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. Author manuscript; available in PMC: 2015 May 1.
Published in final edited form as: Mucosal Immunol. 2014 Mar 26;7(6):1312–1325. doi: 10.1038/mi.2014.19

NOD2 Down-Regulates Colonic Inflammation by IRF4-Mediated Inhibition of K63-Linked Polyubiquitination of RICK and TRAF6

Tomohiro Watanabe 1,2,3,*, Naoki Asano 2,4,*, Guangxun Meng 2, Kouhei Yamashita 5, Yasuyuki Arai 5, Toshiharu Sakurai 6, Masatoshi Kudo 6, Ivan J Fuss 2, Atsushi Kitani 2, Tooru Shimosegawa 4, Tsutomu Chiba 3, Warren Strober 2
PMCID: PMC4177019  NIHMSID: NIHMS569678  PMID: 24670424

Abstract

It is well established that polymorphisms of the nucleotide-binding oligomerization domain 2 (NOD2) gene, a major risk factor in Crohn's disease (CD), lead to loss of NOD2 function. However, a molecular explanation of how such loss of function leads to increased susceptibility to CD has remained unclear. In a previous study exploring this question we reported that activation of NOD2 in human dendritic cells by its ligand, muramyl dipeptide (MDP) negatively regulates Toll-like receptor (TLR)-mediated inflammatory responses. Here we show that NOD2 activation results in increased interferon regulatory factor 4 (IRF4) expression and binding to TNF receptor associated factor 6 (TRAF6) and receptor interacting serine-threonine kinase (RICK). We then show that such binding leads to IRF4-mediated inhibition of Lys63-linked polyubiquitination of TRAF6 and RICK and thus to down-regulation of NF-κB activation. Finally, we demonstrate that protection of mice from the development of experimental colitis by MDP or IRF4 administration is accompanied by similar IRF4-mediated effects on polyubiquitination of TRAF6 and RICK in colonic lamina propria mononuclear cells. These findings thus define a mechanism of NOD2-mediated regulation of innate immune responses to intestinal microflora that could explain the relation of NOD2 polymorphisms and resultant NOD2 dysfunction to CD.

Introduction

Nucleotide-binding oligomerization domain 2 (NOD2) is a NLR family member that functions as an intracellular sensor of small peptides (such as muramyl dipeptide, MDP) derived from the peptidoglycan (PGN) component of the bacterial cell wall 1, 2. Activation of NOD2 occurring upon sensing of its ligand through its leucine rich repeat domain is followed by NOD2 oligomerization and exposure of its caspase activation and recruitment domain (CARD). This enables a physical interaction between NOD2 and a downstream adaptor molecule, receptor interacting serine-threonine kinase (RICK) that then results in lysine 63 (K63)-linked polyubiquitination of RICK 1-3. Ubiquitinated RICK then interacts with TGF-β-activated kinase 1 and TNF receptor associated factor 6 (TRAF6) to cause nuclear translocation of NF-κB subunits 4-8.

The functional importance of NOD2 is underscored by the fact that polymorphisms in the CARD15 gene encoding NOD2 are associated with Crohn's disease and other immune disorders such as graft versus host disease 1, 2, 9. However, despite extensive investigation, the molecular mechanisms by which such polymorphisms contribute to these diseases are not completely understood 1, 9. A possible clue to the nature of these mechanisms comes from the fact that MDP activation of NOD2 can both positively and negatively regulate Toll-like receptor (TLR)-mediated inflammatory responses. For example, synergistic production of pro-inflammatory cytokine responses has been observed in human antigen-presenting cells (APCs) upon simultaneous stimulation of MDP and TLR ligands 10, 11. This synergism could contribute to the control of the gastrointestinal commensal microflora that is necessary for the prevention of Crohn's disease 12.

However, the above described capacity of NOD2 activation to augment innate immune responses is accompanied by the fact that such activation also has a negative effect on TLR signaling. Thus, we and others have shown that pre-activation of NOD2 by MDP induces decreased pro-inflammatory cytokine responses in human APCs upon subsequent challenge with TLR ligands 13-17. In addition, Hedl et al. have shown that such tolerogenic responses were not observed in human APCs from patients bearing Crohn's-disease-associated NOD2 mutations 15-17. We have also found that systemic injection of MDP protects NOD2-intact mice from experimental colitis, but not NOD2-or RICK-deficient mice 6, 14, 18. Collectively, these data support the idea that MDP activation of NOD2 down-regulates innate immune responses to intestinal microflora and thus suggest that the absence of such regulation leads to increased susceptibility to Crohn's disease.

In a previous study of the molecular mechanisms underlying NOD2 regulation of TLR response, we showed that MDP activation of NOD2 induces interferon regulatory factor 4 (IRF4) in human dendritic cells (DCs) and that such induction is necessary for the negative regulation of subsequent TLR-induced pro-inflammatory responses 14. In this study, we report that following NOD2 activation, IRF4 interacts with myeloid differentiation factor 88 (MyD88), TRAF6, and RICK and down-regulates K63-linked polyubiquitinylation of RICK and TRAF6; this, in turn, disrupts NOD2- and TLR-MyD88-induced NF-κB activation pathways, respectively. Thus, IRF4 function initiated by NOD2 activation provides new insight into how NOD2 influences colitis and why loss-of-function NOD2 polymorphisms serve as a risk factor in Crohn's disease.

Results

Physical interactions between IRF4 and MyD88, RICK, and TRAF6 in human DCs

In a previous study 14, we showed that NOD2 pre-stimulation of human DCs results in inhibition of subsequent TLR-induced cytokine responses and that such inhibition requires the up-regulation of IRF4. As for the mechanism of this IRF4 effect, we found in over-expression studies that NOD2 down-regulation of TLR-mediated NF-κB activation is associated with IRF4 interaction with MyD88, RICK, and TRAF6; thus it appeared that IRF4 was interfering with TLR signaling in some manner.

In the present study we addressed the molecular basis of this NOD2-IRF4 inhibitory mechanism by first assessing NOD2-induced IRF4 physical interaction with RICK, MyD88, and TRAF6 in human DCs under physiologic conditions. For this purpose, DCs derived from healthy control peripheral blood monocytes (obtained by culturing the latter in the presence of GM-CSF and IL-4) were pre-stimulated with MDP for 24 hours and then re-stimulated with MDP or lipopolysaccharide (LPS). As shown in Figure 1A, MDP pre-stimulation (designated in Figure 1 as 1st stimulation) up-regulated endogenous IRF4 expression in human DCs without altering their constitutive expression of RICK, MyD88, or TRAF6.

Figure 1. IRF4 expression induced by MDP activation of NOD2 and interaction between IRF4 and RICK, TRAF6, and MyD88.

Figure 1

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(A) Monocytes isolated from healthy individuals were cultured in the presence of GM-CSF and IL-4 for 6 days to generate monocyte-derived dendritic cells (DCs). DCs (1×106/ml) were pre-treated with MDP (10 μg/ml) for 24 hours followed by stimulation with MDP (10 μg/ml) or LPS (1 μg/ml) for 30 minutes; whole cell lysates were subjected to immunoprecipitation (IP) with the indicated Ab followed by immunoblotting (IB) with the indicated Ab. The arrow shows TRAF6-specific bands. (B) Human DCs were treated as described in (A). Interaction between IRF4 and RICK, TRAF6, and MyD88 was visualized in immunofluorescence microscopy by the Duolink assay. Magnification x800. Results shown are representative of at least two experiments.

Accompanying studies in which immunoprecipitation (IP) followed by immuno-blotting (IB) was performed to assess signaling component interactions revealed that MDP pre-stimulation enhanced IRF4 binding to RICK, especially when it was accompanied by MDP re-stimulation. In addition, IRF4 binding to TRAF6 was barely seen in un-stimulated cells or cells stimulated with MDP or LPS without pre-stimulation, but was clearly evident in cells pre-stimulated with MDP especially when such pre-stimulation was followed by re-stimulation with MDP or LPS. Finally, IRF4 binding to MyD88 was increased in cells pre-stimulated with MDP and re-stimulated with LPS.

To verify the above IP-IB studies of interactions between IRF4 and various binding molecules in cells subjected to MDP stimulation we employed the Duolink assay which allows fluorescent visualization of interacting proteins 19. As shown in Figure 1B, an IRF4-RICK complex was generated both in cells pre-stimulated with MDP and re-stimulated with MDP or LPS. In addition, IRF4-TRAF6 and IRF4-MyD88 complexes were generated in cells pre-stimulated with MDP and re-stimulated with either MDP or LPS, particularly the latter. Thus, both the IP-IB and Duo-link assays reveal enhanced interactions between IRF4 and RICK, MyD88, TRAF6 in human primary DCs pre-stimulated with MDP.

As also shown in Figure 1A, MDP pre-stimulation of cells was associated with reduced expression of phospho-IκBα and degradation of IκBα. Thus, the enhanced interaction between IRF4, RICK, and MyD88 in MDP pre-stimulated human DCs is associated with down-regulation of the NF-κB signaling pathway.

IRF4 with mutations at two known phosphorylation sites is capable of both RICK-IRF4 interaction and IRF4 negative regulation

Since RICK is a serine-threonine kinase, NOD2 activation of RICK could be regulating IRF4 function by enhancing RICK phosphorylation of IRF4. To investigate this possibility we first determined the ability of RICK mutated at K47 (K47A) and/or S176 (S176A), sites previously shown to be necessary for RICK kinase activity20, 21. As shown in Figure 2A, binding of IRF4 to RICK (in proportion to RICK expression) was observed in 293 cells after the transfection of FLAG-tagged IRF4 along with RICK mutants lacking kinase activity.

Figure 2. Phosphorylation of IRF4 is not necessary for its negative regulatory activity.

Figure 2

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(A) 293 cells were transfected with vectors expressing FLAG-tagged IRF4 and several forms of mutated RICK. Whole cell lysates were isolated 48 hours after the transfection and were subjected to immunoprecipitation (IP) with the indicated Ab followed by immunoblotting (IB) with the indicated Ab. (B) 293 cells were transfected with vectors expressing either wild type-IRF4 (Wt-IRF4) or Mutated-IRF4 (Mut-IRF4) in which serine residues at 447 and 448 are replaced with alanine; whole cell lysates were isolated 48 hours after transfection and were subjected to IP with anti-V5 Ab followed by IB with the indicated Ab. (C) HT29 cells were transfected with either empty control vector, Wt-IRF4 or Mut-IRF4 expressing vector together with RICK expressing vector, NF-κB luciferase reporter vector and pSV-β-galactosidase vector. The cells were then cultured for 24 hours after which relative luciferase activity values were calculated. Results are expressed as mean ± SD. **P<0.01, as compared with cells transfected with RICK vector alone. # P<0.01. (D) THP1 cells were transfected with either empty control (con) vector, wt-IRF4 or mut-IRF4 vector. The cells were then stimulated with LPS or Pam3CSK4 (PAM) for 24 hours after which culture fluids were analyzed for cytokine concentration by ELISA. NS; no stimulation. Results were expressed as mean ± SD. *P<0.05, **P<0.01, as compared with control vector. # P<0.01. Results shown are representative of at least two experiments.

In related studies, we determined the ability of IRF4 mutated at both S447 (S447A) and S448 (S448A), potential serine phosphorylation sites previously shown to be necessary for IRF4 function in relation to IL-21 regulation, to bind to RICK 22. As shown in Figure 2B, both wild type IRF4 and mutated IRF4 bound to RICK in 293 cells over-expressing V5-tagged RICK and FLAG-tagged IRF4. Thus, phospholylation of IRF4 at these two potential phosphorylation sites were not required for the interaction between RICK and IRF4.

Finally, to assess the capacity of IRF4 lacking two serine phosphorylation sites to regulate NF-κB activity we transfected plasmids expressing either wild type or mutated IRF4 into HT-29 cells (i.e., non-hematopoietic cells not likely to express endogenous IRF4 23) co-transfected with a RICK-expressing plasmid as well as an NF-κB luciferase reporter-expressing plasmid. As shown in Figure 2C, transfection with mutated IRF4 led to a significant reduction in RICK activation of NF-κB as compared to that of wild type (WT) IRF4. In complementary studies to address the same question in TLR-stimulated cells, we transfected either wild type or mutated IRF4 into human THP1 cells, which lack expression of IRF4 either before or after stimulation with MDP as shown in our previous study 14, and then cultured the cells with TLR2 ligand (Pam3CSK4, PAM) or TLR4 ligand (LPS) to determine their capacity to produce NF-κB-dependent cytokines. As shown in Figure 2D, transfection of mutated IRF4 into THP1 cells led to a significant decrease in TLR2 induction of IL-12p40 as compared to that of WT IRF4. Thus, these data provide evidence that loss of potential serine phosphorylation sites enhances increased IRF4-mediated negative regulation of NF-κB activation and its down-stream effect on cytokine production.

IRF4 regulates Lys63-linked polyubiquitination of RICK

TLR and NLR activation of NF-κB requires Lysine 63 (K63)-polyubiquitination of signaling components such as RICK and TRAF6 5-7, 24, 25. It was therefore possible that IRF4 expression induced by NOD2 activation inhibits NF-κB activation by down-regulation of such polyubiquitination. To address this question we first investigated the effect of IRF4 on RICK polyubiquitination in 293 cells transfected with plasmids expressing HA-tagged ubiquitin (Ub), V5-tagged RICK, and FLAG-tagged IRF4 and then lysed to obtain cell lysates that were subjected to IP with anti-HA antibody (Ab) and IB with anti-V5 Ab.

As shown in Figure 3A, polyubiquitination of RICK was seen in 293 cells expressing HA-tagged wild type Ub and V5-tagged RICK alone but not in cells also expressing IRF4. Consistent with previous studies showing that the E3 ligases, TRAF6 and cellular inhibitors of apoptosis proteins (cIAPs) induce K63-linked polyubiquitination of RICK 6, 26, co-transfection of plasmids expressing TRAF6 or cIAP1 or cIAP2 enhanced polyubiquitination of RICK; however, such enhanced polyubiquitination of RICK was markedly reduced in cells also expressing IRF4 (Figures 3A and 3B). In further studies to determine the linkage type of poly-Ub chains on RICK, 293 cells were transfected with plasmids expressing mutant forms of Ub that specifically ubiquitinate via either K48 or K63 linkages. As shown in Figure 3A (middle and right panels), 293 cells expressing IRF4 exhibited reduced K63-linked polyubiquitination of RICK, even in cells co-transfected with TRAF6 that expressed increased amounts of K63-polyubiquitinated RICK; however, IRF4 expression had little or no effect on the marginal amount of K48-linked polyubiquitination observed, even in the presence of TRAF6.

Figure 3. IRF4 regulates polyubiquitination of RICK.

Figure 3

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(A) 293 cells (1×106/6 well plate) were transfected with vectors (1 μg) expressing HA-tagged wild type ubiquitin (Ub), K48 Ub, K63 Ub, FLAG-tagged IRF4, V5-tagged RICK, and TRAF6; whole cell lysates were prepared 48 hours after the transfection and subjected to immunoprecipitation (IP) with the indicated Ab followed by immunoblotted (IB) with the indicated Ab. (B) 293 cells (1×106/6 well plate) were transfected with vectors (1 μg) expressing FLAG-tagged IRF4, Myc-DDK-tagged cIAP1, Myc-DDK-tagged cIAP2, V5-tagged RICK, and HA-tagged K48 or K63 Ub; whole cell lysates were subjected to IP with the indicated Ab followed by IB with the indicated Ab. (C) 293 cells (1×106/6 well plate) were transfected with vectors (1 μg) expressing HA-tagged wild type Ub, V5-tagged RICK, TRAF6, FLAG-tagged IRF4, FLAG-tagged mutated IRF4 (Mut IRF4) in which serine residues at 447 and 448 are replaced with alanine; whole cell lysates were prepared 48 hours after the transfection and subjected to IP with the indicated Ab followed by IB with the indicated Ab. (D) 293 cells stably expressing NOD2 (1×106/6 well plate) were transfected with vectors (1 μg) expressing HA-tagged wild type Ub, FLAG-tagged IRF4, and V5-tagged RICK. 48 hours after the transfection, cells were stimulated with MDP (10 μg/ml) for 30 min; whole cell lysates were subjected to IP with the indicated Ab followed by IB with the indicated Ab. Results shown are representative of two experiments.

As shown in Figure 3B, enhanced K63-linked polyubiquitination of RICK induced by cIAP1 or cIAP2 (but not K48-linked polyubiquitination) was also inhibited in cells expressing IRF4 whereas K63-linked polyubiquitination of RICK by ITCH, another E3 ligase known to induce such polyubiquitination 25 was not reduced in cells expressing IRF4 (data not shown). In addition, as shown in Figure 3C, reduced RICK polyubiquitination was seen in cells expressing either wild type IRF4 or mutated IRF4 lacking its phosphorylation site, indicating that the inhibitory effect of IRF4 was not dependent on its phosphorylation status. Finally, as shown in Figure 3D, polyubiquitination of RICK induced by 30 min of stimulation with MDP in 293 cells stably expressing NOD2 was barely seen upon co-transfection of IRF4; thus the inhibitory effect of IRF4 also applies to RICK activated by NOD2.

In related studies we identified RICK domains that interact with IRF4 and that are necessary for IRF4 inhibition of polyubiquitination. RICK is composed of a kinase domain, an intermediate domain, and a CARD domain. We therefore transfected plasmids expressing V5-tagged RICK mutants lacking each of these domains as well as RICK fragments composed of each of these domains into 293 cells co-transfected with plasmids expressing FLAG-IRF4. As shown in Figure 4A, the interaction between RICK and IRF4 (defined by IP-IB studies) required the presence of the kinase and/or the intermediate RICK domains since the interaction could be detected in 293 cells over-expressing kinase and intermediate domain RICK mutants but not in cells expressing the CARD domain mutant. Thus, the interaction between RICK and IRF4 was mediated by the binding of IRF4 to either the kinase or the intermediate domain but not to the CARD domain. With this information in hand we next conducted ubiquitination studies of RICK domains in 293 cells transfected with plasmids expressing V5-RICK mutants or RICK fragments and co-transfected with plasmids expressing HA-Ub in the absence of IRF4 co-transfectlon. In previous studies, Hasegawa et al. showed that polyubiquitination of RICK at K209 in the kinase domain is essential for RICK-mediated NF-κB activation 7. As shown in Figure 4B, consistent with this finding, 293 cells over-expressing mutant RICK lacking the kinase domain exhibited grossly defective polyubiquitination whereas those over-expressing RICK mutants lacking the intermediate or CARD domains still exhibited polyubiquitination, albeit less than that of WT RICK; in addition, as also shown in Figure 4B, whereas a kinase domain fragment of RICK was polyubiquitinated, an intermediate domain fragment of RICK was not. Thus, these studies demonstrate that the IRF4 inhibition of RICK polyubiquitination shown above involves polyubiquitination of the kinase domain of RICK and this inhibition is facilitated by IRF4 binding to the kinase and/or intermediate domains of RICK.

Figure 4. IRF4 inhibition of RICK polyubiquitination is facilitated by IRF4 binding to the kinase and/or intermediate domains of RICK.

Figure 4

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(A) 293 cells were transfected with vectors expressing FLAG-tagged IRF4 and various forms of V5-tagged mutated RICK; whole cell lysates were isolated 48 hours after the transfection and were then subjected to immunoprecipitation (IP) with the indicated Ab followed by immunoblotting (IB) with the indicated Ab. (B) 293 cells were transfected with vectors expressing various forms of V5-tagged mutated RICK and HA-tagged Ub; whole cell lysates were isolated 48 hours after the transfection and were subjected to IP with the indicated Ab followed by IB with the indicated Ab. Results shown are representative of two experiments.

IRF4 regulates polyubiquitination of TRAF6

Stimulation of the TLRs leads to the recruitment of MyD88 and TRAF6 to the receptor complex 27. This process activates TRAF6 E3 ligase activity and TRAF6-mediated K63-linked polyubiquitination of downstream target proteins as well as TRAF6 itself 24. Since IRF4 binds to TRAF6 following MDP pre-stimulation it seemed possible that as in the case of RICK polyubiquitination, TRAF6 polyubiquitination was regulated by IRF4. To address this question, 293 cells were transfected with HA-tagged TRAF6, His-tagged Ub, and FLAG-tagged IRF4 and subjected to IP-IB studies as described above. As shown in Figures 5A and 5B, cells expressing wild type or mutated IRF4 exhibited greatly reduced polyubiquitination of TRAF6 in the presence or absence of RICK. In addition, as shown in Figure 5C, robust TRAF6 polyubiquitination induced by 30 min of stimulation with LPS in 293 cells stably expressing TLR4, MD2, and CD14, was abolished in cells also expressing IRF4.

Figure 5. IRF4 regulates polyubiquitination of TRAF6.

Figure 5

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(A, B) 293 cells (1×106/6 well plate) were transfected with vectors (1 μg) expressing His-tagged wild type ubiquitin (Ub), FLAG-tagged IRF4, V5-tagged RICK and HA-tagged TRAF6; whole cell lysates were prepared 48 hours after the transfection and subjected to IP with the indicated Ab followed by IB with the indicated Ab. (C) 293 cells stably expressing TLR4 (1×106/6 well plate) were transfected with vectors (1 μg) expressing His-tagged wild type Ub, FLAG-tagged IRF4, and HA-tagged TRAF6. 48 hours after the transfection, cells were stimulated with LPS (1 μg/ml) for 30 min; whole cell lysates were subjected to IP with the indicated Ab followed by IB with the indicated Ab. Results shown are representative of two experiments.

Taken together, these studies strongly suggest that IRF4 negatively regulates polyubiquitination of RICK and TRAF6 either in cells in which target proteins are being over-expressed and are being activated by NLR or TLR ligands, respectively.

Pre-stimulation of human DCs with MDP inhibits Lys63-linked polyubiquitination of RICK and TRAF6

To verify the results of the above over-expression studies of IRF4 under physiologic conditions we next investigated whether IRF4 expression induced by NOD2 inhibits K63-linked polyubiquitination of RICK and/or TRAF6 in human DCs. To this end, cell lysates prepared from human DCs that were pre-stimulated with MDP for 24 hours and then re-stimulated with MDP or LPS were subjected to IP with Abs specific to K63- or K48-ubiquitin and then IB with Abs specific for RICK or TRAF6.

As shown in Figure 6A, pre-stimulation of human DCs with MDP greatly reduced K63-linked, but not K48-linked polyubiquitination of RICK upon secondary stimulation with MDP of human DCs. Similarly, pre-stimulation with MDP greatly reduced K63-linked, but not K48-linked polyubiquitination of TRAF6 upon secondary stimulation with LPS. It should be noted that LPS stimulation did not induce K63-linked polyubiquitination of RICK and MDP stimulation did not induce K63-linked polyubiquitination of TRAF6; thus the possible effect of pre-stimulation of cells with MDP in these situations could not be evaluated.

Figure 6. IRF4 expression induced by MDP activation of NOD2 inhibits K63-linked polyubiquitination of RICK and TRAF6.

Figure 6

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(A) Human monocyte-derived dendritic cells (DCs) were generated as described in Figure 1. DCs (1×106/ml) were pre-treated with MDP (10 μg/ml) for 24 hours followed by treatment with MG132 (10 μg/ml) for two hours and then were stimulated with MDP (10 μg/ml) or LPS (1 μg/ml) for 30 minutes. Whole cell lysates were subjected to immunoprecipitation (IP) with the indicated Ab followed by immunoblotted (IB) with the indicated Ab. (B) Human DCs were transfected with IRF4-specific siRNA or control siRNA (100 nM). One day after the transfection, DCs (1×106/ml) were treated with MDP (10 μg/ml) for 24 hours and then cell lysates were subjected to IB with the indicated Ab. (C) Human DCs were transfected with IRF4-specific siRNA or control siRNA (100 nM). One day after the transfection, DCs (1×106/ml) were pre-treated with MDP (10 μg/ml) for 24 hours followed by treatment with MG132 (10 μg/ml) for two hours and then were stimulated with MDP (10 μg/ml) or LPS (1 μg/ml) for 30 minutes; whole cell lysates were subjected to IP with the indicated Ab followed by IB with the indicated Ab. (D) Human DCs were transfected with IRF4-specific siRNA or control siRNA (100 nM). One day after the transfection, DCs (1×106/ml) were pre-treated with MDP (10 μg/ml) for 24 hours and then were stimulated with MDP (10 μg/ml) or LPS (1 μg/ml) for 30 minutes; whole cell lysates were subjected to IB with the indicated Ab. Results shown are representative of two experiments.

To determine if the negative effect of MDP pre-stimulation on K63-linked polyubiquitination was in fact due to IRF4 we next conducted studies of cells in which IRF4 was down-regulated by IRF4-specific siRNA (Figure 6B). As shown in Figure 6C, whereas MDP pre-stimulation of cells again led to inhibition of MDP-stimulated RICK and LPS-stimulated TRAF6 K63-linked polyubiquitination, respectively, such inhibition was reversed in cells treated with IRF4 siRNA. These studies show that in physiologic human DCs MDP activation of NOD2 and generation of IRF4 result in subsequent inhibition of MDP-induced RICK K63-linked polyubiquitination and LPS-induced TRAF6 K63-linked polyubiquitination. They thus fully corroborate the over-expression studies conducted with 293 cells.

Since K63-polyubiquitination of RICK and TRAF6 have been shown to be necessary for TLR-NLR activation of NF-κB 5, 24 we next asked if down-regulation of IRF4 expression by exposure to IRF4 siRNA also results in reversal of MDP pre-stimulation induced inhibition of NF-κB activation. As shown in Figure 6D, culture of DCs in the presence of IRF4 siRNA did in fact abolish the capacity of MDP pre-stimulation to inhibit either MDP or LPS induction of NF-κB activation as assessed by expression of phospho-IκBα whereas control siRNA had no effect on inhibition. These results strongly suggest that IRF4 inhibition of RICK and TRAF6 K63-linked polyubiquitination results in down-stream inhibition of NF-κB activation

Administration of MDP protects mice from trinitrobenzene sulfonic acid (TNBS) colitis via regulation of K63-linked polyubiquitination of RICK and TRAF6

The above results derived from in vitro studies of both 293 cells and human DCs suggest that MDP/NOD2-induced effects on K63-linked polyubiquitination in RICK and TRAF6 could explain our previous studies showing that MDP administration ameliorates experimental colitis 14. To address this possibility we next determined the effect of MDP administration on K63-linked polyubiquitination in RICK and TRAF6 in mice with TNBS-colitis. As shown in Figures 7A, and 7B, and in the photomicrographs displayed in S1A, systemic administration of MDP protected mice from the induction of TNBS-colitis induced by intra-rectal instillation of TNBS and such protection was accompanied by reduced nuclear translocation of NF-κB subunits (p65, p50, and c-Rel) in colonic lamina propria mononuclear cells (LPMCs) 14.

Figure 7. Administration of MDP protects mice from trinitrobenzene sulfonic acid (TNBS)-colitis via regulation of K63-linked polyubiquitination of RICK and TRAF6.

Figure 7

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C57BL/10 mice were administered MDP on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. (A) Upper panel: Changes in body weight of mice not-treated or treated with MDP (n=10) and challenged with intra-rectal administration of TNBS. Lower panel: Pathology scores of mice not-treated or treated with MDP on day 4. Results were expressed as means ± SD. ** P<0.01, as compared with untreated group. (B) NF-κB activation in colonic LPMCs in mice challenged with TNBS. Nuclear extracts were isolated from colonic LPMCs on day 1 and subjected to a Transfactor Binding Assay. Results are expressed as means ± SD. ** P<0.01, as compared with untreated group. (C) IRF4 expression in the colonic tissue of mice challenged with TNBS on day 1. (D) Interaction between IRF4 and RICK, MyD88, and TRAF6 in the colonic tissue of TNBS-challenged mice on day 1. Molecular interactions were visualized by Duolink assay (red color). (E) K48- or K63-linked polyubiquitination of RICK and TRAF6 in colonic LPMCs of TNBS-challenged mice. Whole cell lysates prepared from colonic LPMCs on day 1 were subjected to immunoprecipitation (IP) with the indicated Ab followed by immunoblotting (IB) with the indicated Ab.

Importantly, several IRF4-related effects accompanied this MDP-mediated protection from colitis. Thus, as shown in Figure 7C, MDP administration led to markedly enhanced IRF4 expression in colonic tissue of MDP-treated mice and, as shown in Figure 7D, Duolink assays revealed that such administration also caused enhanced interaction between IRF4 and RICK, MyD88 or TRAF6 in such colonic tissue. Furthermore, as shown in Figure 7E, MDP-administration led to reduced K63-linked polyubiquitination of RICK and TRAF6 in colonic LPMCs that was unaccompanied by reduced K48-linked polyubiquitination. These in vivo studies are therefore consistent with the in vitro studies described above in showing that MDP-induced IRF4 expression and inhibition of K63-linked polyubiquitination of RICK and TRAF6 is associated with a down-regulation of NF-κB; however, in this case they show that this IRF4 effect is also associated with greatly reduced colonic inflammation.

Prevention of TNBS-colitis by administration of IRF4-expressing plasmids

Whereas the above studies show that MDP-induced up-regulation of IRF4 and the latter's effect on K63-linked ubiquitination of RICK and TRAF6 is associated with down-regulation of NF-κB and colitis it remained possible that MDP inhibition of NF-κB activation was occurring through another mechanism that does not involved IRF4. To address this possibility we conducted further in vivo studies in which we explored the possibility that exogenous IRF4 administration can directly prevent TNBS-colitis, thereby by-passing MDP stimulation. Accordingly, we administered a FLAG-tagged IRF4 plasmid as well as a control plasmid encapsulated in a Hemagglutinin Virus of Japan-Envelope (HVJ-E) viral coat to mice by intra-rectal instillation on each of the two days before and on the day of intra-rectal challenge with TNBS. This method of inducing in vivo protein expression following plasmid administration had proven to be highly efficient in previous studies 14 and, indeed, most of the colonic LPMCs expressing CD11b or CD11c were positive for the expression of FLAG-IRF4 in flow-cytometric analysis two days after the induction of TNBS-colitis (Figure S2). As shown in Figures 8A and S1B, intra-rectal administration of FLAG-tagged IRF4 plasmids prevented the development of TNBS-colitis as assessed by body weight loss and colonic pathology analysis. Thus, exogenous IRF4 administration, like MDP administration, is an effective inhibitor of TNBS-colitis.

Figure 8. Prevention of TNBS-colitis by administration of an IRF4-expressing plasmid.

Figure 8

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C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. (A) Changes of body weight in mice (n=5; each group, top panel) and pathology scores of mice on day 4. Results were expressed as means ± SD. ** P<0.01, as compared with control vector group. (B) Interaction between FLAG-tagged IRF4 and RICK, MyD88, and TRAF6 in the colonic tissue of mice. Whole protein lysates were prepared from the colon tissues of TNBS-challenged mice on day 2 and were subjected to immunoprecipitation (IP) with the indicated Ab followed by immunoblotting (IB) with the indicated Ab. Two colon extracts from each group were used for the assay. (C) Activation of NF-κB and MAPK in the colon tissues of TNBS-challenged mice on day 2. Two colon extracts from each group were used for the immunoblotting. (D) NF-κB activation in colon tissues in mice challenged with TNBS. Nuclear extracts were isolated from colon tissues on day 2 and subjected to a Transfactor Binding Assay. Results were expressed as means ± SD. ** P<0.01, as compared with control vector group. (E, F) Production of IL-12p40 and IFN-γ by colon LPMCs isolated from TNBS-challenged mice on day 4. Colon LPMCs (1×106/ml) were stimulated with MDP, PAM, LPS, Flagellin, and CpG for 24 hours or with anti-CD3 Ab for 48 hours after which culture fluids were assayed for IL-12p40 or IFN-γ levels by ELISA, as indicated. Results were expressed as means ± SD. ** P<0.01, as compared with group administered control vector. Results shown are representative of two experiments.

In further studies, we investigated the interaction between the exogenously administered FLAG-tagged IRF4 and RICK, TRAF6 and MyD88 in the colonic mucosa of the mice subjected to intra-rectal TNBS challenge accompanied by IRF4 administration. To this end, whole protein extracts isolated from the colonic mucosa were subjected to IP with FLAG Ab and then IB with Abs specific for RICK, TRAF6 and MyD88. As shown in Figure 8B, administered FLAG-tagged IRF4 was bound to RICK, MyD88, and TRAF6. In a final set of studies we determined the effect of the exogenously administered IRF4 on NF-κB and MAP kinase expression as well as on down-stream pro-inflammatory cytokine expression. As shown in Figures 8C and 8D, exogenously administered IRF4 led to markedly reduced expression of phospho-κBa, phospho-p38, and phospho-ERK as well as reduced nuclear translocation of NF-κB subunits in the colonic mucosa of mice treated with intra-rectal administration of FLAG-tagged IRF4 plasmids as compared with treated those with control plasmid. In addition, evidence of reduced activation of NF-κB was associated with reduced pro-inflammatory cytokine responses by colonic LPMCs. Thus, as shown in Figures 8E and 8F, colonic LPMCs produced markedly less IL-12p40 and IFN-γ upon stimulation with MDP, Pam3CSK4 (PAM, a TLR2 ligand), LPS, flagellin (a TLR5 ligand), CpG (a TLR9 ligand), and anti-CD3 Ab.

Taken together, these data show that IRF4 administration mimics the effect of MDP administration and increased NOD2 signaling during induction of TNBS-colitis as previously reported 14. As such, they show that prevention of TNBS-colitis by MDP administration is most likely acting via the induction of IRF4.

Treatment of TNBS-colitis by administration of IRF4-expressing plasmids

The striking effect of IRF4-expressing plasmid administration on TNBS colitis shown above suggested that such administration could have therapeutic value. To address this possibility we determined if administration of IRF4-expressing plasmid could reverse previously established TNBS-colitis. Accordingly, mice were challenged with TNBS as described above but in this case they were administered FLAG-tagged IRF4 plasmid encapsulated in the HVJ-E vector three days after TNBS administration rather than at the time of TNBS administration. As shown in Figure 9A, expression of FLAG was again shown to be present in the colonic mucosa of mice following FLAG-tagged IRF4 plasmid administration. In addition, as shown in Figures 9B and S1C, such mice promptly regained body weight and exhibited improved microscopic inflammation scores. Moreover, as shown in Figures 9C, 9D, and 9E, administration of IRF4 was followed by reduced nuclear translocation of NF-κB components in the colonic mucosa as well as greatly decreased production of pro-inflammatory cytokines by mesenteric lymph node (MLN) cells upon stimulation with TLR ligands and anti-CD3 mAb. These data thus provide further proof that MDP activation of NOD2 and generation of IRF4 leads to down-regulation of NF-κB activation and colonic inflammation. In addition, they suggest that IRF4 administration might have clinical value.

Figure 9. Treatment of TNBS-colitis by administration of an IRF4-expressing plasmid.

Figure 9

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C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on day 3 after challenge with TNBS on day 0. (A) Expression of FLAG-tagged IRF4 in the colonic tissues of mice. Whole protein lysates were prepared from the colonic tissues of TNBS-challenged mice on day 6 and were subjected to immunoblotting. Two colonic extracts from each group were used for the immunoblotting. (B) Changes of body weight in mice (n=7; each group, top panel) and pathology scores of mice on day 6. Results were expressed as means ± SD. Results shown are a pool of two independent experiments. **P<0.01, as compared with control vector group. (C) NF-κB activation in colon tissues in mice challenged with TNBS. Nuclear extracts were isolated from colon tissues on day 6 and subjected to Transfactor binding assay. Results were expressed as means ± SD. *P<0.05, **P<0.01, as compared with control vector group. (D, E) Production of IL-12p40, TNF, IL-6 and IFN-γ by mesenteric lymph node (MLN) cells isolated from TNBS-challenged mice on day 6. MLN cells (2×106/ml) were stimulated with MDP, PAM, LPS, Flagellin, and CpG for 24 hours to determine the protein levels of IL-12p40, TNF and IL-6. Cells were also stimulated with anti-CD3 Ab for 48 hours to determine the protein levels of IFN-γ. Results were expressed as means ± SD. *P<0.05, **P<0.01, as compared with control vector group.

Discussion

In a previous study, we demonstrated that MDP activation of NOD2 has down-regulatory effects on multiple TLR signaling pathways 14. We now provide a mechanism for such down-regulation by showing that MDP activation of NOD2 induces IRF4-mediated inhibition of molecular events essential to the activation of NF-κB, namely K63-linked polyubiquitination of RICK and TRAF6. The chain of evidence supporting this conclusion consisted first of the fact that MDP pre-stimulation of human DCs leads to binding of RICK to IRF4 and the binding of IRF4 to TRAF6 and MyD88. As shown in over-expression studies conducted in a cell line and more importantly in physiologic human DCs, these interactions set the stage for MDP/NOD2-induced IRF4 inhibition of K63-linked polyubiquitination of RICK and TRAF6; in addition, such inhibition could be linked to down-regulation of NF-κB activation by the demonstration that siRNA down-regulation of IRF4 reverses the negative effect by NOD2 signaling on K63-linked polyubiquitination and NF-κB activation. These in vitro studies were then supported by in vivo studies showing that protection from the development of TNBS-colitis by MDP administration is accompanied by greatly increased IRF4 expression and interaction with RICK, TRAF6 and MyD88 as well as inhibition of K63-linked polyubiquitination of RICK and TRAF6 in colonic cells and this, in turn, is associated with greatly reduced NF-κB activation. A final step in the chain of evidence consisted of studies showing that administration of an IRF4-expressing plasmid to mice both prevented TNBS-colitis and reversed already established TNBS-colitis. These latter studies established that MDP activation of NOD2 in vivo was in fact acting via IRF4 to inhibit NF-κB activity. Overall, these data provide a mechanistic explanation of how MDP-NOD2 stimulation of APCs negatively regulates inflammatory responses induced by TLR ligands and therefore explain how defective NOD2 function can lead to excessive TLR responses in the gut that contribute to the pathogenesis of Crohn's disease.

IRF4 has been shown in previous reports to function as a negative regulator of TLR signaling pathways in innate immune cells such as DCs 14, 28, 29. As for the mechanisms accounting for such negative regulation, Negishi et al. provided evidence that IRF4 expression is up-regulated by activation of TLRs and then competes with IRF5 for binding to and activation of MyD88 28. While this mechanism of IRF4 inhibitory activity may be valid, it cannot be the only mechanism in play because we have shown previously as well in the present studies that MDP pre-stimulation acting through NOD2 inhibits LPS and other TLR ligand cytokine responses, including TLR responses that do not involve MyD88 14. It should be noted in this context that whereas NOD2 activation leads to RICK-IRF4 binding, LPS activation in the absence of MDP-induced NOD2 interaction does not have this effect (Watanabe T, Asano N, Strober W, unpublished observation). Thus, it is possible that NOD2 activation leads to RICK-IRF4 complexes that have inhibitory functions not shared by IRF4 alone. In any case, we have shown that systemic administration of MDP to mice challenged with TNBS to induce TNBS-colitis leads to enhanced expression of IRF4 in colonic LPMCs and inhibition of inflammation due to reduced K63-linked polyubiquitination of TRAF6 and RICK in those cells. In addition, intra-rectal administration of an IRF4-expressing plasmid to mice challenged with TNBS had a similar anti-inflammatory effect. Thus, our study disclosed a molecular mechanism by which NOD2-induced IRF4 inhibits intestinal inflammation driven, at least in part, by activation of TLR signaling pathways that are not regulated by TLR-induced IRF4.

In the above studies of TNBS-colitis the development of colitis was inhibited either by systemic injection of MDP or intrarectal administration of IRF4 cDNA. These treatments were parallel in that administration of MDP resulted in enhanced interaction between IRF4 and RICK, TRAF6, and MyD88 and administration of IRF4 cDNA led to interaction of IRF4 with the same signaling molecules; moreover, reduction of NF-κB activation was seen in both treatments. Thus, it is likely that MDP activation of NOD2 prevents experimental colitis via induction of IRF4 expression. It should be noted that this conclusion leads to the assumption that activation of TLRs with the ability to induce the expression of IRF4 have the potential to inhibit experimental colitis via the same de-ubiquitination mechanism described here for NOD2. However, previous reports show that generation of tolerogenic responses by LPS depends upon the induction of IRAK-M rather than IRF4 14, 29. Thus, tolerogenic responses induced by MDP activation of NOD2 appear to be intrinsically different from those induced by LPS activation of TLR4 and while LPS administration may suppress colitis due to induction of LPS tolerance, such suppression will not by mediated by the de-ubiquitinization function of IRF4.

Of interest, IRF4 may be exerting inhibitory effects by a mechanism similar to that described here in other instances of pro-inflammatory responses. This includes IRF4-mediated suppression of TLR-induced cytokine responses leading to acute post-ischemic renal inflammation by IRF4 generated in renal DCs reacting to oxidative stress 30 and IRF4-mediated reduction of TLR-induced pro-inflammatory responses of liver plasmacytoid DCs by IRF4 generated in such cells by in vivo administration of MDP 13. However, additional studies will be necessary to verify this possibility.

IRF4 is expressed in most types of cells in the lymphoid system and may have cell-specific functions 31. This possibility is illustrated by the fact that, in contrast to the anti-inflammatory role of IRF4 in TNBS-colitis and post-ischemic renal inflammation described above, it has a pro-inflammatory role in experimental T cell-mediated autoimmune disorders 31. The latter may be due to the fact that IRF4 has been shown to be a positive regulator of IL-17 and IL-21 responses in T cells and increased responsiveness to IL-21 in B cells 22, 31, 32. Interestingly, there is evidence that this pro-inflammatory activity by IRF4 plays a critical role in a T cell-dependent colitis. Thus, Mudter et al. have shown that adoptive transfer of naive CD4+ T cells from wild type mice, but not IRF4-deficient mice to immune-deficient mice resulted in severe colitis associated with increased production of IL-6 and Th17 cytokines 33, 34. In our studies, intra-rectal delivery of a plasmid expressing FLAG-tagged IRF4 was shown to lead to marked expression of FLAG-tagged IRF4 in colonic APCs rather than in colonic T cells. Thus, our data support the idea that whereas IRF4 expression in T cells may promote the development of colitis, its expression in APCs has the contrary effect. In this context, it should also be noted that the HVJ-E delivery of IRF4-expressing plasmid could have led to IRF4 expression in non-myeloid cells and thus we cannot rule out the possibility that the ability of exogenous IRF4 expression to affect colitis in these studies could have been mediated by effects on one or another non-myeloid cell.

As shown by the fact that intra-rectal administration of NF-κB decoy oligonucleotides that blocks activation of NF-κB target genes prevents and treats TNBS- or oxazolone-colitis, the pathogenic immune responses underlying experimental colitis depend on NF-κB transcriptional activity 35, 36. In recent years evidence has accumulated that such NF-κB-mediated inflammation is tightly regulated by ubiquitination of various components of the NF-κB signaling cascade. This is well illustrated by the fact that the function of TRAF6, an essential component of the signaling cascade leading to NF-κB activation is dependent on its K63-linked polyubiquitination status. Thus, de-ubiquitination of TRAF6 by the de-ubiquitinating enzyme, A20, leads to inhibition of TLRs-induced NF-κB activation 24, 37 and A20 deficiency results in excessive NF-κB activation associated with the development of autoimmune disease or colitis due to stimulation by TLR ligands derived from the intestinal microflora 24, 38. In this study, we show that down-regulation of K63-linked polyubiquitination of TRAF6 resulting from an inhibitory interaction with IRF4 also leads to decreased NF-κB activation. The mechanism of such IRF4 inhibition is presently unknown. However, given the fact that TRAF6 is an E3-ligase and can therefore facilitate both the polyubiquitination of down-stream signaling molecules as well as its own polyubiquitination, one possible mechanism is that IRF4 interferes with TRAF6 E3-ligase activity.

Despite the fact that NOD2 polymorphisms associated with Crohn's disease are considered to be loss-of-function abnormalities that lead to decreased NOD2-mediated pro-inflammatory function, immune responses linked to Crohn's disease are characterized by production of pro-inflammatory cytokines driven by excessive NF-κB activation 39, 40. One explanation of this paradox is that NOD2 signaling in epithelial cells is necessary for the elaboration of epithelial cell-derived cryptins that ordinarily control bacterial growth in the intestine; thus, loss of NOD2 function can lead to excessive bacterial growth that gives rise to colitis 41, 42. It should be noted, however, that chronic NOD2 activation has been shown to mediate down-regulation of innate TLRs responses to microbial antigens in the intestine, a phenomenon known as cross-tolerance 14-17. Therefore, an alternative explanation of how NOD2 polymorphisms and loss of NOD2 function leads to intestinal disease is that NOD2 regulates innate responses to intestinal microflora by suppressing TLR responses in the healthy intestinal mucosa, whereas in the diseased Crohn's disease intestinal mucosa lack of NOD2 function leads to lack of cross-tolerance and excessive TLR responses. This study together with our previous study of NOD2 signaling shows that defective NOD2-induced IRF4 inhibitory function is likely to be the cause of the loss of cross-tolerance and thus the molecular basis for the role of loss of NOD2 function in Crohn's disease 14.

In conclusion, the present findings provide evidence that CARD15 polymorphisms function as susceptibility factors in Crohn's disease by affecting the generation and activation of a factor, IRF4, that plays a key role in the regulation of TLR responses induced by the gut microflora. In addition, they show in studies of mice with experimental colitis that MDP administration leading to colonic IRF4 expression or intra-rectal delivery of an IRF4 expression plasmid have the potential to both prevent and treat such colitis and possibly Crohn's disease as well.

Methods

Reagents

Recombinant GM-CSF and IL-4 were from Peprotech. Unless otherwise described, the doses of TLR ligands and NOD2 ligands used for stimulation were as follows; Pam3CSK4 (PAM, TLR2 ligand, 10 μg/ml, InvivoGen), LPS (TLR4 ligand, 1 μg/ml, Sigma), flagellin (TLR5 ligand, 1 μg/ml, InvivoGen), CpG (TLR9 ligand, 1 μM, InvivoGen), and MDP (NOD2 ligand, 10 μg/ml, InvivoGen).

Induction of colitis

TNBS-colitis was induced in C57BL10 mice obtained from Japan SLC as described previously 35. On day -2, -1, and 0, mice received intra-peritoneal injection of MDP (100 μg) for a total of three times before intra-rectal administration of 3.75 mg of TNBS in 100 μl of 45 % ethanol. MLN cells and colon LPMCs were isolated at the indicated time points and cultured as described previously 14. Cells were stimulated with anti-CD3 (1 μg/ml, BD Pharmingen) and TLR ligands as described above. Culture supernatants were collected at 24 hrs or 48 hrs and analyzed for cytokine production by ELISA. In some experiments, whole cell extracts were prepared from colon tissue or LPMCs for the immunoprecipitation and immunoblotting analysis. In the experiments in which mice received FLAG-tagged IRF4 vector 29 or control vector, plasmids were encapsulated in HVJ (GenomIdea) using protamine sulfate according to the manufacture's protocol. 75 μg/mouse of encapsulated plasmids were administered via the intra-rectal route on day -2, -1, and 0 for the evaluation of colitis prevention and on day 3 for the evaluation of colitis treatment. Colon was harvested at the indicated time points. Colon tissues were stained with hematoxylin and eosin (H&E) and used for the scoring of the inflammation as described previously 14. Animal use adhered to Kyoto university animal care guidelines and protocols of animal experiments were approved by the review boards of Kyoto University.

Human monocyte-derived DCs

Monocytes were isolated from the peripheral blood of healthy donors by CD14+ microbeads (Miltenybiotec) and were cultured in 6-well plates (1×106/ml) in 5 ml of complete medium (RPMI 1640 medium supplemented with 2 mM L-glutamine, and 10% fetal calf serum) supplemented with recombinant GM-CSF (20 ng/ml) and recombinant IL-4 (20 ng/ml). Ethical permission of this study was granted by the review boards of Kyoto University. After 3 days of culture, half of the medium in each well was exchanged for fresh medium. After 6 days of culture, cells (1×106/ml) were incubated with MDP or medium for 24 hrs in the absence of GM-CSF and IL-4, and then washed three times and stimulated with LPS or MDP. In some experiments, cells were cultured with MG132 (10 μg/ml, Enzo Life Sciences). In siRNA-mediated gene silencing experiments, DCs were transfected with 100 nM of control siRNA or IRF4 siRNA (Hs IRF4 10 FlexiTube siRNA, Qiagen) by a human dendritic cell nucleofection kit (Lonza).

Immunoprecipitation and immunoblotting

HEK293 cells (ATCC) (1×106/cells) were transfected with 1 μg of FLAG-tagged human IRF4 vector 14, HA-tagged human MyD88, TRAF6 (InvivoGen), V5-tagged RICK 14, Myc-DDK-tagged cIAP1, Myc-DDK-tagged cIAP2 (Origene), HA-tagged wild type ubiquitin (Ub), K63 Ub, K48 Ub (kindly provided by Dr. J. Chen), and His-tagged Ub (kindly provided by Dr. H. Kondoh) by Lipofectamine 2000 (Invitrogen) or by Fugene 6 (Promega). Mutant plasmids expressing IRF4 S447A and S448A, RICK K47A and S176A, or RICK lacking the kinase domain, intermediate domain, or CARD were created by QuickChange site-directed mutagenesis kit (Stratagene). Whole cell lysates were prepared 24 or 48 hrs after the transfection and were incubated with anti-FLAG conjugated beads (Sigma), anti-V5 conjugated beads (Sigma), and anti-HA-conjugated beads (Sigma) overnight. In some experiments, whole cell lysates prepared from human DCs, colonic LPMCs, and colon tissue samples were incubated with anti-K63 Ub Ab, anti-K48 Ub Ab (MBL) or anti-IRF4 Ab (Santa Cruz Biotechnology) and protein A/G agarose (Santa Cruz Biotechnology). Anti-MyD88, anti-TRAF6, anti-IRF4, anti-κBα, anti-phospho-κBα, anti-phospho-p38 anti-p38, anti-phospho-ERK, anti-ERK, and anti-His Abs were obtained from Cell signaling technology (CST). Anti-actin Ab (Santa Cruz), anti-RICK Ab (Cayman Chemicals), anti-V5 Ab (Bethyl laboratories), anti-FLAG Ab (Sigma), anti-HA Ab (Sigma), and anti-Myc Ab (MBL) were used.

Immunofluorescence studies

Colon tissues were harvested and fixed in 10% formalin. Deparaffinized colon sections were then obtained and incubated with mouse anti-IRF4 Ab (Invitrogen) followed by Alexa546-conjugated anti-mouse IgG Ab (Invitrogen) by using Can Get Signal immunoreaction enhancer solution (Toyobo) as described previously 43. For visualization of interaction between IRF4 and RICK, MyD88, TRAF6 in colon samples, a Duolink In Situ kit was used (Olink Bioscience). Goat anti-IRF4 Ab (Santa Cruz), rabbit anti-RICK Ab, rabbit anti-MyD88 Ab, and rabbit anti-TRAF6 Ab (Abcam) were used to visualize target protein interactions. For visualization of interaction between IRF4 and RICK, MyD88, TRAF6 in human DCs, cells were fixed in 4% paraformaldehyde and subjected to the protocols suggested by the Duolink In Situ kit.

Elisa

Protein concentrations of cytokines were determined by eBioscience ELISA kits for mouse IL-12p40, mouse IL-6, and mouse TNF-α. Concentration of IFN-γ was determined by BD Bioscience ELISA kit.

NF-κB activation studies

Nuclear extracts were prepared from colon tissues. Nuclear extracts was obtained with the use of a nuclear extraction kit (Active Motif). Binding activity of nuclear extract (5 μg) to NF-κB subunit (p50, p65, c-Rel) was measured using a Transam kit, obtained from Active Motif, as previously described 43.

Statistical analysis

Student's t test was used to evaluate the significance of the differences. Statistical analysis was performed with the Prism (Graphpad software). A value of P < 0.05 was regarded as statistically significant.

Supplementary Material

Supplementary Figure 1. H&E-stained colonic tissue of mice treated with intra-rectal administration of TNBS. (A) C57BL/10 mice were administered MDP on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. Colonic samples were obtained on day 4. Magnification x400. (B) C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. Colonic samples were obtained on day 4. Magnification x400 (C) C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on day 3 after challenge with TNBS on day 0. Colonic samples were obtained on day 6. Magnification x400.

Supplementary Figure 2. Expression of FLAG-IRF4 in colonic lamina propria mononuclear cells in mice treated with administration of an IRF4-expressing plasmid. C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. Colonic lamina propria mononuclear cells were isolated on day 2 and stained with PE-conjugated CD11b, CD11c, or CD3 Ab and Alexa488-conjugated FLAG Ab.

Acknowledgments

This work was supported by Grant-in-Aid for Scientific Research (25293172, 21229009, 24229005, and 24659363) from Japan Society for the Promotion of Science, the Japanese Society of Gastroenterology, and the Special Coordination Funds by the Ministry of Education, Culture, Sports, Science and Technology of Japan and Astellas Pharma Inc. in Creation of Innovation Centers for Advanced Interdisciplinary Research Areas Program, and by the Intramural Research Program of the National Institutes of Health. We thank Ms. M. Tosaka and Dr. H. Ezoe for their assistance.

Footnotes

Conflicts of interest; none

The authors have no conflicting financial interests.

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Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

Supplementary Figure 1. H&E-stained colonic tissue of mice treated with intra-rectal administration of TNBS. (A) C57BL/10 mice were administered MDP on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. Colonic samples were obtained on day 4. Magnification x400. (B) C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. Colonic samples were obtained on day 4. Magnification x400 (C) C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on day 3 after challenge with TNBS on day 0. Colonic samples were obtained on day 6. Magnification x400.

Supplementary Figure 2. Expression of FLAG-IRF4 in colonic lamina propria mononuclear cells in mice treated with administration of an IRF4-expressing plasmid. C57BL/10 mice were administered HVJ-encapsulated FLAG-tagged IRF4 vector or control vector via the intra-rectal route on days -2, -1, and 0 and then challenged with intra-rectal TNBS on day 0. Colonic lamina propria mononuclear cells were isolated on day 2 and stained with PE-conjugated CD11b, CD11c, or CD3 Ab and Alexa488-conjugated FLAG Ab.

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