NLRP1 and CARD8 are related cytosolic sensors that upon activation form supramolecular signalling complexes known as canonical inflammasomes, resulting in caspase−1 activation, cytokine maturation and/or pyroptotic cell death. NLRP1 and CARD8 use their C-terminal (CT) fragments containing a caspase recruitment domain (CARD) and the UPA (conserved in UNC5, PIDD, and ankyrins) subdomain for self-oligomerization, which in turn form the platform to recruit the inflammasome adaptor ASC (apoptosis-associated speck-like protein containing a CARD) or caspase-1, respectively. Here, we report cryo-EM structures of NLRP1-CT and CARD8-CT assemblies, in which the respective CARDs form central helical filaments that are promoted by oligomerized, but flexibly linked, UPAs surrounding the filaments. Through biochemical and cellular approaches, we demonstrate that the UPA itself reduces the threshold needed for NLRP1-CT and CARD8-CT filament formation and signalling. Structural analyses provide insights on the mode of ASC recruitment by NLRP1-CT and the contrasting direct recruitment of caspase-1 by CARD8-CT. We also discover that subunits in the central NLRP1CARD filament dimerize with additional exterior CARDs, which roughly doubles its thickness and is unique among all known CARD filaments. Finally, we engineer and determine the structure of an ASCCARD–caspase-1CARD octamer, which suggests that ASC uses opposing surfaces for NLRP1, versus caspase-1, recruitment. Together these structures capture the architecture and specificity of the active NLRP1 and CARD8 inflammasomes in addition to key heteromeric CARD-CARD interactions governing inflammasome signalling.
Innate immune pathways recognize and respond to a diverse array of intracellular threats. In one such pathway, cells identify and amplify danger signals through supramolecular signaling complexes called canonical inflammasomes1,2. Upon recognition of intracellular molecular patterns indicative of pathogens or endogenous damage, sensor proteins facilitate inflammasome assembly by undergoing large conformational changes that lead to their oligomerization3,4. Nucleotide binding domains (NBDs) often drive this self-oligomerization to cluster death-fold domains5,6, which in turn recruit downstream adapter and effector molecules. These death-fold domains, including pyrin domains (PYD) and caspase recruitment domains (CARD), participate in homotypic (CARD–CARD or PYD–PYD) interactions that ultimately lead to polymerization of caspase-1 into filaments3,4,7,8,9. This process increases the local concentration of caspase catalytic domains to facilitate its homo-dimerization and autoproteolysis, resulting in its activation1,2,3. Active caspase-1, a cysteine protease, then processes pro-inflammatory cytokines, including pro-IL-1β and pro-IL-18, to their bioactive forms and cleaves the pore-forming protein gasdermin-D (GSDMD) to promote cytokine release and often concomitant lytic cell death termed pyroptosis10,11,12.
NLRP1 and CARD8, two related inflammasome sensors, are highly expressed in a number of cell types and play important roles in both host defense and human diseases. Keratinocytes constitutively express high levels of NLRP1 and germline mutations of NLRP1 in humans lead to a number of skin-related inflammatory diseases, including multiple self-healing palmoplantar carcinoma (MSPC), familial keratosis lichenoides chronica (FKLC)13, vitiligo14,15, autoinflammation with arthritis and dyskeratosis (AIADK)16,17, and juvenile-onset recurrent respiratory papillomatosis (JRRP)18. These mutations cause constitutive NLRP1 activation and downstream pyroptosis13,16, leading to damaging inflammation. For CARD8, the most highly expressing cell types are hematopoietic in origin19,20,21, and CARD8 activators are being pursued for treatment of acute myeloid leukemia19. Thus, understanding the molecular mechanisms governing NLRP1 and CARD8 inflammasome signaling will facilitate the discovery of new therapeutics for inflammatory diseases and cancers.
NLRP1 and CARD8 mediate inflammasome formation through their CARD-containing C-terminal fragment (CT) generated upon functional degradation of their respective N-terminal fragment (NT) by the proteasome22,23. This unusual mechanism of inflammasome activation is associated with autoproteolysis of the function-to-find domain (FIIND) common to NLRP1 and CARD8, which splits FIIND into ZU5 (found in ZO-1 and UNC5) and UPA (conserved in UNC5, PIDD, and ankyrins) subdomains and results in noncovalently associated NT and CT24,25 (Fig. 1a). NLRP1-CT and CARD8-CT are therefore repressed by the NT until upstream cues induce proteasomal degradation of the NT and concomitant release of the CT13,26,27,28 (Fig. 1b). Interestingly, one such cue is provided by small-molecule inhibitors of dipeptidyl peptidases DPP9 and DPP8, for which the mechanism of NLRP1 and CARD8 activation is currently unclear16,19,29. Activated CARD8 and NLRP1 inflammasomes are distinctive in that they are only composed of UPA and CARD, unlike others such as NLRC4 and NLRP3 inflammasomes which use NBDs and leucine-rich repeats (LRRs) to facilitate oligomerization and inflammasome activation4,5,6,30.
In addition to having the unique UPA subdomain, the specificity of NLRP1-CT and CARD8-CT for the CARD and PYD-containing adapter ASC (apoptosis-associated speck-like protein containing a CARD) and for caspase-1 differ from most other inflammasome sensors (Fig. 1c). While ASC is a nearly universal adapter that bridges interactions between sensors and the CARD-containing caspase-11,31, CARD8 does not interact with ASC and instead directly engages caspase-132. In contrast to the CARD-containing sensor protein NLRC4, which can activate caspase-1 both with and without ASC6,33,34, human NLRP1 is completely dependent on ASC and cannot engage caspase-1 directly32.
The molecular bases for the assembly of UPA-CARD-mediated NLRP1-CT and CARD8-CT inflammasomes and for their differential specificity to ASC and caspase-1 are unknown. Here, we determined the cryo-electron microscopy (cryo-EM) structures of NLRP1-CT and CARD8-CT filaments and analysed their assembly and specificity. Despite being invisible in the cryo-EM densities, the UPA domain is required for productive NLRP1 and CARD8 inflammasome signaling, suggesting that it promotes CARD clustering and filament formation and serves an analogous function to the NBD and LRRs in many other inflammasome sensors. The CARD filament of CARD8-CT resembles the helical filaments of caspase-1CARD, ASCCARD, and NLRC4CARD7,35,36 with certain structural variations. Surprisingly however, the CARD filament of NLRP1-CT is composed of CARD dimers in which an additional CARD flanks each subunit of the central CARD filament. We also determined the structure of an ASCCARD-caspase-1CARD octamer, which suggests that ASC uses opposing surfaces for caspase-1 versus NLRP1 engagement and suggests a hierarchical inflammasome assembly mechanism. In sum, we discover new mechanisms of inflammasome formation and uncover the structural basis of hetero-oligomeric CARD–CARD interactions.
Cryo-EM structure determination of CARD8 and NLRP1 CARD filaments
In general, inflammasomes leverage supramolecular filamentous structures to nucleate the polymerization of caspase-1, which in turn increases the local concentration of its caspase domain to facilitate dimerization and activation3,7,36. To elucidate if and how CARD8-CT and NLRP1-CT form filaments, we expressed these CTs in fusion with an N-terminal maltose-binding protein (MBP) tag separated by a linker cleavable by the human rhinovirus (HRV) 3C protease. We posited that such a bulky tag would disrupt oligomerization and facilitate purification of monomeric proteins for controlled CT filament formation in vitro (Fig. 1b and Supplementary Figs. 1, 2). However, the MBP-fusion protein still formed small oligomers. By systematically optimizing cleavage conditions to minimize aggregation, we purified short (~100–200 nm) filaments, which behaved well on cryo-EM grids and enabled the calculation of CARD8-CT and NLRP1-CT maps at resolutions of 3.3 Å and 3.6 Å, respectively (Fig. 1d–i and Supplementary Figs. 1, 2, Supplementary Table 1). Unexpectedly, 2D classifications and 3D reconstructions revealed both similarities and differences between these two filament structures (Fig. 1d, i).
Structure of the CARD8-CT filament
Despite being included in the construct (Supplementary Fig. 1b, c), no UPA density was observed in the CARD8-CT cryo-EM reconstruction, which instead only reveals the central helical CARD filament (Fig. 2a, b). One possible explanation is that UPA does not follow the CARD helical symmetry but is orderly associated with the central CARD filament. However, subtracting out the central density followed by 3D classification without imposing symmetry did not reveal any new density. Given the predicted 17-residue unstructured linker between UPA and CARD, we proposed that UPA and any residual MBP molecules must be flexibly linked to the core CARD filament. Thus, their stochastic position relative to the central CARD filament caused them to average out during data processing. In fact, either the UPA itself or any residual uncleaved MBP tag appeared as noisy density surrounding the filaments in 2D class averages (Fig. 1d).
Like other CARD filament structures4,7,35,36,37,38, the CARD8CARD filament also possesses a one-start helical symmetry, with a refined left-handed rotation of 99.1° and an axial rise of 5.2 Å per subunit (~3.6 subunits per helical turn). The filament has a diameter of ~80 Å with a central hole of ~10 Å (Fig. 2a, b). Analysis of the three types of asymmetric interactions (Fig. 2c) that are characteristic of death-fold filaments39 revealed that the type I interaction is unusually small, with only ~150 Å2 buried surface area per partner, in comparison to ~350 and ~560 Å2 for those in ASCCARD and caspase-1CARD filaments7,36. In contrast, the type II interface is substantially more extensive, burying ~490 Å2 surface area per partner, and the type III interface covers ~230 Å2 per partner. Because of the small type I interface, the filament structure looks almost perforated with visible gaps (Fig. 2a).
Detailed inspection of the three interfaces revealed many charge–charge pairs as well as other hydrophilic interactions including R459 at type Ia with D473 and D477 at type Ib, K509 of type IIa with D525 of type IIb, E507 of type IIa with R464 of type IIb, E479 of type IIa with Y527 of type IIb, and E483 and E487 of type IIIa with R495 of IIIb (Fig. 2d). We used these structural insights to design point mutations that would abolish CARD filament formation. To assess the impact of these mutations on filament formation, we cleaved recombinant wild-type and mutant MBP-tagged CARD8CARD proteins for 3 h at 37 °C, followed by EM imaging of the negatively stained samples. While the wild-type protein formed filaments when the bulky MBP tag was removed, seven different point mutants, one at the type I interface, four at the type II interface, and two at the type III interface, completely abolished filament formation in vitro (Fig. 2e). Of note, unlike many CARDs that form filaments at low µM concentrations7,36,38, we had to raise the concentration of CARD8CARD to 15 µM to see consistent filaments in multiple grid areas under negative stain EM.
Next, we employed a reconstituted HEK293T cell system stably expressing caspase-1 and GSDMD to assess whether these mutants were able to signal in cells19. We transfected these cells with plasmid encoding for WT or mutant CARD8UPA-CARD, and 24 h later, analysed the supernatant for lactate dehydrogenase (LDH) activity, a hallmark of pyroptotic cell death, and the lysate by immunoblotting for caspase-1 and GSDMD cleavage (Fig. 2f). As expected, WT CARD8UPA-CARD induced elevated LDH activity in the supernatant and exhibited prominent caspase-1 and GSDMD cleavage. In contrast, five out of the six filament-deficient mutants showed background level LDH release with no discernible caspase-1 or GSDMD cleavage, similar to the empty vector (EV). Only the D511K mutant displayed residual caspase-1 and GSDMD cleavage. Of note, expression of the CARD8CARD itself did not lead to inflammasome signaling under these same conditions (Fig. 2f).
We further expressed CARD8UPA-CARD fused to a C-terminal mCherry tag in HEK293T cells and found that although the WT formed strong punctate structures indicative of filament formation, all the CARD8UPA-CARD constructs with CARD interface mutations showed diffuse distributions consistent with defective filament formation (Fig. 2g). Thus, these cellular data validated the structure and confirmed that filamentous CARD–CARD interactions are crucial for CARD8-CT-mediated inflammasome signaling.
UPA enhances NLRP1-CT and CARD8-CT signaling
Since the CARD8CARD construct itself did not cause cell death while CARD8UPA-CARD did (Fig. 2f), we hypothesized that the presence of the UPA subdomain enhances inflammasome formation. To test this hypothesis, we sought to determine the approximate minimum concentration required to form CARD8CARD versus CARD8UPA-CARD filaments in vitro. CARD8CARD did not form filaments until 15 µM, while only 0.25 µM was required for CARD8UPA-CARD filament assembly (Fig. 3a, b), an almost 100-fold difference. We found that NLRP1CARD did not form any filaments even at 30 µM, but like CARD8UPA-CARD, NLRP1UPA-CARD formed filaments at 0.25 µM (Fig. 3c, d), suggesting that the UPA subdomain significantly decreased the concentration needed to form CARD8 or NLRP1 filaments. Consistent with their ability to promote filament formation, CARD8UPA and NLRP1UPA alone showed aggregation under negative stain EM (Fig. 3e).
Since CARD8CARD formed filaments at very high concentrations in vitro, we posited that higher concentrations of transfected plasmids were required for appreciable cell signaling. To determine whether increasing the amount of transfected plasmid could lead to inflammasome formation and LDH release for the CARD8CARD or NLRP1CARD alone constructs, we raised the plasmid amount from the usual 20 to 200 ng and 2000 ng per transfection (Fig. 3f, g). For CARD8CARD, significant induction of LDH release, and thus cell death, only occurred when 2000 ng of plasmid was used, and at this condition, CARD8UPA-CARD caused a similar level of LDH release (Fig. 3f). For NLRP1CARD, 200 ng per transfection led to significant LDH release, and at 2000 ng per transfection, it triggered similar levels of LDH release to NLRP1UPA-CARD (Fig. 3g). These data suggest that a ~100-fold greater plasmid amount is needed to cause a similar level of CARD-mediated cell death compared to UPA-CARD-mediated cell death. Additionally, we and others recently communicated pre-prints on the cryo-EM structures of the NLRP1-DPP9 complex, which revealed a front-to-back UPA oligomerization interface required for inflammasome signaling40,41. Taken together with these results, we conclude that UPA oligomerization promotes CARD8-CT and NLRP1-CT filament formation and subsequent inflammasome signaling (Fig. 3h).
Structure of the NLRP1-CT filament containing CARD dimers
Similar to the CARD8-CT filament structure, no UPA density was observed in the NLRP1-CT cryo-EM map, suggesting that the UPA subdomain, with the 25-residue predicted unstructured linker to the CARD, is also flexibly connected to the core NLRP1CARD filament (Fig. 4a and Supplementary Fig. 2b). The NLRP1CARD filament has one-start helical symmetry, with a left-handed rotation of 100.8° and an axial rise of 5.1 Å per subunit (~3.6 subunits per helical turn), similar to other CARD filament structures4,7,35,36,37,38. Strikingly however, unlike any other CARD filament structures known to date, the NLRP1CARD filament is composed of NLRP1CARD dimers, rather than monomers (Fig. 4a, b), which is also reflected in the thicker dimensions of NLRP1-CT filaments compared to CARD8-CT filaments in both 2D classes and the 3D volume (Fig. 1d, f, g, i). The inner NLRP1CARD filament is roughly equivalent to other CARD filament structures, and for all NLRP1CARD subunits in the inner filament, the dimerically related NLRP1CARD subunits form the outer layer of the NLRP1CARD filament (Fig. 4a). The total diameter of the NLRP1CARD filament is approximately 140 Å, with an inner hole of ~10 Å (Fig. 4a).
The NLRP1CARD dimer is mediated by reciprocal interactions at helices α5 and α6, burying a substantial ~300 Å2 surface area per partner, and involving residues with large side chains such as Y1445, M1457, W1460, and E1461 (Fig. 4b). These regions of helices α5 and α6 are not involved in the inner core filament interaction, which instead is mediated by the classical type I, II, and III CARD–CARD interactions (Fig. 4c). Different from the CARD8CARD filament, the type I interface in the NLRP1CARD filament is more extensive, with type I, II and III interfaces burying ~300, 430, and 140 Å2 surface area per partner, respectively. Charged and hydrophilic interactions dominate the interactions, including R1386 of type Ia with D1401, Y1413, and H1404 of type Ib, R1427 of type Ia with E1397 and D1401 of type Ib, E1411 of type IIa with S1395 of type IIb, Q1434 and D1437 of type IIa with R1392 of type IIb, and E1414 of type IIIa with T1421 of type IIIb (Fig. 4c).
To elucidate the role of the observed NLRP1CARD filament in signaling, we employed the same reconstituted HEK293T cell system stably expressing caspase-1 and GSDMD used for assessing CARD8 mutants in cells (Fig. 2f). We transfected these cells with plasmids encoding ASC and either WT or mutant NLRP1UPA-CARD and 24 h later, analysed the supernatant for LDH activity, and the lysate for caspase-1 and GSDMD cleavage (Fig. 4d). In contrast to WT NLRP1UPA-CARD, structure-designed mutants including R1427E (Ia), E1397R (Ib), D1401R (Ib), E1411R (IIa), R1392E (IIb), and E1414R (IIIa) compromised cell death measured by both LDH release and caspase-1 processing (Fig. 4d). Together, the mutational analysis demonstrated the validity of the filament structure in NLRP1 signaling.
NLRP1CARD has a propensity for dimerization
To investigate the function of NLRP1CARD dimerization, we compared the signaling activity of WT NLRP1UPA-CARD and NLRP1UPA-CARD with several CARD dimerization mutants (Fig. 4d). Among the NLRP1UPA-CARD constructs with mutations on the CARD dimer interface, Y1445A compromised LDH release but retained caspase-1 processing, suggesting partial defectiveness. However, several other dimerization mutants, including M1457A, W1460A, and E1461R, showed no discernible impact on inflammasome signaling (Fig. 4d and Supplementary Fig. 3a). Furthermore, while the Y1445A mutant abolished NLRP1UPA-CARD filament formation in vitro, the other single mutants still formed filaments (Supplementary Fig. 3b). These results are consistent with lack of strict sequence conservation of these residues among NLRP1 from different species, and with Y1445 as the most conserved residue at the dimerization interface (Supplementary Fig. 3c). Thus, while the UPA is required for UPA-CARD inflammasome signaling, the dimer likely promotes assembly to a much lesser degree.
If the NLRP1CARD dimerizes in the context of NLRP1-CT, why does the CARD8-CT fail to induce CARD8CARD dimerization? To address this question, we inspected the crystal packing interactions in the previously determined MBP-fused NLRP1CARD (PDB ID: 4IFP) and MBP-fused CARD8CARD (PDB ID: 4IKM) structures to see if dimers were observed42,43. In these preparations, the rigid MBP fusion kept NLRP1CARD and CARD8CARD from forming filaments. For NLRP1, all three independent molecules in the crystallographic asymmetric unit form a symmetrical dimer in the crystal lattice, which superimposes well with the dimer observed in the filament (Fig. 4e). These analyses suggest that NLRP1CARD has an intrinsic propensity to form dimers. In contrast, no CARD8CARD dimer was observed in its crystal lattice, and the corresponding CARD8CARD residues are not conserved across different species (Supplementary Fig. 3c). However, since CARD8CARD does not dimerize and the NLRP1CARD dimer interface plays limited functional role, we cannot exclude the possibility that the NLRP1CARD dimer results from the high protein concentrations used for structure determination. Regardless, multivalency drives CARD clustering to facilitate UPA-CARD filament formation and downstream signaling.
The ASC type b surface nucleates caspase-1 polymerization
We next investigated how heterooligomeric CARD-CARD interactions nucleate caspase-1 filament assembly to facilitate downstream signaling. We previously demonstrated unidirectional polymerization of ASC-nucleated caspase-1 filaments by nanogold labeling of ASC36. We further predicted that ASCCARD uses its type Ib, IIb, and IIIb surfaces to interact with the caspase-1CARD type Ia, IIa, and IIIa surfaces, because these interactions bury a larger total surface area than that of the reverse interactions between the type a surfaces of ASC and the type b surfaces of caspase-136. To test this prediction, we designed mutations based on the ASC and caspase-1 filament structures to prevent filament elongation and thus observe a minimal unit of contact between ASC and caspase-17,36. Specifically, we designed the type IIa W169G mutant of ASCCARD and the type IIb G20K mutant of caspase-1CARD and connected them in one polypeptide chain using a 5× GSS linker (Fig. 5a). As expected, these mutations did not impair the formation of an ASCCARD–caspase-1CARD oligomer (Supplementary Fig. 4a), and multi-angle light scattering (MALS) measurement revealed a main peak of molecular mass of 86.3 kDa, corresponding to a tetramer of the ASCCARD–caspase-1CARD fusion protein, or an octamer of CARDs with 4 ASCCARD molecules and 4 caspase-1CARD molecules (Fig. 5b).
We collected a cryo-EM dataset and found that despite its small size, the octamer 2D classes were quite detailed (Supplementary Fig. 4c). We then determined the 3D structure of the octamer at a resolution of 3.9 Å calculated by FSC between half maps (Supplementary Fig. 4d–f). There were eight CARD subunits in the map, four of which are similar to one another but differ from the remaining four, suggesting that there are four ASCCARD and four caspase-1CARD subunits in the map. The ASCCARD and caspase-1CARD structures were clearly distinguishable by their fit into the densities; in particular, the shorter α6 in caspase-1CARD and the longer α6 in ASCCARD allowed unambiguous placement of ASCCARD and capase-1CARD subunits (Fig. 5c, d and Supplementary Fig. 4g). In this assembly, there is one type I interaction and three type III interactions within ASC subunits and within caspase-1 subunits, and there are three type I interactions, four type II interactions, and one type III interaction between ASC and caspase-1 (Fig. 5e), which must have represented the optimal mode of interaction between ASC and caspase-1. In all three types of interactions between ASC and caspase-1, ASC always uses the type b surfaces (Ib, IIb, and IIIb) to interact with the type a surfaces (Ia, IIa, and IIIa) of caspase-1 (Fig. 5e). Of note, this arrangement requires a tetramer layer of ASCCARD to interact with a tetramer layer of caspase-1CARD, suggesting a hierarchical, rather than mixed, assembly of these death domains (Fig. 5f).
Extensive type I and II interfaces dominate the ASCCARD−caspase-1CARD assembly, with calculated buried surface areas of ~450, 600, and 220 Å2 per partner for type I, II, and III interfaces, respectively. Detailed inspection of these interfaces revealed several clear interactions between ASCCARD and caspase-1CARD. These included E130 of ASC with R55 of caspase-1, W131 of ASC with R15 of caspase-1, and Q147 of ASC with D59 of caspase-1 at the type I interface, N128 of ASC with E37/E38 of caspase-1, S184 of ASC with N36 of caspase-1, and Q185/S186 of ASC with R33 of caspase-1 at the type II interface, T154 of ASC with R45 of caspase-1 and P153 of ASC with K42 with at the type III interface (Fig. 5g). Indeed, a previous study demonstrated that K42E and D59R mutations in caspase-1CARD, in addition to the E130R mutation in ASCCARD, resulted in loss of ASC−caspase-1 interaction, supporting our assignment of these interaction surfaces44.
Predicted modes of interactions between NLRP1CARD and ASCCARD and between CARD8CARD and caspase-1CARD
While most CARD-containing inflammasome proteins, including human NLRP1 and NLRC4, amplify signaling through the adapter protein ASC32,34, CARD8 is the only known inflammasome sensor that cannot engage ASC and instead exclusively binds caspase-132. NLRP1, conversely, exclusively interacts with ASC32. These differences in downstream signaling components could lead to different biological outcomes, given the signal amplification afforded by ASC and its differential expression across cell types.
The structures of CARD8CARD and NLRP1CARD filaments determined in this study allowed us to predict the modes of their CARD–CARD interactions, assuming a unidirectional assembly that has been elucidated for several other death domain superfamily members3,36,45. We first investigated the cross-sectional surface charges of CARD8, NLRP1, ASC, and caspase-1 filaments by extracting a layer of tetramer as defined in the ASCCARD−caspase-1CARD octamer from their respective filament structures. We then generated a CARD8CARD−caspase-1CARD hypothetical complex by fitting a layer of capsase-1CARD tetramer to the CARD8CARD filament structure by rigid-body fitting46. Of note, the interfacial side chains of CARD8CARD and caspase-1CARD were not adjusted or energy minimized, therefore these models should be taken as highly suggestive. In the model in which the type b surfaces of the CARD8CARD layer interact with the type a surfaces of the caspase-1CARD layer, the charge complementarity between CARD8CARD and caspase-1CARD is apparent, especially with strong negative (CARD8) and positive (caspase-1) patches both mainly at the outer rim of the filament cross-sections (Fig. 6a). By contrast, in the opposing model wherein type a surfaces of the CARD8CARD layer interact with the type b surfaces of the caspase-1CARD layer, both interfaces display largely negative charges and should repel each other (Fig. 6b). Similarly, if the type a ASCCARD layer is placed below the type b NLRP1CARD layer, there is obvious charge complementarity with negative (NLRP1) and positive (ASC) patches both mainly near the center of the filament cross-sections (Fig. 6c). The reverse arrangement of ASCCARD above NLRP1CARD reveals repelling positive charges in the cross-sections of both ASCCARD and NLRP1CARD (Fig. 6d).
To further investigate the structural basis for CARD8CARD-caspase-1CARD and NLRP1CARD–ASCCARD interaction, we analysed the modeled interfaces type by type (Fig. 6e, f). Consistent with the surface charge analysis, the modeled CARD8CARD (type b)−caspase-1CARD (type a) interfaces are dominated by charged pairs including K469 of CARD8 to D52 of caspase-1 and D473 of CARD8 to R55 of caspase-1 at the type I interface, E523 of CARD8 to R33 of caspase-1, D467 and K469 of CARD8 to E38 and K42 of caspase-1, and a cluster of interactions involving Y527 and Y531 of CARD8 and K64 and Q67 of caspase-1 at the type II interface, and K493–S497 of CARD8 to K37, E38, K42, and R45 of caspase-1 at the type III interface (Fig. 5e).
The NLRP1CARD (type b)−ASCCARD (type a) interfaces are dominated by both charged pairs and hydrophilic pairs including E1397 and D1401 of NLRP1 with R119 and R160 of ASC at the type I interface, T1394 and S1395 of NLRP1 with E144 and Q145 of ASC at the type II interface, and R1427 of NLRP1 with D143 and E144 of ASC at the type III interface (Fig. 6f). Thus, the structural analysis confirmed favorable interactions between the type b interfaces of NLRP1 and CARD8 with the type a interfaces of ASC and caspase-1, respectively (Fig. 6g). By contrast, ASC uses its type b surface to recruit caspase-1, suggesting a hierarchical inflammasome formation that proceeds through an ordered manner from NLRP1, to ASC, then to caspase-1, with potential signal amplification (Fig. 6g). This ordered assembly is made possible by the use of two opposing ASC filament surfaces with specificity towards either NLRP1 or caspase-1.
In addition to the hierarchical NLRP1CARD−ASCCARD−caspase-1CARD assembly, oligomerized ASCCARD could, in principle, also nucleate the associated ASCPYD to form helical filaments, which in turn recruit more ASC through PYD–PYD interactions and allow the recruited ASC to template more caspase-1CARD filament formation through CARD–CARD interactions to further amplify the signal. In either scenario, however, these structural data suggest that ASCCARD uses opposing surfaces for interaction with NLRP1CARD and caspase-1CARD.
The death-fold domain superfamily is widely represented in innate immune signaling pathways and mediates homo-oligomerization and hetero-oligomerization through filament formation4,47,48. In this study, we showed that NLRP1-CT and CARD8-CT also use their CARDs to assemble filamentous structures for inflammasome signaling. We posit that these CARD filaments are decorated by flexibly linked UPA subdomains that are prone to oligomerization, and this additional multivalency reduces the threshold for CARD filament assembly (Fig. 3h). During the preparation of this manuscript, a complementary preprint on the structures of CARD8CARD and NLRP1CARD filaments was released49. Importantly, our studies together bolster the conclusion that the UPA subdomain on NLRP1-CT and CARD8-CT facilitates inflammasome assembly and signaling.
The role of the UPA subdomain in UPA-CARD inflammasomes might be analogous to other oligomerization domains in inflammasome sensors. For example, in the activated NLRC4 inflammasome, NBDs, and LRRs mediate its oligomerization into a disk-shaped signaling platform, clustering the attached CARDs towards the center of the assembly. The clustered CARDs then template the oligomerization of ASC and/or caspase-1 to stimulate inflammasome signaling5,6,36,50. NLRP3, which possesses a similar domain architecture, might also use a similar mechanism, as mutations in predicted NBD and LRR contacts abolished its inflammasome activity30. It was also recently reported that the isolated PYD of NLRP9 was not sufficient for inflammasome filament formation, implicating its other domains (LRR, NBD) in driving CARD oligomerization51,52.
Other immune sensing pathways also employ CARD filament signaling strategies. In the RIG-I RNA sensing pathway, oligomerization of the RIG-I helicase domain on RNA clusters flexibly linked RIG-I 2CARDs, inducing their tetramerization. This RIG-I 2CARD tetramer, which represents one full helical turn, nucleates CARD filament formation of the MAVS adapter to stimulate interferon signaling37,53,54. In the CARMA1/BCL10/MALT1 (CBM) signalosome, CARMA1CARD nucleates the formation of a BCL10 filament through CARD–CARD interactions. However, the presence of an additional CARMA1 domain called the coiled coil region, which stimulates CARMA1 self-oligomerization, enhances BCL10 filament formation38,55. The role of the RIG-I helicase domain and the CARMA1 coiled coil region are thus similar to that of the UPA subdomain, by which self-oligomerization domains cluster flexibly linked CARDs to stimulate filament formation and signaling complex assembly.
Nucleated filament growth underlies the assembly and function of inflammasomes3. Such behavior allows signal amplification from a low concentration of a pathogen-activated or danger-activated sensor that acts as a nucleator to a robust host response47. Our data are consistent with this model, whereby CARD8CARD directly recruits and polymerizes caspase-1CARD through the favorable side of the growing filament seed. NLRP1CARD, however, must recruit the adapter ASC to facilitate caspase-1 interaction and polymerization32. The specificity of the ASCCARD filament for NLRP1CARD on one side and caspase-1CARD on the other makes it a perfect bridge between the NLRP1 sensor and the caspase-1 effector, and polymerization of the ASCPYD might provide additional signal amplification. Thus, the ability to oligomerize and the specificity of the hetero-oligomerization determine the composition of particular signaling pathways and their biological outcomes.
Cloning, protein expression, and purification
For structure determination, the UPA-CARD fragments of CARD8 (S297-L537, T60 isoform, Uniprot ID: Q9Y2G2-5) and NLRP1 (S1213-S1473, isoform 1, Uniprot ID: Q9C000-1) were cloned into a modified pDB-His-MBP vector with an HRV 3C protease linker (His-MBP-3C-UPA-CARD). For in vitro filament formation experiments, the CARDs of CARD8 (P446-L537) and NLRP1 (D1374-S1473) were also cloned into the modified pDB-His-MBP vector. For in vitro analyses, expression constructs encoding CARD8CARD and NLRP1CARD had an additional A452C (α1) or G1467C (α6) mutation, respectively, for cysteine labeling applications. The NLRP1 UPA (S1213–P1364) was also cloned into the modified pDB-His-MBP vector with an HRV 3C protease linker (His-MBP-3C-UPA). To generate the CARD8 His-MBP-3C-UPA (S297-P446) construct, a stop codon was introduced in the above CARD8 His-MBP-3C-UPA-CARD plasmid with Q5 mutagenesis. For cellular studies, the NLRP1-CT was cloned into pcDNA3.1 LIC 6A with a C-terminal FLAG tag (UPA-CARD-FLAG) and the CARD8-CT was cloned pcDNA3.1 LIC 6B encoding a C-terminal mCherry tag (UPA-CARD-mCherry). cDNA encoding ASCCARD (106–195) and caspase-1CARD (1–95) connected by a 5XGSS linker was cloned into the pDB-His-MBP vector with a tobacco etch virus (TEV)-cleavable N-terminal His6-MBP tag using NdeI and Not I restriction sites. Mutations of W169G on ASCCARD (Type IIa) G20K on caspase-1CARD (Type IIb), and site-directed mutagenesis for all other relevant constructs were performed by QuikChange Mutagenesis (Agilent Technologies) or by Q5 mutagenesis (NEB). All plasmids were confirmed by Sanger sequencing. All constructs have been deposited to Addgene (https://www.addgene.org/Hao_Wu/). Study primers are listed in Supplementary Table 2.
To generate NLRP1-CT filaments, constructs were transformed into BL21 (DE3) cells, grown to OD600 0.6–0.8, cold shocked on ice water for 20 min, and induced overnight with 0.4 mM Isopropyl β-d-1-thiogalactopyranoside (IPTG) at 18 °C. The cells were harvested by centrifugation (4000 × g, 20 min) and lysed by sonication (2 s on 2 s off, 4 min total on, 55% power, Branson) in lysis buffer (25 mM Tris-HCl pH 7.5, 150 mM NaCl, 1 mM TCEP, SIGMAFAST protease inhibitor). Cell lysate was then centrifuged (40,000 × g, 1 h) and the soluble proteome was incubated with pre-equilibrated amylose resin for 2 h at 4 °C. Bound resin was then washed by gravity flow with 50 column volumes (CV) lysis buffer and eluted with 3 CV elution buffer (25 mM Tris-HCl pH 7.5, 150 mM NaCl, 1 mM TCEP, 50 mM maltose). Eluate from amylose resin was concentrated and purified as a range of small oligomers on a Superose 6 size exclusion column (Cytiva) in SEC buffer (25 mM Tris-HCl pH 7.5, 150 mM NaCl, 1 mM TCEP), concentrated again (500 μl, A280 = 6) using a 50 kDa spin column (Millipore), and cleaved overnight with MBP-3C protease (50 μl, A280 = 3) on ice. These cleavage conditions were optimized extensively to produce elongated filaments, as aggregation and incorporation of uncleaved MBP-tagged protein in the NLRP1-CT filaments limited further proteolysis of the MBP-tag and filament elongation. Despite extensive optimization, NLRP1-CT filaments still incorporated some uncleaved proteins containing MBP (Supplementary Fig. 2a). Filaments were further purified by size exclusion chromatography on a Superose 6 column (Cytiva) in lysis buffer and recovered from the column void fraction at a suitable concentration for cryo-EM (A280 = 0.4). UPA peptide coverage was confirmed by Mass Spectrometry at the HMS Taplin Mass Spectrometry Facility (Supplementary Fig. 2b).
To express and purify CARD8-CT filaments, expression and purification protocol followed as above until after elution from maltose resin. Eluate was concentrated (500 μL, A280 = 6) using a 50 kDa spin column (Millipore) and cleaved with MBP-3C protease (50 μL, A280 = 3) for 3 h at 37 °C to produce elongated filaments. Despite extensive optimization of these cleavage conditions, CARD8-CT filaments still incorporated some uncleaved proteins containing MBP (Supplementary Fig. 1a). Filaments were further purified by size exclusion chromatography on a Superose 6 column (Cytiva) in SEC buffer, recovered from the column void fraction, and slowly concentrated using a 0.5 mL spin concentrator (Millipore, 100 kDa MW cutoff). UPA peptide coverage was confirmed by Mass Spectrometry at the HMS Taplin Mass Spectrometry Facility (Supplementary Fig. 1b).
To obtain monomeric MBP-CARD proteins or oligomeric MBP-UPA proteins, constructs were expressed and purified similarly to the UPA-CARD filaments. Following elution from amylose resin, monomeric MBP-CARD proteins were concentrated to 0.5 mL (Amicon Ultra, 50 kDa MW cutoff) and further purified by size exclusion chromatography on a Superdex 200 column (Cytiva) in SEC buffer. Oligomeric MBP-UPA proteins were concentrated to 0.5 mL (Amicon Ultra, 50 kDa MW cutoff) and further purified by size exclusion chromatography on a Superose 6 column (Cytiva) in SEC buffer. Oligomeric MBP-UPA fractions were concentrated to 0.5 mL (Amicon Ultra, 50 kDa MW cutoff), followed by MBP cleavage by MBP-3C protease (50 μL, A280 = 3) for 3 h at RT and purified on another Superose 6 column (Cytiva) in SEC buffer. The peak fraction was taken for negative stain analysis.
Expression of ASCCARD-caspase-1CARD was similar to above. Cells were then collected and resuspended in lysis buffer (25 mM Tris-HCl at pH 8.0, 150 mM NaCl, 20 mM imidazole 5 mM β-ME), followed by sonication. The cell lysate was clarified by centrifugation (40,000 × g, 30 min) at 4 °C. The clarified supernatant containing the target protein was incubated with pre-equilibrated Ni-NTA resin (Qiagen) for 30 min at 4 °C. After incubation, the resin–supernatant mixture was poured into a gravity column and the resin was washed with 50 CV lysis buffer. The protein was eluted using lysis buffer supplemented with 500 mM imidazole. The Ni-NTA eluate was then incubated with TEV protease at 16 °C overnight, and the cleaved His6-MBP tag was removed by passing the protein through an amylose resin column (Qiagen). The flow-through fraction containing the tag-free protein was further purified using a Superdex 200 (10/300 GL) gel-filtration column (Cytiva, 25 mM Tris-HCl at pH 8.0, 150 mM NaCl, 2 mM DTT). Purified ASCCARD-caspase-1CARD oligomer was assessed for absolute molecular mass by re-injecting the sample into a Superdex 200 column equilibrated with 25 mM Tris-HCl at pH 8.0, 150 mM NaCl, and 2 mM DTT. The chromatography system was coupled to a three-angle light scattering detector (mini-DAWN TRISTAR) and a refractive index detector (Optilab DSP) (Wyatt Technology). Data were collected every 0.5 s with a flow rate of 0.5 mL/min. Data analysis was carried out using ASTRA V.
Negative stain EM and critical concentration determination
Copper grids coated with layers of plastic and thin carbon film (Electron Microscopy Sciences) were glow discharged before 5 μL of purified proteins (A280 = 0.1) were applied. Samples were left on the grids for 1 min, blotted, and then stained with 1% uranyl formate for 30 s, blotted, and air dried. The grids were imaged on a JEOL 1200EX or Tecnai G2 Spirit BioTWIN microscope at the Harvard Medical School (HMS) EM facility operating at 80 keV. For determining the critical concentration of CARD8CARD and NLRP1CARD, we have purified the MBP fused protein and cleaved the MBP tag at different concentrations ranging from 1 to 30 μM, in order to engage filament formation. Samples were cleaved with 3C protease for 3 h at 37 °C prior to performing negatived stained EM imaging. Similarly, critical concentration of CARD8UPA-CARD and NLRP1UPA-CARD was determined by imaging cleaved protein samples with protein concentration ranging between 0.1 and 2 μM. The peak fractions of CARD8UPA and NLRP1UPA were taken for imaging.
Cryo-EM data collection
Cryo-EM data collection of NLRP1-CT filaments was conducted at the HMS Cryo-EM Center. Purified NLRP1-CT filaments (A280 = 0.50; 25 mM Tris-HCl pH 7.5, 150 mM NaCl, 1 mM TCEP) were loaded onto a glow-discharged C-flat grid (CF-1.2/1.3 400-mesh copper-supported holey carbon, Electron Microscopy Sciences), blotted for 4–5 s under 100% humidity at 4 °C, and plunged into liquid ethane using a Mark IV Vitrobot (ThermoFisher). Grids were screened for ice and particle quality prior to data collection. 1988 movies were acquired using a Titan Krios microscope (ThermoFisher) at an acceleration voltage of 300 keV equipped with a BioQuantum K3 Imaging Filter (slit width 25 eV), and a K3 direct electron detector (Gatan) operating in counting mode at 81,000× (1.06 Å pixel size). Automated data collection with SerialEM varied the defocus range between −0.8 and −2.2 μm with four holes collected per stage movement through image shift. All movies were exposed with a total dose of 52.3 e−/Å2 for 3.5 s fractionated over 50 frames.
Cryo-EM data collection of CARD8-CT filaments was conducted at the Pacific Northwest Center for Cryo-EM (PNCC). Purified CARD8-CT filaments (A280 = 0.75; 25 mM Tris-HCl pH 7.5, 150 mM NaCl, 1 mM TCEP) were loaded onto a glow-discharged Quantifoil grid (R1.2/1.3 400-mesh copper-supported holey carbon, Electron Microscopy Sciences), blotted for 4–5 s under 100% humidity at 4 °C, and plunged into liquid ethane using a Mark IV Vitrobot (ThermoFisher). Grids were screened for ice and particle quality prior to data collection. 1208 movies were acquired using a Titan Krios microscope (ThermoFisher) at an acceleration voltage of 300 keV equipped with a Falcon 3EC direct electron detector (ThermoFisher) operating in counting mode at 96,000× (0.8315 Å pixel size). Automated data collection with EPU varied the defocus range between −0.8 to −2.2 μm with three movies collected per hole through image shift prior to stage movement. All movies had an exposure time of approximately 40 s for a total dose of 40 e−/Å2 fractionated over 50 frames.
Cryo-EM data collection of the ASC-Caspase-1 CARD octamer was conducted at the HMS Cryo-EM Center. The CARD octamer sample (A280 = 0.2; 25 mM Tris-HCl pH 8.0, 150 mM NaCl, 2 mM DTT) was applied to a glow-discharged Quantifoil grid (R1.2/1.3 400-mesh gold-supported holey carbon, Electron Microscopy Sciences) blotted for 3–4 s under 100% humidity at 4 °C, and plunged into liquid ethane using a Mark IV Vitrobot (ThermoFisher). 5377 movies were acquired using a Titan Krios microscope (ThermoFisher) at an acceleration voltage of 300 keV equipped with a BioQuantum K3 Imaging Filter (slit width 20 eV), and a K3 direct electron detector (Gatan) operating in counting mode at 105,000× (0.825 Å pixel size). Automated data collection with SerialEM varied the defocus range between −0.8 to −2.5 μm with two shots collected in each of four holes per stage movement through image shift. All movies were exposed with a total dose of 57.12 e−/Å2 for 1.897 s fractionated over 50 frames.
Cryo-EM data processing
For the CARD8-CT filament, 1208 movies were aligned using RELION’s implementation of the MotionCor2 algorithm56. The defocus values and contrast transfer functions (CTFs) of the motion-corrected micrographs were then computed and corrected for using CTTFFIND4.157. 1181 micrographs were selected for further processing based on a maximum resolution criterion of 10 Å. Subsequently, start-end particle coordinates were manually picked and 287,568 particles were extracted in RELION58, with a box size of 640 pixels, shift of 6 Å for each segment box, and two times binning58,59 (320 pixel box). After 2D classification, 163,233 particles remained. An initial helical symmetry of 99.1° and 5.2 Å was derived from the power spectrum of the best 2D class average. An initial model was built with relion_helix_toolbox58 using the initial helical parameters as input. 111,333 particles were selected after 3D classification, which were re-extracted without binning and used for 3D refinement. Particle polishing and CTF refinement followed by final round of 3D refinement led to a refined helical symmetry −99.07° and 5.20 Å. Postprocessing in RELION led to a 3.3 Å reconstruction (Fig. 1 and Supplementary Fig. 1).
For the NLRP1-CT filament, movie frames were aligned using RELION’s implementation of the MotionCor2 algorithm56. The defocus values and CTFs of the motion-corrected micrographs were then computed and corrected for using CTTFFIND4.157. 1578 micrographs were selected for further processing based on a maximum CTF resolution criterion of 5 Å. Subsequently, start-end particle coordinates were manually picked, and 118,006 particles were extracted in RELION58 with a box size of 512 pixels and shift of 48 Å for each segment box58,59. All particles were downscaled to a box size 360 to reduce processing time. After 2D classification, 55,083 particles remained. An initial helical symmetry of −100.8° and 5.1 Å was derived from the power spectrum of the best 2D class average. An initial model (helical lattice) was built with relion_helix_toolbox58 using these initial helical parameters as input. 12,200 particles were selected after 3D classification and used for final 3D refinement, followed by CTF refinement and particle polishing prior to a final round of 3D refinement. The refined helical symmetry was −100.79° and 5.08 Å. Postprocessing in RELION led to a 3.6 Å reconstruction (Fig. 1 and Supplementary Fig. 2).
For the ASCCARD-caspase-1CARD octamer, frames from 5377 movies were aligned using RELION’s implementation of the MotionCor2 algorithm56. The defocus values and CTFs of the motion-corrected micrographs were then computed and corrected for using Gctf60, and images were pre-screened with MicAssess61. 602,874 particles were picked in crYOLO62, extracted with 1.65 Å pixel size (2× binning), and subjected to 2D and 3D classifications in RELION. 58,875 particles remained. A second round of particle picking was carried on in Gautomatch with selected 2D classes as template, and the previously selected 59,315 particles were excluded. 1,260,583 particles were picked and extracted with 1.65 Å pixel size. 61,147 remained after 2D and 3D classifications. These particles were combined with the previous particle stack to yield 120,462 total particles, followed by 3D refinement and particle polishing in RELION. 9409 particles were considered as duplicates and removed, based on a 60 Å minimum interparticle distance. Final 3D refinement and postprocessing with this set of 111,053 particles in RELION led to a 3.9 Å map. Map sharpening was performed with DeepEMhancer63 using the “tightTarget” model (Fig. S5).
Model building and display
Model building was performed in program Coot64. The monomeric NLRP1CARD or CARD8CARD crystal structure (PDB ID: 4IFP42 or 4IKM43) was fit to the NLRC4CARD filament model (PDB ID: 6N1I36) and used as initial models for refinement. Refinement was performed using Phenix65 and Refmac66. For the ASCCARD-caspase-1CARD octamer, subunit structures from ASCCARD (PDB ID: 6N1H36) and caspase-1CARD filaments (PDB ID: 5FNA7) were fitted individually into the octamer cryo-EM map, and refined using Phenix65 and Refmac66. Structural representations were displayed and rendered using Pymol67, UCSF ChimeraX68, and UCSF Chimera46.
For surface electrostatic analysis, CARD filaments of CARD8, NLRP1, caspase-1 (PDB ID: 5FNA7), and ASC (PDB ID: 6N1H36) were analysed with the Adaptive Poisson-Boltzmann Solver (APBS) in Pymol67. Electrostatics were scaled identically (±5) for comparison (Fig. 5a–d). To analyse the complementarity and the interaction between CARD8 and caspase-1, or between NLRP1 and ASC, a single layer of CARD8 or NLRP1 (four molecules) was extracted from its filament structure and fit to a single layer of caspase-1 or ASC. The UCSF Chimera “Matchmaker”46 alignment tool was used to spread the RMSD resulting from differences in helical parameters among all four molecules. Interactions were analysed both below and above the fitted layer (a or b type).
Cell death assay and immunoblotting
HEK 293T cells stably expressing caspase-1 and GSDMD-V5 were seeded at 2 × 105 cells/well in 12-well tissue culture dishes. The following day, cells were transfected with plasmids encoding for the indicated NLRP1 or CARD8 construct (0.02 μg), ASC for NLRP1 experiments (0.01 µg), and RFP (to 1 µg) using FuGENE HD according to manufacturer’s instructions (Promega). Twenty-four hours later supernatants were analysed for LDH activity using the Pierce LDH Cytotoxicity Assay Kit (ThermoFisher) and lysates were evaluated by immunoblotting for caspase-1 (Cell Signaling Technology, #2225, 1:1000 dilution), GSDMD (Novus, 33422, 1:1000 dilution) and GAPDH (Cell Signaling Technology, 14C10, 1:1000 dilution) with secondary IRDye 800CW donkey anti-Rabbit (LI-COR, 926-32213, 1:10,000 dilution) imaged via Odyssey CLx (LI-COR). For CARD versus UPA-CARD titration experiments, cells seeded as described above were transfected with the indicated amount of CARD or UPA-CARD construct (20, 200, or 2000 ng), ASC for NLRP1 experiments (0.1 µg), and RFP (to 2.1 µg) per 125 µL optimum using FuGENE HD according to manufacturer’s instructions (Promega). For NLRP1 dimer interface mutant titration experiments, cells seeded as described above were transfected with the indicated UPA-CARD construct (20, 2, or 0.2 ng), ASC (10 ng), and RFP (to 2 µg) per 125 µL optimum using FuGENE HD according to manufacturer’s instructions (Promega). Supernatants were analysed for LDH release after 48 h using the Pierce LDH Cytotoxicity Assay Kit (ThermoFisher). Full uncropped gels are available in the accompanying Source Data file.
HEK 293T cultured in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10% fetal bovine serum (FBS) were plated on CELLview 4-compartment dishes (Greiner Bio-One). HEK 293T cells were transfected with CARD8 WT and mutant UPA-CARD-mCherry constructs (0.02 μg) using lipofectamine 2000 (Thermo Fisher Scientific). Forty-eight hours after transfection, cells were fixed with 4% PFA for 10 min at RT. Cells were imaged using a spinning disk confocal Nikon microscope equipped with a Plan Apo 20×/1.3 air objective. Image analysis was performed in Fiji69.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Raw cryo-EM data have been deposited in EMPIAR under the accession numbers EMPIAR-10567 (CARD8-CT filament), EMPIAR-10564 (NLRP1-CT filament), and EMPIAR-10566 (ASCCARD-caspase-1CARD octamer). The cryo-EM structures have been deposited in the Electron Microscopy Data Bank (EMDB) with accession numbers EMD-22219 (CARD8-CT filament), EMD-22220 (NLRP1-CT filament), and EMDB-22233 (ASCCARD-caspase-1CARD octamer). The atomic coordinates have been deposited in the protein databank (PDB) with accession numbers 6XKJ (CARD8-CT filament), 6XKK (NLRP1-CT filament), and 7KEU (ASCCARD-caspase-1CARD octamer). Pymol/chimera session files are available on our Open Science Framework repository [https://doi.org/10.17605/OSF.IO/X7DV8]. Other data are available from the corresponding author upon reasonable request. Source data are provided with this paper.
Martinon, F., Burns, K. & Tschopp, J. The inflammasome: a molecular platform triggering activation of inflammatory caspases and processing of proIL-β. Mol. Cell 10, 417–426 (2002).
Broz, P. & Dixit, V. M. Inflammasomes: mechanism of assembly, regulation and signalling. Nat. Rev. Immunol. 16, 407–420 (2016).
Lu, A. et al. Unified polymerization mechanism for the assembly of ASC-dependent inflammasomes. Cell 156, 1193–1206 (2014).
Shen, C., Sharif, H., Xia, S. & Wu, H. Structural and mechanistic elucidation of inflammasome signaling by cryo-EM. Curr. Opin. Struct. Biol. 58, 18–25 (2019).
Hu, Z. et al. Structural and biochemical basis for induced self-propagation of NLRC4. Science 350, 399–404 (2015).
Zhang, L. et al. Cryo-EM structure of the activated NAIP2-NLRC4 inflammasome reveals nucleated polymerization. Science 350, 404–409 (2015).
Lu, A. et al. Molecular basis of caspase-1 polymerization and its inhibition by a new capping mechanism. Nat. Struct. Mol. Biol. 23, 416–425 (2016).
Park, H. H. et al. The death domain superfamily in intracellular signaling of apoptosis and inflammation. Annu. Rev. Immunol. 25, 561–586 (2007).
Kesavardhana, S., Malireddi, R. K. S. & Kanneganti, T.-D. Caspases in cell death, inflammation, and pyroptosis. Annu. Rev. Immunol. 38, 567–595 (2020).
Lieberman, J., Wu, H. & Kagan, J. C. Gasdermin D activity in inflammation and host defense. Sci. Immunol. 4, 39 (2019).
Xia, S., Hollingsworth, L. R. & Wu, H. Mechanism and regulation of gasdermin-mediated cell death. Cold Spring Harb. Perspect. Biol. 12, a036400 (2019).
Ruan, J., Xia, S., Liu, X., Lieberman, J. & Wu, H. Cryo-EM structure of the gasdermin A3 membrane pore. Nature 557, 62–67 (2018).
Zhong, F. L. et al. Germline NLRP1 mutations cause skin inflammatory and cancer susceptibility syndromes via inflammasome activation. Cell 167, 187–202 (2016).
Levandowski, C. B. et al. NLRP1 haplotypes associated with vitiligo and autoimmunity increase interleukin-1β processing via the NLRP1 inflammasome. Proc. Natl Acad. Sci. USA 110, 2952–2956 (2013).
Jin, Y. et al. NALP1 in vitiligo-associated multiple autoimmune disease. N. Engl. J. Med. 356, 1216–1225 (2007).
Zhong, F. L. et al. Human DPP9 represses NLRP1 inflammasome and protects against auto-inflammatory diseases via both peptidase activity and FIIND domain binding. J. Biol. Chem. 293, 18864–18878 (2018).
Grandemange, S. et al. A new autoinflammatory and autoimmune syndrome associated with NLRP1 mutations: NAIAD (NLRP1-associated autoinflammation with arthritis and dyskeratosis). Ann. Rheum. Dis. 76, 1191–1198 (2017).
Drutman, S. B. et al. Homozygous NLRP1 gain-of-function mutation in siblings with a syndromic form of recurrent respiratory papillomatosis. Proc. Natl Acad. Sci. USA 116, 19055–19063 (2019).
Johnson, D. C. et al. DPP8/DPP9 inhibitor-induced pyroptosis for treatment of acute myeloid leukemia. Nat. Med. 24, 1151–1156 (2018).
Linder, A. et al. CARD8 inflammasome activation triggers pyroptosis in human T cells. EMBO J. 39, e105071 (2020).
Johnson, D. C. et al. DPP8/9 inhibitors activate the CARD8 inflammasome in resting lymphocytes. Cell Death Dis. 11, 628 (2020).
Taabazuing, C. Y., Griswold, A. R. & Bachovchin, D. A. The NLRP1 and CARD8 inflammasomes. Immunol. Rev. 297, 1–13 (2020).
Mitchell, P. S., Sandstrom, A. & Vance, R. E. The NLRP1 inflammasome: new mechanistic insights and unresolved mysteries. Curr. Opin. Immunol. 60, 37–45 (2019).
Finger, J. N. et al. Autolytic proteolysis within the function to find domain (FIIND) is required for NLRP1 inflammasome activity. J. Biol. Chem. 287, 25030–25037 (2012).
D’Osualdo, A. et al. CARD8 and NLRP1 undergo autoproteolytic processing through a ZU5-Like domain. PLoS ONE 6, e27396 (2011).
Xu, H. et al. The N‐end rule ubiquitin ligase UBR2 mediates NLRP1B inflammasome activation by anthrax lethal toxin. EMBO J. 38, e101996 (2019).
Chui, A. J. et al. N-terminal degradation activates the NLRP1B inflammasome. Science 364, 82–85 (2019).
Sandstrom, A. et al. Functional degradation: a mechanism of NLRP1 inflammasome activation by diverse pathogen enzymes. Science 364, eaau1330 (2019).
Okondo, M. C. et al. Inhibition of Dpp8/9 activates the Nlrp1b inflammasome. Cell Chem. Biol. 25, 262–267 (2018).
Sharif, H. et al. Structural mechanism for NEK7-licensed activation of NLRP3 inflammasome. Nature 570, 338–343 (2019).
Srinivasula, S. M. et al. The PYRIN-CARD protein ASC is an activating adaptor for caspase-1. J. Biol. Chem. 277, 21119–21122 (2002).
Ball, D. P. et al. Caspase-1 interdomain linker cleavage is required for pyroptosis. Life Sci. Alliance 3, e202000644 (2020).
Poyet, J. L. et al. Identification of Ipaf, a human caspase-1-activating protein related to Apaf-1. J. Biol. Chem. 276, 28309–28313 (2001).
Broz, P. et al. Redundant roles for inflammasome receptors NLRP3 and NLRC4 in host defense against Salmonella. J. Exp. Med. 207, 1745–1755 (2010).
Matyszewski, M. et al. Cryo-EM structure of the NLRC4CARD filament provides insights into how symmetric and asymmetric supramolecular structures drive inflammasome assembly. J. Biol. Chem. 293, 20240–20248 (2018).
Li, Y. et al. Cryo-EM structures of ASC and NLRC4 CARD filaments reveal a unified mechanism of nucleation and activation of caspase-1. Proc. Natl Acad. Sci. USA 115, 10845–10852 (2018).
Wu, B. et al. Molecular imprinting as a signal-activation mechanism of the viral RNA sensor RIG-I. Mol. Cell 55, 511–523 (2014).
David, L. et al. Assembly mechanism of the CARMA1-BCL10-MALT1-TRAF6 signalosome. Proc. Natl Acad. Sci. USA 115, 1499–1504 (2018).
Ferrao, R. & Wu, H. Helical assembly in the death domain (DD) superfamily. Curr. Opin. Struct. Biol. 22, 241–247 (2012).
Hollingsworth, L. R. et al. DPP9 directly sequesters the NLRP1 C-terminus to repress inflammasome activation. bioRxiv https://doi.org/10.1101/2020.08.14.246132 (2020).
Huang, M. et al. Structural and biochemical mechanisms of NLRP1 inhibition by DPP9. bioRxiv https://doi.org/10.1101/2020.08.13.250241 (2020).
Jin, T., Curry, J., Smith, P., Jiang, J. & Xiao, T. S. Structure of the NLRP1 caspase recruitment domain suggests potential mechanisms for its association with procaspase-1. Proteins 81, 1266–1270 (2013).
Jin, T., Huang, M., Smith, P., Jiang, J. & Xiao, T. S. The structure of the CARD8 caspase-recruitment domain suggests its association with the FIIND domain and procaspases through adjacent surfaces. Acta Crystallogr. F. 69, 482–487 (2013).
Proell, M., Gerlic, M., Mace, P. D., Reed, J. C. & Riedl, S. J. The CARD plays a critical role in ASC foci formation and inflammasome signalling. Biochem. J. 449, 613–621 (2013).
Shen, C. et al. Molecular mechanism for NLRP6 inflammasome assembly and activation. Proc. Natl Acad. Sci. USA 116, 2052 (2019).
Pettersen, E. F. et al. UCSF Chimera—A visualization system for exploratory research and analysis. J. Comput. Chem. 25, 1605–1612 (2004).
Wu, H. Higher-order assemblies in a new paradigm of signal transduction. Cell 153, 287–292 (2013).
Kagan, J. C., Magupalli, V. G. & Wu, H. Supramolecular organizing centres: location-specific higher-order signalling complexes that control innate immunity. Nat. Rev. Immunol. 14, 821–826 (2014).
Gong, X. et al. Structural basis for distinct inflammasome complex assembly by human NLRP1 and CARD8. Nat. Comms https://doi.org/10.1038/s41467-020-20319-5 (2020).
Diebolder, C. A., Halff, E. F., Koster, A. J., Huizinga, E. G. & Koning, R. I. Cryoelectron tomography of the NAIP5/NLRC4 inflammasome: implications for NLR activation. Structure 23, 2349–2357 (2015).
Ha, H. J. & Park, H. H. Crystal structure of the human NLRP9 pyrin domain reveals a bent N-terminal loop that may regulate inflammasome assembly. FEBS Lett. 594, 2396–2405 (2020).
Marleaux, M., Anand, K., Latz, E. & Geyer, M. Crystal structure of the human NLRP9 pyrin domain suggests a distinct mode of inflammasome assembly. FEBS Lett. 594, 2383–2395 (2020).
Peisley, A., Wu, B., Yao, H., Walz, T. & Hur, S. RIG-I forms signaling-competent filaments in an ATP-dependent, ubiquitin-independent manner. Mol. Cell 51, 573–583 (2013).
Peisley, A., Wu, B., Xu, H., Chen, Z. J. & Hur, S. Structural basis for ubiquitin-mediated antiviral signal activation by RIG-I. Nature 509, 110–114 (2014).
Qiao, Q. et al. Structural architecture of the CARMA1/Bcl10/MALT1 signalosome: nucleation-induced filamentous assembly. Mol. Cell 51, 766–779 (2013).
Zheng, S. Q. et al. MotionCor2: anisotropic correction of beam-induced motion for improved cryo-electron microscopy. Nat. Methods 14, 331–332 (2017).
Mindell, J. A. & Grigorieff, N. Accurate determination of local defocus and specimen tilt in electron microscopy. J. Struct. Biol. 142, 334–347 (2003).
He, S. & Scheres, S. H. W. Helical reconstruction in RELION. J. Struct. Biol. 198, 163–176 (2017).
Zivanov, J. et al. New tools for automated high-resolution cryo-EM structure determination in RELION-3. eLife 7, e42166 (2018).
Zhang, K. Gctf: real-time CTF determination and correction. J. Struct. Biol. 193, 1–12 (2016).
Li, Y., Cash, J. N., Tesmer, J. J. G. & Cianfrocco, M. A. High-throughput Cryo-EM enabled by user-free preprocessing routines. Structure 28, 858–869 (2020).
Wagner, T. et al. SPHIRE-crYOLO is a fast and accurate fully automated particle picker for cryo-EM. Commun. Biol. 2, 218 (2019).
Sanchez-Garcia, R. et al. DeepEMhancer: a deep learning solution for cryo-EM volume post-processing. bioRxiv https://doi.org/10.1101/2020.06.12.148296 (2020).
Emsley, P., Lohkamp, B., Scott, W. G. & Cowtan, K. Features and development of Coot. Acta Crystallogr. D 66, 486–501 (2010).
Adams, P. D. et al. PHENIX: a comprehensive Python-based system for macromolecular structure solution. Acta Crystallogr. D 66, 213–221 (2010).
Murshudov, G. N. et al. REFMAC5 for the refinement of macromolecular crystal structures. Acta Crystallogr. D 67, 355–367 (2011).
Schrodinger, L. L. C. The PyMOL Molecular Graphics System Version 1.8 (New York, NY, 2015).
Goddard, T. D. et al. UCSF ChimeraX: meeting modern challenges in visualization and analysis. Protein Sci. 27, 14–25 (2018).
Schindelin, J. et al. Fiji: an open-source platform for biological-image analysis. Nat. Methods 9, 676–682 (2012).
Kucukelbir, A., Sigworth, F. J. & Tagare, H. D. Quantifying the local resolution of cryo-EM density maps. Nat. Methods 11, 63–65 (2014).
We thank Maria Ericsson at the HMS EM facility for advice and training, Zongli Li, Richard Walsh, Sarah Sterling, and Shaun Rawson at the Harvard Cryo-EM Center for Structural Biology for cryo-EM screening, data collection, training, and productive consultation, Paula Montero Llopis at the Microscopy Resources on the North Quad (MicRoN) core at HMS for microscope use, Ross Tomaino at the HMS Taplin Mass Spectrometry Facility, Theo Humphreys for cryo-EM screening and data collection at the Pacific Northwest Center for Cryo-EM (PNCC), Chen Xu and Kangkang Song for cryo-EM screening and data collection at UMass Medical School, BioRender for figure design, and SBGrid for computing support. This work was supported by National Institutes of Health grants DP1 HD087988 and R01 AI124491 to H.W., T32-GM007726 to L.R.H., the CRI Irvington Postdoctoral Fellowship to P.F., T32 GM007739-Andersen and F30 CA243444 to A.R.G., T32 GM115327-Tan to E.L.O., R01 AI137168 to D.A.B., and the Memorial Sloan Kettering Cancer Center Core Grant P30 CA008748 to D.A.B. A portion of this research was also supported by NIH grant U24GM129547 and performed at the PNCC at OHSU and accessed through EMSL (grid.436923.9), a DOE Office of Science User Facility sponsored by the Office of Biological and Environmental Research.
H.W. is a co-founder of Ventus Therapeutics. The other authors declare no competing interests.
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Robert Hollingsworth, L., David, L., Li, Y. et al. Mechanism of filament formation in UPA-promoted CARD8 and NLRP1 inflammasomes. Nat Commun 12, 189 (2021). https://doi.org/10.1038/s41467-020-20320-y