Logo of plospathPLoS PathogensSubmit to PLoSGet E-mail AlertsContact UsPublic Library of Science (PLoS)View this Article
PLoS Pathog. 2013 Jan; 9(1): e1003118.
Published online 2013 Jan 3. doi:  10.1371/journal.ppat.1003118
PMCID: PMC3536698

IRF-3, IRF-5, and IRF-7 Coordinately Regulate the Type I IFN Response in Myeloid Dendritic Cells Downstream of MAVS Signaling

Christopher F. Basler, Editor


Although the transcription factors IRF-3 and IRF-7 are considered master regulators of type I interferon (IFN) induction and IFN stimulated gene (ISG) expression, Irf3−/−×Irf7−/− double knockout (DKO) myeloid dendritic cells (mDC) produce relatively normal levels of IFN-β after viral infection. We generated Irf3−/−×Irf5−/−×Irf7−/− triple knockout (TKO) mice to test whether IRF-5 was the source of the residual induction of IFN-β and ISGs in mDCs. In pathogenesis studies with two unrelated positive-sense RNA viruses (West Nile virus (WNV) and murine norovirus), TKO mice succumbed at rates greater than DKO mice and equal to or approaching those of mice lacking the type I IFN receptor (Ifnar−/−). In ex vivo studies, after WNV infection or exposure to Toll-like receptor agonists, TKO mDCs failed to produce IFN-β or express ISGs. In contrast, this response was sustained in TKO macrophages following WNV infection. To define IRF-regulated gene signatures, we performed microarray analysis on WNV-infected mDC from wild type (WT), DKO, TKO, or Ifnar−/− mice, as well as from mice lacking the RIG-I like receptor adaptor protein MAVS. Whereas the gene induction pattern in DKO mDC was similar to WT cells, remarkably, almost no ISG induction was detected in TKO or Mavs−/− mDC. The relative equivalence of TKO and Mavs−/− responses suggested that MAVS dominantly regulates ISG induction in mDC. Moreover, we showed that MAVS-dependent induction of ISGs can occur through an IRF-5-dependent yet IRF-3 and IRF-7-independent pathway. Our results establish IRF-3, -5, and -7 as the key transcription factors responsible for mediating the type I IFN and ISG response in mDC during WNV infection and suggest a novel signaling link between MAVS and IRF-5.

Author Summary

Host pathogen sensors, including those of the Toll-like receptor and RIG-I like receptor (RLR) families, detect viral infection in cells. Signaling through these receptors triggers expression of type I interferon (IFN) and IFN-stimulated genes (ISGs), in part through the IRF family of transcription factors. Previous studies with West Nile virus (WNV) showed that IRF-3 and IRF-7 control IFN expression in fibroblasts and neurons, whereas macrophages and myeloid dendritic cells (mDC) retained the ability to induce IFN-β without IRF-3 and IRF-7. In the current study, we generated Irf3−/−×Irf5−/−×Irf7−/− (TKO) mice to characterize the contributions of specific IRF transcription factors to IFN and ISG induction in response to WNV infection in cells and in mice. We found that induction of IFN and ISGs was largely abolished in TKO mDC, but sustained in TKO macrophages. Because IFN and ISG induction also was absent in mDC lacking MAVS, a key mediator of RLR signaling, our results suggest a novel signaling link between IRF-5 and MAVS. This study establishes the molecular pathways responsible for IFN induction in mDC and suggests a cross-talk between IRF-5 and RLR signaling pathways.


The type I interferon (IFN) signaling network is an essential component of the innate immune response against viral infections, and also functions to shape adaptive immunity [1][4]. Infected cells initiate an antiviral response upon recognition of non-self pathogen-associated molecular patterns (PAMPs), which are detected by host pattern recognition receptors (PRRs) [2], . PRRs that recognize RNA viruses include members of the Toll-like receptor (TLR3 and TLR7) and the RIG-I-like receptor (RLR; RIG-I and MDA5) families. TLRs and RLRs recognize distinct PAMPs in different locations (extracellular/endosomes and cytoplasm, respectively) and activate signaling cascades to initiate antiviral and inflammatory responses. TLR3 binds to double-stranded RNA and recruits the adaptor molecule TRIF to activate the kinases TRAF and IKK-ε, which in turn activates the latent transcription factors IRF-3, IRF-7, and NF-κB. Single-stranded RNA is recognized by TLR7, which uses the adaptor molecule MyD88 to activate TRAF and IKK-ε, and subsequently NF-κB- and IRF-7-dependent transcription. RLRs interact with the mitochondria-associated adapter molecule MAVS (also called IPS-1, VISA, or CARDIF), which signals through the kinases TBK1 and IKK-ε to activate IRF-3, IRF-7, and NF-κB and initiate type I IFN production.

A canonical model for type I IFN production after RNA virus infection is a two-step positive feedback loop that is regulated by IRF-3 and IRF-7 [9], [10]. In the first phase, viral sensing by TLRs or RLRs induces nuclear localization of IRF-3, which in concert with NF-κB and ATF-2/c-Jun stimulates transcription, synthesis, and secretion of IFN-β and IFN-α4 by infected cells. In the second phase, extracellular IFN-β and IFN-α4 bind to the type I IFN receptor (IFNAR), which triggers activation of the JAK-STAT signaling pathway and induction of IFN-stimulated genes (ISGs) [11]. ISGs act by a variety of mechanisms to render cells resistant to viral replication [12], [13]. Although type I IFN signaling is required to activate the full antiviral response, a subset of ISGs is induced directly by IRF-3 [14], [15]. While IRF-3 is constitutively expressed in many tissues, IRF-7 is an ISG required for the expression of most IFN-α subtypes, and thus a key mediator of the type I IFN amplification loop [2], [9], [10]. Certain cells, including plasmacytoid dendritic cells and macrophages, express IRF-7 constitutively, which makes them poised for rapid IFN-α production [16][20].

West Nile virus (WNV) is a mosquito-transmitted, enveloped, positive-sense RNA virus and member of the Flaviviridae family. Studies in mice with targeted gene deletions have provided insight into mechanisms of innate immune restriction of WNV infection. The type I IFN response is essential to the control of WNV infection, as mice that are defective at producing or responding to IFN cannot control virus replication and succumb rapidly to infection [17], [21][25]. The host antiviral response in vivo is dependent upon both TLR and RLR signaling, as deficiencies in TLRs, RLRs, or their downstream adaptor molecules (including MyD88 and MAVS) result in enhanced viral replication and lethality [8], [22], [26][30].

Recent studies with WNV have suggested that some cell types use non-canonical signaling pathways to induce type I IFN responses. The combined absence of IRF-3 and IRF-7 resulted in uncontrolled WNV replication and more rapid death in Irf3−/−×Irf7−/− double knockout (DKO) mice compared to the individual single gene knockout mice [17], [21], [22], [31]. However, even without IRF-3 or IRF-7, type I IFN was produced by DKO mice infected with WNV or murine cytomegalovirus, albeit at reduced levels compared to wild type mice [22], [32]. Consistent with the sustained production of type I IFN, lethality in DKO mice infected with WNV or chikungunya virus was not as rapid or complete as in Ifnar−/− mice [22], [31], [33], [34]. Ex vivo experiments with primary myeloid dendritic cells (mDC) and macrophages revealed that the IFN-β response after WNV infection was sustained in DKO cells but abrogated in the absence of MAVS [22], [27]. In contrast, the IFN-β response in neurons and fibroblasts was abolished in the absence of either IRF-3 and IRF-7 or MAVS [22], [27]. These studies suggested cell type-specific requirements for the transcription factors that induce IFN-β expression in response to WNV infection.

To define the transcription factor(s) responsible for the IRF-3 and IRF-7-independent production of IFN-β in myeloid cells, we considered another member of the IRF family, IRF-5. Although IRF-5 was originally identified as an inducer of inflammatory cytokines (IL-6 and TNF-α) downstream of TLR-7 and MyD88 signaling, subsequent studies suggested that it could contribute to type I IFN production after viral infection [35][37]. In response to Newcastle disease virus (NDV) infection, IRF-5 induced overlapping and distinct sets of genes compared to IRF-7, including stronger induction of IFN-β and the antiviral gene Rsad2 (Viperin) [38]. We generated Irf3−/−×Irf5−/−×Irf7−/− triple knockout (TKO) mice and found that these mice were highly vulnerable to infection with WNV. The combined loss of IRF-3, IRF-5, and IRF-7 largely abrogated type I IFN and ISG expression in mDC, and microarray analysis of WNV-infected mDC revealed a set of genes induced in DKO but not in TKO cells. Because the limited set of genes induced in WNV-infected TKO mDCs was absent in Mavs−/− mDCs, we conclude that the RLR-MAVS signaling pathway dominantly regulates innate immune gene induction in mDCs during WNV infection, and that IRF-3, IRF-5, and IRF-7 coordinately mediate this response. Our results establish a new linkage between the IRF-5 and the RLR signaling pathways in induction of the antiviral IFN response.


TKO mice are highly vulnerable to viral infections

We hypothesized that IRF-5 might be responsible for the residual IFN-β production in DKO mice, because IRF-5 contributes to Ifnb mRNA expression downstream of the PRR TLR7 and adaptor molecule MyD88, both of which limit WNV pathogenesis in vivo [28], [30], [39]. To test this, we generated Irf3−/−×Irf5−/−×Irf7−/− TKO mice (Figure S1) and defined their response to viral infection. TKO mice were viable, fertile, and produced progeny according to normal Mendelian frequencies (data not shown). We infected WT, DKO, and TKO mice with a virulent WNV strain (New York 2000, WNV-NY) and found that TKO mice succumbed to infection earlier than DKO mice (mean time to death (MTD): 4.0 days versus 5.7, P<0.0001). TKO mice died marginally later than Ifnar−/− mice, which do not respond to type I IFN and fail to control WNV replication (MTD: 4.0 days versus 3.7, P<0.05) (Figure 1A) [25], [31]. Because TKO, DKO and Ifnar−/− mice all succumbed so rapidly to WNV-NY infection, it was difficult to appreciate biologically meaningful differences in susceptibility among the three genotypes. To address this, we infected these mice with an attenuated WNV strain (Madagascar 1978, WNV-MAD) that inefficiently antagonizes JAK/STAT signaling [23]. With this virus, we observed a pronounced increase in mortality of TKO compared to DKO mice (Figure 1B). Whereas 100% of TKO mice succumbed to WNV-MAD infection, only 20% of DKO mice died (P<0.001). TKO mice were equally vulnerable to WNV-MAD infection as Ifnar−/− mice (P>0.05), and no statistical difference in MTD was observed (9.0 days for TKO versus 8.2 days for Ifnar−/− mice, P>0.05). Similar results were observed upon infection with murine norovirus (MNV), an unrelated non-enveloped positive-sense RNA virus. TKO mice were more vulnerable to MNV infection than DKO mice, with only 1 of 11 TKO mice surviving, compared to 100% survival for DKO mice (P<0.0001) (Figure 1C). However, the TKO mice did not show the same susceptibility as Ifnar−/− mice (P<0.0001), and the MTD was greater in TKO compared to Ifnar−/− mice (7.8 days versus 5.3 days, P<0.001). The observation that lethality in TKO mice more closely matched that of Ifnar−/− mice after WNV infection compared to MNV suggests that there may be virus-specific differences in the particular transcription factors responsible for mediating the antiviral response. Overall, the loss of IRF-5 in the setting of an IRF-3 and IRF-7 deficiency renders mice more vulnerable to viral infection and early death, approaching that seen in mice that cannot respond to type I IFN.

Figure 1
Lethality and viral burden after virus infection.

To understand the basis of the increased susceptibility of TKO mice to viral infection, we infected WT, DKO, TKO, and Ifnar−/− mice with WNV-NY or WNV-MAD and measured viral burden in the draining lymph node, serum, spleen and brain at 2 days (WNV-NY) or 6 days (WNV-MAD) after infection (Figure 1D–G). Viral infection in TKO mice was similar to that observed in Ifnar−/− mice (P>0.05) in all tissues examined, except for the spleen after WNV-MAD infection where titers in TKO mice were greater than in Ifnar−/− mice (25-fold, P<0.05). After infection with WNV-NY, TKO mice had higher viral loads than DKO mice in the draining lymph node (13-fold, P<0.01), spleen (5-fold, P<0.01), and brain (9-fold, P<0.05). After infection with WNV-MAD, TKO mice had higher viral loads than DKO mice in the serum (124-fold, P<0.01) and spleen (169-fold, P<0.01).

Serum antiviral activity

To determine whether the enhanced vulnerability of TKO mice was due to an inability to generate a systemic antiviral response, we measured type I IFN levels in the serum of mice infected with WNV-NY (2 days after infection) or WNV-MAD (6 days after infection) (Figure 2). Unexpectedly, we detected type I IFN activity in the serum of TKO mice infected with WNV-NY or WNV-MAD, and the amount present was not different from DKO mice (P>0.05). While the serum levels of type I IFN in TKO and DKO mice were diminished compared to WT mice after WNV-NY infection and equivalent to WT after WNV-MAD infection, substantially higher levels of type I IFN were detected in the serum from Ifnar−/− mice (29-fold after WNV-NY infection, P<0.01; 416-fold after WNV-MAD infection, P<0.0001). The high level of type I IFN in Ifnar−/− mice likely is a result of high viral replication in the absence of IFN-mediated antiviral effector functions combined with the absence of IFNAR molecules to bind and internalize type I IFN in the serum. Despite the combined absence of IRF-3, IRF-5, and IRF-7, TKO mice still produced type I IFN after WNV infection, albeit at lower levels in the context of markedly enhanced infection.

Figure 2
Type I IFN activity in serum.

Virus control and ISG induction is ablated in TKO mDC but not macrophages

Myeloid cells retain the ability to produce IFN-β during WNV infection despite the lack of IRF-3 and IRF-7 [22]. To determine if this IFN-dependent antiviral activity was mediated by IRF-5, we performed multi-step growth analyses with WNV-NY in primary mDC and macrophages derived from WT, DKO, TKO, and Ifnar−/− mice (Figure 3A and B). Viral replication in TKO mDC was greater than in DKO mDC (74-fold, P<0.0001) and equivalent to Ifnar−/− mDC (P>0.05), suggesting that IRF-3, IRF-5, and IRF-7 regulate innate immune defense to control WNV replication in mDC. In comparison, TKO macrophages showed little increase in WNV-NY replication compared to DKO cells, and reached lower (11-fold, P<0.0001) peak titers compared to Ifnar−/− macrophages. This suggests that macrophages can restrict WNV-NY infection through an alternative pathway that is independent of IRF-3, IRF-5, and IRF-7, possibly through IRF-1 and/or other transcription factors [40].

Figure 3
ISG and IFN-β induction in primary myeloid cells in response to WNV infection.

To establish whether the disparate ability of TKO mDC and macrophages to control WNV-NY replication was associated with differences in antiviral gene induction, we infected cells and performed western blots to assay expression of ISGs, specifically RIG-I (DDX58), MDA5 (IFIH1), STAT1, IFIT2 (ISG54) and IFIT3 (ISG49) (Figure 3C and D). In TKO mDCs, we did not detect expression of any of the tested ISGs, although these were highly expressed in WNV-infected WT and DKO mDC (Figure 3C and [22]). In contrast, most of these proteins were induced in TKO macrophages, although their expression was delayed compared to WT cells: ISG expression was detected in TKO macrophages at only 48 hours after infection, whereas expression was detected in WT cells within 12 hours of infection. Unlike other ISGs, IFIT3 was not expressed in TKO macrophages even at 48 hours after infection, despite being induced in DKO macrophages [22]. The lack of virus-induced ISG expression in TKO mDC resembled the phenotype observed in cells lacking the RLR-signaling adaptor, MAVS [27].

To further define the ISGs expressed in an IRF-3, IRF-5, or IRF-7 dependent manner, we infected mDC and macrophages from WT, DKO, TKO, and Ifnar−/− mice with WNV-NY and measured the induction of Ifnb, Oas1a, Rsad2, and Cxcl10 mRNA at 24 hours after infection by quantitative reverse transcription polymerase chain reaction (qRT-PCR) (Figure 3E and F). These genes were selected as known representatives of different ISG induction pathways. Rsad2 and Cxcl10 can be induced directly by PRR signaling and IRF-3 mediated transcriptional regulation, whereas expression of Oas1a depends more strictly upon IFN-β signaling [14], [15], [20]. Consistent with the western blot results, all four genes were induced strongly in WT and DKO mDC, but not in TKO mDC. In contrast, TKO macrophages retained the ability to express Ifnb and the tested ISGs, although the level of gene induction was equivalent to or less than WT cells, even in the context of enhanced viral replication. As expected, Oas1a was not induced in Ifnar−/− cells, although these cells expressed high levels of Rsad2, Cxcl10 and Ifnb. ISG expression in Ifnar−/− macrophages was especially high, likely secondary to increased viral replication and IRF-3-dependent gene induction.

TKO mDC respond to IFN-β treatment but not to PRR stimulation

Since TKO mDC failed to induce expression of selected ISGs in response to WNV-NY infection, we tested their capacity to express ISGs in response to other inflammatory stimuli including IFN-β and the PRR agonists poly(I∶C) and lipopolysaccharide (LPS) (Figure 4). Although TKO mDC failed to induce Ifnb expression after WNV-NY infection, they retained the ability to respond to its signaling, inducing WT levels of Ifnb, Oas1a, Rsad2, and Cxcl10 at 24 hours after IFN-β treatment. However, these cells showed an ablated response to poly(I∶C) or LPS, with no induction of Ifnb or the tested ISGs. Thus, TKO mDC are defective in transmitting MyD88- and TRIF-dependent signals after PAMP sensing, whereas the JAK/STAT-ISGF3 signaling pathway remains intact. As observed previously, although DKO mDC induced a WT-like pattern of ISGs after WNV infection, they had a diminished response to stimulation by the TLR4 ligand LPS or by poly(I∶C), which is recognized by TLR3 and MDA5 [22]. This suggests that WNV infection activates a broader range of PRRs than poly(I∶C) or LPS treatment alone.

Figure 4
ISG induction by IFN-β and TLR agonists in WT and deficient mDC.

Microarray analysis reveals a MAVS-dependent signal through IRF-5 in mDCs

Analysis of selected ISGs in TKO mDC infected with WNV-NY suggested a profound loss of gene induction, results that also were seen previously in Mavs−/− cells [27]. To evaluate this in greater detail, we performed a microarray analysis to profile gene expression patterns in TKO and Mavs−/− mDC 24 hours after WNV-NY infection at a multiplicity of infection (MOI) of 25. To identify the specific contributions of IRF-5 and type I IFN signaling to the transcriptional response, studies also were performed with WT, DKO, and Ifnar/− mDCs. The level of WNV infection of the cells used for the microarray was assessed by flow cytometry using an anti-WNV monoclonal antibody (Figure 5A). TKO and Mavs−/− mDC had significantly higher rates of infection compared to WT cells (P<0.05 and P<0.01, respectively), whereas infection of DKO and Ifnar−/− mDC surprisingly was not different than WT (P>0.05). Nonetheless, for all genotypes tested, only a fraction (up to 15%) of cells stained positive for WNV antigen at 24 hours after infection, suggesting that uninfected cells contributed substantially to the gene induction profile observed in this experiment.

Figure 5
Microarray analysis of WNV infected mDC.

Gene induction was measured by comparing WNV-infected samples to mock-infected cells of the same genotype, to control for differential basal expression of some genes. We considered genes to be expressed differentially in response to WNV infection if they exhibited a fold change of ≥1.5 and a P-value<0.05. WNV-infected WT mDCs showed a broad transcriptional response, particularly of genes that are induced by PRR and type I IFN signaling. 445 genes were expressed differentially in WNV-infected mDC compared to mock-infected cells (Table S1). The 50 most upregulated genes (Figure 5B) included ISGs with previously described antiviral activity (Rsad2, Ifit2, Ifit3, Isg15, Isg20, and Parp12) [13], [41][43], members of the 2′-5′-oligoadenylate synthetase family (Oas1g, Oas2, Oasl1, and Oasl2) [12], [44], [45], components of the PRR/type I IFN (Ddx58, Dhx58, Ifnb1, Ifna2, Irf7, Stat1, and Stat2) and ISG15 (Isg15, Ube2l6, Usp8) [12] pathways, as well as nucleotide metabolism factors (Cmpk2 and Nt5c3). The particular genes upregulated in DKO mDC were similar to those in WT cells, although the magnitude of induction was lower in DKO cells, consistent with previous observations [22]. In contrast, a restricted set of 22 genes was expressed differentially in WNV-infected Ifnar/− mDCs (Figure 5B and Table S2). Remarkably few genes were expressed differentially in either TKO or Mavs/− mDC upon WNV-NY infection, suggesting that the RLR signaling pathway is critical for initiating the type I IFN and antiviral responses in this cell type.

To validate the results of the microarray analysis, we performed qRT-PCR with the same RNA samples that were used for transcriptional profiling (Figure 5C) and measured the expression of Cxcl10, Rsad2, Ifit2, Ifnb, Ddx58, Ccl5, Ifitm3, and Ccl2. The induction pattern measured by qRT-PCR corroborated the microarray results. These eight genes (listed above in order of relative expression level) were induced in WT and DKO cells but not in TKO or Mavs−/− cells. Consistent with the patterns observed by microarray, Cxcl10, Rsad2, Ifit2, Ifnb, and Ccl5 were induced in Ifnar−/− cells (i.e., are IFN-independent), whereas Ddx58, Ifitm3, and Ccl2 were not (i.e., are IFN-dependent). Ifit1 (ISG56) is an ISG that is highly upregulated upon WNV infection [17], [21], [27], [46][49], thus its absence from the infection-induced bioset was unexpected. Upon further analysis by qRT-PCR, we found that Ifit1 was induced to high levels in infected WT, DKO, and Ifnar−/− mDC but not TKO or Mavs−/− cells. This quality control assessment reveals that the single Ifit1 probe on our microarray chip was defective, and that Ifit1 expression is induced in Ifnar/− cells after WNV infection.

To identify genes whose expression was dependent strictly upon IRF-5 and MAVS, we considered those upregulated in WT but not in Mavs−/− cells (MAVS-dependent) or in WT and DKO but not in TKO cells (IRF-5 dependent). Since TKO and Mavs−/− mDC failed to produce IFN-β in response to WNV infection (Figure 3 and [27]), we stratified our analysis to consider only genes that were upregulated in Ifnar−/− mDC, so as to exclude those whose differential expression might be secondary to the lack of IFN signaling in Mavs−/− and TKO cells. The IFN-independent set of genes (Figure 6A and Table S2 and S3) included Ifnb1, Rsad2, Isg15, Cxcl10, Ifit2, and Ifit3, all of which are induced by IRF-3 without a requirement for IFNAR-mediated signaling [14], [15]. Further analysis revealed that IFN-independent genes included cytokines (Ifnb1, Tnf, Il6), chemokines (Cxcl10, Ccl5, Ccrl2), antiviral restriction factors (Rsad2, Isg15, Ifit2, Ifit3), and components of the unfolded protein response (Ppp1r15a (GADD34), Ddit3 (CHOP, GADD153), Chac1). To corroborate this analysis, we measured the expression of Trib3, Ddit3, Ppp1r15a, Rgs1, Nfkbiz, and Chac1 by qRT-PCR using the same RNA samples used for the microarray (Figure 6B). We confirmed that three of these genes were upregulated in WNV-infected TKO mDC (Trib3, Ddit3, and Gadd45a) (Figure 6C). The qRT-PCR data did however, yield some differences: (a) Trib3 induction was not detected in Mavs−/− mDC by qRT-PCR; (b) Ddit3 was upregulated in a MAVS-independent manner; (c) Rgs1 and Nfkbiz were not upregulated in TKO cells; (d) while Ppp1r15a was upregulated in Ifnar−/− mDC, it also was induced in DKO mDC; and (e) by qRT-PCR we failed to detect expression of Chac1 in mock- or WNV-infected mDC of any genotype, although it was induced in WNV-infected cortical neurons (data not shown).

Figure 6
Type I IFN signaling mediates gene induction by IRF-5 and MAVS.

The absence of gene induction in TKO mDC compared to DKO cells could reflect a direct role for IRF-5 in ISG induction or an indirect effect of the loss of IFN-β production in TKO mDC. To test this, we inhibited type I IFN signaling in DKO cells using an IFNAR-blocking monoclonal antibody (MAR1-5A3, [50]) and used qRT-PCR to measure gene induction in response to WNV-NY infection (Figure 6D). As expected, the IFNAR-blocking antibody prevented induction of Oas1a, a known IFN-dependent ISG [15], but did not impair induction of Ifnb. Ccl5 and Tnf were induced too weakly to observe differences between the IFNAR-blocking and control MAbs. However, the IFNAR-blocking antibody abolished induction of Cxcl10, Rsad2, Ifit1, and Ifit2, even though these genes are considered to be IFN-independent [14], [15] and were induced in Ifnar−/− mDC (Figure 5C). Collectively, these results suggest that IRF-5 contributes to the induction of IFN-β expression after WNV infection in mDC, but does not induce ISG expression directly. To further define the contribution of IRF-5 to IFN and ISG induction in mDC, we infected WT, Irf5−/−, and DKO mDC with WNV (Figure 6E) and WT, Irf5−/−, DKO, and TKO cells with Sendai virus (SeV), a negative sense RNA paramyxovirus (Figure 6F) and measured gene expression by qRT-PCR. We found no change in the induction of Ifnb, Oas1a, Rsad2, or Cxcl10 in Irf5−/− mDC compared to WT cells (P>0.05), indicating that loss of IRF-5 alone in mDCs is not sufficient to impact the antiviral response, analogous to results seen with IRF-3 [21]. Consistent with this observation, we observed no significant difference in WNV-NY replication between Irf5−/− and WT mDC (P>0.05) (Figure 6G). Although DKO mDC retained intact IFN and ISG responses after WNV infection, this pattern surprisingly was not observed following SeV infection: the induced expression of several ISGs (Oas1a, Rsad2, and Cxcl10) was lost in both DKO and TKO mDC. While our results with DKO and TKO cells after WNV infection establish that IRF-5 contributes to the type I IFN response in mDCs, the critical nature of the IFN induction pathways in these key sentinel cells may have resulted in the maintenance of redundant signaling pathways to sustain antiviral gene programs. Indeed, the distinct ISG induction phenotypes after WNV and SeV infection in DKO and TKO mDCs suggest that activation of these parallel pathways may differ among diverse viruses.

The similar gene induction profiles observed between TKO and Mavs−/− mDC by microarray and qRT-PCR suggested a functional interaction between IRF-5 and MAVS. To test this hypothesis, we transfected WT, DKO, and TKO immortalized mouse embryonic fibroblasts (MEFs) with plasmids encoding myc-tagged forms of a constitutively active RIG-I (N-RIG) and/or IRF-5. Ectopic expression of N-RIG and IRF-5 was detected in MEFs 24 hours after transfection by western blotting (Figure 7A) and qRT-PCR (data not shown). As expected, we observed increased expression of ISGs (e.g., Rsad2, Ifit1, and Oas1a) in WT MEFs transfected with N-RIG compared to untransfected cells (Figure 7B–D). Transfection of N-RIG alone in DKO cells failed to induce these ISGs, suggesting that endogenous IRF-5 in MEFs is not adequately expressed or activated to induce ISGs after a MAVS-dependent signal; these results agree with prior studies showing that the combined loss of IRF-3 and IRF-7 in MEFs abolished the ISG response after WNV infection [22], [27]. In comparison, co-transfection of N-RIG and IRF-5 together but not IRF-5 alone enhanced ISG induction in DKO and TKO MEFs. Thus, MAVS-dependent induction of ISGs can occur through an IRF-5-dependent yet IRF-3 and IRF-7-independent pathway.

Figure 7
WT, Irf3−/−×Irf7−/− DKO, and Irf3−/−×Irf5−/−×Irf7−/− TKO immortalized MEFs were transfected with plasmids expressing myc-tagged IRF-5 or residues 1–229 ...


In the present study, we generated Irf3−/−×Irf5−/−×Irf7−/− TKO mice to establish that these three IRF family transcription factors coordinately regulate IFN-β production and ISG expression in mDC. We found that antiviral gene induction was ablated almost entirely in mDC from TKO or Mavs−/− mice, suggesting a dominant role for MAVS in initiating the antiviral response and pointing to a novel signaling interaction between IRF-5 and the RLR signaling pathway.

As TKO mice succumbed to WNV infection with similar kinetics compared to Ifnar−/− mice, we expected they would be completely defective at producing type I IFN. Nonetheless, we detected type I IFN activity in the serum of infected TKO mice, suggesting that some cells must produce type I IFN by a pathway that is independent of IRF-3, IRF-5, and IRF-7. Macrophages or related cells (e.g., inflammatory monocytes) may be one source of this residual type I IFN in vivo, as TKO macrophages cultured ex vivo expressed Ifnb as well as a subset of ISGs in response to WNV infection. Type I IFN induction in TKO macrophages could be mediated in part by IRF-1, which regulates expression of antiviral genes independently of type I IFN in the context of several other viral infections [13], [51], [52]. Consistent with this, Irf1−/− macrophages supported enhanced WNV replication compared to WT controls [40], and viral replication in TKO macrophages did not phenocopy Ifnar/− cells. Nonetheless, IRF-1 was not sufficient to induce the full complement of ISGs in macrophages, as Ifnb and ISG expression in TKO macrophages was diminished and delayed compared to WT cells. Furthermore, IFIT3 was not expressed in TKO macrophages, although it was sustained in DKO cells [22]. It remains unclear whether the genes upregulated in TKO macrophages were induced by IRF-1 directly, by another transcription factor, or downstream of IFN-β production by these cells.

We measured ISG induction in infected mDC to determine whether a lack of antiviral effector gene expression explained the failure of TKO mice and mDC to control WNV replication. In our experiments, fewer than 15% of mDC were infected at 24 hours, even when a high MOI of 25 was used. Increasing the MOI to 100 achieved only marginally higher rates of infection (data not shown) and was not practical for the scale of the microarray experiments. Sorting infected cells by flow cytometry prior to transcriptional profiling analysis was not feasible as infected cells must be permeabilized to detect intracellular WNV antigens and recombinant WNV expressing green fluorescent protein are attenuated and/or unstable [53][55]. In our microarray studies, uninfected cells likely contributed substantially to the ISG expression signatures observed. Indeed, few genes were induced in WNV-infected TKO or Mavs−/− mDC, even though these cells would be expected to upregulate genes associated with cell stress, survival, and metabolism in response to replication by a cytopathic virus. Some components of the unfolded protein response, including Ddit3 and Gadd45a, were upregulated in infected TKO mDC; additional genes likely were induced in infected cells but may have been below the statistical cutoffs used in our analysis due to dilution of the transcripts in a large pool of mRNA from uninfected cells.

Viral infection induces the expression of ISGs both directly (by IRF-3 after PAMP detection and PRR signaling) and indirectly (by IFN-β production and IFNAR signaling), the latter occurring in both infected and uninfected cells. Given the large proportion of uninfected cells, we would expect genes induced by IFNAR signaling to predominate. Indeed, only a small subset of genes was induced after WNV infection of Ifnar−/− mDC (22 genes, compared to 445 in WT mDC). This may reflect the relatively low infection rates, an inherent inefficiency of IFNAR-independent gene induction pathways, or viral countermeasures that antagonize the type I IFN response in highly infected cells [56]. Of the 22 genes induced in WNV-infected Ifnar−/− mDC, several (Ifnb, Cxcl10, Rsad2, Ifit1, and Ifit2) have direct or indirect antiviral activity against WNV [13], [24], [41], [42], [57][59] and are induced directly by IRF-3 [14], [15]. Other genes induced in WNV-infected Ifnar−/− mDC included components of the unfolded protein response, such as Ddit3 and Ppp1r15a. Ddit3 (CHOP) has been shown to promote expression of Ppp1r15a (Gadd34) and Trib3 [60][62], two IFN-independent induced genes detected in our microarray analysis. While induction of these genes may represent a response to the cellular stress caused by viral infection, the unfolded protein response also constitutes a cellular defense that limits replication of diverse viruses, including WNV [60], [63], [64]. DDIT3 inhibits WNV replication, and WNV may induce expression of Ppp1r15a to reverse DDIT3-mediated translational inhibition [60]. In contrast, PPP1R15A is required for IFN-β production and contributes to controlling replication of chikungunya virus [65].

Although global gene induction in response to WNV infection has been reported previously [46][49], [66], [67], our results represent the first such analysis in DCs, which are a sentinel cell type coordinating the innate and adaptive antiviral immune responses, as well as among the first cells infected following a mosquito bite [8], [68]. Some of the genes we identified in mDCs also were detected in microarray analyses of WNV-infected MEFs [46], human kidney epithelial cells [48], or human retinal pigmented epithelium [47]. Induction of these genes (e.g., Rsad2, Ifit2, Isg15, Isg20, and Stat1) thus does not depend on cell type-specific transcription factors. Other WNV-induced genes, however, may be specific to DCs or restricted cell types. As an example, the chemokine Cxcl10 was one of the most highly induced genes in our analysis, yet it was induced at much lower levels or not at all in fibroblasts and epithelial cells [46][48]. CXCL10 contributes to clearance of WNV infection from the CNS by recruiting effector T cells, and is the dominant chemokine secreted by neurons after WNV infection [57].

Only one of the 22 genes differentially expressed in Ifnar−/− mDC, Ddit3, was induced in Mavs−/− mDC, suggesting that the IFN-independent induction signal is conveyed almost entirely by MAVS. Since Mavs−/− mDC failed to produce IFN-β, we surmise that both type I IFN-dependent and -independent pathways of ISG induction are abrogated in these cells. This conclusion agrees with earlier studies on induction of selected sets of genes in Mavs−/− mDC infected with WNV or rabies virus [27], [69]. Although Mavs−/− cells should retain TLR-mediated antiviral gene induction pathways (which signal through TRIF and MyD88), we observed almost no ISG induction in Mavs−/− mDC after WNV infection. Thus, RLRs likely are the dominant PRRs that sense WNV infection in mDC; these results are consistent with the essentially intact antiviral responses reported in WNV-infected Tlr3−/− and Myd88−/− mDC [26], [28].

Although our microarray and qRT-PCR analyses identified 16 genes that were differentially expressed in WNV-infected Ifnar−/− and DKO but not TKO mDC, when gene expression was analyzed from WNV-infected DKO cells that were treated with an antibody blocking type I IFN signaling, only Ifnb gene induction was sustained. These data suggest that in the absence of IRF-3 and IRF-7, IRF-5 is sufficient to induce IFN-β production in response to WNV infection, but unlike IRF-3 [14], [15], does not induce ISGs directly (Figure 8). Although IRF-5 has been suggested to promote IFN-independent expression of some ISGs including Pkr and Isg20 in NDV-infected cells [38], IRF-3 may have contributed to these responses. The observed anti-WNV response in DKO mDC likely results from IRF-5-dependent IFN-β production, and the uncontrolled viral replication in TKO mDC is secondary to a lack of IFN-β and resultant absence of ISG induction. This model suggests that cell types having ancillary pathways for IFN-β induction (such as IRF-1 in macrophages) can mount antiviral responses even in the absence of IRF-3, IRF-5, and IRF-7.

Figure 8
Model of Type I IFN and ISG induction in mDC.

We did not anticipate that the Mavs/− and TKO mDC would phenocopy one other with respect to ISG induction, since IRF-5 has not been previously implicated in the RLR signaling pathway [35][37]. IRF-5 originally was described as an inducer of pro-inflammatory cytokines (e.g., IL-6 and TNF-α) but subsequently was suggested to contribute to the type I IFN antiviral response. Irf5−/− mice have increased susceptibility to viral infections, slightly reduced levels of type I IFN in serum, and more significantly reduced levels of pro-inflammatory cytokines [35], [37]. IRF-5 expression and antiviral activity, however, appears restricted to a limited set of cell types, including monocytes and DCs [35], [39], [70]. Thus, a relative absence of IRF-5 expression in fibroblasts and neurons may explain the observation that type I IFN induction after WNV infection in these cell types is abolished by the combined deletion of IRF-3 and IRF-7 [22]. However, the ability of alternate IRFs to compensate for IRF-3 and IRF-7 in fibroblasts also may depend on the particular viral stimulus, as type I IFN production was essentially absent in DKO fibroblasts infected with WNV, herpes simplex virus, vesicular stomatitis virus, or encephalomyocarditis virus [19], [22], but low-level production of Ifnb and Ifna2 mRNA was sustained in DKO fibroblasts infected with chikungunya virus [33]. IRF-5 preferentially stimulates the IFN-β and IFN-α4 promoters, rather than other IFN-α subtypes, which also suggests that it contributes to the primary type I IFN response, prior to amplification via autocrine and paracrine signaling [35]. The IFN-α subtypes induced in IRF-5-expressing cells vary from those induced in IRF-7-expressing cells, suggesting that the IRF expression patterns within a cell modulate the breadth of the type I IFN response [70].

Although MAVS previously was known to induce IFN-β production via IRF-3 and IRF-7, our experiments suggest that RLR signaling also activates IRF-5 to induce IFN-β production in mDC; the subcellular location where this occurs (e.g., mitochondrion) and through what signaling intermediates remains unknown. A recent study suggested that activation of RLR signaling acts to inhibit induction of inflammatory cytokines by IRF-5 [71]; although the net result was different, this study is consistent with our observation of a functional interaction between IRF-5 and MAVS and with a prior proteomic study demonstrating a physical interaction between these two proteins [72]. Future studies will be required to delineate the mechanistic and functional intermediates that link and regulate the IRF-5 and RLR signaling pathways.

Materials and Methods


The WNV-NY strain (3000.0259) was isolated in New York in 2000 and passaged once in C6/36 Aedes albopictus cells to generate a virus stock that was used in all experiments except for the microarray analysis [73], [74]. For the microarray studies, mDCs were infected in the Früh laboratory with the WNV New York 1999 strain that was propagated in C6/36 cells [75]. The attenuated strain WNV-MAD was amplified in Vero cells and has been previously described [23]. MNV strain MNV1.CW3 [76] was propagated in RAW 264.7 cells (ATCC) and a concentrated stock was prepared as previously described [77]. The SeV virus strain Fushimi was propagated in chicken embryos and provided by D. Lenschow and M. Holtzman (Washington University, St Louis, MO).

Ethics statement

This study was carried out in strict accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health. The protocol was approved by the Institutional Animal Care and Use Committee at the Washington University School of Medicine (Assurance Number: A3381-01). Dissections and footpad injections were performed under anesthesia that was induced and maintained with ketamine hydrochloride and xylazine, and all efforts were made to minimize suffering.

Mouse experiments

All mice used were on an inbred C57BL/6 background. WT mice were commercially obtained (Jackson Laboratories). Irf3−/−×Irf7−/− DKO, Irf5−/−, and Ifnar−/− mice have been reported previously [22], [31], [36]. Irf3−/−×Irf5−/−×Irf7−/− TKO mice were generated by crossing DKO and Irf5−/− mice. Irf5−/− and TKO mice were genotyped for a mutation in the Dock2 gene, which can arise spontaneously in some Irf5/− mice [78]; none of the TKO mice had homozygous mutations in Dock2. Mavs−/− mice were generated directly from C57BL/6 embryonic stem cells [34]. All deficient mice were bred in the animal facilities of the Washington University School of Medicine and genotyped prior to experimentation. For WNV infections, 102 PFU was diluted in Hank's Balanced Salt Solution supplemented with 1% heat-inactivated fetal bovine serum and 8 to 12 week-old mice were inoculated by footpad injection in a volume of 50 µl. For MNV infections, 7 to 8 week-old mice were inoculated orally with 3×107 PFU in 25 µl of PBS and monitored for survival for 21 days.

Measurement of viral burden

To monitor viral spread in vivo, mice were infected with 102 PFU of virus and sacrificed at 2 days after infection (WNV-NY) or 6 days after infection (WNV-MAD). After extensive perfusion with PBS, organs were harvested, weighed, homogenized and virus was titered by plaque assay on BHK21-15 cells [74]. Viral burden in serum and inguinal lymph node was measured using fluorogenic qRT-PCR using primers and probes to WNV-NY or WNV-MAD envelope gene sequences (Table S4). Viral RNA in the lymph node was normalized to Gapdh levels in tissue samples. Viral RNA from serum was isolated using a Viral RNA Mini Kit (Qiagen). Total RNA from lymph nodes was extracted using the E.Z.N.A. total RNA kit (Omega Bio-tek) and DNase-treated to remove genomic DNA. Quantitative RT-PCR was performed using One-Step RT-PCR Master Mix and a 7500 Fast Real-Time PCR System (Applied Biosystems).

Quantification of type I IFN activity

Levels of biologically active type I IFN in serum were determined using an encephalomyocarditis virus L929 cytopathic effect bioassay as described [79]. The amount of type I IFN per ml of serum was calculated from a standard curve using IFN-β (PBL InterferonSource) and adjusted for the background inhibitory activity of naïve serum (approximately 0.1 IU/ml). The inhibitory activity of naïve serum was type I IFN-independent because it was acid labile but resistant to treatment with heat (56°C) or the IFNAR-blocking antibody MAR1-5A3 [17], [50].

Primary cell infections

Macrophage and mDC cultures were generated as described previously [79]. Briefly, bone marrow was isolated from WT, DKO, TKO, Irf5−/−, or Ifnar−/− mice and cultured for seven days in the presence of 40 ng/ml M-CSF (PeproTech) to generate macrophages or with 20 ng/ml GM-CSF and 20 ng/ml IL-4 (PeproTech) to produce mDC. Multi-step virus growth analysis was performed after infection at a MOI of 0.01 for macrophages or 0.001 for mDCs. Supernatants were titered by focus-forming assay on Vero cells using humanized E16 anti-WNV MAb as the detection antibody [80], horseradish peroxidase conjugated anti-human IgG (Sigma), and True Blue Peroxidase Substrate (KPL). For western blotting, cells were infected at an MOI of 1. For measurement of ISG induction by qRT-PCR, cells were infected at an MOI of 0.1. To block signaling by type I IFN, DKO cells were treated with 25 µg/ml of the IFNAR-blocking MAb MAR1-5A3 for one hour prior to infection. A non-binding MAb against human IFN-γ receptor (GiR-208) was used as an isotype control [50].

Microarray analysis of mDCs

Bone marrow cells were cultured in RPMI supplemented with 10% fetal bovine serum, penicillin/streptomycin, L-glutamine, non-essential amino acids, 55 µM β-mercaptoethanol and 20 ng/ml recombinant mouse GM-CSF (eBioscience) for six days in non-tissue culture treated plates. GM-CSF was replenished after two days and non-adherent cells were sub-cultured after 4 days. Sub-cultured cells were infected at an MOI of 25 with WNV-NY. Total RNA was harvested at 0, 6, 12, and 24 hours post-infection with an RNeasy Mini Kit (Qiagen). RNA was treated with DNase prior to cDNA generation. Gene expression was assayed on Illumina microarray chips. Microarray datasets were processed by quantile normalization and annotated using the illuminaMousev2.db R package version 1.10.0. Data were assessed by linear modeling with the limma package [81]. Differentially expressed genes were identified as those with at least a 1.5-fold change as compared to controls and a P-value<0.05 without correction for false discovery. WNV-infected samples were first compared with mock-infected controls. Microarray data have been deposited in GeoArchive, series number GSE42232.

Transfection and ectopic expression

MEFs prepared from WT, DKO, or TKO mice were immortalized after transfection with the plasmid pSV2, which encodes for the large T antigen of SV40. MEFs were transfected using Lipofectamine 2000 (Invitrogen) with plasmids expressing myc-tagged forms of murine IRF-5 (Origene) or residues 1–229 of human RIG-I (N-RIG) [82]. Cells were lysed 24 hours post-transfection and analyzed by qRT-PCR and western blotting.

Western blotting

Macrophages and mDC were lysed in RIPA buffer (10 mM Tris, 150 mM NaCl, 0.02% sodium azide, 1% sodium deoxycholate, 1% Triton X-100, 0.1% SDS, pH 7.4), with protease inhibitors (Sigma). Samples (20 µg) were resolved by electrophoresis on 10% SDS-polyacrylamide gels. MEFs were lysed in RIPA buffer and lysates were separated by electrophoresis on 4–12% SDS-polyacrylamide gels. Following transfer of proteins, membranes were blocked with 5% non-fat dried milk and probed with the following panel of primary antibodies: rabbit anti-IFIT2 and -IFIT3 (provided by Dr. G. Sen, [83]); rabbit anti-RIG-I and anti-MDA5 (IBL); mouse anti-tubulin (Sigma); rabbit anti-GAPDH (Santa Cruz); rabbit anti-STAT1 (Cell Signaling); goat-anti WNV NS3 (R&D Systems); mouse anti-myc (Santa Cruz). Western blots were incubated with peroxidase-conjugated secondary antibodies (Jackson Immunoresearch and Sigma) and visualized using ECL reagents (Amersham Biosciences and Pierce).

Measurement of ISG expression by qRT-PCR

mDCs were treated for 24 hours with 500 IU/ml of IFN-β (PBL Interferon Source), 50 µg/ml of poly(I∶C) (InvivoGen), or 5 µg/ml of LPS (List Biological Laboratories). Macrophages and mDC were infected with WNV-NY at an MOI 0.1 for 24 hours. MEFs were harvested 24 hours after transfection. Total RNA was extracted using the E.Z.N.A. total RNA kit (Omega Bio-tek) or RNeasy kit (Qiagen) and treated with DNase. Fluorogenic qRT-PCR was performed using One-Step RT-PCR Master Mix and a 7500 Fast Real-Time PCR System (Applied Biosystems) with the indicated Taqman primers and probes (Table S4). Gene induction was normalized to Gapdh levels and expressed on a log2 scale as fold increase over mock according to the ΔΔCt method [84].

Statistical analysis

Data were analyzed with GraphPad Prism software. Viral burdens were compared using the Mann-Whitney test. Serum type I IFN levels, viral growth curves and qRT-PCR were compared using a 2-way ANOVA. Kaplan-Meier survival curves were analyzed by the log rank test and mean times to death were compared by Student's T-test.

Supporting Information

Figure S1

Genotyping of TKO mice. DNA from the tails of the indicated mice was amplified by PCR using primers specific for IRF-3, IRF-5, or IRF-7 and separated by agarose gel electrophoresis. The band sizes confirmed the genotypes of the knockout mice.


Table S1

Gene induction in WNV-NY infected mDC. All genes (445) for which expression level in at least one genotype was ≥1.5-fold changed at 24 hours after WNV infection (P<0.05, without correction for false discovery). Values represent the mean of three independent samples for each genotype. “Fold change” refers to the relative fold change of expression in WNV-infected mDC compared with mock-infected controls of the same genotype. DKO: Irf3−/−×Irf7−/−; TKO: Irf3−/−×Irf 5−/−×Irf7−/−.


Table S2

IFN-independent gene induction. Genes are shown for which expression level in Ifnar−/− mDC was ≥1.5-fold changed at 24 hours after WNV infection (P<0.05, without correction for false discovery). Values represent the mean of three independent samples for each genotype. “Fold change” refers to the relative fold change of expression in WNV-infected mDC compared with mock-infected controls of the same genotype. DKO: Irf3−/−×Irf7−/−; TKO: Irf3−/−×Irf 5−/−×Irf7−/−.


Table S3

Genes induced in IFNAR and DKO, but not TKO mDC. Genes are shown for which expression level in Ifnar−/− and DKO mDC was ≥1.5-fold changed at 24 hours after WNV infection (P<0.05), but which fell short of these cutoffs in TKO cells. Values represent the mean of three independent samples for each genotype. “Fold change” refers to the relative fold change of expression in WNV-infected mDC compared with mock-infected controls of the same genotype. DKO: Irf3−/−×Irf7−/−; TKO: Irf3−/−×Irf 5−/−×Irf7−/−.


Table S4

Primers and probes used for quantitative RT-PCR.



The authors thank M. Noll for help generating and screening the TKO mice, and H. Ramos, G. Blahnik, and E. Duan for assistance with some of the experiments. Transcriptional profiling and some of the bioinformatics analysis was performed by the Collaborative Genomics Center (CGC) at VGTI-Florida.

Funding Statement

The authors would like to acknowledge the National Institutes of Health for support of work in their laboratories: U54 AI081680 and U54 AI057160, Pacific Northwest Regional Center of Excellence for Biodefense and Emerging Infectious Diseases Research (MSD and MG); U19 AI083019 and R01 AI074973 (MSD and MG); NO1 AI50027 (JNZ and KF). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Welsh RM, Bahl K, Marshall HD, Urban SL (2012) Type 1 interferons and antiviral CD8 T-cell responses. PLoS Pathog 8: e1002352. [PMC free article] [PubMed]
2. Paun A, Pitha PM (2007) The innate antiviral response: new insights into a continuing story. Adv Virus Res 69: 1–66 [PubMed]
3. Wang BX, Fish EN (2012) The yin and yang of viruses and interferons. Trends Immunol 33: 190–197 [PubMed]
4. Le Bon A, Tough DF (2002) Links between innate and adaptive immunity via type I interferon. Curr Opin Immunol 14: 432–436 [PubMed]
5. Jensen S, Thomsen AR (2012) Sensing of RNA viruses: a review of innate immune receptors involved in recognizing RNA virus invasion. J Virol 86: 2900–2910 [PMC free article] [PubMed]
6. Ramos HJ, Gale M Jr (2011) RIG-I Like Receptors and Their Signaling Crosstalk in the Regulation of Antiviral Immunity. Curr Opin Virol 1: 167–176 [PMC free article] [PubMed]
7. Wilkins C, Gale M Jr (2010) Recognition of viruses by cytoplasmic sensors. Curr Opin Immunol 22: 41–47 [PMC free article] [PubMed]
8. Diamond MS, Gale M Jr (2012) Cell-intrinsic innate immune control of West Nile virus infection. Trends Immunol 33: 522–530 [PMC free article] [PubMed]
9. Honda K, Takaoka A, Taniguchi T (2006) Type I interferon gene induction by the interferon regulatory factor family of transcription factors. Immunity 25: 349–360 [PubMed]
10. Paun A, Pitha PM (2007) The IRF family, revisited. Biochimie 89: 744–753 [PMC free article] [PubMed]
11. Platanias LC (2005) Mechanisms of type-I- and type-II-interferon-mediated signalling. Nat Rev Immunol 5: 375–386 [PubMed]
12. Sadler AJ, Williams BR (2008) Interferon-inducible antiviral effectors. Nat Rev Immunol 8: 559–568 [PMC free article] [PubMed]
13. Schoggins JW, Wilson SJ, Panis M, Murphy MY, Jones CT, et al. (2011) A diverse range of gene products are effectors of the type I interferon antiviral response. Nature 472: 481–485 [PMC free article] [PubMed]
14. Grandvaux N, Servant MJ, tenOever B, Sen GC, Balachandran S, et al. (2002) Transcriptional profiling of interferon regulatory factor 3 target genes: direct involvement in the regulation of interferon-stimulated genes. J Virol 76: 5532–5539 [PMC free article] [PubMed]
15. Nakaya T, Sato M, Hata N, Asagiri M, Suemori H, et al. (2001) Gene induction pathways mediated by distinct IRFs during viral infection. Biochem Biophys Res Commun 283: 1150–1156 [PubMed]
16. Prakash A, Smith E, Lee CK, Levy DE (2005) Tissue-specific positive feedback requirements for production of type I interferon following virus infection. J Biol Chem 280: 18651–18657 [PMC free article] [PubMed]
17. Daffis S, Samuel MA, Suthar MS, Keller BC, Gale M Jr, et al. (2008) Interferon regulatory factor IRF-7 induces the antiviral alpha interferon response and protects against lethal West Nile virus infection. J Virol 82: 8465–8475 [PMC free article] [PubMed]
18. Izaguirre A, Barnes BJ, Amrute S, Yeow WS, Megjugorac N, et al. (2003) Comparative analysis of IRF and IFN-alpha expression in human plasmacytoid and monocyte-derived dendritic cells. J Leukoc Biol 74: 1125–1138 [PubMed]
19. Honda K, Yanai H, Negishi H, Asagiri M, Sato M, et al. (2005) IRF-7 is the master regulator of type-I interferon-dependent immune responses. Nature 434: 772–777 [PubMed]
20. Schmid S, Mordstein M, Kochs G, Garcia-Sastre A, Tenoever BR (2010) Transcription factor redundancy ensures induction of the antiviral state. J Biol Chem 285: 42013–42022 [PMC free article] [PubMed]
21. Daffis S, Samuel MA, Keller BC, Gale M Jr, Diamond MS (2007) Cell-specific IRF-3 responses protect against West Nile virus infection by interferon-dependent and -independent mechanisms. PLoS Pathog 3: e106. [PMC free article] [PubMed]
22. Daffis S, Suthar MS, Szretter KJ, Gale M Jr, Diamond MS (2009) Induction of IFN-beta and the innate antiviral response in myeloid cells occurs through an IPS-1-dependent signal that does not require IRF-3 and IRF-7. PLoS Pathog 5: e1000607. [PMC free article] [PubMed]
23. Keller BC, Fredericksen BL, Samuel MA, Mock RE, Mason PW, et al. (2006) Resistance to alpha/beta interferon is a determinant of West Nile virus replication fitness and virulence. J Virol 80: 9424–9434 [PMC free article] [PubMed]
24. Lazear HM, Pinto AK, Vogt MR, Gale M Jr, Diamond MS (2011) Beta interferon controls West Nile virus infection and pathogenesis in mice. J Virol 85: 7186–7194 [PMC free article] [PubMed]
25. Samuel MA, Diamond MS (2005) Alpha/beta interferon protects against lethal West Nile virus infection by restricting cellular tropism and enhancing neuronal survival. J Virol 79: 13350–13361 [PMC free article] [PubMed]
26. Daffis S, Samuel MA, Suthar MS, Gale M Jr, Diamond MS (2008) Toll-like receptor 3 has a protective role against West Nile virus infection. J Virol 82: 10349–10358 [PMC free article] [PubMed]
27. Suthar MS, Ma DY, Thomas S, Lund JM, Zhang N, et al. (2010) IPS-1 is essential for the control of West Nile virus infection and immunity. PLoS Pathog 6: e1000757. [PMC free article] [PubMed]
28. Szretter KJ, Daffis S, Patel J, Suthar MS, Klein RS, et al. (2010) The innate immune adaptor molecule MyD88 restricts West Nile virus replication and spread in neurons of the central nervous system. J Virol 84: 12125–12138 [PMC free article] [PubMed]
29. Wang T, Town T, Alexopoulou L, Anderson JF, Fikrig E, et al. (2004) Toll-like receptor 3 mediates West Nile virus entry into the brain causing lethal encephalitis. Nat Med 10: 1366–1373 [PubMed]
30. Town T, Bai F, Wang T, Kaplan AT, Qian F, et al. (2009) Toll-like receptor 7 mitigates lethal West Nile encephalitis via interleukin 23-dependent immune cell infiltration and homing. Immunity 30: 242–253 [PMC free article] [PubMed]
31. Daffis S, Lazear HM, Liu WJ, Audsley M, Engle M, et al. (2011) The naturally attenuated Kunjin strain of West Nile virus shows enhanced sensitivity to the host type I interferon response. J Virol 85: 5664–5668 [PMC free article] [PubMed]
32. Steinberg C, Eisenacher K, Gross O, Reindl W, Schmitz F, et al. (2009) The IFN regulatory factor 7-dependent type I IFN response is not essential for early resistance against murine cytomegalovirus infection. Eur J Immunol 39: 1007–1018 [PubMed]
33. Schilte C, Buckwalter MR, Laird ME, Diamond MS, Schwartz O, et al. (2012) Cutting edge: independent roles for IRF-3 and IRF-7 in hematopoietic and nonhematopoietic cells during host response to Chikungunya infection. J Immunol 188: 2967–2971 [PubMed]
34. Rudd PA, Wilson J, Gardner J, Larcher T, Babarit C, et al. (2012) Interferon response factors 3 and 7 protect against Chikungunya virus hemorrhagic fever and shock. J Virol 86: 9888–9898 [PMC free article] [PubMed]
35. Paun A, Reinert JT, Jiang Z, Medin C, Balkhi MY, et al. (2008) Functional characterization of murine interferon regulatory factor 5 (IRF-5) and its role in the innate antiviral response. J Biol Chem 283: 14295–14308 [PMC free article] [PubMed]
36. Takaoka A, Yanai H, Kondo S, Duncan G, Negishi H, et al. (2005) Integral role of IRF-5 in the gene induction programme activated by Toll-like receptors. Nature 434: 243–249 [PubMed]
37. Yanai H, Chen HM, Inuzuka T, Kondo S, Mak TW, et al. (2007) Role of IFN regulatory factor 5 transcription factor in antiviral immunity and tumor suppression. Proc Natl Acad Sci U S A 104: 3402–3407 [PMC free article] [PubMed]
38. Barnes BJ, Richards J, Mancl M, Hanash S, Beretta L, et al. (2004) Global and distinct targets of IRF-5 and IRF-7 during innate response to viral infection. J Biol Chem 279: 45194–45207 [PubMed]
39. Schoenemeyer A, Barnes BJ, Mancl ME, Latz E, Goutagny N, et al. (2005) The interferon regulatory factor, IRF5, is a central mediator of toll-like receptor 7 signaling. J Biol Chem 280: 17005–17012 [PubMed]
40. Brien JD, Daffis S, Lazear HM, Cho H, Suthar MS, et al. (2011) Interferon regulatory factor-1 (IRF-1) shapes both innate and CD8(+) T cell immune responses against West Nile virus infection. PLoS Pathog 7: e1002230. [PMC free article] [PubMed]
41. Jiang D, Weidner JM, Qing M, Pan XB, Guo H, et al. (2010) Identification of five interferon-induced cellular proteins that inhibit west nile virus and dengue virus infections. J Virol 84: 8332–8341 [PMC free article] [PubMed]
42. Szretter KJ, Brien JD, Thackray LB, Virgin HW, Cresswell P, et al. (2011) The interferon-inducible gene viperin restricts West Nile virus pathogenesis. J Virol 85: 11557–11566 [PMC free article] [PubMed]
43. Atasheva S, Akhrymuk M, Frolova EI, Frolov I (2012) New PARP Gene with an Anti-Alphavirus Function. J Virol 86: 8147–8160 [PMC free article] [PubMed]
44. Eskildsen S, Hartmann R, Kjeldgaard NO, Justesen J (2002) Gene structure of the murine 2′-5′-oligoadenylate synthetase family. Cell Mol Life Sci 59: 1212–1222 [PubMed]
45. Eskildsen S, Justesen J, Schierup MH, Hartmann R (2003) Characterization of the 2′-5′-oligoadenylate synthetase ubiquitin-like family. Nucleic Acids Res 31: 3166–3173 [PMC free article] [PubMed]
46. Scherbik SV, Stockman BM, Brinton MA (2007) Differential expression of interferon (IFN) regulatory factors and IFN-stimulated genes at early times after West Nile virus infection of mouse embryo fibroblasts. J Virol 81: 12005–12018 [PMC free article] [PubMed]
47. Munoz-Erazo L, Natoli R, Provis JM, Madigan MC, King NJ (2012) Microarray analysis of gene expression in West Nile virus-infected human retinal pigment epithelium. Mol Vis 18: 730–743 [PMC free article] [PubMed]
48. Fredericksen BL, Smith M, Katze MG, Shi PY, Gale M Jr (2004) The host response to West Nile Virus infection limits viral spread through the activation of the interferon regulatory factor 3 pathway. J Virol 78: 7737–7747 [PMC free article] [PubMed]
49. Koh WL, Ng ML (2005) Molecular mechanisms of West Nile virus pathogenesis in brain cell. Emerg Infect Dis 11: 629–632 [PMC free article] [PubMed]
50. Sheehan KC, Lai KS, Dunn GP, Bruce AT, Diamond MS, et al. (2006) Blocking monoclonal antibodies specific for mouse IFN-alpha/beta receptor subunit 1 (IFNAR-1) from mice immunized by in vivo hydrodynamic transfection. J Interferon Cytokine Res 26: 804–819 [PubMed]
51. Kanazawa N, Kurosaki M, Sakamoto N, Enomoto N, Itsui Y, et al. (2004) Regulation of hepatitis C virus replication by interferon regulatory factor 1. J Virol 78: 9713–9720 [PMC free article] [PubMed]
52. Pine R (1992) Constitutive expression of an ISGF2/IRF1 transgene leads to interferon-independent activation of interferon-inducible genes and resistance to virus infection. J Virol 66: 4470–4478 [PMC free article] [PubMed]
53. Julander JG, Winger QA, Rickords LF, Shi PY, Tilgner M, et al. (2006) West Nile virus infection of the placenta. Virology 347: 175–182 [PubMed]
54. McGee CE, Shustov AV, Tsetsarkin K, Frolov IV, Mason PW, et al. (2010) Infection, dissemination, and transmission of a West Nile virus green fluorescent protein infectious clone by Culex pipiens quinquefasciatus mosquitoes. Vector Borne Zoonotic Dis 10: 267–274 [PMC free article] [PubMed]
55. Pierson TC, Diamond MS, Ahmed AA, Valentine LE, Davis CW, et al. (2005) An infectious West Nile virus that expresses a GFP reporter gene. Virology 334: 28–40 [PubMed]
56. Diamond MS (2009) Mechanisms of evasion of the type I interferon antiviral response by flaviviruses. J Interferon Cytokine Res 29: 521–530 [PubMed]
57. Klein RS, Lin E, Zhang B, Luster AD, Tollett J, et al. (2005) Neuronal CXCL10 directs CD8+ T-cell recruitment and control of West Nile virus encephalitis. J Virol 79: 11457–11466 [PMC free article] [PubMed]
58. Daffis S, Szretter KJ, Schriewer J, Li J, Youn S, et al. (2010) 2′-O methylation of the viral mRNA cap evades host restriction by IFIT family members. Nature 468: 452–456 [PMC free article] [PubMed]
59. Szretter KJ, Daniels BP, Cho H, Gainey MD, Yokoyama WM, et al. (2012) 2′-O methylation of the viral mRNA cap by West Nile virus evades ifit1-dependent and -independent mechanisms of host restriction in vivo. PLoS Pathog 8: e1002698. [PMC free article] [PubMed]
60. Medigeshi GR, Lancaster AM, Hirsch AJ, Briese T, Lipkin WI, et al. (2007) West Nile virus infection activates the unfolded protein response, leading to CHOP induction and apoptosis. J Virol 81: 10849–10860 [PMC free article] [PubMed]
61. Mungrue IN, Pagnon J, Kohannim O, Gargalovic PS, Lusis AJ (2009) CHAC1/MGC4504 is a novel proapoptotic component of the unfolded protein response, downstream of the ATF4-ATF3-CHOP cascade. J Immunol 182: 466–476 [PMC free article] [PubMed]
62. Smith SM, Moran AP, Duggan SP, Ahmed SE, Mohamed AS, et al. (2011) Tribbles 3: a novel regulator of TLR2-mediated signaling in response to Helicobacter pylori lipopolysaccharide. J Immunol 186: 2462–2471 [PubMed]
63. He B (2006) Viruses, endoplasmic reticulum stress, and interferon responses. Cell Death Differ 13: 393–403 [PubMed]
64. Ambrose RL, Mackenzie JM (2011) West Nile virus differentially modulates the unfolded protein response to facilitate replication and immune evasion. J Virol 85: 2723–2732 [PMC free article] [PubMed]
65. Clavarino G, Claudio N, Couderc T, Dalet A, Judith D, et al. (2012) Induction of GADD34 Is Necessary for dsRNA-Dependent Interferon-beta Production and Participates in the Control of Chikungunya Virus Infection. PLoS Pathog 8: e1002708. [PMC free article] [PubMed]
66. Venter M, Myers TG, Wilson MA, Kindt TJ, Paweska JT, et al. (2005) Gene expression in mice infected with West Nile virus strains of different neurovirulence. Virology 342: 119–140 [PubMed]
67. Bourgeois MA, Denslow ND, Seino KS, Barber DS, Long MT (2011) Gene expression analysis in the thalamus and cerebrum of horses experimentally infected with West Nile virus. PLoS One 6: e24371. [PMC free article] [PubMed]
68. Samuel MA, Diamond MS (2006) Pathogenesis of West Nile Virus infection: a balance between virulence, innate and adaptive immunity, and viral evasion. J Virol 80: 9349–9360 [PMC free article] [PubMed]
69. Faul EJ, Wanjalla CN, Suthar MS, Gale M, Wirblich C, et al. (2010) Rabies virus infection induces type I interferon production in an IPS-1 dependent manner while dendritic cell activation relies on IFNAR signaling. PLoS Pathog 6: e1001016. [PMC free article] [PubMed]
70. Barnes BJ, Kellum MJ, Field AE, Pitha PM (2002) Multiple regulatory domains of IRF-5 control activation, cellular localization, and induction of chemokines that mediate recruitment of T lymphocytes. Mol Cell Biol 22: 5721–5740 [PMC free article] [PubMed]
71. Negishi H, Yanai H, Nakajima A, Koshiba R, Atarashi K, et al. (2012) Cross-interference of RLR and TLR signaling pathways modulates antibacterial T cell responses. Nat Immunol 13: 659–666 [PubMed]
72. Li S, Wang L, Berman M, Kong YY, Dorf ME (2011) Mapping a dynamic innate immunity protein interaction network regulating type I interferon production. Immunity 35: 426–440 [PMC free article] [PubMed]
73. Ebel GD, Dupuis AP 2nd, Ngo K, Nicholas D, Kauffman E, et al. (2001) Partial genetic characterization of West Nile virus strains, New York State, 2000. Emerg Infect Dis 7: 650–653 [PMC free article] [PubMed]
74. Diamond MS, Shrestha B, Marri A, Mahan D, Engle M (2003) B Cells and Antibody Play Critical Roles in the Immediate Defense of Disseminated Infection by West Nile Encephalitis Virus. Journal of Virology 77: 2578–2586 [PMC free article] [PubMed]
75. Xiao SY, Guzman H, Zhang H, Travassos da Rosa AP, Tesh RB (2001) West Nile virus infection in the golden hamster (Mesocricetus auratus): a model for West Nile encephalitis. Emerg Infect Dis 7: 714–721 [PMC free article] [PubMed]
76. Thackray LB, Wobus CE, Chachu KA, Liu B, Alegre ER, et al. (2007) Murine noroviruses comprising a single genogroup exhibit biological diversity despite limited sequence divergence. J Virol 81: 10460–10473 [PMC free article] [PubMed]
77. Chachu KA, Strong DW, LoBue AD, Wobus CE, Baric RS, et al. (2008) Antibody is critical for the clearance of murine norovirus infection. J Virol 82: 6610–6617 [PMC free article] [PubMed]
78. Purtha WE, Swiecki M, Colonna M, Diamond MS, Bhattacharya D (2012) Spontaneous mutation of the Dock2 gene in Irf5−/− mice complicates interpretation of type I interferon production and antibody responses. Proc Natl Acad Sci U S A 109: E898–904 [PMC free article] [PubMed]
79. Samuel MA, Whitby K, Keller BC, Marri A, Barchet W, et al. (2006) PKR and RNase L contribute to protection against lethal West Nile Virus infection by controlling early viral spread in the periphery and replication in neurons. J Virol 80: 7009–7019 [PMC free article] [PubMed]
80. Oliphant T, Engle M, Nybakken GE, Doane C, Johnson S, et al. (2005) Development of a humanized monoclonal antibody with therapeutic potential against West Nile virus. Nat Med 11: 522–530 [PMC free article] [PubMed]
81. Smyth GK (2005) Limma: linear models for microarray data. In: Gentleman R, Carey V, Dudoit R, Irizarry R, Huber W, editors. Bioinformatics and Computational Biology Solutions using R and Bioconductor. New York: Springer. pp. 397–420.
82. Saito T, Hirai R, Loo YM, Owen D, Johnson CL, et al. (2007) Regulation of innate antiviral defenses through a shared repressor domain in RIG-I and LGP2. Proc Natl Acad Sci U S A 104: 582–587 [PMC free article] [PubMed]
83. Fensterl V, White CL, Yamashita M, Sen GC (2008) Novel characteristics of the function and induction of murine p56 family proteins. J Virol 82: 11045–11053 [PMC free article] [PubMed]
84. Livak KJ, Schmittgen TD (2001) Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method. Methods 25: 402–408 [PubMed]

Articles from PLoS Pathogens are provided here courtesy of Public Library of Science
PubReader format: click here to try


Save items

Related citations in PubMed

See reviews...See all...

Cited by other articles in PMC

See all...


  • BioProject
    BioProject links
  • Gene
    Gene records that cite the current articles. Citations in Gene are added manually by NCBI or imported from outside public resources.
  • GEO DataSets
    GEO DataSets
    Gene expression and molecular abundance data reported in the current articles that are also included in the curated Gene Expression Omnibus (GEO) DataSets.
  • GEO Profiles
    GEO Profiles
    Gene Expression Omnibus (GEO) Profiles of molecular abundance data. The current articles are references on the Gene record associated with the GEO profile.
  • HomoloGene
    HomoloGene clusters of homologous genes and sequences that cite the current articles. These are references on the Gene and sequence records in the HomoloGene entry.
  • MedGen
    Related information in MedGen
  • Nucleotide
    Primary database (GenBank) nucleotide records reported in the current articles as well as Reference Sequences (RefSeqs) that include the articles as references.
  • Protein
    Protein translation features of primary database (GenBank) nucleotide records reported in the current articles as well as Reference Sequences (RefSeqs) that include the articles as references.
  • PubMed
    PubMed citations for these articles
  • Taxonomy
    Taxonomy records associated with the current articles through taxonomic information on related molecular database records (Nucleotide, Protein, Gene, SNP, Structure).
  • Taxonomy Tree
    Taxonomy Tree

Recent Activity

Your browsing activity is empty.

Activity recording is turned off.

Turn recording back on

See more...