ORIGINAL RESEARCH article
Sec. Molecular Innate Immunity
Volume 11 - 2020 | https://doi.org/10.3389/fimmu.2020.613079
Chicken cGAS Senses Fowlpox Virus Infection and Regulates Macrophage Effector Functions
- 1Department of Pathology, University of Cambridge, Cambridge, United Kingdom
- 2Department of Veterinary Medicine, University of Cambridge, Cambridge, United Kingdom
- 3ISP, INRAE, Université de Tours, Nouzilly, France
- 4Department of Infectious Diseases, Imperial College London, London, United Kingdom
- 5School of Life Sciences, University of Essex, Colchester, United Kingdom
The anti-viral immune response is dependent on the ability of infected cells to sense foreign nucleic acids. In multiple species, the pattern recognition receptor (PRR) cyclic GMP-AMP synthase (cGAS) senses viral DNA as an essential component of the innate response. cGAS initiates a range of signaling outputs that are dependent on generation of the second messenger cGAMP that binds to the adaptor protein stimulator of interferon genes (STING). Here we show that in chicken macrophages, the cGAS/STING pathway is essential not only for the production of type-I interferons in response to intracellular DNA stimulation, but also for regulation of macrophage effector functions including the expression of MHC-II and co-stimulatory molecules. In the context of fowlpox, an avian DNA virus infection, the cGAS/STING pathway was found to be responsible for type-I interferon production and MHC-II transcription. The sensing of fowlpox virus DNA is therefore essential for mounting an anti-viral response in chicken cells and for regulation of a specific set of macrophage effector functions.
The ability of virally infected cells to mount an effective innate immune response is dependent on the intracellular sensing of nucleic acids by pattern recognition receptors (1). The PRRs that sense and respond to intracellular DNA are well characterized in a number of mammalian and non-mammalian organisms but are less studied in avian species, including chickens (2). The PRR cyclic cAMP-GMP (cGAMP) synthase (cGAS) binds intracellular viral DNA and, via production of the second-messenger 2’3’-cGAMP, triggers a range of signaling outputs including type-I interferon (IFN-I) production, cell death and cellular senescence (3). The absence of cGAS or the adaptor protein, stimulator of interferon genes (STING), which binds cGAMP, results in the susceptibility to DNA virus infection in knockout mice and impairs IFN-I production by cells infected with DNA viruses or transfected with linear double stranded DNA (4). Through its ability to sense mislocalized self-DNA, the cGAS/STING signaling axis is also a potent regulator of autoinflammatory and anti-tumor immune responses (5, 6). People with activating mutations in STING or loss-of function mutations in the 5’-3’ exonuclease TREX1, which removes excess cytoplasmic dsDNA, suffer from interferonopathies (7).
The ability of cGAS/STING signaling to drive multiple downstream signaling outputs is dependent on the activation of a number of distinct signaling mechanisms, some of which are better defined than others. The production of IFN-I in this context is dependent on STING recruiting and facilitating activation of TANK-binding kinase-1 (TBK1) and the transcription factor interferon regulatory factor-3 (IRF3) (8). IRF3 phosphorylation, dimerization, and translocation to the nucleus results in IFN-I transcription. The mechanism or mechanisms by which STING can promote cell death are less well described, but include inflammasome activation (9) and apoptosis of various cell types including myeloid and T cells (10, 11). cGAS can also activate a programme of cellular senescence in fibroblasts by sensing damaged self-DNA (12). It is not currently clear in what contexts these disparate signaling outputs are activated by cGAS/STING and to what extent they cross-talk with each other.
Chickens are economically important livestock birds that are infected by numerous viruses including fowlpox virus (FWPV). Fowlpox is a virus from the poxviridae family that replicates its double stranded DNA genome in the cytoplasm of infected cells. The infection is characterized by proliferative lesions in the skin that progress to thick scabs (cutaneous form) and by lesions in the upper GI and respiratory tracts (diphtheritic form) (13). Transmitted mechanically by biting insects, it causes significant losses to all forms of poultry production systems (from backyard, through extensive to intensive commercial flocks). It is particularly challenging in tropical climes where control of biting insects is difficult. FWPV is also used as a live recombinant vaccine vector in avian and mammalian species (14). Like other poxviruses the cytoplasmic replication cycle of FWPV exposes large amounts of foreign DNA to intracellular DNA sensing PRRs, making cGAS a likely candidate for sensing FWPV infection and making FWPV a potentially useful tool for delineating nucleic acid sensing mechanisms in avian systems. The mechanisms by which FWPV is sensed by PRRs during infection have not, however, been described.
In this study we show the existence of a cGAS/STING pathway in chicken macrophages and determine its downstream signaling outputs. Using cGAS and STING CRISPR/Cas9 knockout HD11 cells and pharmacological inhibitors of STING and TBK1 in primary macrophages, we show that the activation of cGAS by intracellular DNA induces an IFN-I response and that this response can be enhanced by priming cells with IFNα. As well as driving IFN-I production, we show that cGAS/STING signaling in macrophages can enhance transcription of specific immune recognition molecules including genes encoding the class II major histocompatibility complex (MHC-II) and co-stimulatory proteins, but without altering phagocytosis. Using FWPV mutants that are deficient in specific immunomodulators we are able to overcome the immunosuppression of wild type FWPV and show that this virus is sensed by cGAS, resulting in IFN-I and MHC-II transcription. These data show that the cGAS/STING/TBK1 pathway senses viral DNA in chicken macrophages and that this pathway regulates not only the antiviral interferon response but also modulates specific components of macrophage effector function machinery.
Materials and Methods
Calf Thymus (CT) DNA (Sigma), Herring Testes (HT) DNA (Sigma), polyinosinic-polycytidylic acid (poly(I:C), Invivogen), 2’3’-cGAMP (Invivogen) and chicken interferon alpha (Yeast-derived Recombinant Protein, Kingfisher Biotech, Inc) were diluted in nuclease-free water (Ambion, ThermoFisher). H-151 and BX795 (Invivogen) were diluted in DMSO, following the manufacturer’s protocols.
HD11 cells, an avian myelocytomatosis virus (MC29)-transformed chicken macrophage-like cell line (15), were incubated at 37°C, 5% CO2. They were grown in RPMI (Sigma-Aldrich, Germany) complemented with 2.5% volume per volume (v/v) heat-inactivated foetal bovine serum (FBS; Sera Laboratories International Ltd), 2.5% volume per volume (v/v) chicken serum (New Zealand origin, Gibco, Thermo Fisher Scientific), 10% Tryptose Phosphate Broth solution (Gibco, Thermo Fisher Scientific), 2 mM L-glutamine (Gibco, Thermo Fisher Scientific), 50 µg/ml of penicillin/streptomycin (P/S; Gibco, Thermo Fisher Scientific).
Chicken embryonic fibroblasts (CEFs) (Pirbright Institute, Woking) were incubated at 37°C, 5% CO2 and were grown in Dulbecco’s Modified Eagle Medium (DMEM) -F12 with Glutamax (Gibco), 5% v/v FBS, and 50 µg/ml P/S.
Knock-Out HD11 Cell Line Generation by CRISPR-Cas9
CRISPR Guide Design
According to the MB21D1 (cGAS) and TMEM137 (STING) sequences obtained from the Ensembl database (release 94), single guide (sg)RNA sequences (Table 1) were designed targeting the catalytic domain (residues 11-13 and 109) and start of the open reading frame, for cGAS and STING, respectively.
Knock-Out Cell Lines Generation Using CRISPR-Cas9
Genome editing of HD11 was performed using ribonucleoprotein (RNP) delivery. tracrRNA was mixed with the target specific sgRNA (Table 1), followed by an incubation at 95°C. To form the RNP complex, the tracrRNA/sgRNA mix was incubated with the Cas9 protein (IDT, Leuven, Belgium) and electroporation enhancer at 21°C.
To generate knockout cells, 1x106 cells per guide were electroporated with the corresponding RNP complex using Lonza Electroporation Kit V (Lonza). After 48 h, the cells were expanded for future experiments and their DNA were extracted using the PureLink Genomic DNA Kit (Thermo Scientific, Waltham, MA, USA). The knockout efficiency was evaluated by genotyping the polyclonal cell populations using MiSeq (Illumina) according to a published method (16). The primers used for the sequencing are listed Table 2.
The successfully edited populations (using guides cGAS sg3 and STING sg1) were diluted to a concentration of 0.5 cell/well and seeded in 96-well plates. Individual clones were sequenced by MiSeq and the confirmed knockout clones were expanded for experiments.
Chicken bone marrow derived macrophages (BMDM) were generated as previously described (17). Briefly, femurs and tibias of 4 week-old immunologically mature White Leghorn (PA12 line) outbred chickens were removed, both ends of the bones were cut and the bone marrow was flushed with RPMI supplemented with P/S. Cells were then washed and re-suspended in RPMI, loaded onto an equal volume of Histopaque-1077 (Sigma-Aldrich, Germany), and centrifuged at 400 g for 20 min. Cells at the interface were collected and washed twice in RPMI. Purified cells, pooled from three homozygous chickens, were seeded in triplicates at 1×106 cells/ml in sterile 60 mm bacteriological petri dishes in RPMI supplemented with 10% FBS, 25 mM HEPES, 2 mM L-glutamine, P/S and 25 ng/ml recombinant chicken colony stimulating factor 1 (CSF-1) (Kingfisher Biotech, Inc) at 41°C and 5% CO2. Half of the medium was replaced with fresh medium containing CSF-1 at day 3. At day 6, adherent cells were harvested and cultured in RPMI supplemented with 10% FBS, 25 mM HEPES, 2 mM L-glutamine, and P/S prior to stimulation. Procedures were performed in strict compliance with legal dispositions applicable in France, which state that animal euthanasia for the only purpose of organ or tissue use is not considered as an experimental procedure with obligation of submission to ethics committee for approval (Ordinance 2013-118, article R.214-89, published in the Journal Officiel de la République Française # 0032 of the February 7, 2013, pp. 2199).
HD11 (WT, cGAS and STING knockouts) were seeded in 12-well plates at a density of 3×105 cells/well. In the following day, the cells were transfected using TransIT-LT1 (Mirus Bio, USA) with HT-DNA (1, 2, or 5 µg/ml), CT-DNA (1, 2, or 5 µg/ml) or Poly(I:C) (1 µg/ml), and harvested 6 or 16 h post-transfection. In the priming assays, IFNα (200 ng/ml) was added 16 h prior to transfection. 2’3’ cGAMP was added at a concentration of 2.5 µg/ml and cells were harvested 6 h post-treatment.
BMDM were seeded in 6-well plates at 8x105 cells/ml. In the following day, cells were transfected using TransIT-LT1 with HT-DNA (2 µg/ml), CT-DNA (2 µg/ml), or Poly(I:C) (1 µg/ml), and harvested 6 h post-transfection. In the priming assays, IFNα (50 ng/ml) was added 16 h prior transfection to the cells supernatants. 2’3’ cGAMP was added to cells supernatants at the concentration of 10 µg/ml and the cells were harvested 6 h post-treatment.
Chicken IFN-I Bioassay
The presence of IFN-I in supernatants of stimulated BMDM was measured indirectly using a luciferase-based Mx-reporter bioassay (18). Briefly, cells from the quail fibroblast cell line CEC32 carrying the luciferase gene under the control of chicken Mx promoter (kindly provided by Prof. Peter Stäheli, University of Freiburg, Germany) were seeded at 2.5×105 cells/well in 24-well plates and incubated at 41°C under 5% CO2. The next day, cells were incubated for 6 h with the diluted supernatants (1/10 of total volume). Medium was removed and cells were washed twice with PBS. Cells were lysed using the Cell Culture Lysis Reagent (Promega, USA), according to the manufacturer’s instructions, and luciferase activity was measured using the Luciferase assay reagent (Promega, USA) and a GloMax-Multi Detection System (Promega, USA).
BMDM or HD11 viability following different stimuli was assessed using the fluorescent DNA intercalator 7-aminoactinomycin D (7-AAD, BD Biosciences, USA). Briefly, following stimulations, supernatants were discarded, and the cells were harvested and washed in PBS. Cells were stained according to the manufacturer’s protocol and the viability was analyzed by flow cytometry (BD FACS Calibur). Data were expressed as the percentage of 7AAD positive cells over total acquired events (50,000 cells).
Cells were lysed by overlaying with 250 µl of lysis buffer containing 4 M guanidine thiocyanate, 25 mM Tris pH 7, and 143 mM 2-mercaptoethanol. As a second step, 250 µl of ethanol was added, and the solution was transferred to a silica column (Epoch Life Science, Inc., Sugar Land, TX, USA) and centrifuged; all centrifugation steps were performed for 90 s at 16,600 g. The bound RNA was washed by centrifugation with 500 µl of buffer containing 1 M guanidine thiocyanate, 25 mM Tris pH 7, and 10% ethanol, followed by a double washing step with 500 µl of wash buffer 2 [25 mM Tris pH 7 and 70% (v/v) ethanol]. RNA was eluted by centrifugation in 30 µl of nuclease-free water and the concentration was measured using a NanoDrop 2000 Spectrophotometer (Thermo Scientific, Waltham, MA, USA).
cDNA and qPCR
Using 500 ng of RNA extracted from HD11 cells, cDNA was produced using SuperScript III reverse transcriptase, following the manufacture’s protocol (Thermo Scientific, Waltham, MA, USA). Samples were diluted in nuclease-free water in a 1:2.5 ratio. One μl of the diluted product was used for quantitative PCR (qPCR) in a final volume of 10 μl. qPCR was performed using SybrGreen Hi-Rox (PCR Biosystems Inc.) using primers described in Table 3. Fold change in mRNA expression was calculated by relative quantification using hypoxanthine phosphoribosyltransferase (HPRT) as endogenous control.
Total RNA (up to 1 µg per reaction) from BMDM was reverse transcribed with iScript cDNA synthesis kit (Bio-Rad, USA). Quantitative PCR was performed using 1 µl of cDNA, 5 µl of iQ SYBR Green Supermix (Bio-Rad, USA), 0.25 µl of each primer pair and 3.5 µl of nuclease-free water in a total reaction volume of 10 µl. Fold-increase in gene expression was calculated by relative quantification using HPRT and Glyceraldehyde 3-phosphate dehydrogenase (GAPDH) as endogenous controls.
Phagocytosis Assay by Flow Cytometry
HD11 WT cells were seeded at a confluence of 3x105 cells/ml in 12-well plates. The cells were primed with IFNα for 16 h and then with transfected exogenous DNA (HT- and CT-DNA – 2 μg/ml) or treated with 2’3’cGAMP (5 μg/ml) for 6 h. After this, the cells were incubated with Zymosan coated beads conjugated with FITC at a ratio of 30 beads to 1 cell for all conditions for 40 min at 37°C. The cells were wash two times in PBS and fixed in suspension using the solution (missing ref; BD Biosciences) with 4% PFA. Cell populations were counted by analysis on a CytoFLEX cytometer.
Fowlpox Virus Growth and Titration
Fowlpox WT (FP9) and mutants [FPV012 (19) and FPV184 (20)] were propagated in primary chicken embryonic fibroblasts (CEFs) and grown in DMEM-F12 (Thermo Fisher Scientific, Waltham, MA, USA) containing 1% FBS and 5% P/S, and harvested 5 days later. Ten-fold dilutions of cell supernatants were prepared in serum-free DMEM-F12 and used to inoculate confluent monolayers of CEFs for 1.5 h at 37°C. Cells were then overlaid with 2xMEM : CMC (1/1 ratio). The foci were counted 7 days later after staining with Toluidine Blue.
Fowlpox Virus Infection
HD11 cells were seeded in 12-well plates in the day prior infection. Fowlpox viruses were diluted in serum-free DMEM-F12 at a multiplicity of infection (MOI) of 3 and added in the cells (1 ml per well). Infected cells and supernatants were collected from infections at 8 and 24 h post-infection.
Prism 7 (GraphPad) was used to generate graphs and perform statistical analysis. Data were analyzed using an unpaired t test with Welch’s correction unless stated otherwise. Data with P < 0.05 was considered significant and 2-tailed P-value were calculated and presented as: *p < 0.05, **p < 0.01, ***p < 0.001; ****p < 0.0001. Each experiment has at least two biological replicates unless stated.
Intracellular DNA Activates an IFN-I Response in Chicken Macrophages
In order to assess the ability of chicken macrophages to sense and respond to intracellular DNA, we used a combination of the monocytic cell line HD11 and primary bone marrow derived macrophages (BMDM). Transfection of CT DNA, increasing doses of HT-DNA or the RNA analogue poly(I:C) into HD11 cells resulted in transcription of chicken interferon-β (IFNβ) and the interferon stimulated gene (ISG) ISG12.2, an orthologue of mammalian IFI6 (Figure 1A). A dose-dependent response to DNA was observed. Transfection of DNA into primary BMDMs also resulted in IFNβ and ISG12.2 transcription (Figure 1B) and IFN-I secretion as measured by a bioassay (Figure 1C), indicating that this response is present in both primary macrophages and the transformed monocytic HD11 cell line.
Figure 1 Intracellular DNA activates an IFN-I response in chicken macrophages. (A) HD11 cells were transfected with HT-DNA (1, 2, and 5 µg/ml), CT-DNA (5 µg/ml) or Poly(I:C) and transcription of IFNB and ISG12.2 measured by qRT-PCR 6 h later. (B) Chicken BMDM were transfected with HT- DNA, CT-DNA (2 µg/ml) or Poly(I:C) (1 µg/ml) and transcription of IFNB and ISG12.2 measured by qRT-PCR 6 h later. (C) Resting BMDMs or BMDMs primed with IFNα for 6 h were transfected with HT- DNA, CT-DNA (2 µg/ml) or Poly(I:C) (1 µg/ml) and interferon activity in the supernatants was measured after 24 h using a bioassay. IFNα stimulation is a positive control in this assay. (D) HD11 or BMDM were primed with IFNα for 6 h, transfected with HT-DNA, CT-DNA, or Poly(I:C) and transcription of IFNB and ISG12.2 measured by qRT-PCR 6 h later. (E) HD11 (top) or IFNα-primed BMDM (bottom) were transfected with HT-DNA, CT-DNA, or Poly(I:C) and cell viability measured by 7AAD staining 24 or 48 h later. *p < 0.05, **p < 0.01, ***p < 0.001; ****p < 0.0001; ns: no significant difference. Data is representative of two or more replicates.
Since in mammalian systems STING is recognized as an interferon stimulated gene (ISG) (21), we sought to understand the effect of IFN-I priming of macrophages on the response to intracellular DNA. Pre-treatment of HD11 or BMDM with chIFNα resulted in an enhancement of IFNβ transcription following DNA stimulation and confirmed ISG12.2 as an ISG (Figure 1D). This signaling enhancement might be explained by increased transcription of STING and/or IRF7 following IFNα treatment (Supplementary Figure 1). Across all HD11 and BMDM DNA stimulations we found that there was little observable or measurable cell death (Figure 1E), indicating that, in chicken macrophages, cell death is likely not a specific output of STING signaling.
Intracellular DNA Stimulates Transcription of MHC-II and Co-Stimulatory Molecules
The sensing of both intracellular and extracellular pathogens activates macrophages, causing up-regulation or enhancement of effector functions designed to combat infection. We hypothesized that DNA transfection, mimicking the presence of intracellular infection, might result in direct effects on the molecules that contribute to T cell stimulation. In chickens, there are two classical MHC-II genes encoded by BLB1 and BLB2, as well as a DM system that includes the DMB1 and DMB2 genes encoding class II-specific chaperones or peptide editors (22), all of which were transcriptionally upregulated by DNA stimulation in chicken BMDMs (Figure 2A). In HD11 cells, only BLB1 transcription was upregulated by DNA stimulation, while BLB2 transcription was upregulated only by IFNα pre-treatment (Supplementary Figure 2) and DMB1/2 were not altered by any stimuli (not shown), highlighting possible differences between primary and transformed cells in this specific context (Figure 2B). CD86 and CD40 are key co-stimulatory molecules in T cell activation. In BMDM CD86 and CD40 transcription was upregulated in response to DNA stimulation (Figure 2A). There was, however, no measurable impact of DNA stimulation on phagocytosis as measured by bead-uptake assays in HD11 cells (Figure 2C). As such, key molecules involved in T cell activation by macrophages are regulated by DNA stimulation, but not all macrophage effector functions are equally enhanced by this signal.
Figure 2 Intracellular DNA stimulates transcription of MHC-II and co-stimulatory molecules. (A) BMDMs or (B) HD11 cells were transfected with HT-DNA, CT-DNA, or Poly(I:C) and transcription of BLB1, BLB2, DMB1, DMB2, CD40, and CD86 measured by qRT-PCR 6 h later. (C) HD11 cells were stimulated with HT-DNA, CT-DNA, or Poly(I:C) and 6 h later phagocytosis was monitored by FITC-conjugated, zymosan coated bead uptake. Histograms of non-treated versus treated cells (left panels) and respective percentages of FITC positive cells for each treatment tested (right panel) are presented. *p < 0.05, **p < 0.01, ***p < 0.001; ns, no significant difference. Data is representative of two or more replicates.
STING and TBK1 Contribute to DNA-Driven Transcriptional Responses in Chicken BMDMs
In order to dissect the signaling pathway downstream of intracellular DNA sensing, we first used the ligand 2’3’-cGAMP, the enzymatic product of cGAS that directly binds and activates STING (23). Treatment of BMDMs or HD11 cells with 2’3’-cGAMP led to increased transcription levels of IFNb, ISG12.2, BLB1, BLB2, CD86, and CD40 (Figures 3A, B). This response, and the response to DNA and cGAMP stimulation, could be reduced by small molecule inhibitors of STING (H151) and the kinase TBK1 (BX795), indicating the existence of a STING and TBK1-dependent signaling pathway in chicken macrophages and evidencing the cross-species utility of these two pharmacological inhibitors (Figures 3C, D). As with DNA stimulation, there was no measurable impact of cGAMP treatment on phagocytosis in HD11 cells (Figure 3E).
Figure 3 STING and TBK1 contribute to DNA-driven transcriptional responses in chicken BMDMs. (A) HD11 and (B) BMDM cells were treated with 2’3’cGAMP (10 μg/ml) and qRT-PCR carried out 6 h later for the indicated genes. (C) BMDM were treated with the STING inhibitor H-151 (10 uM) or TBK1 inhibitor BX795 (1 uM) for 1 h before transfection with HT-DNA and CT-DNA. Six hours later, RNA was extracted and qRT-PCR carried out for the indicated genes. (D) BMDM were treated with the STING inhibitor H-151 (10 uM) or TBK1 inhibitor BX795 (1 uM) for 1 h before treatment with 2’3’cGAMP (10 μg/ml). Six hours later, RNA was extracted and qRT-PCR carried out for the indicated genes. (E) HD11 cells were treated with 2’3’cGAMP (2.5 µg/ml) 6 h later phagocytosis was monitored by FITC-conjugated, zymosan coated bead uptake. *p < 0.05, **p < 0.01, ***p < 0.001; ****p < 0.0001; ns: no significant difference. Data is representative of two or more replicates.
cGAS Is Essential for Intracellular DNA-Dependent IFN-I and MHC-II Transcription in HD11 Cells
To address the possibility that cGAS is a principle PRR responsible for sensing intracellular DNA in chicken macrophages, we generated HD11 knockout cell lines using CRISPR/Cas9 genome editing. To do this, we analyzed the annotated cGAS sequence in the current release of the Gallus gallus genome and designed gRNA sequences targeting regions of the gene which exhibited high conservation across multiple orthologues. By sequencing single cell clones we generated multiple cGAS knockout cell lines with two different gRNAs. By sequencing across the gRNA PAM target sites, we characterized indels to confirm the knockout status in these clones (e.g., Figure 4A). Stimulation of multiple cGAS knockout HD11 clones, each with a different indel, with DNA resulted in an abrogation of IFN-I and ISG transcription indicating that cGAS is a key PRR for sensing intracellular DNA in chicken macrophages (Figure 4B and Supplementary Figure 3). cGAS knockout also abrogated the upregulation of DNA-driven BLB1 stimulation, indicating the cGAS-dependent signaling is responsible for regulation of MHC class II transcription in this context (Figure 4B). These data were independent of IFNα pre-treatment, which enhanced IFN-I and BLB1 transcription in WT DNA-stimulated cells, but did not affect cGAS KO cells (Figure 4C). Consistent with the mammalian cGAS mechanism, stimulation of WT or cGAS KO cells with 2’3’-cGAMP resulted in robust IFN-I transcription, indicating IFN-I production by direct STING ligation was not affected by cGAS KO (Figure 4D). These data confirm the intracellular DNA PRR function of cGAS in chicken macrophages.
Figure 4 cGAS is essential for intracellular DNA-dependent IFN-I and MHC-II transcription in HD11 cells. (A) Example of identification of indel in clonally selected HD11 cGAS KO using NGS sequencing. (B) WT and cGAS KO HD11 cells were transfected with HT-DNA, CT-DNA (2 μg/ml) or Poly(I:C) (1 μg/ml) for 6 h and transcription of the indicated genes measured by qRT-PCR. (C) cGAS KO HD11 cells were primed with IFNα for 6 h, transfected with HT-DNA, CT-DNA, or Poly(I:C) and transcription of IFNB and ISG12.2 measured by qRT-PCR 6 h later (D) WT or cGAS KO cells were treated with 2’3’cGAMP (10 μg/ml) and transcription of IFNB measured by qRT-PCR 6 h later. *p < 0.05, **p < 0.01, ***p < 0.001; ns, no significant difference. Data is representative of two or more replicates.
STING Is Essential for Intracellular DNA-Dependent IFN-I Transcription in HD11 Cells
In parallel, using the same methodology, we generated multiple STING knockout HD11 cell lines (Figure 5A). Stimulation of these cells with DNA phenocopied the cGAS knockout lines, and neither STING or cGAS KO altered tonic IFNB transcription, confirming the function of chicken STING downstream of cGAS in the intracellular DNA sensing pathway (Figure 5B, Supplementary Figures 4 and 5). These data are consistent with the presence of a cGAS/STING pathway in HD11 cells and, in concert with the data using H151 in BMDMs, indicate the function of STING as a critical adaptor protein for intracellular DNA sensing in chicken macrophages.
Figure 5 STING is essential for intracellular DNA-dependent IFN-I transcription in HD11 cells. (A) Example of identification of indel in clonally selected HD11 STING KO using NGS sequencing. (B) WT and STING KO HD11 cells were transfected with HT-DNA, CT-DNA (2 μg/ml) or Poly(I:C) (1 μg/ml) for 6 h and transcription of the indicated genes measured by qRT-PCR 6 h later. *p < 0.05, ***p < 0.001; 2difference. Data is representative of two or more replicates.
Fowlpox Triggers a cGAS/STING Dependent DNA Sensing Pathway in HD11 Cells
FWPV replication exposes large quantities of DNA to the cytoplasm of infected cells making it a prime target for intracellular DNA sensing PRRs. Despite this, using the wild-type vaccine strain FP9 we, and others (13, 19), observe little or no IFN-I transcription in infected cells, and indeed a downregulation of IFN and MHC transcription (Figure 6A). The lack of IFN-I response in poxvirus infected cells is likely due to the presence of numerous virally-encoded suppressors of PRR signaling and IFN-I production (19, 24), hence deletion of specific innate immunomodulators from the viral genome can result in a virus that stimulates host IFN-I signaling. We made use of FWPV mutants FPV012 and FPV184 (19, 20), each deficient in single genes that are proposed immunomodulators, and both of which induce IFN-I production from infected cells (19), including HD11 cells (Figure 6B). In the absence of cGAS or STING the transcription of IFN-I, ISG12.2, BLB1 and CD40 by FPV184 or FPV012 was significantly lower at 24 h post infection (Figures 6B, C), despite robust infection of HD11 cells by all three virus strains (Figure 6D), indicating that FWPV is sensed in infected cells by the DNA sensing PRR cGAS and that the cGAS/STING pathway is responsible for FWPV-induced IFN-I production and MHC-II transcription. Despite its importance for the IFN-I response, in HD11 cells loss of the cGAS/STING pathway did not affect the replicative capacity of the FP9 or mutant viruses (Figure 6E).
Figure 6 Fowlpox triggers a cGAS/STING dependent DNA sensing pathway in HD11 cells. (A) HD11 cells were infected with FWPV strain FP9 at a multiplicity of infection of three. Twenty-four hours later, RNA was extracted and qRT-PCR carried out for the indicated genes. (B, C) HD11 WT, cGAS or STING KO cells were infected with FP9 (black bars), FPV012 (blue bars), FPV184 (red bars), at a multiplicity of infection of three. Twenty-four hours later, RNA was extracted and qRT-PCR carried out for the indicated genes. (D) HD11 cells were infected with FWPV strain FP9 at a multiplicity of infection of three. Twenty-four hours later, RNA was extracted and qRT-PCR carried out for the indicated FWPV genes. (E) HD11 WT, cGAS or STING KO cells were infected with FP9, FPV012, or FPV184 at a multiplicity of infection of three, cell supernatants harvested and released FP9 was titrated on CEFs to measure focus forming units (ffu) per ml. *p < 0.05, **p < 0.01, ***p < 0.001; ****p < 0.0001; ns, no significant difference. Data is representative of two or more replicates.
The ability of innate immune cells to detect virus infection is dependent on a set of PRRs that directly bind viral nucleic acids. Macrophages act in this context as tissue-resident sentinel sensors of infection that express a broad repertoire of PRRs and mount a rapid and robust innate immune response to viruses and other pathogens. Indeed intracellular DNA sensing was first described in macrophages (25). As well as interferon and cytokine production, activated macrophages use effector functions for pathogen clearance and for activation of adaptive immunity. In mammalian systems the signaling outputs downstream of intracellular DNA detection in macrophages include IRF-dependent IFN and cytokine production and cell death driven by the AIM2 inflammasome. In chicken macrophages, which lack AIM2, we find that intracellular DNA sensing produces IFN but does not result in measurable cell death, rather it upregulates a specific set of antigen presentation machinery including the MHC-II gene BLB1 and co-stimulatory molecules, providing a direct link between anti-viral innate sensing and the initiation of adaptive immunity.
During DNA virus infection, the cGAS/STING-dependent signaling pathway is triggered by viral DNA, resulting in type-I interferon production via activation of TBK1 and the IRF family of transcription factors. Although well defined in mammalian systems, the function of chicken cGAS and STING has only more recently been identified (26, 27). FWPV is an avian poxvirus that causes skin lesions and respiratory infections and can infect multiple cell types including macrophages (28). Here we show that the cGAS/STING pathway in chicken macrophages can sense FWPV infection and is responsible for the IFN-I response as well as for upregulation of BLB1.
In order to escape detection and evade host anti-viral responses, poxviruses like FWPV encode a broad range of immunomodulatory proteins that target PRR signaling pathways resulting in these viruses being able to effectively inhibit IFN production from infected cells. These immune evasion mechanisms mask the signaling outputs of PRR signaling during infection with wild type poxviruses. To overcome this issue, we used two mutant FWPVs with deletions in individual genes that block IFN-I production during infection. Infection of cells with FPV184 and FPV012 (29) resulted in interferon and ISG transcription, which was lost in cGAS and STING knockout lines. FWPV DNA is therefore sensed by the cGAS/STING pathway and the downstream signaling response leading to IFN-I production is effectively blocked by the wild type virus. In culture the loss of cGAS or STING didn’t lead to significant alterations FWPV’s replicative capacity in infected cells (Figure 6E), but it remains to be seen how individual PRRs like cGAS contribute to protection against FWPV infection in vivo. In mice cGAS/STING are essential for the host response to poxvirus infections such as vaccinia and ectromelia viruses, and the protective effects are meditated via IFN-I, despite the presence of large numbers of immunomodulators targeting PRR signaling, including the cGAS/STING systems in these viruses. As such it is likely that cGAS/STING mediated FWPV DNA sensing and IFN-I production has a significant contribution to host defence against FWPV infection in chickens, although mechanistically it remains to be seen exactify how IFN-I mediates this defence against this avian poxvirus.
Birds occupy the same habitats as mammals, have comparable ranges of life span and body mass, and confront similar pathogen challenges, yet birds have a different repertoire of organs, cells, molecules and genes of the immune system compared to mammals (30). It is increasingly evident that the immune system of avian species is rather different from those of model mammalian species. Untested extrapolation from mammalian systems cannot provide the quality of knowledge that is required for understanding host-pathogen relationships in birds. Here, we find that the signaling downstream of chicken cGAS leading to IFN-I transcription is similar to that found in mammalian systems. The presence of orthologues of STING and TBK1 in the chicken genome and their functional inhibition by small molecule compounds (H151 and BX795) is indicative of mechanistic signaling pathway conservation. The chicken genome also contains an orthologue of IRF3, which is the main transcription factor downstream of STING/TBK1 activation, although chicken IRF7 (as this gene is annotated) is not equivalent to mammalian IRF3 or IRF7 and may be considered more as a hybrid these two genes (31). It is likely that chicken IRF7 and TBK1 are recruited by STING following 2’3’-cGAMP ligation and that subsequent phosphorylation, dimerization, and nuclear translocation of IRF7 leads to DNA-induced IFN-I transcription (27, 32). In mammalian systems, the transcription of IFNβ also requires activation of NF-κB, to a greater or lesser extent depending on the species (33, 34). STING can itself be responsible for NF-κB activation following virus infection (35). The extent to which chicken IFNβ transcription downstream of cGAS activation requires NF-κB activity along with IRF7 remains to be explored (32). Recent evidence has implicated chicken cGAS and STING in avian antiviral defence, in particular against Marek’s Disease Virus (MDV) and chicken adenovirus 4 (36, 37) in fibroblasts. Using CRISPR/Cas9 technology to knockout STING and cGAS in a transformed monocytic cell line (HD11) and complementing these data in primary macrophages with pharmacological inhibitors we have been able to show this cGAS/STING/TBK1 pathway is active in chicken macrophages. The use of primary cells in this context is important as transformation or immortalization can significantly alter PRR pathways so as to obscure physiological signaling mechanisms.
IFN-I is one of the most effective anti-viral innate immune mediators. Secretion and subsequent ISG transcription induced by autocrine and paracrine IFN receptor signaling sets an anti-viral/inflammatory state in infected and bystander cells. As an example, chicken IFNβ was shown to be an autocrine/paracrine pro-inflammatory mediator in chicken macrophages (17), with direct effects in macrophage effector functions. Nucleic acid sensing PRRs therefore provide a rapid and potent innate response helping to combat infection and reduce viral spread in infected tissues. At the same time, innate immune responses can initiate and amplify adaptive immune responses for example, by regulating functions of antigen presenting cells (APCs), promoting cross-priming and stimulating antibody production (38–40). In both mammals and birds, macrophages are key regulators of adaptive immunity as principle APCs. By processing and presenting antigen to T and B cells, macrophages directly trigger adaptive responses. The discovery that cGAS/STING signaling can directly regulate the transcription of MHC genes in macrophages provides further evidence linking PRR signaling with the activation of adaptive immunity during infection. It remains to be explored exactly how the transcription of BLB1 and BLB2 is regulated by cGAS/STING signaling. In tissues, macrophages survey the local environment for infection and damage. In this context, macrophage effector functions may be modulated by the presence of innate immune mediators in the tissue. The priming effect of IFNα as an enhancer of macrophage DNA sensing, by upregulating STING expression, suggests a possible mechanism of bystander surveillance. Tissue resident macrophages may respond to signals, including IFN-I and cGAMP, secreted from virally infected stromal cells by enhancing specific effector functions appropriate to defend against viral infection in the tissue (41, 42).
Our data adds to the list of chicken cGAS/STING functions in sensing of avian DNA viruses such as MDV and Adenovirus 4 that replicate in the nucleus or FWPV that replicates in the cytoplasm, and in the regulation of macrophage effector functions. The ability of this pathway to sense a broad range of DNA viruses that replicate in different compartments in avian innate immune cells indicates that this pathway is a primary DNA sensing mechanism for DNA viruses in chickens.
Data Availability Statement
The raw data supporting the conclusions of this article will be made available by the authors, without undue reservation.
BF and CB provided the funding and supervised the work. MO, DR, RG, VG, and EK performed the experiments and statistical analysis. SG and MS generated the mutant fowlpox viruses. BF, CB, RG designed the study and wrote the manuscript. All authors contributed to the article and approved the submitted version.
This work was funded by BBSRC grants BB/S001336/1 (BF and CB), BB/E009956/1, BB/G018545/1, BB/H005323/1 & BB/K002465/1 (MS) and by EUROFERI (Région Centre-Val-de-Loire, France, RG).
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
This manuscript has been released as a Pre-print at BioRxiv. We thank the experimental facility PFIE (Plateforme d’Infectiologie Expérimentale, Centre INRAE Val de Loire, Nouzilly, France) for providing the animals used for the isolation of primary macrophages.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fimmu.2020.613079/full#supplementary-material
Supplementary Figure1 | Effect of IFNα priming on expression levels of STING and IRF7 in BMDM and HD11. BMDM or HD11 cells were treated with IFNα for 6 h and transcription of STING and IRF7 measured by qRT-PCR 6 h later. Data is representative of two or more replicates.
Supplementary Figure 2 | BLB2 but not BLB1 is an ISG in HD11 cells. HD11 cells were treated with IFNα for 6 h and the indicated genes were measured by qRT-PCR. Data is representative of two or more replicates.
Supplementary Figure 3 | cGAS is essential for intracellular DNA-dependent IFN-I transcription in HD11 cells. WT or three individual cGAS knockout clones with different indels were stimulated with HT-DNA (2 μg/ml) and IFNB transcription measured by qRT-PCR 6 h later. Data is representative of two or more replicates.
Supplementary Figure 4 | STING is essential for intracellular DNA-dependent IFN-I transcription in HD11 cells. WT or three individual cGAS knockout clones with different indels were stimulated with HT-DNA (2 μg/ml) and IFNB transcription measured by qRT-PCR 6 h later. Data is representative of two or more replicates.
Supplementary Figure 5 | STING or cGAS loss does not significantly alter tonic IFN-I transcription. IFNB transcription measured by qRT-PCR in WT, cGAS KO or STING KO HD11 cells (data shown relative to WT cells).
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Keywords: DNA, fowlpox, chicken, macrophages, cyclic GMP-AMP synthase, stimulator of interferon genes, pattern recognition receptor
Citation: Oliveira M, Rodrigues DR, Guillory V, Kut E, Giotis ES, Skinner MA, Guabiraba R, Bryant CE and Ferguson BJ (2021) Chicken cGAS Senses Fowlpox Virus Infection and Regulates Macrophage Effector Functions. Front. Immunol. 11:613079. doi: 10.3389/fimmu.2020.613079
Received: 01 October 2020; Accepted: 16 December 2020;
Published: 01 February 2021.
Edited by:Chunfu Zheng, Fujian Medical University, China
Reviewed by:Henrique De Paula Lemos, Newcastle University, United Kingdom
Lei Huang, Newcastle University, United Kingdom
Copyright © 2021 Oliveira, Rodrigues, Guillory, Kut, Giotis, Skinner, Guabiraba, Bryant and Ferguson. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Brian J. Ferguson, email@example.com
†These authors share senior authorship