Toll-like receptors (TLRs) and proteinase-activated receptors (PARs) function as innate immune biosensors in mucosal epithelial cells (ECs). We previously reported the functional and physical interactions between TLR4 and PAR2. We have extended these findings herein by showing the cooperation between PAR2 and TLR2, TLR3, or TLR4 for activation of nuclear factor-κB-dependent signaling in mucosal EC lines. In contrast, activation of PAR2 negatively regulated TLR3-dependent antiviral pathway, blunting the expression of TLR3/interferon regulatory factor-3 (IRF-3)-driven genes, as well as activation of IRF-3 and STAT1. Consistent with these in vitro observations, PAR2−/− and TLR4−/− mice, which were refractory to footpad edema induced by PAR2 agonist peptide, were protected from mouse-adapted H1N1 influenza A virus-induced lethality when compared to wild-type (WT) mice. These data support and extend our recently described, novel model of PAR2–TLR4 “receptor cooperativity” and highlight the complexity of signaling integration between heterologous innate immune biosensors.
Pathogen recognition is a critical function of innate immunity. Distinct germline-encoded pattern-recognition receptors (PRRs) expressed on innate immune cells detect microbial structures and virulence factors, including microbial proteinases (reviewed in Gribar et al.1 and Vroling et al.2). Toll-like receptors (TLRs) and proteinase-activated receptors (PARs) represent two structurally distinct classes of transmembrane receptors that have key roles in the innate immune response to pathogens. For example, influenza A virus infection activates multiple PRRs, including TLR3,3, 4 but also generates extracellular proteinases5, 6 that could activate PARs.
“Classical” PRRs sense pathogen-associated molecular patterns (PAMPs), structural molecular motifs that are evolutionarily conserved and shared among members of a given microbial class (reviewed in Janeway and Medzhitov,7 Akira and Takeda,8 and Akira et al.9). In mouse and man, the TLRs represent a family of >10 single-transmembrane classical PRRs that detect chemically conserved microbial components, for example, lipopolysaccharide (LPS), lipopeptides, and RNA. Ligand engagement of TLR N-terminal ectodomains induces receptor dimerization that brings the intracytoplasmic “Toll/interleukin-1 (IL-1) receptor resistance” (TIR) domains into close proximity. This interaction facilitates subsequent recruitment of TIR-domain-containing adapter proteins, kinases, and other signaling molecules to the “signaling platform” generated by the interacting TIR domains of the TLR dimer.
The innate immune system also senses proteolytic enzymes generated during infection through a family of “nonclassical” PRRs, for example, PARs. The PARs are a family of four 7-transmembrane, G protein-coupled receptors (7-TM GPCRs) that detect serine proteinases derived from pathogens and the host (reviewed in Steinhoff et al.10 and Ramachandran and Hollenberg11). PAR1, PAR3, and PAR4 are activated by thrombin; PAR2 mediates the cellular effects of trypsin and trypsin-like enzymes, including several microbial proteinases. PAR-activating enzymes cleave each PAR irreversibly at a specific site in the extracellular N-terminus to expose a tethered neo-ligand that binds to the second extracellular loop (ECL2) of each GPCR to trigger receptor activation. In this sense, the PARs function as a novel class of nonclassical PRRs that might serve as additional pathogen/tissue damage biosensors. Synthetic PAR agonist peptides (APs), corresponding to the hexapeptide sequences of the tethered neo-ligands of PAR1, PAR2, and PAR4, activate the native, uncleaved PARs nonenzymatically by binding directly to the corresponding PAR ECL2 to mediate signaling.
Proteinase-activated receptors and TLRs are distributed ubiquitously, yet strategically, in the body. Of the four PARs, PAR2 has been most extensively studied with respect to the inflammatory response to microbial exposure. PAR2 is expressed highly in the respiratory and gastrointestinal (GI) tracts on epithelial cells (ECs), endothelial cells, macrophages, and dendritic cells (DCs) (reviewed in Steinhoff et al.10 and Ramachandran and Hollenberg11). Exposure of human ECs to proteinases purified from certain pathogens activates PAR2 to induce antimicrobial and inflammatory responses.12, 13, 14, 15 In mice, PAR2 deficiency reduces clearance of bacterial, parasitic, and fungal infections.16, 17, 18 Similar to PARs, TLRs are also expressed on ECs, endothelial cells, macrophages, and DCs in the airway and GI tract. In general, TLR2 and TLR4 recognize Gram-positive and Gram-negative bacteria, respectively; TLR3 detects double-stranded RNA (dsRNA) from viruses (reviewed in Akira and Takeda8). Experimentally, TLR2 is activated by synthetic di- or triacylated lipopeptides that mimic bacterial cell wall constituents. TLR3 is stimulated by the synthetic dsRNA analog, polyinosine–polycytidylic acid (poly I:C). TLR4 is triggered by Gram-negative bacterial LPS. Signals originating from independently engaged, heterologous receptors may converge synergistically or antagonistically to modify cellular responses to different exogenous stimuli (reviewed in Trinchieri and Sher19 and O’Neill20). PAR2 activation delivers intracellular signals that intersect with TLR/IL-1R signaling pathways.21, 22, 23, 24 We reported previously that PAR2 AP augmented LPS-induced IL-8 secretion synergistically in SW620 human colonic ECs.23 Our studies in HEK293T cells transfected with PAR2 and/or TLR4 revealed a novel mechanism of “receptor cooperativity” in which PAR2 AP-induced NF-κB activation was synergistically enhanced by TLR4 coexpression.23 These findings were strengthened by the observation that PAR2 AP-induced NF-κB-dependent IL-1β mRNA expression in TLR4−/− macrophages was diminished.23 Moreover, an AP-dependent, physical interaction between PAR2 and TLR4 was shown in HEK293T cells by co-immunoprecipitation.23
Given that TLRs and PARs are concurrently present on mucosal ECs (reviewed in Vroling et al.2), we hypothesized that intracellular signaling pathways utilized by TLRs and PAR2 would converge either cooperatively or non-cooperatively when co-engaged. As the mucosal epithelium is the frontline innate immune barrier of the respiratory and GI tracts, we analyzed lung (A549) and colonic (SW620) ECs for responsiveness to stimulation of PAR2 and/or TLRs. Specifically, cellular responses to agonists of TLR2, TLR3, or TLR4 were examined to determine the potential effects of PAR2 activation on the inflammatory responses associated with bacterial and viral infections in mucosal ECs. Cooperation between PAR2 and TLR2, TLR3, or TLR4 for nuclear factor-κB (NF-κB)-dependent IL-8 mRNA induction was observed. However, our data also revealed a novel role for PAR2 in the negative regulation of TLR3 antiviral pathway, leading to reduced expression of TLR3-, interferon (IFN) regulatory factor-3 (IRF-3)-driven genes, and diminished activation of IRF-3 and signal transducer and activator of transcription 1 (STAT1). In vivo, both PAR2−/− and TLR4−/− mice were highly refractory to footpad edema induced by PAR2 AP, and less susceptible to lethality following intranasal infection with a mouse-adapted H1N1 influenza A virus than wild-type (WT) C57BL/6J mice. Collectively, this study highlights the complexity of signaling integration between heterologous innate immune biosensors that result in modulation of host inflammatory responses.
We reported recently that PAR2 AP synergized with the TLR4 agonist, LPS, to enhance IL-8 secretion in SW620 human colonic ECs.23 As PAR2 is expressed highly and strategically on ECs of the respiratory and GI tracts, we postulated that PAR2 might function as a novel, nonclassical PRR. We also hypothesized that cross talk between the two heterologous PRR classes, that is, PAR2 and TLR2, 3, and 4, would modulate the inflammatory response.
PAR2 AP responsiveness in human mucosal EC lines
Human lung (A549) and colonic (SW620) ECs were examined for responsiveness to PAR2 AP. Both responded rapidly to PAR2 AP with IL-8 mRNA induction that peaked rapidly at 0.5–1 h after stimulation (Figure 1a); SW620 ECs responded similarly, but somewhat less robustly than A549 ECs. PAR2 AP-treated A549 ECs also expressed a broader array of proinflammatory mediator genes examined, for example, MIP-3α, tumor necrosis factor-α (TNF-α), IL-6, IL-8, MIP-2α, MCP-1, and COX-2 (Figure 1b) than SW620 ECs (data not shown). A549 and SW620 ECs responded to PAR2 AP with peak AP activities at ∼100 vs. ∼300 μm, respectively (Figure 1c). A control, reverse peptide (RP) was inactive in both cell lines.
Cooperative PAR2–TLR signaling integration in human mucosal EC lines
A549 and SW620 ECs were next examined for responsiveness to TLR2, TLR3, or TLR4 agonists, that is, Pam2CSK4 (or P2C), poly I:C, or LPS, respectively, in the absence or presence of PAR2 AP. In both EC lines, PAR2 AP enhanced IL-8 mRNA expression induced by these TLR agonists (Figure 2); a control RP had no effect. In A549 ECs, the effect of concurrent PAR2 AP and LPS co-stimulation on IL-8 mRNA expression was additive (Figure 2a). However, in SW620 ECs, PAR2 AP potentiated LPS-induced IL-8 mRNA synergistically (Figure 2b). As for PAR2 and TLR2, cooperative signaling for IL-8 mRNA induction was detected in both EC lines (Figure 2). In addition, PAR2 AP, together with the TLR3 agonist, poly I:C, induced robust, synergistic augmentation of IL-8 mRNA levels in both EC lines (Figure 2).
Cooperative and non-cooperative PAR2-TLR3 signaling integration
As the synergy between PAR2 and TLR3 was the strongest observed for any of the agonist combinations tested, we examined PAR2–TLR3 signaling interactions further. Poly I:C stimulates MyD88-independent signaling by recruiting the adapter protein, TRIF, to the TLR3 dimer. Although MyD88-dependent signaling is predominantly associated with NF-κB activation, TRIF-dependent signaling results in the activation of IFN regulatory factor-3 (IRF-3) and delayed NF-κB activation (reviewed in Akira and Takeda8 and Akira et al.9). Although NF-κB is most often associated with the induction of proinflammatory cytokines and chemokines, for example, IL-8 and MIP-3α, IRF-3 is a potent transcriptional activator of many MyD88-independent genes, including IFN-β, IP-10, and RANTES.25, 26 In both EC lines, PAR2 AP induced mRNA expression of IL-8 and MIP-3α, but did not stimulate the expression of IFN-β, IP-10, or RANTES mRNAs (Figure 3). PAR2 AP synergistically enhanced poly I:C-induced mRNA expression of IL-8 and MIP-3α (Figure 3, top panels). In contrast, PAR2 AP significantly downregulated poly I:C-induced mRNA expression of IFN-β, IP-10, and RANTES (Figure 3). In A549 ECs, poly I:C-induced IFN-β mRNA expression peaked at ∼2 h after stimulation (Figure 4); IP-10 mRNA expression was relatively delayed, consistent with its IFN-β dependence.25, 26, 27 PAR2 AP suppressed poly I:C-induced IFN-β mRNA levels significantly at 2–4 h and markedly inhibited poly I:C-induced mRNA expression of IP-10 and RANTES at 3–6 h after stimulation. In contrast, PAR2 AP enhanced poly I:C-induced IL-8 and MIP-3α mRNAs at all time points examined (Figure 4). Poly I:C, but not PAR2 AP, induced TLR3 mRNA expression (Figure 4),26, 28 and the delayed induction kinetics reflects its IFN-β dependence.26 Consistent with its inhibitory effect on poly I:C-induced IFN-β gene expression, PAR2 AP also inhibited poly I:C-induced TLR3 mRNA expression (Figure 4). Kinetic analysis of SW620 ECs stimulated with PAR2 AP and/or poly I:C yielded similar results (data not shown). In contrast to its effects on poly I:C-induced IFN-β, IP-10, RANTES, and TLR3 mRNAs in A549 ECs, PAR2 AP enhanced mRNA expression of other TLR3-driven, NF-κB-regulated genes, that is, MCP-1, MIP-2α, TNF-α, IL-6, and IL-1β (data not shown). Consistent with the mRNA data, PAR2 AP augmented poly I:C-induced IL-8 and MIP-3α protein production synergistically, but suppressed poly I:C-induced IP-10 and RANTES secretion significantly in A549 ECs (Figure 5).
PAR2 AP differentially modulates TLR3-mediated activation of NF-κB and IRF-3
Consistent with the observation that the NF-κB-responsive genes, for example, IL-8 and MIP-3α, were significantly upregulated by PAR2 and TLR3 co-stimulation, NF-κB p65 activation (phospho-Ser536) was enhanced in A549 ECs co-stimulated with AP and poly I:C vs. AP or poly I:C alone (Figure 6a). This observation was supported by a significant reduction in the levels of the negative regulator of NF-κB, IκBα (Figure 6b). In contrast to augmented NF-κB activation, PAR2 AP downregulated poly I:C-induced IRF-3 activation (phospho-Ser396) significantly (Figure 6c). Total IRF-3 levels were unaffected (Figures 6a–c). Experiments in HEK293T cells transiently transfected with PAR2, TLR3, and luciferase reporter constructs driven by promoters having either interferon-stimulated response element (ISRE) or NF-κB binding sites showed similar results: PAR2 AP co-stimulation inhibited poly I:C-induced ISRE-luciferase activity, whereas AP and poly I:C co-treatments induced higher NF-κB-luciferase reporter activity than AP or poly I:C alone (data not shown).
PAR2 AP suppresses TLR3-induced STAT1 activation
Poly I:C triggers the TLR3/IRF-3 pathway to induce the expression of IFN-β that then binds to the type I interferon-α/β receptor (IFN-α/βR),25, 26, 27 resulting in the activation of several transcription factors, including STAT1. As PAR2 AP suppressed poly I:C-induced IRF-3 activation and mRNA expression of IRF-3-dependent genes, including IFN-β, we predicted that AP would also suppress poly I:C-induced STAT1 activation. In A549 ECs, STAT1 Tyr701 phosphorylation (p-STAT1) was prominently induced at ∼3 h after stimulation with poly I:C, but not with PAR2 AP at any time point examined; however, AP significantly inhibited p-STAT1 levels in poly I:C-treated ECs (Figure 6d). Total STAT1 levels were unaffected. Together, these data support the finding that PAR2 engagement can simultaneously augment TLR3-driven NF-κB activation while inhibiting TLR3-mediated IRF-3 responses, leading to downregulation of the second wave of signaling induced by the IFN-β/IFN-α/βR/STAT1 pathway.
We next asked whether PAR2 AP would also inhibit IFN-β-induced STAT1 activation. In contrast to its inhibitory effect on poly I:C-induced STAT1 activation, PAR2 AP co-stimulation did not inhibit recombinant IFN-β (rIFN-β)-induced p-STAT1 levels in A549 ECs (Figure 6e).
PAR2−/− and TLR4−/− mice are protected from influenza-induced lethality
As PAR2 activation inhibited the TLR3/IRF-3 antiviral pathway in mucosal ECs, we hypothesized that PAR2−/− mice would exhibit a de-repressed TLR3/IRF-3-mediated antiviral response and, thus, would exhibit increased protection against virus infection. Influenza A virus infection activates multiple PRRs, including MDA-5, RIG-I, and TLR3,3, 4 but also generates significant tissue damage that produces extracellular proteinases,5, 6 including elastase,5 that could activate PAR2 (reviewed in Vroling et al.2). WT C57BL/6J and PAR2−/− mice were infected intranasally with mouse-adapted H1N1 influenza virus, strain A/PR/8/34. At 200 p.f.u. (plaque-forming unit), ∼80% of WT mice died by day 14 after infection; in contrast, most of the PAR2−/− mice survived the infection (Figure 7a). At 600 p.f.u., all mice from both strains succumbed equally (data not shown). We reasoned that if PAR2−/− mice were resistant to influenza virus-induced lethality secondary to a de-repressed TLR3/IRF-3/IFN-β-mediated antiviral response, IFN-β−/− mice would exhibit the opposite phenotype. Although most of the PAR2−/− mice survived the influenza infection (200 p.f.u.) vs. WT mice, all the IFN-β−/− mice died (Figure 7b). Taken together, these in vivo data support our observations in EC lines that PAR2 activation inhibits the antiviral response induced by innate immune biosensors, such as TLR3. The absence of PAR2 conferred a protective phenotype on influenza-infected mice.
Previously, we showed receptor cooperativity between PAR2 and TLR4 in vitro.23 In HEK293T transfectants, PAR2 engagement by its AP resulted in NF-κB activation that was synergistically enhanced by the coexpression of TLR4. TLR4-mediated enhancement of PAR2 signaling was MyD88 dependent, whereas PAR2 signaling in the absence of TLR4 was TRIF dependent.23 Conversely, PAR2 AP-treated TLR4−/− macrophages exhibited significantly diminished expression of NF-κB-dependent IL-1β mRNA vs. WT macrophages. In the HEK293T transfection system, PAR2 AP induced a physical association between PAR2 and TLR4.23 We concluded from our earlier study that optimal PAR2 signaling leading to NF-κB activation occurs when in complex with TLR4 and its adapter protein, MyD88.23
Given that optimal PAR2 signaling requires TLR4,23 and as PAR2−/− mice were resistant to influenza-induced lethality, we hypothesized that TLR4−/− mice would be similarly protected. Similar to PAR2−/− mice, most of the TLR4−/− mice survived H1N1 influenza A virus infection, under conditions in which most of the WT mice died (Figure 7c).
TLR4 contributes to PAR2-mediated inflammation in vivo
To test further the hypothesis that PAR2–TLR4 receptor cooperativity occurs in vivo, we also used a well-characterized footpad edema model.29 Injection of PAR2 AP, but not saline or an inactive, control (reverse) peptide (RP), into the hind footpads of WT C57BL/6J mice rapidly induced edema that peaked at 1 h (Figure 8). Neither PAR2 AP nor RP induced footpad edema in PAR2−/− mice (Figure 8a). Compared to the WT response, PAR2 AP-induced footpad edema was significantly diminished in both TLR4−/− and MyD88−/− mice (Figures 8a and b). Together, these in vivo data further support our recently described novel model of PAR2–TLR4 receptor cooperativity23 in which optimal PAR2 signaling leading to an inflammatory response requires TLR4 and MyD88.
Signaling pathways coordinately triggered by distinct innate immune PRRs on activation by microbial components, for example, PAMPs, proteinases, have the potential to synergize with or antagonize one another to modulate an inflammatory response to infection. Results from our recent study showed that PAR2 and TLR4 synergized in vitro to augment a MyD88-mediated, NF-κB-dependent inflammatory response.23 In this study, we have extended these original observations by studying signaling interactions between the classical PRRs, that is, TLR2, TLR3, and TLR4, and a nonclassical PRR, that is, PAR2, in A549 and SW620 ECs derived from human respiratory and colonic mucosa, respectively. Our data presented herein support the conclusion that PAR2–TLR signaling integration drives “customized” inflammatory responses to combinatorial “danger” stimuli from the environment. We observed cooperative signaling convergence between PAR2 and TLR2, TLR3, or TLR4 for mRNA induction of NF-κB-dependent IL-8, a potent neutrophil chemoattractant; cooperation between PAR2 and TLR3 was highly synergistic. We also showed, for the first time, that PAR2 coactivation led to differential signaling outcomes in TLR3-stimulated mucosal ECs. We revealed a novel role for PAR2 in the negative regulation of TLR/IRF-3 antiviral pathway, leading to reduced expression of TLR3-, IRF-3-driven genes, for example, IFN-β, IP-10, and RANTES. Mechanistically, these PAR2-mediated differential effects on TLR3 signaling were traced to changes in the level of activation of the transcription factors, NF-κB and IRF-3. The inhibitory effect of PAR2 AP on TLR3-driven IRF-3 activation resulted in reduced IFN-β expression and significant suppression of TLR3-inducible STAT1 activation. These in vitro observations in EC lines were supported by results showing that PAR2−/− mice were more resistant to lethality following intranasal infection with H1N1 influenza A virus than WT C57BL/6J mice, whereas IFN-β−/− mice were hypersusceptible.
During viral infection, RNA from viruses can be sensed by TLRs 3, 7, and 8, as well as the RNA helicase cytosolic sensors, RIG-I and MDA-5 (reviewed in Kawai and Akira30). We examined the cellular responses to TLR3 stimulation as a representative TLR-dependent antiviral pathway in mucosal ECs. Ligand-bound TLR3 activates several transcription factors, including IRF-3 and NF-κB.31 Ligand-activated TLR3 dimerizes, binds its sole adapter, TRIF, and recruits IκB kinase ɛ (IKKɛ) and TANK-binding kinase 1 (TBK1).32 In turn, IKKɛ/TBK1 activates IRF-3 through C-terminal phosphorylation. The TLR3–TRIF complex also recruits receptor-interacting protein 1 (RIP1) to couple signaling to the IKKα/β/γ complex for NF-κB activation.33 Although activated NF-κB translocates to the nucleus and induces transcription of many proinflammatory cytokine or chemokine genes, for example, IL-8, MIP-3α, phosphorylated IRF-3 homodimers translocate to the nucleus to induce transcription of type I IFNs and many other IRF-3-regulated genes, for example, IFN-β, IP-10, and RANTES.34 Induction of type I IFNs is critical for evoking the expression of additional antiviral genes through the IFN-α/βR/STAT1 signaling pathway.25, 26, 27
Both IRF-3 and NF-κB are required for transcriptional activation of the potent antiviral protein, IFN-β (reviewed in Kawai and Akira30). Although PAR2 AP enhanced poly I:C-induced NF-κB activation, AP markedly inhibited poly I:C-driven IRF-3 activation, consistent with AP-mediated suppression of TLR3-driven IFN-β mRNA expression. The inhibitory effect of AP on the TLR3/IRF-3 signaling pathway appears to be very early, at the level of IKKɛ/TBK1 phosphorylation of IRF-3, rather than a result of altered IRF-3 protein stability. This is further supported by the observation that poly I:C-induced, but not rIFN-β-induced, phosphorylation of STAT1 was inhibited by concurrent stimulation of PAR2 by AP. The LPS-transducing receptor, TLR4, is the only other TLR that signals through the TRIF/IKKɛ/TBK1/IRF-3 pathway (reviewed in Akira and Takeda8). In SW620 ECs, LPS-induced expression of IFN-β and IP-10 mRNAs was attenuated significantly by PAR2 AP co-stimulation (Supplementary Figure S1a online). In A549 ECs, PAR2 AP co-stimulation also inhibited LPS-induced IP-10 mRNA expression significantly (Supplementary Figure S1b). Taken together, these data suggest that PAR2 activation exerts a more generalized inhibitory effect on the TLR/TRIF, that is, TLR3/TRIF and TLR4/TRIF, signaling pathway.
Consistent with previous reports attributing a positive, cooperative signaling outcome between PAR2 and TLRs,22, 23, 24 we showed positive cooperativity between PAR2 and TLRs at the level of NF-κB activation. The cooperative convergence of NF-κB signaling derived from these two distinct PRR families supports our contention of their proposed roles as biosensors of infection. Enhanced NF-κB activation is predicted to be critical for optimal induction of inflammatory mediators, including the expression of chemokines and cytokines necessary for the recruitment and activation of circulating leukocytes to the nidus of infection. However, selective augmentation and suppression of cytokine/chemokine expression likely has an important role in the pathogenesis and persistence/clearance of a given infection. That PAR2 activation augmented TLR3-driven expression of some chemokines, for example, IL-8 and MIP-3α, yet suppressed the expression of others, for example, IP-10 and RANTES, suggests that proteinase-rich microenvironments might drastically alter the composition of infiltrating leukocytes and, thus, significantly alter the inflammatory outcome of an infection.
Under physiological conditions, extracellular proteinases are tightly regulated by many mechanisms, including the regulation of proteinase expression and their negative control by anti-proteinases. Reduced expression of anti-proteinases and/or enhanced local levels of pathogen- and/or host-derived proteinases can lead to a dysregulated proteinase/anti-proteinase balance at anatomical sites where extracellular proteolysis is undesirable (reviewed in Antalis et al.35). Given that PAR2 activation negatively regulated the TLR3/IRF-3 antiviral pathway, we speculated that in tissues in which both PAR2 and TLR3 are present, for example, the airway, disease processes with dysregulated and de-repressed extracellular PAR2-activating trypsin-like proteolytic activities might be more susceptible to infection with TLR3-triggering viruses such as influenza A.3, 4 We confirmed this hypothesis by infecting WT C57BL/6J and PAR2−/− mice with mouse-adapted H1N1 influenza A virus that can activate TLR3 and also generates extracellular proteinases that can trigger PAR2. In support of our in vitro observations in EC cultures, in three separate experiments, PAR2−/− mice were protected from challenge with influenza A virus. In contrast, IFN-β−/− mice were hypersusceptible to influenza virus-induced lethality. Taken together, both the in vitro and in vivo data support our model that PAR2 activation inhibits TLR/IRF-3 antiviral pathway; the absence of PAR2 conferred a protective phenotype in influenza-infected mice. The absence of PAR2 might also mitigate the NF-κB-mediated cytokine storm induced by influenza infection leading, in part, to the resistance of PAR2−/− mice to influenza-induced lethality.
In contrast to our findings using 200 p.f.u. influenza virus per mouse, Khoufache et al.36 recently reported that PAR2−/− mice were more susceptible to intranasal infection with cell culture-propagated H1N1 influenza A/PR/8/34 virus (30–60 p.f.u. per mouse). Differences in infectious dose, method of virus propagation (i.e., cell culture vs. allantoic fluid of embyonated eggs), and housing conditions may account for the discrepancies between results reported by us and Khoufache et al. and warrant further investigation. It is unlikely, though, that our viral dose (200 p.f.u.) was less infectious because it killed ∼80% of the WT mice, whereas their dose of 30–60 p.f.u. was nonlethal in PAR2+/+ mice. However, we hypothesize that different infectious doses used in the two studies (200 p.f.u. vs. 30–60 p.f.u.) perhaps led to differential levels of PAR2 receptor expression or activation that could potentially account for the opposite findings. The extent of tissue damage, the level of PAR2-activating enzymes generated, and the degree of PAR2 receptor activation secondary to influenza infection are likely to be different at the two viral doses. In support of this hypothesis, it has been shown that differential stimulus dosage, for example, low vs. high agonist concentrations, can result in opposite biological effects. For example, Eisenbarth et al.37 showed that low levels of LPS induced T-helper cell type 2 responses to an inhaled antigen, whereas high levels of inhaled LPS with the same antigen resulted in strong Th1 responses. The genetic backgrounds of the PAR2−/− mice used in the two studies were also different. The different gene-targeted deletion approaches used to generate PAR2−/− mice and the extent of genetic backcross may also have contributed to the opposite observations.38, 39 In addition, PAR2 activation has been reported to exhibit opposite effects in other host inflammatory responses,40, 41, 42, 43 and perhaps this is attributable to the balance of synergistic or antagonistic effects reported herein between PAR2 and activation of other PRRs by PAMPs that are concurrently present in the environment. Future studies will be necessary to determine how differences in experimental designs might have contributed to the different findings. Nevertheless, like PAR2−/− mice, we observed that TLR4−/− mice were similarly protected from H1N1 influenza A virus infection, findings that are consistent with our recently described model of PAR2–TLR4 receptor cooperativity. Moreover, PAR2 AP induced footpad edema in WT C57BL/6J mice that was absent in PAR2−/− mice and significantly diminished in both TLR4−/− and MyD88−/− mice. We also observed significantly diminished secretion of KC and MIP-2α chemokines by TLR4−/− vs. WT C57BL/6J colonic intestinal tissues cultured ex vivo and treated with PAR2 AP (data not shown). Moretti et al.18 reported recently that PAR2 signaling in murine polymorphonuclear neutrophils depended on the presence of TLR4.
Interference of host innate antiviral defense by influenza virus is known to be achieved by the nonstructural NS1 viral protein, which dampens the induction of IRF-3-responsive antiviral genes, including IFN-β.44 However, infection of host cells by orthomyxoviruses and paramyxoviruses can also be enhanced by host/pathogen-derived proteinases45 (and reviewed in Kido et al.46). For example, co-infection with Staphylococcus aureus strains that secrete trypsin-like serine proteinases enhances influenza virus infectivity significantly by mediating cleavage of viral fusion glycoproteins, for example, hemagglutinin.45 In this study, we have provided evidence for an additional mechanism by which host/pathogen-derived proteinases might diminish TLR-mediated host antiviral response through the activation of PAR2. It is tempting to speculate that natural selection and host–virus co-evolution led to the utilization of proteinases for enhanced virus infectivity by simultaneously facilitating host–virus membrane fusion and interfering with host antiviral defense.
In summary, results from this study provide compelling data that suggest that regulating the extracellular proteinase/anti-proteinase balance might represent an effective therapeutic approach to controlling orthomyxovirus and paramyxovirus infections. The results from this study also represent a novel example of cooperative and non-cooperative signaling integration between heterologous PRRs of the innate immune system.
Reagents, virus, cell culture, and mice. Human PAR2 AP, SLIGKV-NH2, and an inactive control RP, VKGILS-NH2, were synthesized (>96% purity) by Phoenix Pharmaceuticals (Belmont, CA). Protein-free, phenol/water-extracted LPS from Escherichia coli strain K235 was purified as referenced.23 S-[2,3-bis(palmitoyloxy)-(2-RS)-propyl]-[R]-Cys-Ser-Lys4-OH (Pam2CSK4 or P2C) and poly I:C (pI:C) were purchased from Invivogen (San Diego, CA). Human rIFN-β 1a was purchased from PBL InterferonSource (Piscataway, NJ). Mouse-adapted H1N1 influenza virus (A/PR/8/34) was purchased from American Type Culture Collection (ATCC) (Manassas, VA) and grown in the allantoic fluid of 10-day old embryonated chicken eggs (Charles River Laboratories, Wilmington, MA) as previously described.47 Human A549 lung and SW620 colonic ECs (ATCC) were propagated in Dulbecco's modified Eagle's medium (DMEM) or RPMI-1640 (CellGro, Herndon, VA), respectively. DMEM was supplemented with 10% heat-inactivated fetal calf serum (FCS; Hyclone, Logan, UT), 100 U ml−1 penicillin, 100 μg ml−1 streptomycin, and 2 mM L-glutamine. RPMI-1640 received the same supplements, but with 2% heat-inactivated FCS. ECs were harvested from tissue culture flasks (Corning, Corning, NY) using CellStripper solution (CellGro) and seeded in 6-well plates at 4 × 105 (A549) or 1 × 106 (SW620) cells per well. Cells were allowed to rest for 2 days with a medium change on day 1, and treated with agonists, as indicated. WT C57BL6/J mice and PAR2−/− mice backcrossed onto a C57BL/6 background (N5) were purchased from The Jackson Laboratories (Bar Harbor, ME). TLR4−/− and MyD88−/− mice (N8 on a C57BL/6 background), originally obtained from Dr Shizuo Akira (Osaka University, Osaka, Japan), and IFN-β−/− mice (N8 on a C57BL/6 background), originally obtained from Dr Eleanor Fish (University of Toronto, Ontario, Canada), were bred at UMB. Mice were housed in a SPF barrier facility (UMB). Administration of AP or influenza to mice is described in the figure legends. All mice were age matched and used between 6–10 weeks of age. All experiments were conducted with institutional approval.
Preparation of total RNA and cDNA. Total RNA from EC cultures was extracted, and oligo(dT)-primed cDNA was synthesized as previously described.28
qPCR. Quantitative real-time PCR (qPCR) primers ( Table 1) were designed and synthesized as previously described.28 qPCR was carried out on ABI Prism 7500 Fast Real-time PCR System (Applied Biosystems, Foster City, CA) in a 25 μl reaction containing 20 ng cDNA, 0.3 μm each of sense/anti-sense primers, and 12.5 μl of Fast SYBR Green Master Mix (Applied Biosystems) under the manufacturer's pre-set thermal conditions: 20 s at 95 °C, 40 cycles of 3 s at 95 °C and 30 s at 60 °C, followed by a dissociation stage. Relative gene expression was calculated using the 2−ΔΔCt method as previously referenced,28 with hypoxanthine guanine phosphoribosyltransferase as the housekeeping gene.
Western analysis. A549 cells were seeded at 8 × 105 cells per well in 6-well plates and allowed to rest for 3 days, with a medium change on day 1. After treatment, whole-cell lysates were collected, processed, resolved by gel electrophoresis, transferred to polyvinylidene difluoride membranes, probed with antibodies, and target protein bands detected as previously described.28 Primary and horseradish peroxidase-conjugated secondary antibodies used in this study were purchased from Cell Signaling Technology (Danvers, MA) and used at 1:1,000 and 1:2,000 dilutions, respectively.
Analysis of secreted proteins by ELISA. The concentrations of secreted proteins were determined by enzyme-linked immunosorbent assay (ELISA) by the Cytokine Core Laboratory (UMB).
Statistical analysis. Using GraphPad PRISM 4.0 (GraphPad Software, San Diego, CA), one-way analysis of variance (ANOVA) with Tukey's post-test or two-way ANOVA with Bonferroni post-test was performed to assess statistical significance (P-values <0.05).
The authors declared no conflict of interest.
The authors thank Ms Rachel Griffin for breeding TLR4−/−, MyD88−/−, and IFN-β−/− mice, and Dr Prasad Rallabhandi for helpful discussion. This work was supported by the NIH Grants R37 AI-18797 (SNV), R01 DK048373 (AF), R01 HL084387, R01 DK081376, R01 CA098369 (TA), and R01 AI050632 (DF). QMN was supported, in part, by the NIH Training Grant (T32 AI-07540) and is currently supported by AI-18797 (SNV). JRT was supported by a minority supplement R01 AI50632S1. This work was carried out in partial fulfilment of the PhD requirements (QMN).
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Journal of Natural Medicines (2016)