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Nlrp6 regulates intestinal antiviral innate immunity

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Science  13 Nov 2015:
Vol. 350, Issue 6262, pp. 826-830
DOI: 10.1126/science.aab3145

Nlrp6 keeps gut infections in check

Most viruses infect only certain cells of the body. Enteric viruses, such as norovirus and rotavirus, specifically infect the gut. Wang et al. now show that the response to such viruses is tissue-specific, too. Antiviral immunity to enteric but not systemic viral infections in mice required Nlrp6, a member of the NOD-like receptor family of proteins that play important roles in host defense. Together with the RNA helicase protein Dhx15, Nlrp6 bound viral RNA and elicited downstream antiviral immune responses necessary for viral clearance. These included the production of type I and type III interferons and the expression of interferon-stimulated genes.

Science, this issue p. 826

Abstract

The nucleotide-binding oligomerization domain–like receptor (Nlrp) 6 maintains gut microbiota homeostasis and regulates antibacterial immunity. We now report a role for Nlrp6 in the control of enteric virus infection. Nlrp6−/− and control mice systemically challenged with encephalomyocarditis virus had similar mortality; however, the gastrointestinal tract of Nlrp6−/− mice exhibited increased viral loads. Nlrp6−/− mice orally infected with encephalomyocarditis virus had increased mortality and viremia compared with controls. Similar results were observed with murine norovirus 1. Nlrp6 bound viral RNA via the RNA helicase Dhx15 and interacted with mitochondrial antiviral signaling protein to induce type I/III interferons (IFNs) and IFN-stimulated genes (ISGs). These data demonstrate that Nlrp6 functions with Dhx15 as a viral RNA sensor to induce ISGs, and this effect is especially important in the intestinal tract.

Nucleotide oligomerization domain (NOD)–like receptors (NLRs) play a central role in the immune response to diverse microorganisms and react to environmental insults and cellular danger signals (1, 2). Some NLRs contribute to antiviral immunity. NOD2 recognizes single-stranded RNA (ssRNA) viruses to induce type I interferons (IFNs) via mitochondrial antiviral-signaling protein (MAVS) (3), and the NLRP3 inflammasome is crucial for the control of diverse viral infections in vivo (47). Several NLRs, on the other hand, dampen antiviral immune responses. NLRX1 and NLRC5 negatively regulate type I IFNs and nuclear factor κB (NF-κB) signaling via distinct molecular mechanisms (812); NLRC3 attenuates Toll-like receptor signaling and the stimulator of interferon genes (STING)–mediated anti-DNA virus immune signaling (13, 14). A role for Nlrp6 in the regulation of antibacterial immune responses has recently been documented (1518); however, whether Nlrp6 regulates viral infection has not yet been elucidated.

Nlrp6 exhibits a tissue- and cell-type–specific pattern of expression, with the highest level in intestinal epithelial cells (IECs) (15) (figs. S1 and S2). We therefore determined whether Nlrp6 plays a prominent role in inhibiting enteric virus infection at the intestinal interface. We used a (+) ssRNA virus, encephalomyocarditis virus (EMCV), which is transmitted via the fecal-oral route in nature. We infected both wild-type (WT) and Nlrp6−/− mice with EMCV systemically via intraperitoneal injection and noted that the survival curve of Nlrp6−/− mice was similar to that of WT animals (Fig. 1A). Viral dissemination was also the same in the blood, brains, and hearts of Nlrp6−/− and WT mice. The intestinal viral burden of Nlrp6−/− mice was, however, higher than that of WT animals (Fig. 1B)—suggesting that Nlrp6 plays an important role in limiting EMCV replication at this location. In support of this, Nlrp6 mRNA expression was much higher in the intestines than other tissues after EMCV infection (Fig. 1C). We therefore reasoned that Nlrp6 prevents systemic infection and mortality when EMCV is delivered orally to its principal site of infection—the intestine. Indeed, Nlrp6−/− mice were more susceptible to oral infection with EMCV than WT animals (Fig. 1D and Fig. 3E).

Fig. 1 Nlrp6 controls EMCV infection of the intestine.

(A) The survival curves of WT and Nlrp6−/− mice infected with EMCV via the intraperitoneal route. N = 12 mice per group. (B and C) Quantitative polymerase chain reaction (qPCR) analyses of (B) EMCV viral loads and (C) Nlrp6 in various tissues 72 hours after infection with EMCV intraperitoneally Intestinal epithelial cells (IEC). (D) The survival curves of WT mice, WT mice cohoused with Nlrp6−/− [WT (Nlrp6−/−)], Nlrp6−/− mice cohoused with WT [Nlrp6−/−(WT)], and Casp1−/− mice after oral infection with EMCV. N = 10 to 16 mice per group. *P < 0.05 (log-rank test). Results were pooled from two independent experiments. (E and F) qPCR analysis of EMCV loads (E) in the whole blood cells 72 hours after oral infection or (F) in the intestines 72 hours after intraperitoneal infection. Each symbol in (B), (C), (E), and (F) represents one mouse; small horizontal lines indicate the median of the result. *P < 0.05; **P < 0.01 (nonparametric Mann-Whitney analysis). The data are representative of at least two to three independent experiments.

Alterations in microbiota and inflammasome activation are two potential processes that may influence the ability of Nlrp6−/− mice to control intestinal EMCV infection. The intestinal microbial ecology of Nlrp6−/− mice is different from that of WT mice (15), which could affect antiviral immunity. We therefore cohoused mice for 4 weeks before EMCV infection, which we previously showed was sufficient to equilibrate the microbiota between WT and Nlrp6−/− mice. WT and Nlrp6−/− mice had similar levels of TM7 and Prevotellacae bacteria (15) after cohousing (fig. S3A), indicating stabilization of the microbiota. Nlrp6−/− mice, however, died of EMCV infection more rapidly than WT and cohoused WT animals (Fig. 1D), and viremia was ~10-fold higher in Nlrp6−/− than WT animals (Fig. 1E). When inoculated systemically via intraperitoneal injection, EMCV loads in the intestines of cohoused Nlrp6−/− mice were also more than 10-fold higher than those of cohoused WT animals (Fig. 1F). Similar survival results were noted for Nlrp6−/− and Nlrp6+/+ littermates (fig. S3B). These data demonstrate that the increased viral susceptibility of Nlrp6−/− mice is not a result of altered intestinal microbial ecology. To extend our finding further, we examined another enteric virus, murine norovirus 1 (MNV-1), a (+) ssRNA virus. MNV-1 was rapidly cleared by the innate immune system in WT mice (19) but persisted much longer in Nlrp6−/− mice (fig. S3, C to E). Nlrp6 initiates inflammasome signaling via caspase-1. We therefore determined whether Nlrp6 requires caspase-1 to control EMCV at the intestinal epithelia. In agreement with a previous report (20), following EMCV challenge, the survival of Casp1−/− and WT mice was similar (Fig. 1D). These data suggest that intestinal Nlrp6 controls EMCV infection by an alternative mechanism.

To understand how Nlrp6 contributes to antiviral innate immune responses, we used an Nlrp6 antibody to immunoprecipitate Nlrp6 binding partners from mouse primary IECs and a FLAG-Nlrp6 overexpression system in human embryonic kidney 293 T (HEK293T) cells. We identified DEAH (Asp-Glu-Ala-His) box helicase 15 (Dhx15) by mass spectrometry (fig. S4) and confirmed it using a specific antibody to Dhx15 (Fig. 2A and fig. S5A). Glutathione S-transferase–Dhx15 expressed in Escherichia coli pulled down FLAG-Nlrp6 expressed using a mammalian in vitro translation system (fig. S5B), suggesting a direct interaction. Nlrp6 is composed of three functional domains: an N-terminal pyrin domain (PYD), a NACHT domain, and a C-terminal leucine-rich repeat domain (LRR). Each individual domain failed to bind Dhx15 when compared with full-length Nlrp6 (fig. S5C). A fragment encompassing the NATCH and NACHT-associated domain (NAD) interacted with Dhx15 (Fig. 2B). NLRP3, a close relative of Nlrp6, did not interact with Dhx15, demonstrating specificity (fig. S5C).

Fig. 2 Nlrp6 binds viral RNA via Dhx15.

(A) Coimmunoprecipitation (co-IP) of Nlrp6 with Dhx15 from WT and Nlrp6−/− mouse intestinal epithelial cells using an antibody to Nlrp6. IB, immunoblotting. (B) Co-IP of FLAG-Nlrp6 NACHT+NAD (amino residues 170 to 715) and the full-length (1-end) with endogenous DHX15 from HEK293T cells overexpressing FLAG-tagged proteins using an antibody to FLAG. (C) Co-IP of FLAG-tagged proteins with endogenous MAVS from HEK293T cells, as in (B). WCE, whole-cell extract; GAPDH, glyceraldehyde 3-phosphate dehydrogenase. (D) qPCR analyses of viral RNA bound by FLAG-tagged proteins from EMCV-infected and FLAG fusion protein–expressing HEK293T cells. The data are presented as relative increase over vector (FLAG). (E) Binding of endogenous Nlrp6 to viral RNA. (Left) qPCR analyses of viral RNA bound by endogenous FLAG-Nlrp6 in IECs. (Right) Immunoblots of FLAG-Nlrp6 in WCE and IP. 3xFLAG-Nlrp6 denotes three FLAG motifs tagged to Nlrp6. (F) (Top) qPCR analyses of EMCV RNA bound by FLAG-Nlrp6 from GFP or DHX15 siRNA-treated HEK293T cells. (Bottom) Immunoblots of WCE and IP. (G) Immunoblots showing FLAG-tagged proteins (purified from HEK293T) bound by biotin-labeled RNA analogs. polyIC(H), high molecular weight (1.5 to 8 kb); polyIC(L), low molecular weight (0.2 to 1 kb). (H) Co-IP of Mavs with Dhx15 from IECs of WT and Nlrp6−/− mice infected with EMCV using a rabbit polyclonal antibody to Mavs. (I) The survival curves of WT and Mavs−/− mice after oral infection with EMCV. N = 5 mice per group; *P < 0.05 (log-rank test). The data are representative of at least two independent experiments.

Dhx15 is a putative pre-mRNA-splicing factor and adenosine triphosphate (ATP)–dependent RNA helicase that modulates antiviral immune responses via MAVS, an adaptor protein for retinoic acid inducible gene 1 (RIG-I)–like receptors (RLRs) (21, 22). We reasoned that the Nlrp6-Dhx15 complex might use MAVS to trigger type I IFN responses. Indeed, FLAG-Nlrp6 bound endogenous MAVS, as did Nlrp3 ((23)) and RIG-I (2427) (Fig. 2C). The negative controls FLAG-NLRC5 (11) or Nlrp10 did not coprecipitate with MAVS (fig. S5D), confirming the specificity of the Nlrp6-MAVS interaction. Because Dhx15 is a putative RNA helicase and viral RNA sensor (22), we then determined whether Nlrp6-Dhx15 forms a viral RNA-sensing complex. Both Nlrp6 and Dhx15 showed high affinity for viral RNA (Fig. 2D and fig. S6A). The Nlrp6 NACHT domain was sufficient for RNA binding but weaker than full-length Nlrp6 (fig. S6B). To exclude nonspecific binding due to overexpression, we examined endogenous Nlrp6 binding to viral RNA in WT and FLAG-Nlrp6 knock-in mice (fig. S2). Both Nlrp6 and FLAG-Nlrp6 was coimmunoprecipitated with EMCV RNA from infected IECs (Fig. 2E and fig. S6C). Because the RNA binding capacity of Dhx15 was much greater than that of Nlrp6, we reasoned that Nlrp6-RNA binding was dependent on Dhx15. Indeed, the amount of Nlrp6-bound viral RNA was reduced significantly in Dhx15 small interfering RNA (siRNA)–treated cells (Fig. 2F). In contrast, Dhx15-RNA binding was not altered in Nlrp6−/− cells (fig. S6D). Like Dhx15 (22), Nlrp6 bound only RNA but not DNA viruses (fig. S6E). To assess the nature of viral RNA bound by Nlrp6, we tested several synthetic RNA analogs. Nlrp6 preferably bound the long double-stranded RNA (dsRNA) analog polyinosinic-polycytidylic acid (polyIC) (Fig. 2G). To provide in vivo evidence for a functional interaction between MAVS, Dhx15, and Nlrp6, we examined MAVS-Dhx15 interactions in WT and Nlrp6−/−IECs. Consistent with a previous report (22), MAVS binding to Dhx15 was enhanced by EMCV infection in WT IECs, but the interaction was weaker in Nlrp6−/− (Fig. 2H). Mavs−/− mice were also much more susceptible to EMCV administered orally when compared with WT mice (Fig. 2I). These data suggest that the Dhx15-Nlrp6-MAVS axis plays an important role in restricting EMCV infection of the intestine.

To validate a role for Nlrp6 in Dhx15-Mavs–mediated antiviral immunity, we examined the expression of type I/III IFN-induced genes (ISGs). The mRNA and protein expression of a number of ISGs was reduced in Nlrp6−/− IECs compared with WT (fig. S7A and Fig. 3, A and B). Although both types I and III IFNs can elicit antiviral responses, type III IFNs are particularly critical for controlling viral infection in IECs (2830). IFN-λ (also known as IL-28a) protein and mRNA, and Ifnb mRNA, were reduced in Nlrp6/– intestines after EMCV infection (fig. S7B). ISG mRNA amounts were, however, similar in other WT and Nlrp6−/− tissues (fig. S8).

Fig. 3 Nlrp6 regulates type I/III IFN and ISG expression in the intestine.

(A to C) Mouse tissues were analyzed on day 3 after intraperitoneal infection with EMCV. (A) qPCR analyses of selected ISG mRNA expression in IECs and whole intestine. (B) Immunoblotting analyses of ISG protein abundance in whole intestine of cohoused mice. (Right) Relative ISG abundance normalized to a housekeeping protein, Gapdh. (C) qPCR analyses of cellular EMCV loads and immune gene expression in MEFs after EMCV infection (multiplicity of infection = 0.1). (D) Enzyme-linked immunosorbent assay of IFN-β concentrations in the culture medium of MEFs after EMCV infection and quantification of infectious viral particles in the culture medium 16 hours after EMCV infection. (E) (Upper) The survival curves of WT and Nlrp6−/− mice treated with 0.9% saline (mock) or 25 μg of recombinant mouse IFN-λ2 4 hours before oral infection with EMCV. (Lower) qPCR analysis of EMCV loads in the whole blood cells 72 hours after infection. N = 7 to 10 mice per group. *P < 0.05 (log-rank test). In (A) and (E), the data are normalized with mouse beta actin and are presented as relative change over the mean of the results of WT [Mock-WT in (E)] mice. Each band/dot represents an animal. The horizontal lines in the figures indicate the median of the results. *P < 0.05; **P < 0.01; ***P < 0.001 (nonparametric Mann-Whitney analysis). In (C) and (D), scale bars show mean + SEM; n = 3 mice. *P < 0.05; **P < 0.01 (unpaired Students’ t test). The data are representative of at least two independent experiments.

To assess whether the Nlrp6-caspase-1 inflammasome regulates antiviral immunity in the intestine, we compared ISG expression in Nlrp6−/− with Casp1−/− and WT mice. The viral loads and ISG expression were similar in the intestines of Casp1−/− and WT mice (fig. S9), demonstrating an inflammasome-independent antiviral mechanism for Nlrp6. In support of the in vivo findings, EMCV loads in Nlrp6−/− embryonic fibroblasts (MEFs) were sixfold higher than those in Nlrp6+/− cells at 16 hours after infection, while antiviral gene expression was significantly lower (Fig. 3, C and D, and fig. S10, A and B). We also observed a decrease in polyIC-induced Ifnb1 expression in Nlrp6−/− compared with Nlrp6–/+ MEFs (fig. S10C). In agreement with the results from Nlrp6−/− cells, overexpression of Nlrp6 enhanced Ifnb1 and Il6 expression modestly (fig. S11). All these data demonstrate a pivotal role for Nlrp6 in inducing type I/III IFNs and ISGs. Type III IFNs are particularly critical for control of viral infection of IECs (2830). Indeed, exogenous IFN-λ fully protected WT and Nlrp6−/− mice against lethal EMCV infection and reduced viremia significantly (Fig. 3E). We next determined whether the antiviral function of Nlrp6 is specific for RNA viruses. Neither herpes simplex virus–1 (HSV-1) titers nor Ifnb1 expression in Nlrp6−/− was different from those in Nlrp6–/+ cells (fig. S12A). IFN-α, polydAT, or lipopolysaccharide-induced ISGs or cytokine expression in Nlrp6−/− was also similar to that in Nlrp6-/+ MEFs (fig. S12, B to D).

As viral infections and the ligands that can induce robust type I IFN expression also up-regulated Nlrp6 expression (Fig. 3C and figs. S10C, S12C, and S13), we reasoned that Nlrp6 per se might be an ISG. Indeed, induction of Nlrp6 mRNA expression by EMCV or polyIC treatment was almost abolished in Irf3/7−/− or Ifnar1−/− MEFs. Consistent with this, recombinant IFN-α, but not tumor necrosis factor–α (TNF-α) was able to induce Nlrp6 expression vigorously, suggesting that interferon regulatory factor (IRF)/IFN signaling, but not NF-κB signaling controls Nlrp6 expression (Fig. 4 and fig. S14A). Nlrp6 mRNA expression was also induced by recombinant IFN-λ2 (fig. S14B). These results indicate that Nlrp6 expression is regulated by type I/III IFNs via IRF3/7.

Fig. 4 Nlrp6 is an ISG.

qPCR analyses of the transcripts of (A) Nlrp6 and (B) Mda5 in WT, Irf3/7−/−, and Ifnar−/− MEFs treated with EMCV, polyIC, recombinant IFN-α, or TNF-α. The data are expressed as percentage of a housekeeping gene Hprt. Scale bars, mean + SD. The data are representative of at least two independent experiments.

The above-mentioned data demonstrate that Dhx15-Nlrp6 senses long dsRNA in the cytoplasm (Fig. 2G), a well-established feature for MDA5. We then determined whether Nlrp6-mediated signaling is also dependent on MDA5. siRNA knockdown of Nlrp6 reduced Ifnb1 and Isg15 mRNA expression after polyIC stimulation in Mda5−/− MEFs (fig. S15A), suggesting an MDA5-independent antiviral role for Nlrp6. Similar results were noted with Rig-I−/− MEFs (fig. S15B). Nlrp6-RNA binding was unchanged in Mda5−/− or Rig-I−/− MEFs compared with WT (fig. S15C), and there was no interaction between Nlrp6 and MDA5 or RIG-I (fig. S15D). We next examined the relative antiviral role for MDA5 in the intestine in comparison with Nlrp6. The viral loads in both Nrp6−/− and Mda5−/− IECs were similar but were much higher than those in WT mice (fig. S15E). These results, in conjunction with the Nlrp6, Dhx15, and MDA5 expression data (fig. S1), suggest that Dhx15-Nlrp6 constitutes the first line of anti-EMCV defense in the intestinal epithelia, whereas MDA5 is dominant in myeloid cells.

Our results demonstrate that Nlrp6 controls enteric virus infection in the intestine by interacting with an RNA sensor, Dhx15, to trigger MAVS-dependent antiviral responses. This inflammasome-independent response provides a mechanism for Nlrp6 to elicit pleotropic effects in the host and demonstrates its importance against diverse classes of microbes.

Supplementary Materials

www.sciencemag.org/content/350/6262/826/suppl/DC1

Materials and Methods

Figs. S1 to S15

References (3137)

References and Notes

  1. Acknowledgments: The data presented in this manuscript are tabulated in the main paper and in the supplementary materials. This work was supported by National Institutes of Health grants N01-HHSN272201100019C, AI099625, and AI103807. E.F. and R.F. are Investigators of the Howard Hughes Medical Institute. S.Z. was supported by a fellowship from Howard Hughes Medical Institute–The Helen Hay Whitney Foundation.
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