonsils at 24 hpi. Overall, most affected pathways were related to interferon production and the heat-shock response. Research on these candidate genes and pathways is warranted to decipher underlying mechanisms of immunity against LPAIV in chickens.
Avian influenza viruses (AIVs) pose major public health threats and significant economic losses to the poultry industry1,2. AIVs possess an error-prone RNA polymerase making them susceptible to reassortment, which occasionally results in the emergence of zoonotic viruses3,4. Low pathogenic (LP) AIVs of subtype H9N2 are widespread pathogens of poultry. They are listed by the World Health Organization as a zoonotic influenza virus and ranked by Centers for Disease Control and Prevention (CDC) as potential pandemic viruses5,6. A novel influenza A (H7N9) virus is likely to have acquired six viral segments from circulating avian H9N2 viruses7.
The subtype of the virus is a critical factor in understanding the host’s ability to regulate the immune responses against AIV8,9,10,11. LPAIVs principally replicate in the avian respiratory and gastrointestinal tract (GIT), causing mild signs of illness12. Replication of LPAIVs in the GIT disrupts the gut microbiota and dysregulates type I interferons (IFN)13,14,15. The GIT plays a critical role in immune homeostasis, balancing the protection of the host against invading pathogens and interacting with commensal microbiota16,17,18. The well-developed gut-associated lymphoid tissues in the GIT are the first line of defence against invading pathogens and consist of various lymphoid cells found in Peyer’s patches, cecal tonsils and epithelial lining and lamina propria of the GIT19. Peyer’s patches are located at the anti-mesenterial side of the chicken jejunum, and one Peyer’s patch is consistently found in ileum at the proximal ileocecal transition20. Peyer’s patches epithelium has specialized cells called M cells that overlay follicles of defined T and B cell areas. Cecal tonsils are located at the cecum–rectum junction and have a structure similar to Peyer’s patches20,21. Antigen recognition through M cells or by direct antigen sampling by macrophages and dendritic cells induce intestinal immune responses22,23.
There has been significant interest in understanding how influenza viruses interact with their host. To this end, several studies have interrogated transcriptomics of host responses to LPAIV and highly pathogenic AIV24,25,26. These studies have revealed a complex network of immune responses initiated by avian influenza viruses, at cellular and tissue levels, in the respiratory tract24,27,28,29,30, ileum8,31, dendritic cells25 and chicken embryonic fibroblasts32. It has become evident that avian influenza viruses trigger the innate receptors of their host. Pattern-recognition receptors (PRRs) are the host's innate immune sensors, and at least three distinct classes of PRRs recognize influenza virus infection33,34. This recognition leads to secretion of cytokines, chemokines and antimicrobial peptides by cells, including dendritic cells and macrophages. Additional immune responses occur at immunological induction sites, including activation of IFN-stimulated genes (ISG)35,36. Remarkably, viral mechanisms antagonizing Toll-like receptor-mediated signaling by influenza viruses have not been described37. However, the influenza virus non-structural 1 (NS1) protein limits type I IFN responses. Deletions in influenza virus NS1 provoke augmented caspase‐1 activity post-infection of macrophages resulting in enhanced secretion of interleukin (IL)‐1β and IL-18, which indicates an antagonizing function of NS137. Viral NS1 also targets melanoma differentiation-associated protein 5 (MDA5) and directly interferes with the function of different ISGs37,38.
The increasing appreciation of the complexity of GIT immune responses has increased research efforts to decipher the mechanisms behind their induction and regulation. However, there is still a paucity of information about underlying mechanisms of chicken immunity against pathogens, including AIV in the GIT. The largest lymphoid aggregates of avian gut-associated lymphoid tissue are cecal tonsils. Along with Peyer's patches in the intestine, cecal tonsils elicit protective immune responses against bacterial and viral pathogens in avian species. Therefore, the present study was designed to examine gene expression in ileum and cecal tonsils, as potential sites for virus replication and induction of immune responses. Our findings could facilitate the development of effective measures to enhance immunity against AIV in poultry.
RNA-seq data analysis
The average number of reads that passed the quality control was 23.7 and 25.5 million reads per sample for cecal tonsils and ileum, respectively. The average percentage of reads uniquely mapped to the chicken reference genome was 89.7% and 91.7% of the reads for cecal tonsils and ileum, respectively.
Global profiles of DE genes in chicken infected with low pathogenic AIV subtype H9N2
Transcriptomic changes were detectable in cecal tonsils and peaked at 24 hpi
Comparing the gene expression in cecal tonsil tissues between infected and non-infected groups, the highest number of DE genes was 24 hpi and reduced to near baseline at 72 hpi (Table 1; Fig. 1A). The significant changes were also illustrated for DE genes with volcano plots (Fig. 2).
At 12 hpi (Fig. 1A), there were no DE genes between AIV-infected and non-infected chickens’ cecal tonsil tissues (FDR < 5%). However, using FC-based significance (FC < 1.5), we found a downregulated gene (FGF19), which is involved in mitogen-activated protein kinase (MAPK)1/MAPK3 signaling and cytokine signaling in immune system pathways.
Changes in DE genes began in cecal tonsils at 24 hpi (Fig. 1A). Ninety-five genes had a significant fold-change in expression (84 upregulated, 11 downregulated) (Table 1). The fold-change of gene expression between infected and non-infected groups ranged from 7.27 to -3.41. The gene with the highest upregulation was a novel gene called T-complex protein 1 subunit gamma-like. This gene is an orthologue of turkey’s CCT3 (Chaperonin Containing T-complex protein 1 subunit 3) gene and encodes for a chaperonin member containing TCP1 complex. T-complex protein 1 (TCP1) is a chaperonin class of protein involved in intracellular assembly and folding of various proteins. Specifically, this protein’s gamma subunit plays a crucial role in folding and assembling cytoskeleton proteins, exploited by viruses during early viral infection. TCP1 is also a cytosolic HSP60 family protein. Another gene with significant upregulation was the early endosome antigen 1-like, a novel long non-coding RNA (lncRNA). We also found upregulation of HSPs (HSP90AA1, HSPH1, HSPA8) and some genes involved in innate immune and antiviral responses, including IFN-inducible genes and ISGs (DDX60, IFI6, RSAD2, IFIT5, MX1, OASL, CMPK2, RNF213, ERAP1, IFIH1, STAT1, DHX58, IFITM5 (interferon-induced transmembrane) and C1S (complement C1s)). The MX1 gene prevents the import of nuclear material into viral nucleocapsids, which is known to have a disruptive effect on influenza A viruses by disrupting lipid rafts of the virus. CMPK2 is involved in the differentiation of monocytes and is involved in metabolism. The ERAP1 gene is involved in class I major histocompatibility complex (MHC)-mediated antigen processing and presentation. The DNAJA1 gene is an important paralog of DNAJA4, and response to heat and protein folding are some of its related annotations (GO:0,009,408, GO:0,006,457). C1S was an upregulated gene in the present study and is involved in the innate immune system and regulation of complement cascade pathways. A novel chicken gene characterized as an orthologue to human USP18, was upregulated. This novel chicken gene is involved in interferon signaling, antiviral mechanisms by IFN-stimulated genes and ISG15. Another novel chicken gene, described as guanylate binding protein 1, was also upregulated and among its GO term was cellular response to interferon-gamma. Downregulated genes in cecal tonsils at 24 hpi included a novel gene (an orthologue of human SAA gene). This gene is expressed in granulocytes and involved in the biological process of acute-phase responses (GO:0,006,953, acute inflammatory response to infection) and the innate immune system pathway (R-GGA-168249).
At 72 hpi, only HSPA5 had a significant upregulated expression (FDR < 5%) (Fig. 1A; Table 1). The FDR threshold was set to 10% to examine genes under a relaxed level of significance. Five HSPs were significantly different at this level. Additionally, one of these upregulated genes was CIDEC (with the greatest FC > 1.5). CIDEC (cell death-inducing DFFA (DNA fragmentation factor-alpha)-like effector c) is involved in regulating the apoptotic process. The DOP1B gene was among the results for both FC > 1.5 and FDR < 10% and is known to increase during responses to infections.
Transcriptomic changes were detected in the ileal tissue at 12 hpi and peak at 24 hpi
Differential gene expression in ileal tissue samples of infected chickens was detected as early as 12 hpi, and further increased at 24 hpi and then decreased 72 hpi (Fig. 1B; Table 1). This changing dynamic and the number of significant changes were somewhat different from the cecal tonsil samples; the number of DE genes at 72 hpi was maintained above ileum baseline. The differences in DE genes and changing dynamics for each time point post-infection were further illustrated in volcano plots, which give a more detailed display of the magnitude of changes in contrast to the measure of statistical significance (Fig. 2).
In ileum at 12 hpi, only three genes were significantly upregulated (FC > 1.5). RNF213 is related to class I MHC-mediated antigen processing and presentation pathways and adaptive immune system pathways. TRANK1 is a protein-coding gene, and its GO annotations for molecular functions include protein binding and ATP (Adenosine Triphosphate) binding. RNF213 and TRANK1 have orthologues in humans. NCKAP5 is involved in the formation and modification of the microtubules.
At 24 hpi, the number of gene expression changes in ileum increased substantially (Fig. 1B). Ninety genes had significant fold-changes (76 genes upregulated, and 14 genes downregulated) (FDR < 5% and FC > 1.5; Table 1). The fold-change of gene expression between infected and non-infected groups ranged from 2.38 to − 1.41. The gene with the greatest significant upregulation was the early endosome antigen 1-like, a novel lncRNA. The significant upregulation of RNF213 and TRANK1 continued from 12- to 24-hpi time point. There was also augmented expression of antiviral factors, including innate immune responses, IFN-inducible genes and ISGs (IFIT5, IFI6, IFIH1 (MDA5), IFITM5, IFI27L2, STAT1, MX1, DHX58, DDX60, and OASL). The RSAD2 gene was also one of the top upregulated genes. GO terms for RSAD2 were related to (1) defence responses to viruses, (2) CD4+ αβT cell activation and differentiation, (3) negative regulation of protein secretion and viral genome replication and (4) positive regulation of Toll-like receptor (TLR) 7/9 signaling pathways and T-helper 2 cell cytokine production. The ZBTB32 gene was also among the significantly upregulated genes; its GO terms were related to negative regulation of transcription by RNA polymerase II. The ZBTB32 orthologue in humans is ZBTB16, which is involved in the adaptive immune system and class I MHC-mediated antigen processing and presentation pathways. Heat-shock protein genes were also among the top results of upregulated genes, including HSPH1, HSPA2, HSP90AA1, HSPB9, HSPA4L and HSPA8. The C1R gene was also upregulated. It is involved in complement activation and the classical antibody-mediated complement activation pathway. TLR3 was upregulated in this study. This gene encodes TLR 3, which recognizes double-stranded RNA and plays a vital role in pathogen recognition and activation of innate immunity.
Among the significantly downregulated genes in ileum at 24 hpi were GNLY, CD3D, CST7, PTPN7, WAS and XCL1. GNLY, CD3D and CST7 are involved in the innate immune system. The PTPN7 annotation was cytokine signaling in the immune system, and WAS is involved in the Fc-gamma receptor-dependent phagocytosis pathway. XCL1 is involved in chemokine-mediated signaling pathways, G protein-coupled receptor signaling pathway, and cellular responses to IFN-gamma, IL-1 and tumour necrosis factor.
Of the 37 DE genes in ileum of infected chickens at 72 hpi, 25 genes had significant fold-changes (Table 1). HSPs were in the top results (HSPH1 (HSP110), HSP90AA1 (HSP90), HSPA4L, HSPA5 and HSPA8 (HSP70)). Additionally, PDK4, CHAC1, DNAJA4 and DNAJA1 were upregulated. In mice with severe influenza, inhibition of PDK4 using a therapeutic agent results in prevention of multiorgan failure39. CHAC1 gene annotations included the intrinsic apoptotic signaling pathway in response to endoplasmic reticulum stress, which usually results from the accumulation of unfolded or misfolded proteins in the lumen of the endoplasmic reticulum lumen (GO:0,070,059), and negative regulation of the Notch signaling pathway (GO:0,045,746). Like cecal tonsils results, DNAJA4 and its paralog DNAJA1 gene were also upregulated in ileum at 72 hpi. The DNAJA4 gene has related annotations, including unfolded protein binding and HSP binding (GO:0,051,082, GO:0,031,072). TGIF1 gene was upregulated and involved in signaling by the transforming growth factor (TGF)-β receptor complex pathway.
The genes that were most downregulated in ileum at 72 hpi included P2RY4, which is involved in the G protein-coupled receptor signaling pathway. ELF3 was also downregulated, and one of its gene ontogeny biological processes terms was inflammatory response to infection (GO:0,006,954). ELF1 is a protein encoded by the ELF1 gene, which is a paralog of ELF3 gene and regulates broad antiviral responses distinct from the type I IFN response40.
Functional annotation analysis
Functional analysis of Reactome pathways of DE genes
Functional annotation analysis of Reactome pathways using the PANTHER overrepresentation test among significantly upregulated genes resulted in three statistically significant (FDR < 5%, Fisher’s exact test) Reactome pathways in cecal tonsils and ileum at 24 hpi. In both tissues, the highest enriched pathway was the ISG15 antiviral mechanism (Table 2).
Functional analysis of gene ontology of DE genes
Functional annotation analysis of GO using the PANTHER overrepresentation test among upregulated genes gave results in cecal tonsils at 24 hpi and ileum at 24 and 72 hpi. In cecal tonsils at 24 hpi, the significantly upregulated genes were classified into 27 biological processes and 27 molecular functions with FDR of < 5% (Supplementary Tables 7 and 8) according to the GO project, respectively. The top 10 results of enriched biological processes are shown in Fig. 3A. The main GO categories of biological processes for the upregulated genes were protein ADP (Adenosine Diphosphate)-ribosylation, positive regulation of PRR signaling pathways, positive regulation of cytokine production (e.g. positive regulation of type I IFN production) and regulation of viral life cycle (e.g. negative regulation). The top 10 results of enriched molecular functions are shown in Fig. 3B. The GO terms of the molecular functions for the upregulated genes included protein folding chaperone, single-stranded RNA binding and HSP binding.
In ileum at 24 hpi, the upregulated genes were classified into 30, 21 and one functional groups (FDR < 5%) of biological processes, molecular functions and cellular components, respectively (Supplementary Tables 9, 10 and 11). The top 10 results of enriched biological processes are shown in Fig. 3A. The main GO categories of the biological processes were regulation of PRR signaling pathways, positive regulation of cytokine production (e.g. IFN-β), negative regulation of viral process (e.g. negative regulation of viral genome replication) and response to stress (e.g. defense response to virus). The top 10 results of enriched molecular functions are shown in Fig. 3B. The GO terms of the molecular functions included protein folding chaperone, double- and single-stranded RNA binding, chaperone binding and unfolded protein binding. Figure 3C shows the cellular component (cytosol) as the only enriched GO term relevant to ileum at 24 hpi.
In ileum at 72 hpi, the DE upregulated genes were classified into 19 biological processes, 19 molecular functions and one cellular component at FDR < 5% (Supplementary Tables 12, 13 and 14) according to the GO project, respectively. The top 10 results of enriched biological processes are shown in Fig. 3A. The main biological processes were negative regulation of inclusion body assembly, negative regulation of transcription from RNA polymerase II promoter in response to stress and protein refolding. Figure 3B presents the top 10 enriched molecular functions, including C3HC4-type RING (Really Interesting New Gene) finger domain binding, protein folding chaperone, misfolded protein binding, chaperone binding and HSP binding. The cellular component (cytosol) was the only enriched GO term in ileum at 72 hpi (Fig. 3C).
Immunity against AIV is the result of an orchestrated effort between innate and adaptive immune responses to this virus. Transcriptomic studies have been carried out in the GIT of chickens during infection with various subtypes of influenza A viruses. Infection with H5N1 or H5N2 in chickens results in differential expression of genes associated with innate immune responses in ileum8. Also, transcriptome analysis of ileum from birds infected with high (H5N1) and low (H5N2) pathogenic influenza viruses has revealed very different IFITM responses in ducks and chickens31. Yet, there is no comprehensive understanding of the mechanisms of immune response to LPAIV, such as H9N2, in the GIT. The present study was designed to evaluate the global gene expression changes in cecal tonsils and ileum of chickens after infection with H9N2 AIV. The induced expression patterns of different genes in ileum and cecal tonsils of AIV-infected chickens were revealed with some important observations.
Comparing the gene expression profiles of cecal tonsils and ileum, we observed some shared and unique responses to AIV infection. At 24 and 72 hpi, the comparison of differentially expressed genes showed that there were no genes displaying an opposite expression pattern between the two tissues and between the time points post-infection (Supplementary Fig. 2A-D). None of the sets resulted in any pathway with FDR < = 5%, except the upregulated genes in ileum at 24 hpi. The most enriched pathways were the regulation of gene expression by hypoxia-inducible factor (HIF) pathway (R-GGA-1234158) and the TRAF6-mediated interferon regulatory factor (IRF7) activation pathway (R-GGA-933541). The mechanism of viral activation of the HIF-1 pathway is that influenza A virus infection causes impaired proteasome function, resulting in HIF-1α accumulation, and decreases expression of factor inhibiting HIF-1, further boosting HIF-1 activity41. Nuclear translocation of HIF-1α induced by influenza A infection is crucial to pro-inflammatory cytokines production, and deficiency of HIF-1α in lung epithelial cells enhances autophagy, facilitating influenza A virus replication42,43. Activation of IRF7 is triggered by TLR7 recognition of RNA released from the influenza virus, which is followed by the production of type I IFNs. Moreover, TRAF6-mediated IRF7 activation establishes innate immune responses and the absence of TRAF6 ensues enhanced viral replication and a significant reduction in IL-6 and type I IFNs production after infection with RNA virus44.
In the present study, RNF213 was upregulated gene in ileum at 12 and 24 hpi and cecal tonsils at 24 hpi. The Rnf213 gene was identified as highly expressed among a cluster of ISGs with known antiviral activity in a mouse model45. The model revealed that the heterogeneity of influenza replication from cell to cell is not derived by cell type. Also, the cells with no or low viral replication have high induction of the Rnf213 gene45. Additionally, a low abundance of virus transcripts is associated with the host innate response (response to type I IFN) gene cluster, including the RNF213 gene, which is significantly highly expressed in response to influenza infection46. Further, a transcriptomic analysis has revealed new genes and networks in response to H5N1 infection in ducks; among them, the RNF213 gene is expressed differentially in the brain post-infection47.
Here, we report that a novel gene called early endosome antigen 1-like and identified as a lncRNA had significant upregulation in cecal tonsils and ileum at 24 hpi. Although little is known about lncRNAs, a lncRNA is upregulated due to viral delivery and is required to induce antiviral effects by promoting an increase in IFN production48. Furthermore, an evolutionarily conserved role for lncRNAs has been suggested, as conserved sequences are found to define virus-specific effector and memory CD8+ T cells49. Early endosome antigen 1 (EEA1), a protein-coding gene, is involved in vesicular trafficking and is affected by bacterial infections50,51. Intracellular pathogens target molecular factors, including EEA1, and inhibit its recruitment, triggering phagosomal maturation arrest50,52. Influenza A viruses benefit from EEA1 to infect human cells; following internalization of virus particles in dendritic cells, the influenza virus traffic through EEA1+ early endosomes to gain access to the cytoplasm53. Chicken EEA1 is a coding orthologue of human EEA1. It is hypothesized that lncRNA is involved in competing for endogenous RNA (ceRNA), which could regulate a protein-coding gene by sponging up microRNA54. The infected cells may increase early endosome antigen 1-like expression to limit viral entry to cells in the current study.
DExD/H-box helicases, such as DDX3, have been involved as sensors in innate antiviral immunity55,56,57,58. DDX60 is involved in RIG-I-dependent and independent antiviral responses59. Several DEAD/DEAH-box RNA helicases are hijacked by RNA viruses in infected cells to facilitate their replication60,61,62,63,64. Chicken DDX60 and DHX58 have orthologues in humans. In the present study, two IFN-inducible cytoplasmic helicases were upregulated in chicken GIT post-infection: DDX60 (DExD/H-box helicase 60) and DHX58 (DExH-box helicase 58, also known as LGP2 (laboratory of genetics and physiology 2)). Our observations supported the role of DExD/H-box helicases in innate antiviral immunity and their manipulation by viruses. DDX60 upregulation started at 12 hpi in ileum but not in cecal tonsils, which then reached significant upregulation at 24 hpi in both tissues, and then subsided at 72 hpi. This gene expression may imply a broader function of chicken DExD/H-box helicases and provide a deeper understanding of immune mechanisms and pathogenesis of AIV in chicken GIT.
Heat shock proteins shared across Archea, bacteria and eukaryotes, are associated with cellular injury. Expression of HSPs is elevated to protect cells under stress and is involved in protein folding, the immune system and antiviral response. However, viruses lack HSPs and depend on host HSPs for their protein folding65. Therefore, viruses can hijack HSPs, including hsp40, hsp70 and hsp90, to increase viral replication66. Exogenous administration of HSPs can enhance immune responses in cancer and infectious diseases by activation of protective T cell responses67,68. HSPs can also interact with various viral proteins; for example, HSPA8 can interact with influenza virus protein M1. This interaction inhibits the nuclear export of matrix protein 1 and nucleoprotein and subsequently inhibits viral assembly69. Upregulation of HSPs has been reported in the chicken respiratory tract27. In the present study, we found that HSPs were upregulated significantly at 24 and 72 hpi in ileum and cecal tonsils of AIV-infected chickens. Targeting HSPs could provide a platform for prophylactic or therapeutic strategies to manipulate immune responses against AIV in poultry.
Viruses also exploit cytoskeleton proteins during early viral replication70,71. TCP1 is a chaperonin and a cytosolic HSP60 family protein72. The gamma subunit of TCP1 plays a vital role in the folding and assembling of cytoskeleton proteins73,74. Chicken TCP1 has a human orthologue—section of the gene that codes for the gamma-like subunit. T-complex protein 1 subunit gamma-like, a novel gene in the chicken genome, is a paralogue of chicken TCP1. In the present study, we found the most upregulation of the T-complex protein 1 subunit gamma-like gene in cecal tonsils at 24 hpi. This unique gene upregulation in cecal tonsils may signal this gene's employment by H9N2 AIV in the current study for its purposes in protein folding and assembly.
We found that MX1 gene was upregulated in ileum and cecal tonsils. This may draw a link to an anti-viral response in chicken cecal tonsils to AIV infection. MX1 protein inhibits the import of nuclear material into viral nucleocapsids, which is known to have a disruptive effect on influenza A viruses by disrupting lipid rafts of the virus. Other transcriptomic studies in poultry have also shown upregulation of this gene in repertory tract and ileum8,24,27.
IFITM is a family of genes known to have a role in limiting influenza infection75. Transcriptomic analysis shows that chickens mount a weak IFITM response in ileum post-infection with LPAIV H5N231. However, the findings of our study showed upregulation of IFITM5 in cecal tonsils and ileum at 24 hpi. This discrepancy of IFITM response may be because of the different subtypes used.
The results of the functional analyses of the DE genes were related to the immune responses to influenza infection. GO terms and Reactome pathways results were almost exclusively associated with response to viral infection. In cecal tonsils and ileum at 24 hpi, one of the highest enriched pathways was the ISG15 antiviral mechanism (Supplementary Fig. 1). IFN-induced ISG15 targets the non-structural 1 (NS1A) protein of the influenza A virus, causing a loss of function of the NS1A protein and the inhibition of influenza A virus replication in virus-infected cells76. Additionally, ISG15 plays various roles in the defence against viral infections and the activation of immune system cells such as lymphocytes, monocytes, and natural killer cells77. Interestingly, the NS1A protein of influenza A viruses is responsible for inhibiting host immune responses by limiting production of IFNs and, therefore, antiviral effects of IFN-induced proteins78.
In conclusion, our study illustrated the differential expression of several innate immune system genes following AIV infection in ileum and cecal tonsils. The results of the present study revealed that there is some degree of similarity between immune responses in GIT and those induced in the respiratory tract, although further research is required to determine whether there are spatial and temporal differences in gene expression between the gastrointestinal and respiratory tracts. Our study highlighted some of the DE genes that are known to be exploited by the influenza virus to support viral replication. Some of the DE genes have been consistently identified in chicken LPAIV studies, hinting that they may be the best candidates for future research. One important finding was the enriched antiviral pathway of ISG15. ISG15 plays a critical role in innate responses, and future research studying this mechanism might provide a platform for strategies against AIV in poultry.
Materials and methods
This study included two main factors: treatment (challenged versus nonchallenged) and time (three time points post-infection), resulting in six groups. Each group contained six biological replicates. A total of 36 one-day-old specific pathogen-free White Leghorn layers were purchased from the Canadian Food Inspection Agency (Ottawa, Canada) and housed in the isolation facility at the Ontario Veterinary College at the University of Guelph. All experimental procedures were approved by the University of Guelph Animal Care Committee and conducted according to specifications of the Canadian Council on Animal Care. Experiments in the manuscript followed the recommendations in the ARRIVE guidelines.
Twenty-one days after hatching, 18 chickens in the challenged group were inoculated via oculo-nasal and oral routes with 250 μL of 3.1 × 107 TCID50/mL of LPAIV H9N2. Eighteen chickens in the nonchallenged group were inoculated via the same route with 200 μL of phosphate-buffered saline. The ileal samples at proximal ileocecal transition and cecal tonsils were collected from six chickens per time point at 12, 24, and 72 h post-infection (hpi) per treatment. The collected samples were transferred into tubes containing 1 mL of RNAlater solution (Invitrogen, Burlington, ON, CAN) for RNA stabilization and storage for later processing. The above time points were chosen that coincides with induction of innate responses to the virus.
Virus strain and virus propagation
A/TK/IT/13VIR1864-45/2013 (H9N2) from the Istituto Zooprofilattico Sperimentale delle Venezie (IZSVe), Italy, was used in this study. The virus was propagated in 10-day-old embryonated specific pathogen-free chicken eggs. After 72 h of incubation at 37 °C, eggs were refrigerated at 4 °C overnight. Allantoic fluid was collected and purified by centrifuging at 400 × g for 5 min at 4 °C and then stored at -80 °C until further use. The propagated virus titer was determined with 50% tissue culture infectious dose (TCID50) on Madin-Darby canine kidney (MDCK) cells.
Extraction, library preparation and RNA sequencing
Total RNA was extracted using the RNeasy Mini kit (Qiagen, Toronto, ON, CAN) according to the manufacturer’s instructions. Library construction, quality control testing and sequencing were performed by Novogene (Sacramento, USA). Briefly, quantification and quality control testing were performed on 1% agarose gels, the NanoPhotometer spectrophotometer (IMPLEN, CA, USA) and the RNA Nano 6000 Assay Kit in a Bioanalyzer 2100 system (Agilent Technologies, CA, USA). A total amount of 1 μg of RNA per sample was used for library preparation using a NEBNext Ultra RNA Library Prep Kit for Illumina (New England Biolabs, USA). Library quality was assessed on the Agilent Bioanalyzer 2100 system. The clustering of the index-coded samples was performed on a cBot Cluster Generation System using a PE Cluster Kit cBot-HS (Illumina). cDNA libraries were sequenced on an Illumina HiSeq-4000 platform, and 150 base pair paired-end reads were generated.
RNAseq data analysis interpretation
RNA-seq analysis was performed on the Trimmomatic-STAR-RSEM-DESeq2 pipeline previously established79. Raw reads were processed for quality control. Clean data were obtained based on Phred score (a quality measure to assess the accuracy of a sequencing) by trimming adapters and nucleotides with a Phred score of less than 30 at the beginning and end of the reads and discarding nucleotides with a Phred score of less than 20 in the window of five nucleotides using Trimmomatic80. The minimum length of surviving reads was set at 36 nucleotides. All downstream analyses were based on clean data with high quality.
Reads were mapped to a Gallus gallus reference genome (GRCg6a, release 98) using Spliced Transcripts Alignment to a Reference (STAR) (version 2.7.0a)81. The number of reads per gene was quantified by RNA-Seq by Expectation–Maximization (RSEM)82. RSEM output files were used in DESeq2 (version 1.24.0) to calculate differentially expressed (DE) genes by comparing challenge group versus control group for each tissue per time point83. Genes with an absolute fold-change (FC) of more than a 1.5 (|FC|> 1.5; |log2FC|> 0.584) and with a significant p-value when False Discovery Rate (FDR) was controlled at 5% were considered DE. VennDiagram package in R was used to compare DE genes between cecal tonsils and ileum at 24 and 72 h time points84.
Functional annotation analysis of DE genes
Overrepresentation analysis was performed on PANTHER (version 15) (http://www.pantherdb.org/) using the PANTHER Overrepresentation Test (Released 20,200,728) on DE genes of each tissue at each time point. Gene ontology (GO) database https://doi.org/10.5281/zenodo.3954044 Released 2020–07-16 (http://www.geneontology.org) was used to analyze the overrepresentation of GO terms in all gene lists. Reactome pathways (from Reactome database version 65, Released 2019–12-22) was used to analyze the overrepresentation of pathways among genes in all gene lists (https://reactome.org/). Both tests were performed using Fisher's exact test with FDR correction.
The datasets generated and analyzed during the current study are available in SRA database, BioProject ID PRJNA735215.
Jakhesara, S. J., Bhatt, V. D., Patel, N. V., Prajapati, K. S. & Joshi, C. G. Isolation and characterization of H9N2 influenza virus isolates from poultry respiratory disease outbreak. Springerplus 3, 196 (2014).
Qi, X. et al. Deterioration of eggshell quality in laying hens experimentally infected with H9N2 avian influenza virus. Vet. Res. 47, 35 (2016).
Horman, W. S. J., Nguyen, T. H. O., Kedzierska, K., Bean, A. G. D. & Layton, D. S. The drivers of pathology in zoonotic avian influenza: the interplay between host and pathogen. Front. Immunol. 9, 19 (2018).
Li, X. et al. Genetics, receptor binding property, and transmissibility in mammals of naturally isolated H9N2 avian influenza viruses. PLoS Pathog. 10, 1200 (2014).
CDC. Summary of Influenza Risk Assessment Tool (IRAT) Results |Pandemic Influenza (Flu)| CDC. The Centers for Disease Control and Prevention https://www.cdc.gov/flu/pandemic-resources/monitoring/irat-virus-summaries.htm (2020).
WHO, W. H. O. Influenza (Avian and other zoonotic). The World Health Organization https://www.who.int/news-room/fact-sheets/detail/influenza-(avian-and-other-zoonotic) (2018).
Kageyama, T. et al. Genetic analysis of novel avian A(H7N9) influenza viruses isolated from patients in China. Science 18, 16 (2013).
Cao, Y. et al. Differential responses of innate immunity triggered by different subtypes of influenza a viruses in human and avian hosts. BMC Med. Genom. 10, 70 (2017).
Josset, L., Zeng, H., Kelly, S. M., Tumpey, T. M. & Katze, M. G. Transcriptomic characterization of the novel avian-origin influenza a (H7N9) virus: specific host response and responses intermediate between avian (H5N1 and H7N7) and human (H3N2) viruses and implications for treatment options. mBio 5, 1900 (2014).
Samy, A. A. et al. Different counteracting host immune responses to clade 126.96.36.199 and 188.8.131.52 Egyptian H5N1 highly pathogenic avian influenza viruses in naïve and vaccinated chickens. Vet. Microbiol. 183, 103–109 (2016).
Suzuki, K. et al. Association of increased pathogenicity of Asian H5N1 highly pathogenic avian influenza viruses in chickens with highly efficient viral replication accompanied by early destruction of innate immune responses. J. Virol. 83, 7475–7486 (2009).
Payne, S. Chapter 23 - Family Orthomyxoviridae. in Viruses (ed. Payne, S.) 197–208 (Academic Press, 2017). https://doi.org/10.1016/B978-0-12-803109-4.00023-4.
Li, H. et al. Avian influenza virus subtype H9N2 affects intestinal microbiota, barrier structure injury, and inflammatory intestinal disease in the chicken Ileum. Viruses 10, 196 (2018).
Yitbarek, A., Weese, J. S., Alkie, T. N., Parkinson, J. & Sharif, S. Influenza A virus subtype H9N2 infection disrupts the composition of intestinal microbiota of chickens. FEMS Microbiol. Ecol. 94, 290 (2018).
Yitbarek, A. et al. Gut microbiota modulates type I interferon and antibody-mediated immune responses in chickens infected with influenza virus subtype H9N2. Benef. Microbes 9, 417–427 (2018).
Ahluwalia, B., Magnusson, M. K. & Öhman, L. Mucosal immune system of the gastrointestinal tract: maintaining balance between the good and the bad. Scand. J. Gastroenterol. 52, 1185–1193 (2017).
Montalban-Arques, A., Chaparro, M., Gisbert, J. P. & Bernardo, D. The innate immune system in the gastrointestinal tract: role of intraepithelial lymphocytes and lamina propria innate lymphoid cells in intestinal inflammation. Inflamm. Bowel Dis. 24, 1649–1659 (2018).
Nochi, T., Jansen, C. A., Toyomizu, M. & van Eden, W. The well-developed mucosal immune systems of birds and mammals allow for similar approaches of mucosal vaccination in both types of animals. Front. Nutr. 5, 1036 (2018).
Bar-Shira, E., Sklan, D. & Friedman, A. Establishment of immune competence in the avian GALT during the immediate post-hatch period. Dev. Comp. Immunol. 27, 147–157 (2003).
Casteleyn, C. et al. Locations of gut-associated lymphoid tissue in the 3-month-old chicken: a review. Avian Pathol. 39, 143–150 (2010).
Kitagawa, H., Hiratsuka, Y., Imagawa, T. & Uehara, M. Distribution of lymphoid tissue in the caecal mucosa of chickens. J. Anat. 192, 293–298 (1998).
Aliberti, J. Immunity and tolerance induced by intestinal mucosal dendritic cells. Mediators Inflamm 2016, e3104727 (2016).
Flannigan, K. L., Geem, D., Harusato, A. & Denning, T. L. Intestinal antigen-presenting cells. Am. J. Pathol. 185, 1809–1819 (2015).
Wang, Y. et al. Integrated analysis of microRNA expression and mRNA transcriptome in lungs of avian influenza virus infected broilers. BMC Genom. 13, 278 (2012).
Liu, Q. et al. Transcriptomic profile of chicken bone marrow-derive dendritic cells in response to H9N2 avian influenza A virus. Vet. Immunol. Immunopathol. 220, 109992 (2020).
Reemers, S. S. et al. Reduced immune reaction prevents immunopathology after challenge with avian influenza virus: a transcriptomics analysis of adjuvanted vaccines. Vaccine 28, 6351–6360 (2010).
An, J. et al. A homeostasis hypothesis of avian influenza resistance in chickens. Genes 10, 543 (2019).
Kuchipudi, S. V. et al. Highly pathogenic avian influenza virus infection in chickens but not ducks is associated with elevated host immune and pro-inflammatory responses. Vet. Res. 45, 118 (2014).
Meyer, L. et al. Transcriptomic profiling of a chicken lung epithelial cell line (CLEC213) reveals a mitochondrial respiratory chain activity boost during influenza virus infection. PLOS ONE 12, e0176355 (2017).
Wang, Y., Lupiani, B., Reddy, S. M., Lamont, S. J. & Zhou, H. RNA-seq analysis revealed novel genes and signaling pathway associated with disease resistance to avian influenza virus infection in chickens. Poult. Sci. 93, 485–493 (2014).
Smith, J. et al. A comparative analysis of host responses to avian influenza infection in ducks and chickens highlights a role for the interferon-induced transmembrane proteins in viral resistance. BMC Genom. 16, 574 (2015).
Kim, T. H., Kern, C. & Zhou, H. Knockout of IRF7 highlights its modulator function of host response against avian influenza virus and the involvement of MAPK and TOR signaling pathways in chicken. Genes 11, 385 (2020).
Suresh, R. & Mosser, D. M. Pattern recognition receptors in innate immunity, host defense, and immunopathology. Adv. Physiol. Educ. 37, 284–291 (2013).
Vidya, M. K. et al. Toll-like receptors: significance, ligands, signaling pathways, and functions in mammals. Int. Rev. Immunol. 37, 20–36 (2018).
Chen, X. et al. Host immune response to influenza a virus infection. Front. Immunol. 9, 1000 (2018).
Koutsakos, M., Kedzierska, K. & Subbarao, K. Immune responses to avian influenza viruses. J. Immunol. 202, 382–391 (2019).
Schmolke, M. & García-Sastre, A. Evasion of innate and adaptive immune responses by influenza A virus. Cell. Microbiol. 12, 873–880 (2010).
Liniger, M., Summerfield, A., Zimmer, G., McCullough, K. C. & Ruggli, N. Chicken cells sense influenza A virus infection through MDA5 and CARDIF signaling involving LGP2. J. Virol. 86, 705–717 (2012).
Yamane, K. et al. Diisopropylamine dichloroacetate, a novel pyruvate dehydrogenase kinase 4 inhibitor, as a potential therapeutic agent for metabolic disorders and multiorgan failure in severe influenza. PLoS ONE 9, 1113 (2014).
Seifert, L. L. et al. The ETS transcription factor ELF1 regulates a broadly antiviral program distinct from the type I interferon response. PLOS Pathog. 15, e1007634 (2019).
Ren, L. et al. Influenza A virus (H1N1) triggers a hypoxic response by stabilizing hypoxia-inducible factor-1α via inhibition of proteasome. Virology 530, 51–58 (2019).
Guo, X. et al. Nuclear translocation of HIF-1α induced by influenza A (H1N1) infection is critical to the production of proinflammatory cytokines. Emerg. Microbes Infect. 6, 1–8 (2017).
Zhao, C. et al. Deficiency of HIF-1α enhances influenza A virus replication by promoting autophagy in alveolar type II epithelial cells. Emerg. Microbes Infect. 9, 691–706 (2020).
Konno, H. et al. TRAF6 establishes innate immune responses by activating NF-κB and IRF7 upon sensing cytosolic viral RNA and DNA. PLoS ONE 4, e5674 (2009).
Sjaastad, L. E. et al. Distinct antiviral signatures revealed by the magnitude and round of influenza virus replication in vivo. Proc. Natl. Acad. Sci. 115, 9610–9615 (2018).
Wang, C. et al. Cell-to-cell variation in defective virus expression and effects on host responses during influenza virus infection. mBio 11, 1298 (2020).
Huang, Y. et al. Transcriptomic analyses reveal new genes and networks response to H5N1 influenza viruses in duck (Anas platyrhynchos). J. Integr. Agric. 18, 1460–1472 (2019).
Huang, X. et al. Determination of antiviral action of long non-coding RNA loc107051710 during infectious bursal disease virus infection due to enhancement of interferon production. Virulence 11, 68–79 (2020).
Hudson, W. H. et al. Expression of novel long noncoding RNAs defines virus-specific effector and memory CD8 + T cells. Nat. Commun. 10, 196 (2019).
Fratti, R. A., Backer, J. M., Gruenberg, J., Corvera, S. & Deretic, V. Role of phosphatidylinositol 3-kinase and Rab5 effectors in phagosomal biogenesis and mycobacterial phagosome maturation arrest. J. Cell Biol. 154, 631–644 (2001).
Malik, Z. A. et al. Cutting edge: mycobacterium tuberculosis blocks Ca2+ signaling and phagosome maturation in human macrophages via specific inhibition of sphingosine kinase. J. Immunol. 170, 2811–2815 (2003).
Fratti, R. A., Chua, J. & Deretic, V. Induction of p38 mitogen-activated protein kinase reduces early endosome autoantigen 1 (EEA1) recruitment to phagosomal membranes. J. Biol. Chem. 278, 46961–46967 (2003).
Baharom, F. et al. Visualization of early influenza A virus trafficking in human dendritic cells using STED microscopy. PLOS ONE 12, e0177920 (2017).
Song, X. et al. Analysing the relationship between lncRNA and protein-coding gene and the role of lncRNA as ceRNA in pulmonary fibrosis. J. Cell. Mol. Med. 18, 991–1003 (2014).
Fullam, A. & Schröder, M. DExD/H-box RNA helicases as mediators of anti-viral innate immunity and essential host factors for viral replication. Biochim. Biophys. Acta BBA-Gene Regul. Mech. 1829, 854–865 (2013).
Lai, M.-C., Sun, H. S., Wang, S.-W. & Tarn, W.-Y. DDX3 functions in antiviral innate immunity through translational control of PACT. FEBS J. 283, 88–101 (2016).
Perčulija, V. & Ouyang, S. Diverse roles of DEAD/DEAH-box helicases in innate immunity and diseases. Helicases Domains Life https://doi.org/10.1016/B978-0-12-814685-9.00009-9 (2019).
Taschuk, F. & Cherry, S. DEAD-box helicases: sensors, regulators, and effectors for antiviral defense. Viruses 12, 1956 (2020).
Oshiumi, H. et al. DDX60 Is involved in RIG-I-dependent and independent antiviral responses, and its function is attenuated by virus-induced EGFR activation. Cell Rep. 11, 1193–1207 (2015).
Diot, C. et al. Influenza A virus polymerase recruits the RNA helicase DDX19 to promote the nuclear export of viral mRNAs. Sci. Rep. 6, 33763 (2016).
Lorgeoux, R.-P., Guo, F. & Liang, C. From promoting to inhibiting: diverse roles of helicases in HIV-1 replication. Retrovirology 9, 79 (2012).
Ma, J. et al. The requirement of the DEAD-box protein DDX24 for the packaging of human immunodeficiency virus type 1 RNA. Virology 375, 253–264 (2008).
Xu, L. et al. The cellular RNA helicase DDX1 interacts with coronavirus nonstructural protein 14 and enhances viral replication. J. Virol. 84, 8571–8583 (2010).
Xu, Z., Anderson, R. & Hobman, T. C. The capsid-binding nucleolar helicase DDX56 is important for infectivity of West Nile virus. J. Virol. 85, 5571–5580 (2011).
Marques, M., Ramos, B., Soares, A. R. & Ribeiro, D. Cellular proteostasis during influenza A virus infection—friend or foe?. Cells 8, 569 (2019).
Bolhassani, A. & Agi, E. Heat shock proteins in infection. Clin. Chim. Acta 498, 90–100 (2019).
Binder, R. J. Functions of heat shock proteins in pathways of the innate and adaptive immune system. J. Immunol. 193, 5765–5771 (2014).
Wieten, L. et al. A novel heat-shock protein coinducer boosts stress protein Hsp70 to activate T cell regulation of inflammation in autoimmune arthritis. Arthritis Rheum. 62, 1026–1035 (2010).
Watanabe, K. et al. Identification of Hsc70 as an influenza virus matrix protein (M1) binding factor involved in the virus life cycle. FEBS Lett. 580, 5785–5790 (2006).
Döhner, K. & Sodeik, B. The Role of the Cytoskeleton During Viral Infection. in Membrane Trafficking in Viral Replication (ed. Marsh, M.) 67–108 (Springer, 2005). https://doi.org/10.1007/3-540-26764-6_3.
Walsh, D. & Naghavi, M. H. Exploitation of cytoskeletal networks during early viral infection. Trends Microbiol. 27, 39–50 (2019).
Archibald, J. M., Logsdon, J. M. Jr. & Doolittle, W. F. Origin and evolution of eukaryotic chaperonins: phylogenetic evidence for ancient duplications in CCT genes. Mol. Biol. Evol. 17, 1456–1466 (2000).
Frydman, J. et al. Function in protein folding of TRiC, a cytosolic ring complex containing TCP-1 and structurally related subunits. EMBO J. 11, 4767–4778 (1992).
Grantham, J., Ruddock, L. W., Roobol, A. & Carden, M. J. Eukaryotic chaperonin containing T-complex polypeptide 1 interacts with filamentous actin and reduces the initial rate of actin polymerization in vitro. Cell Stress Chaperones 7, 235–242 (2002).
Everitt, A. R. et al. IFITM3 restricts the morbidity and mortality associated with influenza. Nature 484, 519–523 (2012).
Zhao, C., Hsiang, T.-Y., Kuo, R.-L. & Krug, R. M. ISG15 conjugation system targets the viral NS1 protein in influenza A virus–infected cells. Proc. Natl. Acad. Sci. 107, 2253–2258 (2010).
dos Santos, P. F. & Mansur, D. S. Beyond ISGlylation: functions of free intracellular and extracellular ISG15. J. Interferon Cytokine Res. 37, 246–253 (2017).
Hale, B. G., Randall, R. E., Ortín, J. & Jackson, D. The multifunctional NS1 protein of influenza A viruses. J. Gen. Virol. 89, 2359–2376 (2008).
Emam, M. et al. Transcriptomic profiles of monocyte-derived macrophages in response to Escherichia coli is associated with the host genetics. Sci. Rep. 10, 271 (2020).
Bolger, A. M., Lohse, M. & Usadel, B. Trimmomatic: a flexible trimmer for Illumina sequence data. Bioinformatics 30, 2114–2120 (2014).
Dobin, A. et al. STAR: ultrafast universal RNA-seq aligner. Bioinformatics 29, 15–21 (2013).
Li, B. & Dewey, C. N. RSEM: accurate transcript quantification from RNA-Seq data with or without a reference genome. BMC Bioinf. 12, 323 (2011).
Love, M. I., Huber, W. & Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 15, 550 (2014).
Chen, H. & Boutros, P. C. VennDiagram: a package for the generation of highly-customizable Venn and Euler diagrams in R. BMC Bioinf. 12, 35 (2011).
We would like to acknowledge the isolation unit staff at the Ontario Veterinary College, University of Guelph, for their help with the care and housing of chickens. Funding was provided in part by Agriculture and Agri-Food Canada. The Ontario Ministry of Agriculture Food and Rural Affairs, the Natural Sciences and Engineering Research Council of Canada, Egg Farmers of Canada, Chicken Farmers of Saskatchewan, and the Canadian Poultry Research Council provided funding as well. This research was also supported in part by the University of Guelph’s Food from Thought initiative and the Canada First Research Excellence Fund. We are also thankful for the kind support from the Istituto Zooprofilattico Sperimentale delle Venezie, Italy, by providing the virus used in this study.
The authors declare no competing interests.
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Alqazlan, N., Emam, M., Nagy, É. et al. Transcriptomics of chicken cecal tonsils and intestine after infection with low pathogenic avian influenza virus H9N2. Sci Rep 11, 20462 (2021). https://doi.org/10.1038/s41598-021-99182-3