The transcription coactivator YAP plays a vital role in Hippo pathway for organ-size control and tissue homeostasis. Recent studies have demonstrated YAP is closely related to immune disorders and inflammatory diseases, but the underlying mechanisms remain less defined. Here, we find that YAP promotes the activation of NLRP3 inflammasome, an intracellular multi-protein complex that orchestrates host immune responses to infections or sterile injuries. YAP deficiency in myeloid cells significantly attenuates LPS-induced systemic inflammation and monosodium urate (MSU) crystals-induced peritonitis. Mechanistically, YAP physically interacts with NLRP3 and maintains the stability of NLRP3 through blocking the association between NLRP3 and the E3 ligase β-TrCP1, the latter increases the proteasomal degradation of NLRP3 via K27-linked ubiquitination at lys380. Together, these findings establish a role of YAP in the activation of NLRP3 inflammasome, and provide potential therapeutic target to treat the NLRP3 inflammasome-related diseases.
The NLRP3 inflammasome is a multiple protein complex that plays critical role in host immune responses to infections or sterile injuries1,2,3. It consists of the nucleotide-binding domain, leucine-rich repeat, pyrin domain-containing protein 3 (NLRP3), the apoptosis-associated speck like protein containing a CARD (ASC) and caspase-1. NLRP3 can be activated by a broad range of microbial components, endogenous danger signals and environmental irritants1. Once activated, the NLRP3 inflammasome serves as a platform for the activation of caspase-1, which induces the maturation of interleukin (IL)-1β and IL-18, as well as gasdermin d-mediated pyroptotic cell death1,2,3. It is well-known that the deregulated NLRP3 inflammasome drives the progression of many inflammatory, metabolic, degenerative and aging-related diseases, such as atherosclerosis, gout, type 2 diabetes, autoimmune disorders, and Alzheimer’s disease4,5,6,7. Therefore, NLRP3 inflammasome activity must be tightly regulated to maintain immune homeostasis and avoid detrimental effects. Although the mechanisms by which NLRP3 inflammasome is activated has been studied extensively, its endogenous regulatory networks remain largely unknown.
The Hippo-YAP pathway, which is highly evolutionarily conserved in mammals, is a key regulator to control the organ size8,9. This pathway integrates a variety of cellular stress signaling to maintain tissue homeostasis, including mechanical stress, DNA damage and oxidative stress under physiological and pathological conditions10. Upon activation of the Hippo pathway, the transcription co-activators YAP and TAZ are phosphorylated by Lats1/2 and retained in the cytoplasm for degradation. When the signaling is turned off, YAP/TAZ are predominantly localized in the nucleus, binding to transcription factors of the TEAD family and other factors to promote gene transcription8,9. Recent studies have revealed the role of the Hippo-YAP pathway in innate antibacterial11,12,13 and antiviral immune responses14,15 via transcriptional or non-transcriptional activity, providing new insights into the crosstalk between the innate immune system and the Hippo-YAP pathway. Moreover, the elevated expression of YAP is associated with the progression of atherosclerosis16, inflammatory bowel disease (IBD)17, sepsis18, and pancreatitis19. Together with the findings that these inflammatory disorders involve the deregulated NLRP3 inflammasome activity, we postulated that YAP might regulates the activation of NLRP3 inflammasome.
In this work, we demonstrate that YAP promotes the activation of NLRP3 inflammasome. Deletion of YAP in myeloid cells significantly attenuates lipopolysaccharide (LPS)-induced systemic inflammation and monosodium urate (MSU) crystals-induced peritonitis. Activation of the Hippo signaling that induces the degradation of YAP markedly decreases the activity of the NLRP3 inflammasome in vitro. Mechanistically, YAP physically interacts with NLRP3 and maintains its stability through blocking the association between NLRP3 and the E3 ligase β-TrCP1, the latter promotes the proteasomal degradation of NLRP3 via K27-linked ubiquitination at lys380. Thus, we uncover a role of YAP in regulation of the NLRP3 inflammasome activation, and provide potential therapeutic target to treat a number of inflammatory disorders, such as atherosclerosis, gout, colitis, and sepsis.
YAP specifically promotes NLRP3 inflammasome activation
To investigate the role of YAP in the NLRP3 inflammasome activation, we diminished the YAP expression in primary mouse macrophages using small-interfering RNA (siRNA) (Supplementary Fig. 1a). Knockdown of YAP expression markedly suppressed ATP-, nigericin-, or MSU-induced caspase-1 cleavage and release of IL-1β and IL-18, without affecting the tumor necrosis factor alpha (TNF-α) secretion (Fig. 1a, b). We also examined whether YAP specifically regulates the NLRP3 inflammasome activation and found that silencing of YAP expression had no effect on either poly (dA:dT)-induced AIM2 inflammasome or flagellin (FLA) transfection-induced NLRC4 inflammasome activation (Fig. 1a). To confirm this phenomenon, we generated Yapfl/fl lyz2-Cre mice with Yap deletion in myeloid cells20. ATP, nigericin or MSU-induced cleavage of caspase-1 and release of IL-1β and IL-18 were markedly suppressed in YAP-deficient (Yapfl/fl lyz2-Cre) macrophages as compared to that of YAP-sufficient (Yapfl/fl) macrophages (Fig. 1c, d). By contrast, YAP deletion did not alter the release of IL-1β and IL-18 upon poly (dA:dT) or flagellin transfection (Fig. 1c, d). The NLRP3 inflammasome activation induces the oligomerization of ASC, resulting in formation of ASC specks through the pyrin domain1,2,3. Accordingly, deletion of YAP markedly inhibited the ASC oligomerization and ASC-speck formation (Fig. 1e, f). NLRP3 is pivotal for caspase-1-dependent IL-1β maturation upon non-canonical inflammasome activation21. As expected, YAP deficiency suppressed both caspase-1 cleavage and IL-1β release in macrophages transfected with LPS (Supplementary Fig. 1b, c). Taken together, our data demonstrate that YAP deficiency specially impairs the NLRP3 inflammasome activation.
Cytoplasmic YAP inhibits the proteasomal degradation of NLRP3
Next, we sought to investigate the mechanisms by which YAP promotes the NLRP3 inflammasome activation. It is well-established that the activation of NLRP3 inflammasome requires two steps, termed priming and assembly1. The priming step involves the stimulation of NLRP3 expression, which is critical for the subsequent inflammasome activation1,3. We examined the expression of NLRP3 inflammasome components in mouse macrophages following LPS stimulation and found that YAP deficiency markedly decreased the protein expression of NLRP3 without affecting the expression of caspase-1, pro-IL-1β, and ASC (Fig. 2a). Intriguingly, deletion of YAP failed to affect the mRNA expression of NLRP3 (Supplementary Fig. 2a), clearly suggest that YAP promotes NLRP3 expression at the post-transcriptional level. In line with the previous findings that NLRP3 degradation impairs the NLRP3 inflammasome activation1, YAP deficiency significantly promoted the protein degradation of NLRP3 but not ASC or caspase-1 (Fig. 2b, c). NLRP3 degradation was reversed by the proteasome inhibitor MG-132, but not the lysosome inhibitor chloroquine or the autophagy inhibitor 3-MA (Fig. 2d–f). suggesting that YAP inhibits the proteasomal degradation of NLRP3.
Previous studies22,23 have reported that substitution of YAP residue Ser112 with Ala (S112A) generates a nuclear protein with constitutive transcriptional activity (Supplementary Fig. 2b). Using genetically modified HEK293T cells expressing the NLRP3 inflammasome components, we observed that overexpression of wild-type but not S112A mutant YAP markedly increased the IL-1β release (Fig. 2g) and promoted the NLRP3 expression in a dose-dependent manner (Fig. 2h), while the S112A YAP mutant had no such effect (Fig. 2g, h). Moreover, YAP predominantly localized in the cytoplasm of macrophages upon LPS stimulation (Supplementary Fig. 2c, d). These results suggest that cytoplasmic YAP is critical for maintaining the stability of NLRP3.
Hippo signaling suppresses the NLRP3 inflammasome activation in a YAP-dependent manner
The Hippo pathway, activated by various cellular stresses, is known to induce the degradation of YAP8,9. We then asked whether cellular stresses-induced Hippo signaling could affect the NLRP3 inflammasome activation, and subjected cells to serum starvation or high cell confluence, both of which are well-known cellular stress conditions that activate the Hippo signaling24,25, this led to YAP Ser127 phosphorylation and YAP degradation, indicative of the activation of Hippo signaling (Supplementary Fig. 3a, b). Serum starvation or high cell confluence markedly inhibited the NLRP3 inflammasome-induced release of IL-1β and IL-18 in WT but not YAP-deficient macrophages, without affecting the secretion of TNF-α (Fig. 3a, b). Upon activation of the Hippo signaling, Lats1/2 mediates YAP phosphorylation, leading to its polyubiquitination and degradation24,25. To further confirm that the Hippo signaling regulates the activation of NLRP3 inflammasome through YAP, we next investigated the role of Lats1/2 in activation of the NLRP3 inflammasome. Silencing of Lats1/2 expression in macrophages prevented the decrease of YAP expression (Supplementary Fig. 3c, d), and enhanced NLRP3 agonists-induced IL-1β and IL-18 secretion during serum starvation (Fig. 3c). The coactivator TAZ is a downstream effector of Hippo signaling8,9. However, in contrast to the lung tissues, macrophages did not express detectable TAZ expression in the presence or the absence of LPS stimulation (Supplementary Fig. 3e, f). Taken together, our findings indicated that the Hippo signaling suppresses the NLRP3 inflammasome activation in a YAP-dependent manner.
YAP suppresses K27-linked ubiquitination of NLRP3
Protein ubiquitination is a crucial step in the ubiquitin–proteasome degradation pathway26. We next determined whether YAP participates in the ubiquitination of NLRP3. We found that NLRP3 ubiquitination was markedly decreased in HEK293T cells over-expressing YAP (Fig. 4a). By contrast, deletion of YAP in myeloid cells increased the NLRP3 ubiquitination (Fig. 4b). Since different types of polyubiquitin linkages mediate distinct biological functions, we expressed Myc-tagged NLRP3 in HEK293T cells together with a series of ubiquitin mutants (K6, K11, K27, K29, K33, K48, and K63), all of which contained only one indicated lysine available for poly-linkage. Notably, over-expressing YAP markedly decreased K27-linked polyubiquitination of NLRP3 but had no appreciable effect on the NLRP3 ubiquitination of other types of linkages (Fig. 4c). When we replaced K27 with an arginine (K27R), YAP was no longer able to decrease the polyubiquitination of NLRP3 (Fig. 4d). Taken together, these data suggest that YAP selectively suppresses the K27-linked ubiquitination of NLRP3.
YAP suppresses β-TrCP1-mediated K27-linked ubiquitination of NLRP3
Since YAP could block the ubiquitination of NLRP3, we speculated that there may exist a YAP-associated enzyme that mediates NLRP3 ubiquitination. The 14-3-3 protein has been reported to bind to phosphorylated YAP, sequestering it in the cytoplasm8,9. Previous studies have suggested that 14-3-3σ promotes the ubiquitination of c-myc and COP127,28, prompting us to examine the role of 14-3-3σ in NLRP3 ubiquitination. However, expressing 14-3-3σ did not enhance the ubiquitination of NLRP3 (Supplementary Fig. 4a).
Other studies report that β–transducin repeat containing E3 ubiquitin protein ligase 1 (β-TrCP1), targets YAP for ubiquitination and degradation29,30,31,32. Thus, we next determined whether β-TrCP1 could mediate the ubiquitination of NLRP3. To address this, we first measured the interaction between β-TrCP1 and NLRP3. We found that β-TrCP1 co-immunoprecipitated with NLRP3 in HEK293T cells expressing both Flag-tagged β-TrCP1 and Myc-tagged NLRP3 (Supplementary Fig. 4b). Co-immunoprecipitation assays confirmed that endogenous β-TrCP1 interacted with NLRP3 in LPS-stimulated primary macrophages (Supplementary Fig. 4c). Further, confocal microscopy revealed the colocalization of β-TrCP1 and NLRP3 in primary macrophages (Supplementary Fig. 4d). As shown by previous studies33,34, the classic DSG(X)2+NS motif and “atypical” XSG(X)2+NS motif are important characteristics of substrates for β-TrCP1 binding. We therefore scanned the NLRP3 protein sequence and identified two potential phosphodegron motifs, namely 193-DSPMSS-198 and 890-NSGLTS-895; the latter is conserved among species (Supplementary Fig. 4e). Given that serine phosphorylation within the degron is crucial for the recognition by β-TrCP1, we generated mutants in which all serine residues within the putative degron motifs were replaced with alanine. The NLRP3 S891A/S895A mutant lost its ability to bind to β-TrCP1, while NLRP3 S194A/S197A/S198A bound to β-TrCP1 in a manner similar to that of wild-type NLRP3 (Supplementary Fig. 4f), suggesting that the 890-NSGLTS-895 motif of NLRP3 is crucial for its binding to β-TrCP1.
Next, we tested whether β-TrCP1 mediates the ubiquitination of NLRP3. We found that the K27-linked ubiquitination and the overall polyubiquitination of NLRP3 was markedly increased in HEK293T cells overexpressing β-TrCP1 (Fig. 5a). Silencing β-TrCP1 expression in primary macrophages decreased the ubiquitination of NLRP3 (Fig. 5b). These data clearly suggest that β-TrCP1 binds to NLRP3 and mediates the ubiquitination of NLRP3. To further investigate the relationship between YAP and β-TrCP1 in mediating NLRP3 ubiquitination, we expressed YAP, β-TrCP1, and NLRP3 in HEK293T cells and observed that YAP over-expression blocked β-TrCP1-induced polyubiquitination and K27-linked ubiquitination of NLRP3 (Fig. 5a). Accordingly, the decreased NLRP3 expression mediated by β-TrCP1 was rescued by YAP overexpression (Fig. 5c). Collectively, these data indicate that YAP blocks β-TrCP1-mediated K27-linked ubiquitination and polyubiquitination of NLRP3.
YAP disrupts the interaction between NLRP3 and β-TrCP1 through competing with β-TrCP1 to bind NLRP3
To explore the mechanism by which YAP blocks β-TrCP1-mediated K27-linked ubiquitination of NLRP3, we determined whether YAP affects the physical interaction between β-TrCP1 and NLRP3. Co-expression of YAP decreased the interaction between β-TrCP1 and NLRP3 (Fig. 5d), whereas YAP deficiency increased the capacity of β-TrCP1 to bind NLRP3 (Fig. 5e), indicating that YAP disrupts the interaction between β-TrCP1 and NLRP3. Three possible explanations might explain the underlying mechanisms. First, YAP may affect the serine phosphorylation of NLRP3, leading to the decreased binding between NLRP3 and β-TrCP1. Second, YAP might directly interact with β-TrCP1 and thereby mask the NLRP3 binding site of β-TrCP1. Third, YAP might directly interact with NLRP3 and thereby mask the β-TrCP1 binding site of NLRP3.
To test the first possibility, we overexpressed YAP in iBMDMs and assessed NLRP3 serine phosphorylation. LPS stimulation led to the increase of NLRP3 serine phosphorylation, which was not affected by YAP overexpression, excluding the first possibility (Supplementary Fig. 5a). To test the second possibility, we overexpressed YAP-S366A mutant (in humans, the homologous mutant is YAP-S381A), which lost the β-TrCP1 binding capacity31 (Supplementary Fig. 5b). However, the S366A substitution in YAP did not affected the NLRP3 and β-TrCP1 binding (Supplementary Fig. 5c), suggesting that YAP interrupts the NLRP3 and β-TrCP1 interaction independent of its direct binding to β-TrCP1. Next, we tested the third possibility and observed an association between YAP and NLRP3 (Supplementary Fig. 5d). This phenomenon was confirmed by using Proximity Ligation Assay (PLA), which could visualize the protein-protein interactions in vivo (Supplementary Fig. 5e, f). As shown by co-immunoprecipitation assay, we found that the C-terminal transactivation domain (residues 151–488) rather than the N-terminal TEAD binding domain of YAP physically interacted with NLRP3 (Supplementary Fig. 5g, h). Co-expression of wild-type YAP or its C-terminal transactivation domain but not the N-terminal TEAD-binding domain interrupted the interaction between NLRP3 and β-TrCP1 (Supplementary Fig. 5i), indicating that the NLRP3-YAP binding inhibits the NLRP3-β-TrCP1 interaction. Further, we observed that both YAP and β-TrCP1 bound to the same domain of NLRP3 (NACHT and LRR domain) (Supplementary Fig. 5j, k, l). Taken together, these results demonstrate that YAP disrupts the interaction between NLRP3 and β-TrCP1 through competing with β-TrCP1 to bind NLRP3.
β-TrCP1 inhibits NLRP3 inflammasome activation
To determine whether β-TrCP1 might inhibit the NLRP3 inflammasome activation, we knocked down the expression of β-TrCP1 in primary macrophages by using siRNA. Silencing of β-TrCP1 expression in primary macrophages markedly enhanced the release of IL-1β or IL-18, but did not affect the TNF-α secretion, upon stimulation by NLRP3 agonists (Fig. 6a). Accordingly, silencing of β-TrCP1 expression markedly decreased the NLRP3 expression (Fig. 6b). Moreover, upon silencing of β-TrCP1 in YAP-deficient macrophages from Yapfl/fllyz2-Cre mice, the decline in IL-1β or IL-18 secretion and NLRP3 expression was rescued as compared to that of in macrophages from control Yapfl/fl mice (Fig. 6c, d), which further confirmed that YAP could suppress β-TrCP1-mediated NLRP3 degradation. These results clearly suggest that β-TrCP1 inhibits NLRP3 inflammasome activation.
Lys380 in NLRP3 is essential for its ubiquitination and degradation
Next, we sought to identify the β-TrCP1-mediated ubiquitination site of NLRP3. HEK293T cells were transfected with plasmids encoding a series of truncation mutants of NLRP3(▵PYD, ▵NACHT and▵LRR) (Supplementary Fig. 5j) and HA-ubiquitin-K27, with or without exogenous β-TrCP1 expression. Notably, deletion of the NACHT domain prevented NLRP3 ubiquitination upon β-TrCP1 co-expression (Supplementary Fig. 6a), suggesting that β-TrCP1 mediates the ubiquitination of the NACHT domain of NLRP3. We further analyzed the most conserved lysine residues within the NACHT domain among species and constructed plasmids encoding mutated NLRP3 with individual lysine residue replaced by arginine (K/R) (Supplementary Fig. 6b). The K380R substitution rather than other point mutations abolished β-TrCP1-mediated K27-linked ubiquitination of NLRP3 (Fig. 7a). We next tested whether K27-linked ubiquitin chains on K380 might function as a degradation signal for NLRP3, and observed a significantly slower degradation rate of the K380R NLRP3 mutant as compared to that of wild-type NLRP3 (Fig. 7b). Further, co-expression of β-TrCP1 failed to promote the degradation of the K380R NLRP3 mutant (Fig. 7c).
To further address the functional importance of K380 ubiquitination, we reconstituted the NLRP3 inflammasome in HEK293T cells and observed that the expression of K380R mutant enhanced IL-1β secretion as compared to that of wild-type NLRP3 (Fig. 7d). To confirm this phenomenon in immune cells, we induced the expression of WT NLRP3 or its K380R mutant in NLRP3−/− iBMDMs using lentivirus, and then stimulated the LPS-primed iBMDMs with ATP or nigericin. We found that expression of the K380R mutant significantly increased the release of IL-1β but not TNF-α secretion as compared to that of cells expressing WT NLRP3 (Fig. 7e, f). Taken together, these data indicate that K380 of NLRP3 is an important site for the K27 ubiquitination and the degradation of NLRP3.
YAP promotes NLRP3 inflammasome activation in vivo
Finally, we investigated the role of YAP in NLRP3 inflammasome activation in vivo. Intraperitoneal (i.p.) injection of LPS induces IL-1β secretion and neutrophil infiltration in a NLRP3-dependent manner35,36. Notably, the secretion of IL-1β but not TNF was significantly reduced in Yapfl/fllyz2-Cre mice, as compared to that of in control Yapfl/fl mice (Fig. 8a). Moreover, deletion of YAP in myeloid cells markedly attenuated endoxemia-induced lung injury, as evaluated by histopathology (Fig. 8b). To confirm the role of YAP in regulating NLRP3 inflammasome activation in vivo, we injected i.p. the mice with monosodium urate (MSU), which induces neutrophil infiltration and peritonitis in a NLRP3 dependent manner35,36. We observed that deletion of YAP in myeloid cells significantly inhibited MSU-induced IL-1β release and neutrophil infiltration as compared to that of in control Yapfl/fl mice (Fig. 8c, d and Supplementary Fig. 7). Collectively, these findings demonstrated that YAP promotes NLRP3 inflammasome activation in vivo.
The Hippo pathway participates in the innate immune responses in multiple aspects, including antibacterial immune response, antiviral immune response and macrophage polarization17,37,38. Accumulating evidence suggest that up-regulation of YAP expression is associated with the development of inflammatory diseases, such as atherosclerosis16, inflammatory bowel disease(IBD)17, sepsis18 and pancreatitis19. However, the underlying mechanisms by which YAP regulates inflammation and promotes the pathogenesis of inflammatory diseases are not fully understood. In this study, we demonstrated that myeloid YAP deficiency specifically impairs NLRP3 inflammasome activation both in vitro and in vivo. In addition, serum starvation- or high cell confluence-induced Hippo signaling activation that induces the degradation of YAP markedly decreased the activity of the NLRP3 inflammasome. Mechanistically, YAP maintains the stability of NLRP3 by direct binding to NLRP3, thereby blocking the accessibility of E3 ligase β-TrCP1, the latter promotes the proteasomal degradation of NLRP3 via K27-linked ubiquitination at K380 (Fig. 8e). Thus, our study provides a mechanistic insight into the regulatory roles of YAP in inflammation.
Accumulated evidence reveal that altered NLRP3 expression is associated with the pathogenesis of several inflammatory disorders, including atherosclerosis39,40, type-2 diabetes (T2D)41, and autoimmune diseases42. Our study suggests that YAP may be a potential therapeutic target to regulate NLRP3 protein expression in many inflammatory diseases. This is consistent with a recent report43 showing elevated YAP expression in atherosclerotic plaques, which are enriched in NLRP3 expression40,41. It was also found that YAP protein levels correlate with plasma IL-1β levels in patients with ST-segment elevated myocardial infarction (STEMI)43, suggesting that YAP could be a potential target for the treatment of atherosclerosis. Serum starvation and high cell confluence, the well-known cellular stresses that activate Hippo signaling, could inhibit the NLRP3 inflammasome activation in a YAP-dependent manner. Given that other cellular stresses, including matrix stiffness, mechanical stress, and long-range hormonal signals, are able to activate the Hippo-YAP pathway, we propose that these stress signaling might also regulate the NLRP3 inflammasome activation in the lung, a highly mechanical organ44.
Ubiquitination of NLRP3 plays an important role in the regulation of inflammasome1,45. To date, NLRP3 has been reported to be ubiquitinated with both K48 and K63 linkages. A series of enzymes that are responsible for K48-linked ubiquitination of NLRP3 have been identified, including PAI246, MARCH735, FBXL247, Trim3148, and Cbl-b49. All of these bind to NLRP3 and mediate the degradation of NLRP3 either by the autophagy-lysosomal pathway or the ubiquitin-proteasome pathway. BRCC3-mediated deubiquitination of NLRP3 is required for NLRP3 inflammasome assembly and activation50, in which the ubiquitination of NLRP3 consists of both K48 and K63 linkages. In our study, we found that NLRP3 can be ubiquitinated with K27 linkage, leading to subsequent NLRP3 degradation in the ubiquitin-proteasome pathway. This finding provides insights into the regulation of NLRP3 degradation. Although most studies have shown that K48-linked ubiquitination is the signal that mediates proteasomal degradation51,52, our work provides compelling evidence that K27-linked ubiquitination could also lead to the proteasomal degradation of target proteins53,54,55. Moreover, we identified that Lys380 is the K27-linked ubiquitination site by screening the most-conserved lysine residues in the NACHT domain of NLRP3. When we replaced lysine with arginine, the degradation of NLRP3 was inhibited. Accordingly, cells expressing the NLRP3 K380R mutant released more IL-1β as compared to cells expressing WT NLRP3. Thus, our study revealed a ubiquitination site for NLRP3 degradation and inactivation.
β-TrCP1, one of the best-characterized mammalian F-box proteins of SCF ligase, has been reported to be involved in the ubiquitination of well-established substrates, such as YAP, β-catenin, IκB, caspase-334,56. All of these studies have suggested that β-TrCP1-mediated substrate ubiquitination is K48-linked. However, in current study, we did not observe that β-TrCP1-mediated K48-linked ubiquitination of NLRP3. Instead, β-TrCP1 promoted K27-linked ubiquitination of NLRP3 and its subsequent degradation. It has been well-documented that β-TrCP1’s substrates contain a consensus DSG(X)2+nS degron33,34. The serine residues in this degron could be phosphorylated by specific protein kinases, resulting in β-TrCP1 recognition and subsequent ubiquitination of the substrates. We identified the 890-NSGLTS-895 motif, an “atypical” XSG(X)2+NS motif in NLRP3, is essential for β-TrCP1 binding. However, the kinase responsible for NLRP3 serine phosphorylation remains unknown. Previous studies have shown that kinases JNK136, PKA57,58, PKD59, and AKT60 could mediates serine phosphorylation of NLRP3. However, the reported phosphorylation site was neither serine 891 nor 895. Whether these kinases could also mediate serine 891/895 phosphorylation and whether unrecognized kinases account for NLRP3 phosphorylation, are interesting questions for future studies. Previous studies have suggested that 14-3-3 family members including 14-3-3ε, 14-3-3η, and14-3-3τ, can bind to pyrin and regulate the activation of the pyrin inflammasome61,62. Although we found that 14-3-3σ has no effect on the ubiquitination of NLRP3, the role of the14-3-3 family in NLRP3 inflammasome activation deserves further investigation.
In this work, our study uncovers a role of YAP in regulation of the NLRP3 inflammasome activation, and provides potential therapeutic target to treat a number of inflammatory disorders, such as atherosclerosis, gout, colitis and sepsis.
Yapfl/fl mice and Lyz2-Cre mice on the C57BL/6 background were from Jackson laboratories20. Yapfl/fl mice were crossed with Lyz2-Cre mice to obtain Yapfl/fl lyz2-Cre mice. Wild-type C57BL/6 mice (8–10 weeks old) were purchased from Hunan SJA Laboratory Animal Co.Ltd (Changsha, China). All the animals were generated in specific pathogen-free (SPF) levels and daily cycles of 12 h of light at 23 °C and 12 h of dark at 21 °C. All animal experiments were conducted in accordance with the Institutional Animal Care and Use Committee of Central South University.
Ultrapure LPS (E. coli 0111:B4), Standard LPS (E. coli 0111:B4), Pam3CSK4, ATP, Nigericin, MSU, FLA-ST, Poly(dA:dT) naked, DyLight 488-labeled secondary antibody (A120-100D2, 1:50 for immunofluorescence), Alexa Fluor 594-conjugated secondary antibody (405326, 1:50 for immunofluorescence) were purchased from InvivoGen. Lipofectamine 2000 Transfection Reagent, Pierce™ Anti-c-Myc Agarose were from ThermoFisher Scientific. Anti-Caspase-1 antibody (ab179515, 1:1000 for WB), mouse IL-18 ELISA kit (Ab218808) were purchased from Abcam. Anti-IL-1β antibody (AF-401-NA; RRID: AB_416684, 1:1000 for WB) was from RD systems. Anti-YAP1 antibody (A1002, 1:1000 for WB), Anti-TAZ antibody (A15806, 1:1000 for WB) were from ABclonal. Anti-NLRP3 antibody (Cryo-2, 1:1000 for WB, 1:400 for IP), Anti-ASC antibody (AL177, 1:1000 for WB) were purchased from Adipogen. Anti-β-actin antibody (BH10D10, 1:10000 for WB), Anti-Phospho-YAP(Ser127) antibody (4911, 1:1000 for WB), Anti-β-TrCP antibody (D13F10, 1:1000 for WB), Cell Lysis Buffer were from Cell Signaling Technology. Anti-LATS1 antibody (AF7669, 1:1000 for WB) was from Affinity.
Anti-Ub antibody (Sc-8017, 1:200 for WB), mouse immunoglobin IgG protein (SC-2025, 1:160 for IP), Protein A/G PLUS-Agarose were from Santa cruz. Anti-HA-tag (M180-3, 1:5000 for WB), Anti-DDDDK-tag (M185-3L, 1:5000 for WB), Anti-Myc-tag (M047-3, 1:5000 for WB), Anti-His-tag (D291-3, 1:5000 for WB) were from MBL. FITC anti-mouse/human CD11b (101216, 1:500 for flow cytometry) and APC anti-mouse Ly-6G (127614, 1:500 for flow cytometry) were from Biolegend. Cholera Toxin B Subunit (Choleragenoid) from Vibrio cholerae was purchased from List Biological Laboratories, INC. Anti-Flag affinity gel was from Sigma. pLenti-CRISPR v2 was from Addgene. First-Strand cDNA Synthesis SuperMix was purchased from TransGen Biotech. SYBR quantitative PCR (qPCR) Master Mix was from Vazyme Biotech. Mouse IL-1β ELISA kit (88-7013), Mouse TNF-α ELISA kit (88-7324) were purchased from eBioscience. Duolink In Situ Red Starter Kit Goat/Rabbit kit, Duolink In Situ PLA Probe Anti-Mouse MINUS were purchased from Sigma.
To obtain mouse primary peritoneal macrophages, mice were injected intraperitoneally with 3% thioglycolate. Three days later, peritoneal exudate cells were harvested and incubated. Two hours later, nonadherent cells were removed and the adherent monolayer cells were used as peritoneal macrophages. HEK293T cells were obtained from American Type Culture Collection (Manassas, VA). The cells were cultured in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10% fetal bovine serum and 1% penicillin and streptomycin.
The concentration of agonists or stimuli were used as below: For NLRP3 inflammasome activation: peritoneal macrophages were primed with LPS (100 ng/mL) for 3 h followed by stimulation with 5 mM ATP (1 h); 10 μM Nigericin (1 h); 200 μg/mL MSU (6 h). For non-canonical NLRP3 inflammasome activation, macrophages were primed for 4 h with Pam3CSK4 (100 ng/mL), then treated with LPS (2 μg/mL) combined with CTB (5 μg/mL) (CTB + LPS), or LPS (2 μg/mL) transfected with FuGENE HD (0.25% v/v) for 16 h. For AIM2 inflammasome activation, Pam3CSK4- primed macrophages were transfected with Poly (dA:dT) (1 μg/mL) using Lipofectamine 2000 (3 μL/mg DNA) following the manufacturer’s protocol (Invitrogen). For NLRC4 inflammasome activation, macrophages were primed with LPS (100 ng/mL) for 3 h, then transfected with Flagellin (2 μg/mL) by Lipofectamine 2000 for 1 h.
Reconstitution of NLRP3 inflammasome in HEK293T cells
A standard reconstitution system in HEK293T cells was referred63. HEK293T cells were seeded into 24-well plates at density of 2 × 105 cells per well in complete cell culture medium overnight before transfection. The cells were transfected with plasmids expressing pro-IL-1β-flag (200 ng/well), pro-caspase-1-myc (100 ng/well), ASC-myc (20 ng/well), NLRP3-myc (200 ng/well) using Linear Polyethylenimine. Twenty-four to 36 h later, replace the medium with 250 μL DMEM cell culture medium, then 10 μM nigericin was added one hour before supernatant collection.
Plasmids and transfection
NLRP3, caspase-1, pro-IL-1β, ASC, 14-3-3σ, and β-TrCP1 full-length sequences were obtained from mouse peritoneal macrophage cDNA and YAP full-length sequences was obtained from mouse testis tissue cDNA, then cloned into pcDNA3.1 vector that contained different tags. Deleted, truncated, and point mutants were generated by PCR-based amplification and the construct encoding the wild-type protein as the template. All constructs were confirmed by DNA sequencing. Ubiquitin and its mutants (K6, K11, K27, K29, K33, K48, K63and K27R) genes were synthesized (Sangon Biotech, Shanghai, China) and cloned into pcDNA3.1-HA eukaryotic expression vectors respectively. Plasmids were transiently transfected into HEK293T cells with Linear Polyethylenimine. For iBMDMs, we generate NLRP3, NLRP3 K380R, and YAP plasmids, which cloned in the lentiviral vector, pCDH-MCS-T2AcopGFP. Lentivirus was produced in HEK293T cells by co-transfection of lentiviral vectors (pCDH-MCS-EF1-copGFP), pSPAX2, and pVSV-G with a ratio of 3:2:1. Virus-containing supernatants were filtered through a 0.45-μm-pore-size filter (Millipore) and supplemented with polybrene (8 μg/mL) before adding to cells. NLRP3−/− iBMDMs were re-transduced with lentivirus encoding NLRP3 WT or NLRP3 K380R mutant in pCDH-MCS-EF1-copGFP vectors (System Biosciences). GFP-positive cells were then sorted by flow cytometry (FACS Aria II, BD Biosciences).
ASC oligomerization and ASC speck formation
Peritoneal macrophages were plated in 6-well plates (2 × 106 cells per well), then stimulated with 100 ng/mL LPS for 3 h, followed by stimulation with or without 10 μM nigericin (1 h). The cells were lysed with Triton Buffer [50 mM Tris-HCl (pH 7.5), 150 mM NaCl, 0.1% Triton X-100, 0.1 mM PMSF and EDTA-free protease inhibitor cocktail] at 4 °C for 10 min, then remove 30 μL as whole cell lysates. The rest of cell lysates were centrifuged at 6000 × g at 4 °C for 15 min, the supernatant was collected and pellet was washed twice and re-suspended in 200 μL Triton Buffer, and cross-linked for 30 min at 37 °C with 2 mM disuccinimidyl suberate (DSS). The pellets were collected after centrifuged for 15 min at 6000 × g, and dissolved in SDS loading buffer for immunoblot analysis
For ASC speck formation, peritoneal macrophages were seeded on chamber slides and allowed to attach overnight. The next day, the cells were treated with indicated stimulators. Then the cells were fixed in 4% paraformaldehyde followed by permeabilization with 0.1% Triton X-100 for 30 min. Then the slides were blocked with phosphate-buffered saline (PBS) containing 1% Bovine serum albumin (BSA), followed by ASC and DAPI staining.
Cells were visualized by fluorescence microscope (Nikon Ti2-U).
Proximity ligation assay
Proximity ligation assays were carried out to detect protein-protein interactions in situ by using Duolink reagents (Sigma). Briefly, primary macrophages were cultured on a six-well object glass in RPMI medium 1640. After stimulated with LPS for 4 h or not, cells were fixation in 4% paraformaldehyde and permeabilization with PBS containing 0.1% Triton X-100, then incubated over night with primary antibody pair of different species directed to NLRP3 (1:200), YAP (1:200), β-TrCP1 (1:200). Probe incubation, ligation and amplification reaction were carried out according to the manufacturer instructions. Thus, each individual pair of proteins generated a spot that could be visualized using fluorescent microscopy (Nikon Ti2-U).
CRISPR/Cas9-mediated generation of NLRP3−/− iBMDM cells
CRISPR/Cas9 genomic editing for gene deletion according to the previous publication64. Guide RNA sequences targeting NLRP3(5′- gtcctcctggcataccatag- 3′) with BsmbI sticky end were annealed and inserted into the lentiviral vectors pLenti-CRISPR v2(Addgene #52961) digested with BsmBI (NEB). Lentivirus was produced in HEK293T cells by co-transfection of plenti-sgRNA plasmid, pSPAX2, and pMD2.G with a ratio of 3:2:1. Virus-containing supernatants were filtered through a 0.45-μm-pore-size filter (Millipore) and supplemented with polybrene (8 μg/mL) before adding to cells. iBMDMs then were transduced with lentivirus encoding NLRP3 guide RNA. Stable transduced cells were selected with 5 mg/mL puromycin for 72 h, and single colonies were obtained by serial dilution and amplification. Clones were identified by immunoblotting with anti-NLRP3 antibodies, and the NLRP3−/− clone was used for the indicated analyses.
RNA interference assay
Peritoneal macrophages were seeded in 24 well (2 × 105 cells per well) or 6-well plates (1 × 106 cells per well), then transfected with siRNA using Lipofectamine RNAiMAX (Thermo Fisher Scientific) according to the manufacturer’s instructions. The siRNA sequences for mouse YAP (GGUCAAAGAUACUUCUUAATT), Mouse β-TrCP1 (CCAUCGCUGUGUGGGAUAUTT), Mouse Lats1(GCAAGUCACUCUGCUAAUUTT), Mouse Lats2(GCCUCAAUGCUGACUUGUATT) and the negative control (UUC UCCGAACGUGUCACGUTT) were chemically synthesized by Sangon Biotech Co., Shanghai, China.
Primary macrophages were stimulated with LPS for indicated hours, then cells were fixed with 4% paraformaldehyde for 15 min and permeabilized with 0.1% Triton X-100 for 10 min. After blocking with 3% BSA for 1 h, cells were incubated overnight with anti-NLRP3 antibody (1:100 in PBS containing 3% BSA) and β-TrCP1 antibody (1:100 in PBS containing 3% BSA), followed by staining with DyLight 488-labeled secondary antibody (Invitrogen) and Alexa Fluor 594-conjugated secondary Ab (Invitrogen) (1:50 in PBS containing 3% BSA). Nuclei were co-stained with DAPI (Invitrogen). Stained cells were viewed using a confocal fluorescence microscope (SpinSR10; Olympus).
Total RNA was extracted by using RNA Fast 200 kit according to the manufacturer’s instructions (FASTAGEN). Complementary DNA was synthesized by using TransScript All-in-One First-Strand cDNA Synthesis SuperMix for qPCR (TransGen Biotech) according to the manufacturer’s protocols. Quantitative PCR was performed using SYBR Green (Vazyme Biotech) on a LightCycler 480 (Roche Diagnostics), and data were normalized by the level of β-actin expression in each individual sample. The 2−ΔΔCT method was used to calculate relative expression changes.
Immunoprecipitation and western blot
HEK293T cells after transfection or peritoneal macrophages after stimulation, then lysed in IP buffer, which contained 1% (v/v) Nonidet P-40, 50 mM Tris-HCl (pH 7.4), 50 mM EDTA, 150 mM NaCl, and a protease inhibitor cocktail, pre-cleared cell lysates were then subjected to anti-Flag M2 affinity gel or anti-Myc affinity gel for 2 h or with specific Abs and protein G plus-agarose overnight, then washed four times with IP buffer. Immunoprecipitates were eluted by boiling with 1% (w/v) SDS sample buffer.
For ubiquitination analysis, cells were lysed in IP buffer supplemented with 10 mM NEM (Sigma), 1% SDS, protease inhibitor cocktail and PMSF. Obtained cell lysates were subsequently boiled for 5 min at 95 °C, diluted to 0.1% SDS with IP buffer, and immunoprecipitated.
For immunoblot analysis, cells were lysed with CLB buffer (CST) supplemented with protease inhibitor cocktail and PMSF, and then protein concentrations in the extracts were measured with a bicinchoninic acid assay (Pierce). Equal amounts of extracts were separated by sodium dodecyl sulphate–polyacrylamide gel electrophoresis, and then they were transferred onto nitrocellulose membranes for immunoblot analysis.
ELISA assay for cytokines
Levels of IL-1β, TNF-α, and IL-18 collected from cell culture and sera were determined using quantitative ELISA kits (eBioscience or abcam) according to the manufacturer’s instructions.
In vivo LPS challenge
Yapfl/fl lyz2-Cre mice and Yapfl/fl littermates were injected intraperitoneally with LPS (20 mg/kg body weight), after 6 h, the mice were killed, and the serum concentrations of IL-1β, and TNF-α were measured by ELISA.
MSU-induced peritonitis in vivo
Yapfl/fl lyz2-Cre mice and Yapfl/fl littermates were i.p. injected with 1 mg MSU (dissolved in 500 μL PBS) for 6 h. Peritoneal cavities were washed with 10 mL ice-cold PBS. The peritoneal lavage fluids were collected and concentrated for ELISA analysis with Amicon Ultra 10 K filter (UFC900308) from Millipore. Peritoneal exudate cells were collected and analyzed by FACS.
The data were analyzed by GraphPad Prism 8.0 software and were presented as the mean ± SD or mean ± SEM. Two-tailed unpaired Student’s t-test was used to compare the differences between two groups. One-way ANOVA or two-way ANOVA with Bonferroni’s post hoc test were used for comparisons of more than two groups. Differences were considered significant when *P < 0.05, **P < 0.01 and ***P < 0.001.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
The authors declare that the data supporting the findings of this study are available within the paper and its supplementary information files or available from the corresponding author upon reasonable request. Source data are provided with this paper.
Swanson, K. V., Deng, M. & Ting, J. P. The NLRP3 inflammasome: molecular activation and regulation to therapeutics. Nat. Rev. Immunol. 19, 477–489 (2019).
Guo, H., Callaway, J. B. & Ting, J. P. Inflammasomes: mechanism of action, role in disease, and therapeutics. Nat. Med. 21, 677–687 (2015).
Schroder, K. & Tschopp, J. The inflammasomes. Cell 140, 821–832 (2010).
Davis, B. K., Wen, H. & Ting, J. P. The inflammasome NLRs in immunity, inflammation, and associated diseases. Annu. Rev. Immunol. 29, 707–735 (2011).
Lamkanfi, M. & Dixit, V. M. Inflammasomes and their roles in health and disease. Annu. Rev. Cell Dev. Biol. 28, 137–161 (2012).
Wen, H., Ting, J. P. & O’Neill, L. A. A role for the NLRP3 inflammasome in metabolic diseases–did Warburg miss inflammation? Nat. Immunol. 13, 352–357 (2012).
Afonina, I. S., Zhong, Z., Karin, M. & Beyaert, R. Limiting inflammation-the negative regulation of NF-kappaB and the NLRP3 inflammasome. Nat. Immunol. 18, 861–869 (2017).
Yu, F. X., Zhao, B. & Guan, K. L. Hippo Pathway in organ size control, tissue homeostasis, and cancer. Cell 163, 811–828 (2015).
Pan, D. The hippo signaling pathway in development and cancer. Dev. Cell 19, 491–505 (2010).
Mao, B., Gao, Y., Bai, Y. & Yuan, Z. Hippo signaling in stress response and homeostasis maintenance. Acta Biochim. Biophys. Sin. 47, 2–9 (2015).
Liu, B. et al. Toll receptor-mediated hippo signaling controls innate immunity in Drosophila. Cell 164, 406–419 (2016).
Geng, J. et al. Kinases Mst1 and Mst2 positively regulate phagocytic induction of reactive oxygen species and bactericidal activity. Nat. Immunol. 16, 1142–1152 (2015).
Li, W. et al. STK4 regulates TLR pathways and protects against chronic inflammation-related hepatocellular carcinoma. J. Clin. Investig. 125, 4239–4254 (2015).
Wang, S. et al. YAP antagonizes innate antiviral immunity and is targeted for lysosomal degradation through IKKvarepsilon-mediated phosphorylation. Nat. Immunol. 18, 733–743 (2017).
Zhang, Q. et al. Hippo signalling governs cytosolic nucleic acid sensing through YAP/TAZ-mediated TBK1 blockade. Nat. Cell Biol. 19, 362–374 (2017).
Wang, L. et al. Integrin-YAP/TAZ-JNK cascade mediates atheroprotective effect of unidirectional shear flow. Nature 540, 579–582 (2016).
Zhou, X. et al. YAP aggravates inflammatory bowel disease by regulating M1/M2 macrophage polarization and gut microbial homeostasis. Cell Rep. 27, 1176–1189 e1175 (2019).
Lv, Y. et al. YAP controls endothelial activation and vascular inflammation through TRAF6. Circ. Res. 123, 43–56 (2018).
Morvaridi, S., Dhall, D., Greene, M. I., Pandol, S. J. & Wang, Q. Role of YAP and TAZ in pancreatic ductal adenocarcinoma and in stellate cells associated with cancer and chronic pancreatitis. Sci. Rep. 5, 16759 (2015).
Zhang, N. et al. The Merlin/NF2 tumor suppressor functions through the YAP oncoprotein to regulate tissue homeostasis in mammals. Dev. Cell 19, 27–38 (2010).
Kayagaki, N. et al. Non-canonical inflammasome activation targets caspase-11. Nature 479, 117–121 (2011).
Chen, Q. et al. Homeostatic control of Hippo signaling activity revealed by an endogenous activating mutation in YAP. Genes Dev. 29, 1285–1297 (2015).
Xin, M. et al. Hippo pathway effector Yap promotes cardiac regeneration. Proc. Natl Acad. Sci. USA 110, 13839–13844 (2013).
Yu, F. X. et al. Regulation of the Hippo-YAP pathway by G-protein-coupled receptor signaling. Cell 150, 780–791 (2012).
Mo, J. S., Yu, F. X., Gong, R., Brown, J. H. & Guan, K. L. Regulation of the Hippo-YAP pathway by protease-activated receptors (PARs). Genes Dev. 26, 2138–2143 (2012).
Jiang, X. & Chen, Z. J. The role of ubiquitylation in immune defence and pathogen evasion. Nat. Rev. Immunol. 12, 35–48 (2011).
Su, C. H. et al. 14-3-3sigma exerts tumor-suppressor activity mediated by regulation of COP1 stability. Cancer Res. 71, 884–894 (2011).
Phan, L. et al. The cell cycle regulator 14-3-3σ opposes and reverses cancer metabolic reprogramming. Nat. Commun. 6, 7530 (2015).
Zhao, B., Li, L., Lei, Q. & Guan, K. L. The Hippo-YAP pathway in organ size control and tumorigenesis: an updated version. Genes Dev. 24, 862–874 (2010).
Zhao, B., Tumaneng, K. & Guan, K. L. The Hippo pathway in organ size control, tissue regeneration and stem cell self-renewal. Nat. Cell Biol. 13, 877–883 (2011).
Zhao, B., Li, L., Tumaneng, K., Wang, C. Y. & Guan, K. L. A coordinated phosphorylation by Lats and CK1 regulates YAP stability through SCF(β-TRCP). Genes Dev. 24, 72–85 (2010).
Ma, S., Meng, Z., Chen, R. & Guan, K. L. The Hippo pathway: biology and pathophysiology. Annu. Rev. Biochem. 88, 577–604 (2019).
Liu, J. et al. β-TrCP restricts lipopolysaccharide (LPS)-induced activation of TRAF6-IKK pathway upstream of IκBα signaling. Front. Immunol. 9, 2930 (2018).
Bi, Y., Cui, D., Xiong X. & Zhao Y. The characteristics and roles of β-TrCP1/2 in carcinogenesis. FEBS J. https://doi.org/10.1111/febs.15585 (2020).
Yan, Y. et al. Dopamine controls systemic inflammation through inhibition of NLRP3 inflammasome. Cell 160, 62–73 (2015).
Song, N. et al. NLRP3 phosphorylation is an essential priming event for inflammasome activation. Mol. Cell 68, 185–197.e186 (2017).
Zhang, Y., Zhang, H. & Zhao, B. Hippo signaling in the immune system. Trends Biochem. Sci. 43, 77–80 (2018).
Hong, L., Li, X., Zhou, D., Geng, J. & Chen, L. Role of Hippo signaling in regulating immunity. Cell. Mol. Immunol. 15, 1003–1009 (2018).
Baldrighi, M., Mallat, Z. & Li, X. NLRP3 inflammasome pathways in atherosclerosis. Atherosclerosis 267, 127–138 (2017).
Abbate, A. et al. Interleukin-1 and the inflammasome as therapeutic targets in cardiovascular disease. Circ. Res. 126, 1260–1280 (2020).
Lee, H. M. et al. Upregulated NLRP3 inflammasome activation in patients with type 2 diabetes. Diabetes 62, 194–204 (2013).
Li, Z., Guo, J. & Bi, L. Role of the NLRP3 inflammasome in autoimmune diseases. Biomed. Pharmacother. 130, 110542 (2020).
Liu, M. et al. Macrophage K63-linked ubiquitination of YAP promotes its nuclear localization and exacerbates atherosclerosis. Cell Rep. 32, 107990 (2020).
Solis, A. G. et al. Mechanosensation of cyclical force by PIEZO1 is essential for innate immunity. Nature 573, 69–74 (2019).
Shim, D. W. & Lee, K. H. Posttranslational regulation of the NLR family pyrin domain-containing 3 inflammasome. Front. Immunol. 9, 1054 (2018).
Chuang, S. Y. et al. TLR-induced PAI-2 expression suppresses IL-1beta processing via increasing autophagy and NLRP3 degradation. Proc. Natl Acad. Sci. USA 110, 16079–16084 (2013).
Han, S. et al. Lipopolysaccharide primes the NALP3 inflammasome by inhibiting its ubiquitination and degradation mediated by the SCFFBXL2 E3 ligase. J. Biol. Chem. 290, 18124–18133 (2015).
Song, H. et al. The E3 ubiquitin ligase TRIM31 attenuates NLRP3 inflammasome activation by promoting proteasomal degradation of NLRP3. Nat. Commun. 7, 13727 (2016).
Tang, J. et al. Sequential ubiquitination of NLRP3 by RNF125 and Cbl-b limits inflammasome activation and endotoxemia. J. Exp. Med. 217, e20182091 (2020).
Py, B. F., Kim, M. S., Vakifahmetoglu-Norberg, H. & Yuan, J. Deubiquitination of NLRP3 by BRCC3 critically regulates inflammasome activity. Mol. Cell 49, 331–338 (2013).
Malynn, B. A. & Ma, A. Ubiquitin makes its mark on immune regulation. Immunity 33, 843–852 (2010).
Weissman, A. M. Themes and variations on ubiquitylation. Nat. Rev. Mol. Cell Biol. 2, 169–178 (2001).
Jin, S. et al. Tetherin suppresses type i interferon signaling by targeting MAVS for NDP52-mediated selective autophagic degradation in human cells. Mol. Cell 68, 308–322.e304 (2017).
Zhao, C. et al. The E3 ubiquitin ligase TRIM40 attenuates antiviral immune responses by targeting MDA5 and RIG-I. Cell Rep. 21, 1613–1623 (2017).
Ashida, H. et al. A bacterial E3 ubiquitin ligase IpaH9.8 targets NEMO/IKKgamma to dampen the host NF-kappaB-mediated inflammatory response. Nat. Cell Biol. 12, 66–73 (2010). sup pp 61–69.
Fuchs, S. Y., Spiegelman, V. S. & Kumar, K. G. The many faces of beta-TrCP E3 ubiquitin ligases: reflections in the magic mirror of cancer. Oncogene 23, 2028–2036 (2004).
Guo, C. et al. Bile acids control inflammation and metabolic disorder through inhibition of NLRP3 inflammasome. Immunity 45, 802–816 (2016).
Mortimer, L., Moreau, F., MacDonald, J. A. & Chadee, K. NLRP3 inflammasome inhibition is disrupted in a group of auto-inflammatory disease CAPS mutations. Nat. Immunol. 17, 1176–1186 (2016).
Zhang, Z. et al. Protein kinase D at the Golgi controls NLRP3 inflammasome activation. J. Exp. Med. 214, 2671–2693 (2017).
Zhao, W. et al. AKT regulates NLRP3 inflammasome activation by phosphorylating nlrp3 serine 5. J. Immunol. (Baltim., Md: 1950) 205, 2255–2264 (2020).
Jéru, I. et al. Interaction of pyrin with 14.3.3 in an isoform-specific and phosphorylation-dependent manner regulates its translocation to the nucleus. Arthritis Rheum. 52, 1848–1857 (2005).
Park, Y. H., Wood, G., Kastner, D. L. & Chae, J. J. Pyrin inflammasome activation and RhoA signaling in the autoinflammatory diseases FMF and HIDS. Nat. Immunol. 17, 914–921 (2016).
Shi, H., Murray, A. & Beutler, B. Reconstruction of the mouse inflammasome system in HEK293T cells. Bio Protoc. 6, e1986 (2016).
Ran, F. A. et al. Genome engineering using the CRISPR-Cas9 system. Nat. Protoc. 8, 2281–2308 (2013).
We thank Dr. Feng Shao (National Institute of Biological Sciences) for providing immortalized mouse macrophages. We thank Qianqian Xue for assisting in raising the animals. This work was supported by National Natural Science Foundation of China (81801967, 82025021, 81930059, 81971893), Innovation-driven Project of Central South University (2018CX030, 2019CX013), Natural Science Foundation of Hunan Province, China (2020JJ5873), Fundamental Research Funds for the Central Universities of Central South University (CX20190076).
The authors declare no competing interests.
Peer review information Nature Communications thanks Keiichi Nakayama and the other, anonymous, reviewer(s) for their contribution to the peer review of this work. Peer reviewer reports are available.
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Wang, D., Zhang, Y., Xu, X. et al. YAP promotes the activation of NLRP3 inflammasome via blocking K27-linked polyubiquitination of NLRP3. Nat Commun 12, 2674 (2021). https://doi.org/10.1038/s41467-021-22987-3
This article is cited by
Deubiquitinase OTUD6A in macrophages promotes intestinal inflammation and colitis via deubiquitination of NLRP3
Cell Death & Differentiation (2023)
Cardiac fibroblasts and mechanosensation in heart development, health and disease
Nature Reviews Cardiology (2023)
Theaflavin mitigates acute gouty peritonitis and septic organ injury in mice by suppressing NLRP3 inflammasome assembly
Acta Pharmacologica Sinica (2023)
NLRP10 promotes AGEs-induced NLRP1 and NLRP3 inflammasome activation via ROS/MAPK/NF-κB signaling in human periodontal ligament cells
Role of the Hippo pathway in liver regeneration and repair: recent advances
Inflammation and Regeneration (2022)
By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.