RESULTS IL-22 and IL-18 activate their receptors on epithelial cells to protect against RV
We previously reported that systemic administration of bacterial flagellin elicits TLR5-mediated production of IL-22 and NLRC4-mediated generation of IL-18 that can act in concert to prevent or treat RV and some other enteric viral infections (5). Specifically, as shown in fig. S1 and our previous work, chronic RV infections that developed in RV-inoculated immune-deficient C57BL/6 Rag-1/ mice were cured by combined systemic treatment with IL-18 and IL-22, whereas injection of either cytokine alone reduced RV loads but did not clear the virus, regardless of cytokine dose and duration of administration. In these particular experiments, RV infection was assayed by measuring fecal RV antigens by enzyme-linked immunosorbent assay (ELISA), but measurement of RV genomes in the intestine yields similar results (5). In wild-type (WT) mice, a sufficiently high doses of recombinant IL-22 can, by itself, fully prevent RV infection, whereas lower doses of exogenously administered IL-22 and IL-18 markedly reduced the extent of RV infection, while the combination of these cytokines eliminated evidence of infection (Fig. 1A). The central goal of this study was to elucidate mechanisms by which these cytokines act in concert to control and prevent RV infection.
Mice were administered PBS, IL-22 (2 g), and/or IL-18 (1 g) via intraperitoneal injection, 2 hours before, or 2, 4, 6, or 8 days after (indicated by arrows) oral inoculation with mRV. Fecal RV levels were measured over time by ELISA. (A) C57BL/6 mice n = 4. (B) IL-22/ mice, n = 5 and 7 for PBS and IL-18, respectively. (C) IL-18/ mice, n = 5. * indicates significantly different from PBS by two-way analysis of variance (ANOVA), P < 0.0001. dpi, days post-inoculation.
In the context of parasitic infection, both IL-18 and IL-22 promote expression of each other, and loss of either impairs immunity to Toxoplasma gondii (6). We thus hypothesized that administration of IL-18 might impede RV as a result of its ability to induce IL-22 expression. This hypothesis predicted that the ability of IL-18 to protect against RV infection would be largely absent in IL-22/ mice. However, administration of IL-18 upon RV inoculation clearly reduced the extent of RV infection in IL-22/ mice, which argued strongly against this hypothesis (Fig. 1B). We considered the converse hypothesis, namely, that IL-22 might impede RV infection by elicitation of IL-18, but we observed that recombinant IL-22 markedly prevented RV infection in IL-18/ mice (Fig. 1C). Although IL-18 and IL-22 may play important roles in inducing each others expression, our results indicate that they each activate distinct signaling pathways that cooperate to impede RV infection.
Next, we examined the extent by which IL-18 and IL-22 acted upon the hematopoietic or nonhematopoietic compartment to impede RV infection. We used WT, IL-18-R/, and IL-22-R/ mice to generate irradiated bone marrow chimeric mice that expressed the receptors for IL-22 or IL-18 in only bone marrowderived or radioresistant cells. Such mice were inoculated with RV, treated with recombinant IL-22 or IL-18, and RV infection was monitored via measuring fecal RV antigens by ELISA. Figure 1 used a relatively low dose of cytokine that highlighted the cooperativity of IL-18 and IL-22, but successive experiments used fivefold higher doses to enable a robust effect that could be dissected via bone marrow chimeric mice. Mice that expressed the IL-22 receptor only in bone marrowderived cells were not protected from RV infection by treatment with IL-22 (Fig. 2A), whereas mice with IL-22 receptor only in radioresistant cells were almost completely protected by this cytokine (Fig. 2B). These results suggest that IL-22 protects mice from RV infection by acting on IEC, which are known to be populated from radioresistant stem cells and responsive to IL-22 (7). In accord with this notion, we observed that multiple IEC cell lines are responsive to IL-22 in vitro via STAT3 phosphorylation, although IL-22, like flagellin and IL-18, did not affect RV infection in vitro (fig. S2). Studies with IL-18-R chimeric mice similarly revealed that expression of this receptor in only bone marrowderived cells conferred only a modest nonsignificant reduction (12 3.8%) in the extent of RV infection upon IL-18 administration (Fig. 2C). In contrast, in mice that expressed IL-18-R in only radioresistant cells, IL-18 reduced extent of RV infection by 76 8.7% (Fig. 2D). Together, these results suggest that agonizing IL-18 and IL-22 receptors on IEC result in generation of signals that impede RV in vivo but not in vitro.
Indicated bone marrowirradiated chimeric mice were administered PBS (control), IL-22 (10 g), or IL-18 (2 g) via intraperitoneal injection, 2 hours before or 2, 4, 6, or 8 days after oral inoculation with mRV. Fecal RV levels were measured over time by ELISA. Differences between control and cytokine groups for each chimera/panel were analyzed by two-way ANOVA. (A) n = 7, P = 0.7715. (B) n = 4 and 7 for PBS and IL-22, respectively. (C) n = 7 and 6 for PBS and IL-18, respectively. (D) n = 4 and 6 for PBS and IL-18, respectively. * indicates significantly different from PBS by two-way ANOVA, P < 0.0001.
In cell culture and organoid models, IL-22 promotes IEC proliferation, migration, and stem cell regeneration (810), which together are thought to contribute to ability of IL-22 to promote healing in response to an array of insults, including exposure to radiation and dextran sodium sulfate in vivo (1114). In contrast to such severe injuries, RV infection is generally characterized by a lack of overt intestinal inflammation (15, 16). We hypothesized that IL-22 may promote IEC proliferation and/or migration that might reduce the extent of RV infection by increasing the rate of IEC turnover, especially near villus tips, which is the predominant site of RV infection (24). We further reasoned that IL-18 might trigger the same kind of response and further increase IEC proliferation and turnover. Mice were administered 5-bromo-2-deoxyuridine (BrdU) and treated with IL-22 and/or IL-18. Sixteen hours later, mice were euthanized, and intestines were subjected to fluorescence microscopy to measure rates at which IEC migrated toward villus tips (17). In accord with our hypothesis, administration of IL-22 approximately doubled the rate at which IEC migrated toward villus tips (Fig. 3, A and B). IL-18 administration also increased the rate of IEC migration to a lesser extent. The combination of these cytokines did not result in a faster rate of IEC migration relative to IL-22 alone. Epidermal growth factor (EGF) is known to promote IEC proliferation and migration (18, 19), so we tested whether this cytokine might protect against RV infection. In accord with EGF promoting proliferation in a variety of tissues, EGF treatment induced IEC migration up the crypt villus axis (Fig. 3, C and D), albeit not quite as robustly as IL-22 (1.43- versus 1.95-fold increase respectively). Moreover, EGF had the ability to reduce the extent of RV infection (Fig. 3E), but not as completely as IL-22. Together, these results support the hypothesis that IL-22 and IL-18 promote IEC replication and migration, which contributes to protection against RV infection.
Mice were intraperitoneally injected with PBS, IL-22, (10 g) IL-18 (2 g), both cytokines, or mEGF. One hour later, mice were administered BrdU. Mice were euthanized 16 hours after BrdU administration, and BrDU was visualized (A and C) and migration was measured (B and D) by microscopy and image analysis, respectively. Images shown in (A) and (C) are representative. Scale bar equals 50 m. For (B) and (D), sections were scored at least from 50 villus per group of mice (n = 5). Distance of the foremost migrating cells along the crypt-villus axis was measured with ImageJ software. Results are presented as means SEM. Statistical significance was evaluated by Students t test (****P < 0.0001). (E) Mice were intraperitoneally injected with PBS or EGF (10 g) mEGF 2 hours before or 2, 4, 6, or 8 days after oral inoculation with mRV. Fecal RV levels were measured over time by ELISA. Data are means SEM, n = 5 * indicates significantly different from PBS by two-way ANOVA, P < 0.0001.
We next considered how promoting IEC proliferation might impede RV infection. Increased extrusion of IEC into the lumen is a likely consequence of increased IEC proliferation/migration, which is thought to occur such that cells remain alive until extrusion is completed to preserve the gut barrier (20). We hypothesized that increased proliferation/migration induced by IL-22 and/or IL-18 treatments might result in increased extrusion of villus tip cells, which are the site of RV infection. We investigated this hypothesis using a previously described method (21) in which cross sections of hematoxylin and eosinstained pieces of ileum are examined for visual evidence of cell shedding. We were unable to consistently distinguish IEC from other luminal contents, so we visualized cells using the DNA stain. This approach suggested a greater presence of IEC in the lumen of mice treated with cytokines, particularly IL-22 (Fig. 4A), but it was difficult to quantitate such a difference via cell counting, so we sought to evaluate levels of host cells via quantitative polymerase chain reaction (qPCR) of 18S DNA in the ileum. The highly degradative environment of the intestine would likely degrade IEC shed into the lumen, but because such cells are extruded in a relatively intact state, their DNA might survive long enough to enable quantitation by qPCR. Small intestinal contents were extracted, and 18S DNA quantitated and expressed as number of cells per 100 mg of luminal content using known numbers of mouse epithelial cells to generate a standard curve. This approach indicated that IL-22 treatment markedly increased the level of IEC present in the lumen (Fig. 4B), suggesting increased IEC shedding. IL-18 induced only a modest level of IEC shedding that appeared to be additive to the shedding induced by IL-22. A generally similar pattern was observed in the cecum (Fig. 4C). In contrast, these cytokines did not affect levels of 18S DNA present in the lumen of the colon (Fig. 4D), perhaps reflecting that the impact of these cytokines on IEC shedding is specific to the ileum/cecum and/or that the DNA of shed IEC is quickly degraded in the bacterial-dense colon. An even greater amount of shedding of IEC into the ileum was induced by treating mice with flagellin, although two treatments of IL-18/22 could match this level, which suggested that production of these cytokines might be sufficient to recapitulate the IEC shedding induced by flagellin (Fig. 4E). The greater potency of flagellin may reflect ability of IL-18 and IL-22 to promote each others expression. Use of IL-22/ and IL-18/ mice revealed that these cytokines, both of which are necessary for flagellins anti-RV action (5), were both necessary for flagellin-induced cell shedding (Fig. 4F). Collectively, these results support the notion that increased extrusion of IEC, particularly in response to IL-22, might be central to this cytokines ability to impede RV infection, but these data did not offer insight into how IL-22 and IL-18 cooperate to offer stronger protection against this virus.
Mice [WT or indicated knockout (KO) strain] received a single (except where indicated otherwise) intraperitoneal injection of PBS, IL-22, (10 g), IL-18 (2 g), both cytokines or bacterial flagellin, FliC (15 g). Eight hours later, mice were euthanized, intestine was isolated, and luminal content was collected. (A) Microscopic appearance of DAPI-stained section to visualize shed cells in lumen. Scale bar equals 50 m. (B to F) Measurements of shed cells in different regions of the gastrointestinal tract via 18s by q-PCR (B, E, and F) small intestine, (C) cecum, (D) colon [double doses of IL-22 and IL-18 in (E) were 12 hours apart]. Data in (B) to (F) are means SEM (B), with significance assessed by Students t test, n = 5 to 15 mice as indicated by number of data points. *P < 0.05, **P < 0.01, ***P < 0.001, and ****P < 0.0001. n.s., not significant; SI, small intestine.
Next, we examined how IL-22 and IL-18 might affect IEC in the presence of an active RV infection. We used WT mice 3 days after inoculation with RV, a time approaching peak levels of RV shedding (Fig. 1A). RV-infected and uninfected mice were administered IL-22 and/or IL-18 and euthanized 6 hours later, and small intestinal content was isolated. Like IL-18/22 administration, RV infection up-regulated IEC extrusion, with a marked further increase in IEC extrusion being observed by administration of IL-18/22 to RV-infected mice (Fig. 5A). This suggests that increased IEC extrusion may normally contribute to innate defense against RV (2) and that exogenously administered IL-18/22 (or flagellin) may enhance this protective mechanism. Yet, like the case in uninfected mice, the promotion of IEC extrusion appeared to be driven by IL-22 and not IL-18 (Fig. 5B).
Mice were orally inoculated with mRV, or not(sham?) and were intraperitoneally injected at 3 dpi with PBS, IL-22, (10 g) IL-18 (2 g), or both cytokines. Mice were euthanized 6 hours later and following assays were carried out. (A and B) Assay of cell extrusion (i.e., measure of cells in lumen) as performed in response to cytokines in Fig. 4. (C and D) Assay cleaved caspase-3 in IEC was assayed by SDS-PAGE immunoblotting. (E and F) Visualization of cell death by TUNEL staining, counterstained with DAPI. (G) Quantitation of TUNEL-positive cells at villus tip region based on visual counts. Data in (A), (B), and (G) are means SEM. Panels (A) and (B) used five mice per condition to generate one value per mouse. Panel (G) used five mice per condition and assayed 6 to 10 villi per mouse, which are indicated by data points. Significance was determined by Students t test. *P < 0.05 and ****P < 0.0001.
Next, we sought to investigate events in IEC that remained part of the small intestine at the time of increased IEC extrusion. Specifically, we examined whether IL-18 and/or IL-22 might affect cell death. We observed that IL-18/22 or RV induced modest and variable induction of cleaved caspase-3. In contrast, administration of these cytokines to RV-infected mice induced marked elevations in cleaved caspase-3 (Fig. 5C). Caspase-3 cleavage was also observed in response to IL-18 but not IL-22 (Fig. 5D). Quantitation of cell death by terminal deoxynucleotidyl transferasemediated deoxyuridine triphosphate nick end labeling (TUNEL) yielded a similar pattern of results. Specifically, both IL-18/22 and RV by themselves resulted in a modest increase in TUNEL-positive cells, which appeared sporadically throughout the villi (Fig. 5E and fig. S3, A and B). In contrast, treating RV-infected mice with IL-18 or the combination of IL-18 and IL-22, but not IL-22 itself, resulted in notable TUNEL positivity at the villus tips (Fig. 5, E to G), known sites of RV infection. Cytokine-induced TUNEL positivity, which did not occur in the absence of RV, appeared to localize in the villus tip, where RV was localized before cytokine treatment, thus suggesting that IL-18 was promoting cell death in RV-infected cells (fig. S3C).
Cell death can occur via numerous pathways, so we hypothesized that IL-18induced cell death might occur via pyroptosis, which appears to be a frequent form of cell death for infected cells (22). In accord with this possibility, IL-18 administration to RV-infected mice results in cleaved gasdermin D (Fig. 6A), whose activity is essential for pyroptosis. To test the role of gasdermin D activation in IL-18induced cell death, we performed experiments in mice lacking gasdermin D and gasdermin E, the latter of which is thought to compensate for lack of gasdermin D in some scenarios. Our initial experiments found that gasdermin-deficient mice were highly resistant to RV infection (fig. S4). However, such resistance was associated with high levels of segmented filamentous bacteria (SFB), which we have recently shown drives spontaneous resistance to RV in Rag1/ mice (23). Cross-fostering on gasdermin-deficient mice removed SFB and restored susceptibility to RV infection, thus extending our recent findings to mice with functional adaptive immunity. This model could also address if the IL-18induced cell death that associates with clearance of RV is mediated by pyroptosis. IL-18 administration did not induce cleaved gasdermin D in mice lacking this gene (Fig. 6A), thus verifying the specificity of the antibody we used. IL-18induced cell death of RV-infected mice proceeded at least as robustly as had been observed in WT mice (Fig. 6B). Specifically, although gasdermin-deficient mice had mild elevations in basal caspase-3, they still up-regulated this caspase in response to IL-18, albeit at markedly lower levels compared with WT mice. IL-18 induced marked TUNEL positivity in these mice (Fig. 6, C and D) and fully protected gasdermin-deficient mice against RV infection (Fig. 6E). These results argue that IL-18induced cell death and associated clearance of RV are not mediated by pyroptosis.
(A to D) Gasdermin-deficient, or WT, mice were administered PBS or IL-18 (2 g) 3 days after mRV inoculation. Mice were euthanized 6 hours later and jejunums were analyzed. (A and B) IEC were analyzed by SDS-PAGE immunoblotting for detection of gasdermin D, cleaved gasdermin D, and cleaved caspase-3, respectively. (C) Cell death by TUNEL, counterstained with DAPI. (D) Quantitation of TUNEL-positive cells at villus tip region based on visual counts. Experiments included five mice per condition. Data in (D) was based on assay 6 to 8 villi per mouse, which are indicated by data points ****P < 0.0001 by Students t test. (E) Gasdermin-deficient mice were administered PBS or IL-18 (2 g) via intraperitoneal injection, 2 hours before, or 2, 4, 6 or 8 days after (indicated by arrows), oral inoculation with mRV. Fecal RV levels were measured over time by ELISA. Data are means SEM. n = 5. * indicates significantly different from control by two-way ANOVA, P < 0.0001.
We examined the extent by which IL-22induced IEC extrusion and IL-18induced IEC death were associated with RV reduction in the ileum at 6 and 24 hours after administration of these cytokines. We measured the levels of RV genomes and the ratio of positive to negative (+/) RV strands in both the lumen and IEC, which reflects levels of active replication because most positive strands encode RV proteins and do not get incorporated into virions (24). In accord with our previous work, we observed that, in the epithelium, both IL-22 and IL-18 led to a clear reduction in both the level of RV genomes and RV replication by 6 hours (Fig. 7, A and B). In contrast, the small intestinal lumen had a marked but variable increase in the level of RV genomes and a stark increase in RV +/ strand ratios 6 hours after administration of IL-18 with the combination of IL-18 and IL-22 but not IL-22 alone (Fig. 7, C and D). By 24 hours, levels of RV in the lumen had dropped markedly, whereas the miniscule levels of remaining virus appeared to not be actively replicating (Fig. 7, E and F). Collectively, these results support a model wherein IL-18induced cell death interrupts active RV replication, spewing incompletely replicated virus into the lumen while IL-22 induces IEC migration and subsequent extrusion of the mature IEC that RV targets, thus together working in concert to resolve RV infection.
mRV-infected mice were intraperitoneally injected with PBS, IL-22 (10 g), IL-18 (2 g), or both cytokines on day 3 post-mRV inoculation. Six or 24 hours later, mice were euthanized, and contents of jejunums were isolated. RNA was extracted and used to measure of mRV genomes and replication status as reflected by NSP3 RNA levels and the ratio of NSP3 (+) RNA strand to complimentary NSP3 () RNA strand. (A and B) The overall mRV genome and efficacy of virus replication in small intestinal epithelial cells. (C to F) The overall mRV genome and efficacy of virus replication in luminal content from small intestine (one-way ANOVA, n = 5 to 10, *P < 0.05, **P < 0.01, ***P < 0.001, and ****P < 0.0001).
The central focus of this study was to determine the mechanisms by which IL-18 and IL-22, which are elicited by bacterial flagellin, contribute to preventing or curing RV infection. We initially considered that the ability of IL-18 and IL-22 to promote each others expression allowed them to use a shared mechanism to promote RV clearance. We found that irrespective of such mutual promotion, IL-18 and IL-22 both impeded RV independent of each other and did so by distinct mechanisms, which is illustrated in Fig. 8. Specifically, IL-22 drove IEC proliferation and migration toward villus tips, thus accelerating the ongoing process of extrusion of highly differentiated IEC at the major site of RV replication. In contrast, administration of IL-18 to RV-infected mice induced rapid cell death, as defined by TUNEL, at villus tips where RV is localized. Such induction of TUNEL positivity, which is not typically seen at significant levels in the intestine, was associated with rapid abortion of the RV replication cycle followed by a marked reduction of RV antigens in the intestinal tract. These actions of IL-22 and IL-18 together resulted in rapid and complete expulsion of RV, thus providing a mechanism that explains how this combination of cytokines prevents and cures RV infection.
IL-22 increases epithelial proliferation thus increasing extrusion of epithelial cells, including RV-infected cells. Into lumen the intestinal lumen, i.e., anoikis. IL-18 induces rapid cell death, associated with loss of cell rupturing of RV-infected cells.
RV does not induce detectable increases in IL-22 expression nor does genetic deletion of IL-22 appear to markedly augment RV infection (5), thus arguing that IL-22 does not normally play a major role in clearance of this pathogen. The known cooperation of IL-22 and interferon- in activating antiviral gene expression (3) suggests the possibility that RV may have evolved strategies to deliberately avoid or block IL-22 induction. Nonetheless, the downstream action of IL-22, particularly its promotion of IEC turnover, may be shared by endogenous anti-RV host defense mechanisms. The role of adaptive immune-independent host defense against RV is most easily appreciated in immune compromised mice wherein RV loads decline markedly from their peak levels, but it may also play a role in protecting against RV even in immune competent mice. Innate host defense against RV is likely multifactorial and may involve type III interferon (3), particularly in neonate mice. Our observations in adult mice indicate that RV infection increases IEC extrusion, and this mechanism combined with previous observations that RV infection activates intestinal stem cell proliferation suggests that increased IEC turnover may limit RV infection (2). We do not think that such a mechanism is necessarily unique to IL-22 as EGF has ability to drive similar events. Moreover, we recently showed that SFB also drives enterocyte proliferation independent of IL-22 and is not required for adaptive immunity (23). Hence, we presume that IL-22 can activate a primitive mechanism of host defense against a variety of challenges, especially those affecting IEC.
IEC are rapidly proliferating cells with average lifetimes of about 3 days (24), which means that the intestine must eliminate vast numbers of cells continuously. The overwhelming majority of IEC are eliminated via cell extrusion at villus tips through a process termed anoikis. A central tenet of anoikis is that cells remain alive at the time of extrusion followed by the lack of attachment to other cells resulting in induction of a programmed death process (25). A key aspect of this process is that cells can be eliminated without comprising gut barrier function, thus avoiding infection and inflammation that might otherwise occur. Accordingly, administration of IL-22 is associated with few adverse effects and has been shown to resolve inflammation in several different scenarios. (26). Moreover, IL-22 plays a broad role of maintaining gut health in the intestinal tract, including mediating microbiota-dependent impacts of dietary fiber (27). It is possible that increasing anoikis via IL-22 results in extrusion of RV-containing cells in a manner that prevents viral escape and, consequent infection of other IEC. However, inability of IL-22 to induce detectable increases in luminal RV argues against this possibility. Rather, we envisage that the cell death process after IEC extrusion might result in destruction of RV in these cells. We also hypothesize that the accelerated IEC turnover induced by IL-22 may result in villus IEC being less differentiated and less susceptible to RV infection. In accord with this possibility, we observed that that flagellin administration resulted in an IL-22dependent increase in CD44+26 IEC (fig. S5), which are known to be RV resistant (28). It is difficult to discern the relative importance of IL-22 in the induction of IEC extrusion versus its impact on differentiation state of villus IEC. IL-22induced reduction in RV levels in chronically infected Rag-1/ mice occurs over a course of several days that supports a role for the latter mechanism. Use of IL-22 receptor bone marrow chimera mice demonstrated that IL-22 acts directly on IEC to affect RV infection. (7). IL-22induced signaling is generally thought to be mediated by STAT3 (5, 10), and IL-22 induced phosphorylation of STAT3 in IEC in vivo. However, we observed that IEC-specific STAT3-knockout mice could still be protected against RV by IL-22, suggesting that this mechanism of action may not proceed by a characterized signaling mechanism (fig. S6). Thus, how the IL-22 receptor signals to affect IEC phenotype remains incompletely understood.
In contrast to IL-22, recent work indicates that induction of IL-18 plays a role in endogenous immunity against RV, wherein caspase-1mediated IL-18 production results from activation of the NLR9pb inflammasome. Such IL-18 induction paralleled gasdermin-dependent cell death, the absence of which resulted in delayed clearance of RV (29, 30). On the basis of this work, we hypothesized that exogenously administered IL-18 might enhance RV-induced death of RV-infected cells and/or increase IEC turnover analogous to IL-22. Administration of IL-18 in the absence of RV elicited a modest increase in the number of TUNEL-positive cells as well as a modest increase in IEC proliferation/migration that was not accompanied by increased IEC extrusion, suggesting the increased proliferation compensated for cell death. However, TUNEL-positive cells were scattered along the villus. In RV-infected mice, IL-18 led to TUNEL-positive cells at the villus tips, which is also the primary site of RV infection. It is tempting to envisage localized impacts of IL-18 reflect the pattern of expression of the IL-18 receptor, including localization to villus tips and/or induced by RV, but limited knowledge of the determinants of its expression and lack of available reagents to study it render these ideas as speculative.
The manner of IL-18induced cell death, namely, its notable TUNEL induction, which was associated with spewing of RV replication intermediates, suggested pyroptotic cell death. However, we found that lack of gasdermin D and E, which are thought to be essential for pyroptosis, did not impede IL-18induced cell death in RV-infected cells thus arguing such cell death does not fit perfectly into any known cell death pathways. Induction of IL-18 receptor-mediated signaling by itself is not sufficient to induce cell death in villus tip epithelial cells but triggers death in cells primed as a result of RV infection. The nature of such priming is not understood but may involve IEC signaling pathways, including NLR9pb, TLR3, and RNA-activated protein kinase, which are capable of recognizing RV components and/or responding to intracellular stress in general (3032). In this context, the ability of IL-22 to enhance IL-18induced TUNEL positivity in RV-infected cells may reflect an intersection of IL-22-R and IL-18-R signaling or be a manifestation of these cytokines to promote each others expression.
The central limitation in our study was that our approaches were largely correlative. Specifically, we lacked modalities to specifically block IEC migration or cell death in response to IL-22 and IL-18, respectively. Another limitation is that we were not able to demonstrate that the TUNEL-positive cells actually contained RV. Our attempts to do so via double-staining were not successful, possibly reflecting that the disappearance of RV after cytokine treatment likely occurs early in the cell death process while the DNA fragmentation that underlies TUNEL positivity is considered a late event in the cell death process. Thus, more specific identification of processes that mediate cell death of RV-infected IEC in response to IL-18 is an important target of future studies.
The improved understanding of the mechanism by which IL-18/22 controls RV infection reported herein should inform use of these cytokines to treat viral infection in humans. Chronic RV infections can occur in immune compromised humans, suggesting that IL-18/22 may be explored as a possible treatment for this and other chronic viral infections. Our results suggest that this cytokine treatment may be effective for viruses that preferentially infect villus epithelial cells and possibly other epithelia that have high cell turnover rates. In contrast, this combination of cytokines seems unlikely to affect viruses that inhabit more long-lived cells, including hematopoietic cells that are generally not responsive to IL-22. We observed that flagellin and IL-18/22 has some efficacy against reovirus, particularly early in infection when it infects gut epithelial cells, as well as some efficacy against influenza, which initially infects lung epithelial cells, but did not show any impact on hepatitis C virus as assayed in mice engrafted with human hepatocytes, which are thought to be long-lived cells. IL-18/22 can protect mice against norovirus infection, which infects B cells and tuft cells (33, 34), but human norovirus is thought to primarily infect epithelial cells, particularly in immunocompromised persons who develop chronic norovirus infections (35). SARS-CoV-2, the causative agent of coronavirus disease 2019 (COVID-19) has also been observed to replicate in IEC (36), and like RV, appears to replicate in mature IEC, which express the SARS-CoV-2 receptor angiotensin-converting enzyme 2. Intestinal replication of SARS-CoV-2 is thought to contribute to extrarespiratory pathologies associated with COVID-19 (37). As such, the use of IL-18/22based therapy may be a potential strategy to treat chronic RV and/or norovirus infections in person with immune dysfunction and, moreover, might serve to mitigate severe cases of COVID-19.
This study sought to ascertain the mechanism by which IL-22 and IL-18 prevent and cure RV infection. Mice were orally administered RV. Extent of infection was assayed my measuring viral genomes and proteins in the intestine. IL-18 and or IL-22 were administered to mice with various genetic deficiencies. Cell extrusion and cell death were measured. All procedures involving mice were approved by GSUs animal care and use committee (Institutional Animal Care and Use Committee no.17047).
All mice used herein were adults (i.e., 4 to 8 weeks old) on a C57BL/6 background bred at Georgia State University (GSU) (Atlanta, GA). RV-infected mice were housed in an animal biosafety level 2 facility. WT, Rag-1/, IL-18/, IL-18-R/, Stat3flox, and Villin-cre were purchased from the Jackson laboratory (Bar Harbor, ME, USA). NLRC4/, IL-22/, and IL-22-R/ mice were provided by Genentech (South San Francisco, CA, USA). TLR5/ and TLR5//NLRC4/ and WT littermates were maintained as previously described (5). Gasdermin D/E/ mice, whose generation and initial characterization were previously described (22), were shipped to GSU and studied in original and cross-fostered state as indicated in results.
Murine Fc-IL-22 was provided by Genentech Inc. Murine IL-18 was purchased from Sino Biological Inc. (Beijing, China). Procedures for isolation of flagellin and verification of purity were described previously (5). Recombinant murine EGF (mEGF) was purchased from PeproTech.
Age- and sex-matched adult mice (8 to 12 weeks of age) were orally administered 100 l of 1.33% sodium bicarbonate (Sigma-Aldrich) and then inoculated with 105 SD50 of murine RV EC strain. Approach used to determine SD50 has been described previously (5).
Five-week-old Rag-1/ mice were infected with murineRV (same infection procedure as described in the Acute models section). Feces were collected 3 weeks after RV inoculation to confirm the establishment of chronic infection.
Cell culture-adapted rhesus RV (RRV) was trypsin-activated [trypsin (10 g/ml)] in serum-free RPMI-1640 (cellgro) at 37C for 30 min. The basolateral side of the polarized Caco-2 cells was stimulated with cytokines, 1.5 hours before expose to RRV infection as previously described (5). The upper chamber of transwells was infected with trypsin-pretreated RRV and allowed to adsorb at 37C for 40 min before being washed with serum-free medium. The presence of cytokines was maintained at a constant level throughout the experiment.
Fecal pellets were collected daily from individual mouse on days 0 to 10 after RV inoculation. Samples were suspended in phosphate-buffered saline (PBS) [10% (w/v)], after centrifugation, supernatants of fecal homogenates were analyzed by ELISA, and after multiple serial dilutions, more detailed descriptions of experimental procedures are previously described (5).
Mice were subjected to x-ray irradiation using an 8.5 gray (Gy) equivalent followed by injection of 2 107 bone marrow cells administered intravenously as previously described (5). All mice were afforded an 8-week recovery period before experimental use. For the first 2 weeks after transfer, mice were maintained in sterile cages and supplied with drinking water containing neomycin (2 mg/ml) (Mediatech/Corning).
Intestinal sections were fixed in methanol-Carnoys fixative solution (60% methanol, 30% chloroform, and 10% glacial acetic acid) for 48 hours at 4C. Fixed tissues were washed two times in dry methanol for 30 min each, followed by two times in absolute ethanol for 20 min each, and then incubated in two baths of xylene before proceeding to paraffin embedding. Thin sections (4 m) were sliced from paraffin-embedded tissues and placed on glass slides after floating on a water bath. The sections were dewaxed by initial incubation at 60C for 20 min, followed by two baths in prewarmed xylene substitute solution for 10 min each. Deparaffinized sections were then hydrated in solutions with decreasing concentration of ethanol (100, 95, 70, 50, and 30%) every 5 min in each bath. Last, slides allowed to dry almost completely and were then mounted with ProLong antifade mounting media containing 4,6-diamidino-2-phenylindole (DAPI) before analysis by fluorescence microscopy.
Intestinal sections were fixed in 10% buffered formalin at room temperature for 48 hours and then embedded in paraffin. Tissues were sectioned at 4 m thickness, and IEC death was detected by TUNEL assay using the In Situ Cell Death Detection Kit, Fluorescein (Roche) according to the manufacturers instructions.
IECs lysate (20 g per lane) was separated by SDSpolyacrylamide gel electrophoresis through 4 to 20% Mini-PROTEAN TGX gel (Bio-Rad, USA), transferred to nitrocellulose membranes, and analyzed by immunoblot, as previously described (5). Briefly, isolated IEC was incubated with radioimmunoprecipitation assay lysis buffer (Santa Cruz Biotechnology, USA) for 30 min at room temperature. Subsequently, cell lysates were homogenized by pipette and subjected to full-speed centrifugation. Protein bands were detected for cleaved caspase-3, phosphor-STAT3, and anti-actin (Cell Signaling Technology) and incubated with horseradish peroxidaseconjugated anti-rabbit secondary antibody. Immunoblotted proteins were visualized with Western blotting detection reagents (GE Healthcare) and then imaged using the ChemiDoc XRS+ system (Bio-Rad).
The entire small intestine was harvested from mice according to indicated experimental design and sliced longitudinally before being washed gently in PBS to remove the luminal content. Tissues were processed and maintained at 4C throughout. Cleaned tissue samples were further minced into 1- to 2-mm3 pieces and shaken in 20 ml of Hanks balanced salt solution (HBSS) containing 2 mM EDTA and 10 mM Hepes for 30 min. An additional step of vigorous vortexing in fresh HBSS (10 mM Hepes) after EDTA incubation facilitated cell disaggregation. IECs were then filtered through 70-m nylon mesh strainer (BD Biosciences), centrifuged, and resuspended in PBS.
Bulk leukocytes and IECs isolated above were incubated with succinimidyl esters (NHS ester)Alexa Fluor 430, which permitted determination of cell viability. Cells were then blocked by incubation with anti-CD16/anti-CD-32 (10 g/ml) (clone 2.4G2, American Type Culture Collection). Twenty minutes later, cells were stained with fluorescently conjugated antibodies: CD26-PE (clone H194-112, eBioscience), CD44-PECy7 (clone IM7, eBioscience), CD45fluorescein isothiocyanate (clone, 30-F11, eBioscience), and CD326-allophycocyanin (clone G8.8, eBioscience). Last, stained cells were fixed with 4% formaldehyde for 10 min before whole-cell population was analyzed on a BD LSR II flow cytometer. Collected data were analyzed using FlowJo.
Host DNA was quantitated from 100 mg of luminal content (100 mg) from small intestine by using the QIAamp DNA Stool Mini kit (Qiagen) and subjected to qPCR using QuantiFast SYBR Green PCR kit (Bio-Rad) in a CDX96 apparatus (Bio-Rad) with specific mouse 18S oligonucleotides primers. The sense and antisense oligonucleotides primers used were: 18s-1F: 5-GTAACCCGTTGAACCCCATT-3 and 18s-1R: 5-CCATCCAATCGGTAGTAGCG-3. PCR results were expressed as actual numbers of IEC shedding per 100 mg of luminal content, calculated using a standard curve, which was generated using twofold serial dilutions of mouse colon carcinoma cell line MC26. DNA was extracted from each vial with known number of MC26 cells after serial dilutions, and then real-time qPCR was performed. The cycle quantification (Cq) values (x axis) are inversely proportional to the amount of target genes (18S) (y axis), and a standard curve is applied to estimate the numbers of cell shedding from luminal content based on the quantity of target copies (18S) from each sample.
To extract RNA, cell pellets were homogenized with TRIzol (Invitrogen), and chloroform was added to the homogenate to separate RNA (an upper aqueous layer) from DNA and proteins (a red lower organic layer). Isopropanol facilitated the precipitation of RNA out of solution, and after centrifugation, the impurities were removed by washing with 75% ethanol. RNA pellets were resuspended in ribonuclease-free water and underwent quantitative reverse transcription PCR. Total RNA from luminal content was purified from the RNeasy PowerMicrobiome Kit according to the manufacturers instructions. Primers that target non-structural protein 3 region: EC.C (+) (5-GTTCGTTGTGCCTCATTCG-3 and EC.C () (5-TCGGAACGTACTTCTGGAC-3) were applied to quantify viral genomes from IEC and luminal content. RV replication was quantitated as previously described (38).
A pulse-chase experimental strategy was used to label intestinal enterocytes with BrdU to estimate the IEC migration rate along the crypt-villus axis over a defined period of time. Briefly, 8-week-old mice were intraperitoneally injected with either PBS or cytokine(s) (IL-22 and/or IL-18) 1 hour before BrdU treatment (50 g/mg of mice body weight, ip). After 16 hours, mice were euthanized, and a segment of the jejunum were resected, immediately embedded in optimal cutting temperature compound (OCT) (Sigma-Adrich) and then underwent tissue sectioning. Tissue sections (4 m) were firstly fixed in 4% formaldehyde for 30 min at room temperature and then washed three times in PBS. DNA denaturation was performed by incubating the sections in prewarmed 1.5 N HCl for 30 min at 37C, and then acid was neutralized by rinsing sections three times in PBS. Before BrdU immunostaining, sections were blocked with rabbit serum (BioGenex, Fremont, CA) for 1 hour at room temperature, then incubated with anti-BrdU (Abcam) 2 hours at 37C, and counterstained with DAPI. The BrdU-labeled cells were visualized by fluorescence microscopy.
The proximal jejunum was imbedded into OCT compound, and then sliced into 6-m-thin sections. Tissue slides were incubated in 4% paraformaldehyde for 15 min, followed by 5 min washing of PBS twice. Autofluorescence caused by free aldehydes was quenched by incubating slides in 50 mM NH4Cl in PBS or 0.1 M glycine in PBS for 14 min at room temperature, followed by 5 min PBS washing three times. Bovine serum albuminPBS (3%) was used to block the tissue samples for 1 hour at room temperature. The slides were then washed with PBS for 5 min, followed by incubation with primary antibody (1:100; hyperimmune guinea pig anti-RRV serum) in blocking buffer overnight at 4C. After slides were washed three times with PBS, secondary antibody (donkey antiguinea pig immunoglobulin G, Jackson ImmunoResearch, 706-586-148) was applied to the sample slides for 1 to 2 hours at room temperature. The fluorescence emission of mRV antigen was detected by fluorescence microscopy.
Significance was determined using the one-way analysis of variance (ANOVA) or students t test (GraphPad Prism software, version 6.04). Differences were noted as significant *P < 0.05, **P < 0.01, ***P < 0.001, and ****P < 0.0001.
Funding: This work was supported by NIH grants DK083890 and DK099071 (to A.T.G.). J.Z. is supported by career development award from American Diabetes Association. B.C. is supported by a Starting Grant from the European Research Council, an Innovator Award from the Kenneth Rainin Foundation, and a Chaire dExcellence from Paris University. Author contributions: Z.Z. led performance of all experiments. J.Z. and Z.S. helped with specimen analysis. B.Z., L.E.-M., Y.W., and B.C. advised in experimental design and data interpretation. X.S. and F.S. provided advice and key reagents. A.G. helped design study and drafted manuscript. Competing interests: A.T.G. and B.Z. are inventors on patent application (WO2015054386A1 WIPO) held by GSU that covers Prevention and treatment of rotavirus infection using IL-18 and IL-22. Data and materials availability: All data needed to evaluate the conclusions in the paper are present in the paper or the Supplementary Materials. All mice are either commercially available or available under a material transfer agreement.
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