MLKL is the essential effector of necroptosis, a form of programmed lytic cell death. We have isolated a mouse strain with a single missense mutation, MlklD139V, that alters the two-helix ‘brace’ that connects the killer four-helix bundle and regulatory pseudokinase domains. This confers constitutive, RIPK3 independent killing activity to MLKL. Homozygous mutant mice develop lethal postnatal inflammation of the salivary glands and mediastinum. The normal embryonic development of MlklD139V homozygotes until birth, and the absence of any overt phenotype in heterozygotes provides important in vivo precedent for the capacity of cells to clear activated MLKL. These observations offer an important insight into the potential disease-modulating roles of three common human MLKL polymorphisms that encode amino acid substitutions within or adjacent to the brace region. Compound heterozygosity of these variants is found at up to 12-fold the expected frequency in patients that suffer from a pediatric autoinflammatory disease, chronic recurrent multifocal osteomyelitis (CRMO).
Necroptosis is a lytic form of programmed cell death associated with the production of pro-inflammatory cytokines, the destruction of biological membranes and the release of intracellular damage associated molecular patterns (DAMPs)1. Necroptosis depends on the activation of the mixed lineage kinase domain-like (MLKL) pseudokinase by receptor interacting protein kinase 3 (RIPK3)2,3,4. RIPK3-mediated phosphorylation of MLKL triggers a conformational change4,5 that facilitates the translocation to, and eventual irreversible disruption of, cellular membranes. While the precise biophysical mechanism of membrane disruption is still a matter of debate, common features of contemporary models are the formation of an MLKL oligomer and the direct association of the executioner four-helix bundle domain (4HB) of MLKL with biological membranes6,7,8,9,10. In mouse cells, the expression of the murine MLKL 4HB domain alone (residues 1–125), 4HB plus brace helices (1–180), or the expression of phosphomimetic or other single site pseudokinase domain (PsKD) mutants is sufficient to induce membrane translocation, oligomerization and membrane destruction4,9. While capable of disrupting synthetic liposomes when produced recombinantly, similarly truncated and equivalent single site (PsKD) mutant forms of human MLKL do not robustly induce membrane-associated oligomerization and cell death without forced dimerization11,12,13. Furthermore, both mouse and human MLKL mutants have been reported that have the capacity to form membrane-associated oligomers, but fail to cause irreversible membrane disruption and cell death9,13. Recent studies have revealed that necroptosis downstream of MLKL phosphorylation and membrane association can be modulated by processes that engage the endosomal sorting complex required for transport (ESCRT) family of proteins. One model proposes a role for ESCRT in limiting necroptosis via plasma membrane excision and repair14 while other models limit plasma membrane disruption by ESCRT-mediated release of phosphorylated MLKL in extracellular vesicles15,17,17 and/or the internalization of phosphorylated MLKL for lysosomal degradation17.
In mice, the absence of MLKL does not appear to have obvious deleterious developmental or homeostatic effects4,18. However, genetic deletion of Fadd, Casp8 or Ripk1, leads to inappropriate activation of MLKL and ensuing necroptosis during embryogenesis that is incompatible with life beyond embryonic day (E)10.5, E10.5 and 1–3 days post-natally, respectively19,20,21,22,23,24,25. Exploring the precise physiological consequences of inappropriate MLKL activation in these scenarios is complicated by the fact that FADD, Caspase-8 and RIPK1 also play important roles in cellular processes other than modulation of MLKL-induced necroptotic cell death23,26,27,28,29,30.
Aberrant levels of MLKL-dependent cell death contribute to disease in several genetic and experimental mouse models23,31,32,33,34,35. In humans, MLKL mRNA and protein levels are positively correlated with survival of patients with pancreatic adenocarcinoma, cervical-, gastric-, ovarian- and colon- cancers (reviewed by ref. 36). Interestingly, high levels of phosphorylated MLKL are associated with reduced survival in esophageal and colon cancer patients37. Two missense MLKL somatic mutations identified in human cancer tissue have been found to confer a reduction in necroptotic function in cell-based assays4,13. Very recently, siblings suffering from a novel neurodegenerative disorder were reported as homozygous for a rare haplotype involving a frameshift variant in MLKL, as well as an in-frame deletion of one amino acid in the adjacent fatty acid 2-hydroxylase (FA2H) gene38. The significant enrichment of an ultra-rare MLKL stop-gain gene variant p.Q48X has been reported in Hong Kong Chinese patients suffering from a form of Alzheimer’s disease39, however more common germline MLKL gene variants are only weakly associated with human disease in GWAS databases.
We have identified a single base pair germline mutation of mouse Mlkl that encodes a missense substitution within the MLKL brace region and confers constitutive activation independent of upstream necroptotic stimuli. Given this mutant Mlkl allele is subject to the same developmental and environmental controls on gene expression as wild-type Mlkl, the postnatal lethality in these mice provides insight into the physiological and pathological consequences of dysregulated necroptosis. In parallel, these findings inform the potential functional significance of three common human MLKL polymorphisms that encode non-conservative amino acid substitutions within, or in close proximity to, the brace helix that is mutated in the MlklD139V mouse.
Generation of a constitutively active form of MLKL
Mpl−/− mice, owing to genetic deletion of the major receptor for thrombopoietin, have only 10% the wild-type number of peripheral platelets. An ENU mutagenesis screen was performed to identify mutations that ameliorate thrombocytopenia in Mpl−/− mice via thrombopoietin independent platelet production40. A G1 founder, designated Plt15, had a modestly elevated platelet count of 189 × 106 per mL compared with the mean for Mpl−/− animals (113 ± 57 × 106 per mL) and yielded 19 Mpl−/− progeny. Ten of these mice had platelet counts over 200 × 106 per mL, consistent with segregation of a dominantly acting mutation (Fig. 1a). Linkage analysis and sequencing identified an A to T transversion in Mlkl that was heterozygous in all mice with an elevated platelet count (Fig. 1b). The MlklPlt15 mutation results in a non-conservative aspartic acid-to-valine substitution at position 139 within the first brace helix. In the full-length mMLKL structure, D139 forms a salt bridge with an arginine residue at position 30 (α2 helix) of the MLKL four-helix bundle (4HB) domain4 (Fig. 1c). This salt bridge represents one of a series of electrostatic interactions between residues in helix α2 of the MLKL 4HB domain and the two-helix ‘brace’ region. D139 of mouse MLKL is conserved in all MLKL orthologues in vertebrata reported to date (Fig. 1d). We have shown that the exogenous expression of the 4HB domain of murine MLKL alone is sufficient to kill mouse fibroblasts whereas exogenous expression of full-length MLKL does not, suggesting an important role for this ‘electrostatic zipper’ in suppressing the killing activity of the MLKL 4HB9. To determine if MLKLD139V exhibited altered ability to induce necroptotic cell death relative to MLKLWT, we stably expressed these full-length proteins under the control of a doxycycline-inducible promoter in immortalized mouse dermal fibroblasts (MDF) isolated from Wt, Mlkl−/−, Ripk3−/− or Ripk3−/−;Casp8−/− mice. While expressed at comparable levels, MLKLD139V induced markedly more death than MLKLWt, on each of the genetic backgrounds tested (Fig. 1e–f, Supplementary Fig. 1a), and formed a high molecular weight complex observable by BN-PAGE in the absence of exogenous necroptotic stimuli (Supplementary Fig. 1b). This indicates that MLKLD139V is a constitutively active form of MLKL, capable of inducing necroptotic cell death independent of upstream signaling and phosphorylation by its activator RIPK3. Consistent with this interpretation, exogenous expression of MLKLD139V in Ripk3−/−;Casp8−/− MDFs was sufficient to induce the organelle swelling and plasma membrane rupture characteristic of TNF-induced necroptosis when examined by Transmission Electron Microscopy (Fig. 1g).
Mlkl D139V causes a lethal perinatal inflammatory syndrome
To define the phenotypic consequences of constitutively active MLKL in the absence of any confounding effects resulting from Mpl-deficiency, all subsequent studies were performed on a Mpl+/+ background. Homozygous MlklD139V/D139V pups were born at expected Mendelian frequencies (Supplementary Table 1) and were ostensibly normal macroscopically and histologically at E19.5 (Supplementary Fig. 2a–d). However, by 3 days of age, although outwardly indistinguishable from littermates (Fig. 2a), they exhibited reduced body weight (Supplementary Fig. 2b) and failed to thrive, with a maximum observed lifespan of 6 days under conventional clean housing conditions. Like MlklWt/D139V mice, Mlklnull/D139V compound heterozygotes were present at the expected frequency at P21 and developed normally to adulthood (Supplementary Table 2). Thus, the constitutive activity of MLKLD139V was not affected by the presence of normal MLKL protein suggesting it is the absolute allelic dose of MlklD139V that determines perinatal lethality. To confirm that the phenotype of the ENU derived MlklD139V mice was due to the MlklD139V missense mutation, we independently generated MlklD139V mice using CRISPR-Cas9 genomic editing. Homozygote CRISPR-MlklD139V/D139V mice also died soon after birth (Supplementary Table 3).
Hematoxylin-Eosin stained-sections from both P2 and P3 MlklD139V/D139V pups revealed multifocal acute inflammation characterized by neutrophilic infiltration, dilated blood vessels and edema (Fig. 2b) in the dermis and subcutis of the head and neck. These inflammatory features were not observed in MlklWt/Wt or MlklWt/D139V littermates, nor in Mlkl−/− mice of the same age (Supplementary Fig. 2i). Cells of hematopoietic origin, revealed by immunohistochemical staining for CD45, were sparsely distributed throughout the lower head and neck and confined predominantly to a clearly delineated developing lymph node in MlklWt/Wt and MlklWt/D139V littermates (Fig. 2c). In contrast, CD45+ cells were more numerous and distributed throughout the cutis, subcutis and salivary glands of MlklD139V/D139V pups (Fig. 2c). A mixture of diffuse and focal inflammatory infiltration was also observed within the mediastinum and pericardial space of all P2/P3 MlklD139V/D139V pups examined, as was a paucity of thymic cortical lymphocytes (Fig. 2d, Supplementary Fig. 2e), phenotypes not evident in E19.5 embryos (Supplementary Fig. 2d). No other consistent lesions were observed by histopathology. Consistent with this inflammatory phenotype, significantly elevated levels of several pro-inflammatory cytokines and chemokines were evident in the plasma of both E19.5 and P3 MlklD139V/D139V pups (Fig. 2e, f). Blood glucose levels were normal (Supplementary Fig. 2f, g).
Hematopoietic defects in Mlkl D139V mice
Although blood cell numbers were unchanged in MlklD139V/D139V pups at E19.5 relative to MlklWt/Wt and MlklWt/D139V littermates, by P3 significant deficits were evident in total white blood cell count (due predominantly to reductions in lymphocyte numbers) and platelet numbers (Fig. 3a–c, Supplementary Fig. 3a). Similarly, the numbers of hematopoietic stem and progenitor cells were present at normal proportions in fetal livers of E18.5 MlklD139V/D139V pups, although increased levels of intracellular ROS were uniformly evident in live cells, (Fig. 3d, e, Supplementary Fig. 3b,c). By P2, deficits in CD150+CD48+ and CD150+CD48− populations were present (Fig. 3f), accompanied by increased AnnexinV binding in live cells (which indicates phosphatidyl serine exposure) of all lineages (Fig. 3g). In adult MlklWt/D139V mice, numbers of hematopoietic stem and progenitor cells were unaffected (Fig. 3h); however, upon myelosuppressive irradiation, recovery of hematopoietic cell numbers was delayed and characterized by increased expression of ROS and Annexin V (Supplementary Fig. 3d, e). When challenged with the cytotoxic drug 5-fluorouracil (5-FU), blood cell recovery in MlklWt/D139V mice was similarly delayed (Fig. 3i). In competitive transplants in which test MlklWt/D139V or MlklWt/Wt marrow was co-injected with wild-type competitor marrow in 10:1 excess, as expected, MlklWt/Wt marrow contributed to 90% of recipient blood cells 8 weeks after transplantation and maintained that level of contribution for 6 months (Fig. 3j). In contrast, MlklWt/D139V marrow performed poorly, contributing to 25% and 51% of recipient blood cells at these times (Fig. 3j). Similarly, while wild-type fetal liver cells contributed to the vast majority of blood cells in irradiated recipients up to 6 months after transplantation, cells from MlklD139V/D139V embryos failed to compete effectively during this period (Fig. 3k). Heterozygote MlklWt/D139V fetal liver cells contributed poorly in the first month following the graft but recovered to contribute more after six months (Fig. 3k). Thus, while tolerated under steady-state conditions, heterozygosity of MlklD139V is deleterious under conditions of hematopoietic stress. Bone marrow- derived HSCs from MlklWt/D139V adults and fetal liver- derived HSCs from MlklWt/D139V and MlklD139V/D139V pups also formed fewer and smaller colonies in the spleens of lethally irradiated recipient mice after 8 days (Supplementary Fig. 3f).
Mlkl D139V fibroblasts are less sensitive to necroptosis
To examine if the constitutive activity of exogenously expressed MLKLD139V results in an enhanced propensity for necroptosis in cells that express MLKLD139V under the control of its endogenous promoter, we immortalized MDFs from MlklWt/Wt, MlklWt/D139V and MlklD139V/D139V littermates and from Mlkl−/− E19.5 pups. We observed no significant differences in basal cell death levels, nor any differences in the sensitivity of these cells to an apoptotic stimulus such as TNF plus Smac mimetic (Fig. 4a, Supplementary Fig. 4a). Surprisingly and in apparent contradiction to our initial observations using exogenous expression systems, endogenous expression of this Mlkl mutant revealed a significant and consistent decrease in sensitivity to TNF-induced necroptosis using three different pan-caspase inhibitors Q-VD-OPh, zVAD-fmk and IDN-6556/emricasan in a MlklD139V dose-dependent manner (Fig. 4a, Supplementary Fig. 4a). MDFs isolated from MlklD139V/D139V homozygotes were up to 60% less sensitive to TNF-induced necroptosis compared with MlklWt/Wt MDFs, but were not as resistant as Mlkl−/− MDFs (Fig. 4a).
While there were no obvious differences in the levels of MLKLWt and MLKLD139V protein following doxycycline induced exogenous expression (Fig. 1f), MLKL was virtually undetectable by Western blot in MlklD139V/D139V pup-derived fibroblasts immortalized and cultured ex vivo (Fig. 4b). There was, however, no significant reduction in Mlkl gene transcript levels in these cells (Supplementary Fig. 4b) suggesting that this reduction was post-transcriptional. A reduction in MLKLD139V protein levels was also evident in whole E14.5 embryo protein lysates and in single cell clones derived from HOXA9 factor dependent myeloid cell lines derived from MlklD139V/D139V E14.5 embryos (Supplementary Figs. 4c, j). Lysates from E14.5 embryos also clearly show that MlklWt/D139V heterozygotes have intermediate levels of MLKL, reflecting the intermediate sensitivity of MlklWt/D139V MDFs to necroptotic stimuli (Supplementary Fig. 4c and Fig. 4a).
MLKLD139V protein turnover requires proteasome activity
Measuring the half-life of endogenously expressed MLKLD139V is not possible using conventional ‘pulse chase’ methods because this mutant protein induces necroptotic cell death, so we capitalized on our previous observation that an N-terminally FLAG-tagged MLKL 4HB forms a high molecular weight membrane-associated complex just like the untagged form, but, unlike the untagged version, does not kill cells9. Consistent with this observation, N-FLAG full-length mouse MLKLD139V did not induce cell death when inducibly expressed in Mlkl−/− MDFs (Supplementary Fig. 4f).
Using this system, we were able to measure the cellular turn over of MLKL by inducing N-FLAG-MLKLWT or N-FLAG-MLKLD139V expression in Mlkl−/− MDFs for 15 h using doxycycline then washing and culturing them in the absence of doxycycline for a further 2–24 h. In the absence of a stimulus (UT), the levels of N-FLAG-MLKLWT remained consistent over the 24-h period (Fig. 4c), indicating that non-activated wild-type MLKL is a stable protein in MDFs. However, when these cells were treated with a necroptotic stimulus (TSI) to activate MLKL, the levels of wild-type MLKL rapidly declined even though these cells were unable to undergo a necroptotic cell death. Consistent with the fact that untagged MLKLD139V behaves as an auto-activated form of MLKL (Fig. 1e), the half-life of N-FLAG-MLKLD139V (4–6 h) was similar to the WT version stimulated with TSI (Fig. 4c). Thus, the absence of endogenously expressed MLKLD139V in E14.5 embryo lysates and cultured fibroblasts can be attributed to the reduced post-translational stability of this mutant auto-activated form of the protein.
To determine which cellular mechanism(s) are required for the clearance of activated MLKLD139V, we included a series of proteasome, lysosome and specific protease inhibitors during the ‘chase’ period after doxycycline was withdrawn (schematic in Fig. 4d). The doses of all inhibitors were carefully titrated and combined with pan-caspase inhibitor IDN6556 to minimize any toxicity-associated apoptotic cell loss during the chase period. To exclude any confounding RIPK3-mediated activation of the necroptotic pathway by proteasome inhibitors41 (Supplementary Fig. 4f), the same experiment was also performed in Mlkl−/−, RIPK3−/− MDFs (Supplementary Fig. 4d). Even at the very low doses used, addition of the proteasome inhibitor PS341 was accompanied by reduced clearance of N-FLAG-MLKLD139V and the stabilization of higher molecular weight species that resemble mono- and poly-ubiquitinated MLKL (Fig. 4d, Supplementary Fig. 4d, i). This PS341 mediated protection of activated MLKL was also evident when the same assay was performed for phospho(p)S345-N-FLAG-MLKLWT (Supplementary Fig. 4e). The less potent proteasome inhibitor MG132 did not stabilize MLKLD139V to levels that could be resolved by western blotting of total MLKL in this assay but did facilitate some stabilization of (p)-N-FLAG-MLKLWT. Chloroquine, Bafilomycin and NH4Cl also partially protected against (p)-N-FLAG-MLKLWT clearance, supporting the potential role for lysosome mediated degradation of natively phosphorylated MLKLWT15,17, but this was not observed for constitutively activated N-FLAG-MLKLD139V using this approach (Fig. 4d, Supplementary Fig. 4d).
Based on these findings we hypothesized that this MLKL-clearance mechanism limits the capacity of MLKLD139V to kill MlklWt/D139V and MlklD139V/D139V cells in culture and in vivo by maintaining protein levels below a critical threshold. To test whether this protective mechanism could be overwhelmed, we incubated MDFs with agents that have been shown to induce Mlkl expression (TNF, interferons (IFN) β and γ)42,43,44, or inhibit its turnover (proteasome and lysosome inhibitors). MLKLD139V protein in untreated MlklD139V/D139V MDFs was undetectable by Western blot but became faintly detectable following addition of these stimuli (Fig. 4b and Supplementary Fig. 4g). This correlates with moderate but statistically significant increases in cell death (particularly when compared with the lack of sensitivity to conventional necroptotic stimuli (Fig. 4a)), when exposed to IFN-β alone and in combination with proteasome or lysosome inhibitors (Fig. 4e). A similar allele-dose dependent sensitivity is also evident in primary MDFs (Supplementary Fig. 4h). To examine if this mechanism may explain the reduced capacity of MlklD139V/D139V fetal liver cells to reconstitute an irradiated host (Fig. 2k), ex vivo colony forming assays were performed on fetal liver cells derived from MlklWt/Wt and MlklD139V/D139V E14.5 littermates, alongside E14.5 livers taken from Mlkl−/− mice. MlklD139V/D139V cells showed significantly increased sensitivity to the inhibitory effects of IFN-β, with reduced colony formation at low doses of cytokine that affected MlklWt/Wt and Mlkl−/− colony formation only marginally (Fig. 4f). Factor dependent myeloid cells generated through HOXA9 immortalization of E14.5 liver HSCs also demonstrated high rates of cell death under conventional FDM culture conditions when derived from MlklWt/D139V or MlklD139V/D139V embryos (Supplementary Fig. 4k). Together, these experiments provide further evidence for the existence of steady-state MLKL surveillance and turnover mechanisms that suppress cell death by lowering the abundance of activated MLKL below a killer threshold at the cellular level6,14,15,16 and provide an in vivo precedent for both the existence of this phenomenon and the lethal consequences of its dysregulation in the form of the MlklD139V mouse.
To test whether the lethal inflammation in MlklD139V/D139V neonates was mediated by the direct or indirect activation of the inflammasome by active MLKL we crossed this line with the Caspase 1/11 null mouse strain45,46,47. This did not enhance the lifespan of MlklD139V/D139V pups (Table 1). The combined genetic deletion of Casp8 and Ripk3 did not rescue or extend the life of MlklD139V/D139V mice, indicating that postnatal lethality is not mediated by bystander extrinsic apoptotic cell death that may occur secondary to initial waves of MLKLD139V-mediated necroptosis (Table 1). The genetic deletion of Tnfr1, Myd88 or Ifnar individually did not provide any extension to the lifespan of MlklD139V homozygote pups (Table 1). These data indicate that the removal of any one of these routes to NF-κB- and interferon-mediated gene upregulation, inflammation or apoptotic cell death is not sufficient to protect mouse pups against a double allelic dose of MlklD139V.
Common human missense MLKL variants map to the brace region
Given the severe inflammatory phenotype of murine MlklD139V/D139V neonates and the significant defects in stress hematopoiesis observed in murine MlklWt/D139V adults, we explored the prevalence of brace region variation in human MLKL. Examination of the gnomAD database48, which contains human MLKL exome or genome sequence data from a total of over 140,000 individuals revealed that the second and third highest frequency human MLKL missense coding variants; rs34515646 (R146Q) and rs35589326 (S132P), alter the same brace helix (Table 2, Fig. 5a). The 4th most common human MLKL polymorphism, rs144526386 (G202*V) is a missense polymorphism identified exclusively in the context of a shorter splice isoform of MLKL (*) named ‘MLKL2’49 (Table 2, Fig. 5b). The full-length canonical transcript of MLKL encodes a 471 amino acid protein, while MLKL2 is an alternatively spliced isoform of MLKL that is 263 amino acids long. MLKL2 lacks a large portion of the pseudokinase domain which functions to repress the killing potential of the 4HB domain6,7,8,9 and recruit co-effectors like RIPK3 and HSP9013,50,51,52. Glycine202* is encoded by an extension to exon 9 that is unique to the MLKL2 splice isoform (Fig. 5a, b).
While the amino acid substitution MLKLR146Q is classified as ‘tolerated’ and ‘benign’ by SIFT/POLYPHEN 2 algorithms53,54 (Supplementary Table 1), R146 of human MLKL shows NMR chemical shift perturbations in the presence of the negatively charged IP3 and IP6 phospholipid head groups, indicating a possible role in membrane association and disruption11,55. Ser-132 lies before the first structured residue of the first brace helix in human MLKL (Fig. 5a)13,56,57. A Serine-to-Proline substitution at this position is predicted to significantly impact the conformation of the immediately adjacent W133 (brace helix) and in turn, the proximal W109 within the 4HB domain (Supplementary Fig. 5a). When mapped to a model of MLKL splice-isoform 249 Glycine 202* is predicted to be on an isoform 2-specific helix and to form an interface along with S132 and R146 of brace helix 1. While the precise structural consequence of these three brace polymorphisms is unknown, modeling of human MLKL predicts that disruption in the brace region favors adoption of an activated conformation13. Consistent with this prediction, the murine equivalent of the human S132P variant, mMLKLS131P, formed high molecular weight membrane-associated complexes and killed MDFs in the absence of a necroptotic stimulus (Fig. 5c, d) when expressed at close to endogenous levels (Supplementary Fig. 5b). Similarly to mMLKLD139V, unstimulated mouse dermal fibroblasts generated from the first generation of heterozygote and homozygote mutant pups of a recently generated mMlklS131P CRISPR modified mouse line demonstrated a clear reduction in MLKL protein levels relative to those prepared from wild-type littermates (Supplementary Fig. 5c), though the cellular clearance is not as complete as observed for mMLKLD139V. Together, these data indicate that constitutive activation and reduced protein stability is not a unique, idiosyncratic feature of the mMLKLD139V, but also a feature of a closely situated MLKL brace mutant, mMLKLS131P.
MLKL brace variants occur in trans more frequently in CRMO
To investigate if human MLKL brace region polymorphisms play a role in human autoinflammatory disease we examined their frequency in cohorts suffering from ankylosing spondylitis (AS), chronic recurrent multifocal osteomyelitis (CRMO), Guillain Barré Syndrome (GBS) and Synovitis, Acne, Pustulosis, Hyperostosis and Osteitis (SAPHO) Syndrome. The individual minor allele frequencies of R146Q, S132P, and G*202V are not enriched in these disease cohorts relative to healthy controls when population distribution is accounted for (Supplementary Tables 4 and 5). However, these alleles occur in trans (making ‘compound heterozygotes’—schematic in Fig. 5e) in 3 out of 128 CRMO patients. This is 29 times the frequency that these combinations are observed in healthy NIH 1000 genomes samples (where there are only two compound heterozygotes for these polymorphisms out of 2504 healthy individuals sequenced), or at 10–12 times the frequency when only European CRMO patients and two separate healthy European control populations were compared (Table 3).
In contrast to apoptosis, necroptosis is widely considered to be an inflammatory form of cell death. However, definitive evidence for this proposition has yet to emerge. Because MLKL is activated by inflammatory stimuli such as TNF it is very difficult to separate cause from effect. The serendipitous identification of an auto-activating mutant of MLKL (MlklD139V) in mice has allowed us to explore the consequences of inappropriate necroptosis in the absence of such confounding factors. Furthermore, it has led to significant insights into the critical adult hematopoietic and perinatal developmental processes that are most sensitive to excessive MLKL activation, and into physiological mechanisms that have evolved to neutralize activated MLKL.
In the absence of a robust immunohistochemical marker for RIPK3-independent necroptosis, it is not possible to pinpoint exactly which cell type/s undergo necroptosis in MlklD139V mice. Nevertheless, the presence of high levels of circulating pro-inflammatory cytokines in MlklD139V/D139V pups at E19.5 relative to MlklWt/Wt and MlklWt/D139V littermates suggests that necroptosis and ensuing inflammation begins in the sterile in utero environment. This is not enough to overtly retard prenatal development or affect hematopoietic cell populations. However, upon birth and/or exposure to the outside environment the capacity of homozygous MlklD139V/D139V pups to suppress MLKLD139V activity is overwhelmed and they die within days of birth. This is clearly a dose-dependent effect because both MlklD139V/Wt and MlklD139V/null heterozygous mice are viable. Postnatal death cannot be prevented by combined deficiencies in Ripk3 and Casp8 nor by deficiency of other important inflammatory genes including Tnfr1, Myd88 or Ifnar. In light of the elevated levels of circulating G-CSF, IL-6 and IL-5 observed, the role of these key mediators in the initiation or potentiation of pre- and perinatal inflammation in MlklD139V/D139V pups will be the subject of future investigations.
The MlklD139V mutation was initially identified for its capacity to moderately increase platelet production independent of the thrombopoietin receptor Mpl. While the mechanism underlying this observation remains unclear, it follows observations by others that another member of the necroptotic pathway, RIPK3, plays a role in platelet activation58. The reduced platelet levels observed in MlklD139V/D139V pups is unlikely to be the sole cause of death given much more severe thrombocytopenia is not lethal in Mpl−/− mice40. Difficulty with suckling due to inflammatory infiltration of the head and neck and resulting failure to thrive is one possible explanation for the lethality in MlklD139V/D139V pups. However, the narrow window of mortality for these pups and marked pericardial immune infiltration make heart failure another potential cause of sudden neonatal death.
The MlklD139V mouse reveals that maintaining MLKL levels below a threshold can prevent necroptotic activation. This strain is a potential tool for the mechanistic and physiological examination of MLKL-mediated extracellular vesicle generation or other cell death-independent roles related to inflammation that is unconfounded by RIPK3 activation. While others have recently shown that an ESCRT dependent repair or extracellular vesicle extrusion can help protect membranes from limited MLKL damage14,15,16, and that p-MLKL can be internalized and degraded by the lysosome17 our data also suggest a role for the proteasome in the disposal of activated MLKL, be it directly, or in its capacity to generate free ubiquitin. This creates the possibility that these mechanisms or the previously described ESCRT mechanisms intersect in some way. Finally, the ability of these mechanisms to hold single gene-dose levels of active MLKL in check without deleterious consequences in vivo supports the idea that direct inhibition of activated MLKL may be an effective means to therapeutically prevent unwanted necroptotic cell death. Similarly, the MlklD139V mouse and assorted relevant crosses may prove to be a useful tool for the further examination of whether ROS production is co-incident with-, causative of- or consequential to- necroptotic plasma membrane disruption in varied tissue types and under highly physiologically relevant contexts (recently reviewed by59).
While any mouse MLKL-human MLKL comparisons must be made cautiously in light of the species-specific structural and mechanistic differences5,12,13, it is notable that out of over 140,000 individuals surveyed, there is only one recorded case of a human carrying a substitution equivalent to the mMlklD139V mouse (hMLKLD140V; rs747627247) in the gnomAD database, and this individual is heterozygous for this variant. To our surprise, 3,841 individuals in gnomAD (55 of which are homozygotes) carry a very closely situated MLKL brace region variant –MLKLS132P. Our CRISPR-generated MlklS131P mouse equivalent supports the connection between constitutive MLKL activation and decreased MLKL protein stability. Preliminary observations show that this variant manifests in a much milder and context specific phenotype in mice than mMlklD139V, which is consistent with its high frequency presence in the human population.
Overlaid with structural, biochemical, cell and animal-based evidence of function, it is tempting to speculate that these human MLKL brace region variants lead to altered MLKL function and/or regulation in what is most likely a highly tissue-, context- or even pathogen specific way60,61,62. While increased numbers and examination of independent cohorts will be required to confirm the statistical enrichment of human MLKL brace variants occurring in trans in the autoinflammatory disease CRMO, this patient cohort offers a tantalizing clue into their potential as modifiers of complex, polygenic inflammatory disease in present day humans.
All mice were backcrossed to C57BL/6 mice for >10 generations or generated on a C57BL/6J background. Mlkl−/−, Tnfr1−/−, Myd88−/−, IFNAR1−/−, Ripk3−/−, Casp8−/−, and Casp1/Casp11−/− mice were generated as described4,45,46,63,64,65,66,67. Mice designated as E19.5 were obtained by Caesarean section from mothers that received progesterone injections at E17.5 and E18.5. Independent mouse strains that carry the D139V or S131P mutation in the Mlkl gene (MLKLD139V CRISPR) were generated using CRISPR/Cas9 as previously described68. For D139V, one sgRNA of the sequence GGAAGATCGACAGGATGCAG (10 ng per μL), an oligo donor of the sequence ATTGGAATACCGTTTCAGATGTCAGCCAGCCAGCATCCTGGCAGCAGGAAGATCGACAGGTTGCAGAAGAAGACGGgtgagtctcccaaagactgggaaagagtaggccagggttgggggtagggtgg (10 ng per μL) and Cas9 mRNA (5 ng per μL) were injected into the cytosol of C57BL/6J zygotes. Mice were sequenced across the mutated region to confirm incorporation of the altered codon and analysis was performed after at least 2 back-crosses to C57BL/6. The same procedure was followed for the generation of MLKLS131P CRISPR mice, using sgRNA (CTGTCGATCTTCCTGCTGCC) and oligo donor (CTGTTGCTGCTGCTTCAGGTTTATCATTGGAATACCGTTTCAGATGTCAGCCAGCCAGCACCATGGCAGCAGGAAGATCGACAGGATGCAGAGGAAGACGGgtgagtctcccaaagactggga). Sex was not recorded for mice that were sampled at E19.5, P2 and P3. Experiments using adult mice were performed with a combination of both males and females between 8 and 12 weeks of age. Mice were housed in a temperature and humidity controlled specific pathogen free facility with a 12 h:12 h day night cycle. The WEHI Animal Ethics Committee approved all experiments in accordance with the NHMRC Australian code for the care and use of animals for scientific purposes.
We mapped the chromosomal location of the Plt15 mutation by mating affected mice to 129/Sv Mpl−/− mice to produce N2 (backcross) and F2 (intercross) generations. A genome-wide scan using 20 N2 mice with the highest platelet counts (287 ± 74 × 106 per mL, compared with 133 ± 75 × 106 per mL for the overall population, Fig. 1a) localized the mutation to a region of chromosome 8 between D8Mit242 and D8Mit139 and linkage to this region was then refined. Analysis of the F2 population revealed a significant reduction in the frequency of mice homozygous for C57BL/6 alleles in this interval (e.g., D8Mit200 3/81 F2 mice homozygous C57BL/6, p = 2.2 × 10−5 χ2-test), suggesting the Plt15 mutation results in recessive lethality. The refined 2.01 Mb interval contained 31 annotated genes, only five of which appeared to be expressed both in the hematopoietic system and during embryogenesis (http://biogps.gnf.org/): Dead box proteins 19a and 19b (Ddx19a and Ddx19b), Ring finger and WD repeat domain 3 (Rfwd3), Mixed lineage kinase domain like (Mlkl), and WD40 repeat domain 59 (Wdr59). Sequencing identified a single mutation, an A to T transversion in Mlkl that was heterozygous in all mice with an elevated platelet count.
Antibodies; Rat-anti mRIPK3 and rat anti-mMLKL 8F6 (selected for affinity to residues 1–30 of mouse MLKL) and rat anti-MLKL 3H14 (MLKL brace region) were produced in-house. Anti-Pro Caspase 8 (#4927) and GAPDH (#2113) were purchased from Cell Signaling Technology. Anti-mouse MLKL pS345 (ab196436) and anti-Actin (ab5694) were purchased from Abcam. Anti-VDAC (AB10527) was purchased from Millipore. Fc-hTNF was produced in house and used at a final concentration of 100 ng per mL. Recombinant mouse IFN-γ and β were purchased from R&D Systems (Minneapolis, MN, USA) Q-VD-OPh and zVAD-fmk were purchased from MP Biomedicals (Seven Hills, NSW, Australia). Smac mimetic also known as Compound A, and the caspase inhibitor IDN-6556 were a gift from TetraLogic (Malvern, PA, USA). Propidium iodide, doxycycline, and bafilomycin were purchased from Sigma-Aldrich (Castle Hill, NSW, Australia).
Cell line generation and culture
Primary mouse dermal fibroblasts were prepared from skin taken from the head and body of E19.5 pups delivered by C-section or from the tails of adult mice69. Primary MDFs were immortalized by stable lentiviral transduction with SV40 large T antigen. Immortalized MDFs were stably transduced with exogenous mouse MLKL cloned into the pFTRE 3 G vector, which was generated by Toru Okamoto, and allows doxycycline- inducible expression as described4. The following oligonucleotides were used for the assembly of constructs;
mMlkl fwd; 5′-CGCGGATCCGCGCCACCatggataaattgggacagatcatcaag-3′,
mMlkl rev; 5′-CGGAATTCttacaccttcttgtccgtggattc-3′,
N-FLAG mMlkl fwd; 5′-CGCGGATCCAA gccacc atg gcg cgc cag gac-3′
N-FLAG mMlkl rev; 5′-CGCGGATCC tta cac ctt ctt gtc cgt gga ttc-3′
mMlkl D139V fwd; 5′-gaagatcgacaggTtgcagaggaagac-3′
mMlkl D139V rev; 5′-gtcttcctctgcaAcctgtcgatcttc-3′
mMlkl S131P fwd; 5′-gccagcctgcaCcctggcagcag-3′
mMlkl S131P rev; 5′-ctgctgccaggGtgcaggctggc-3′
Cells were maintained in culture as previously described44. 4-hydroxy-tamoxifen regulated HOXA9 immortalised Factor Dependent Myeloid cells were generated from mouse E14.5 fetal liver cells and cultured as described previously70.
Cell death assays
Flow Cytometry based cell death assays were performed using 5 × 104 MDFs per well in 24 or 48-well tissue culture plates4. Doxycycline (20 ng per mL) was added together with death stimuli. Fc-hTNF was produced in house and used at 100 ng per mL, Compound A Smac mimetic and IDN6556 were used at 500 nM and 5 μM respectively. zVAD-fmk and QVD-OPh were used at 25 and 10 μM respectively. Mouse and human interferons γ and β were used at 30 ng per mL, PS341 and MG132 at 2 and 200 nM respectively and Bafilomycin at 300 nM. For Incucyte automated imaging, MDFs were plated at a density of 8 × 103 cells per well of a 96-well plate and permitted to attach for 3 h. FDMs were plated at a density of 5 and 10 × 103 cells per well of a 48-well plate. 0.2 μg per mL propidium iodide was in media alongside stimuli as indicated. Images were recorded at intervals of 1 and 2 h using an IncuCyte S3 and numbers of PI positive cells per mm2 at each time point quantified and plotted using IncuCyte S3 software.
MLKL turn-over assays
5 × 104 MDFs per well were plated in 24-well tissue culture plates and allowed to settle. Doxycycline (20 ng per mL) +/− TNF, Smac Mimetic and IDN6556 was added. After 15 h, ‘no dox’ and ‘0’ wells were harvested. Media was removed from remaining wells and cells were washed with PBS and fresh media containing IDN6556 was re-added. Wells were then harvested 2, 4, 6, 8, and 24 h from this point. Cells were harvested by direct lysis in reducing SDS-PAGE loading buffer.
MLKL protection assays
5 × 104 MDFs per well were plated in 24-well tissue culture plates and allowed to settle. Doxycycline (20 ng per mL) was added. After 18 hrs, ‘no dox’ and ‘T0’ samples were harvested. Media was removed and cells washed before addition of fresh media containing TSI or IDN alone for 3 h. Cells were washed again and media restored with IDN6556 alone (UT), or IDN6556 + inhibitor (MG132 (200 nM), PS341 (10–40 nM), Chloroquine (50 μM), Bafilomycin (300 nM), Ca-074 Me (20 μM), TLCK (100 μM) and AEBSF (100 μM)) for a further 21 h. Cells were harvested by direct lysis in reducing SDS-PAGE loading buffer.
UBA pull downs
2 × 106 MDFs stably transduced with doxycycline inducible N-FLAG-mMLKLWT or N-FLAG-mMLKLD139V expressing constructs were seeded and settled O/N before stimulation with 1 μg per mL doxycycline +/− TSI for 5 hrs. Cells were lysed in Urea-based UBA-pull down buffer, ubiquitylated proteins enriched and Usp21-treated as described previously71.
Transmission electron microscopy
Murine dermal fibroblasts prepared from mice of the indicated genotypes were untreated or stimulated with the indicated agents for the indicated hours. Then, cells were fixed with 2% glutaraldehyde in 0.1 M phosphate buffer, pH 7.4, postfixed with 2% OsO4, dehydrated in ethanol, and embedded in Epok 812 (Okenshoji Co.). Ultrathin sections were cut with an ultramicrotome (ultracut N or UC6: Leica), stained with uranyl acetate and lead citrate, and examined with a JEOL JEM-1400 electron microscope. The viability of a portion of these cells was determined by measuring LDH release as described previously72.
Caesarian-sectioned E19.5 and Day P2/3 pups were euthanized by decapitation and fixed in 10% buffered formalin. Five-micrometers coronal sections were taken at 200-μm intervals for the full thickness of the head, 5-μm sagittal sections were taken at 300-μm intervals for the full thickness of the body. A thorough examination of these sections was performed by histopathologists Aira Nuguid and Tina Cardamome at the Australian Phenomics Network, Melbourne. Findings were confirmed by Veterinary Pathologist Prof. John W. Finney, SA Pathology, Adelaide and clinical Pathologist Prof. Catriona McLean, Alfred Hospital, Melbourne.
Measurement of relative thymic cortical thickness
Representative images of thymus sections were analysed to determine relative cortical thickness using ImageJ. Briefly, medullary areas were identified on the basis of H and E staining and removed from the larger thymus structure using the Image J Image Calculator function to isolate the cortical region. The thickness of the cortical region, defined by the radius of the largest disk that can fit at a pixel position, was determined using the Local Thickness plugin in ImageJ (http://www.optinav.info/Local_Thickness.htm).
Following terminal blood collection, P0 and P3 pups were fixed for at least 24 h in 10% buffered formalin and paraffin embedded before microtomy. Immunohistochemical detection of cleaved caspase 3 (Cell Signaling Technology #9661) and CD45 (BD) was performed as described previously23.
All plasma was stored at −80 °C prior to cytokine analyses. Cytokines were measured by Bioplex Pro mouse cytokine 23-plex assay (Bio- Rad #M60009RDPD) according to manufacturer’s instructions. When samples were designated ‘<OOR’ (below reference range) for a particular cytokine, they were assigned the lowest value recorded for that cohort (as opposed to complete exclusion or inclusion as ‘zero’ which would artificially inflate or conflate group averages respectively). Values are plotted as fold change relative to the mean value for the Wt/Wt samples, and p values were calculated in Microsoft Excel using a two-tailed TTEST, assuming unequal variance. Data is only shown for cytokines that displayed statistically significant differences between genotypes at either of or both day E19.5 and day P3.
Blood was collected from P0 and P3 pups into EDTA coated tubes using heparinized glass capillary tubes from the neck cavity immediately after decapitation. After centrifugation at 500 G for 5 min, 5–15 μL of plasma was carefully removed and this volume was replaced with PBS. Blood cells were resuspended and diluted between 8–20-fold in DPBS for automated blood cell quantification using an ADVIA 2120 hematological analyzer within 6 h of harvest. Blood was collected from adult mice retro-orbitally into tubes containing EDTA and analyzed using an ADVIA120 automated hematological analyzer (Bayer).
Donor bone marrow or fetal liver cells were injected intravenously into recipient C57BL/6-CD45Ly5.1/Ly5.2 mice following 11 Gy of gamma-irradiation split over two equal doses. Recipient mice received neomycin (2 mg per mL) in the drinking water for 4 weeks. Long term capacity of stem cells was assessed by flow cytometric analysis of donor contribution to recipient mouse peripheral blood and/or hematological organs up to 6 months following engraftment. Recovery from cytotoxic insult was assessed by automated peripheral blood analysis at regular times following treatment of mice with 150 mg per kg 5-fluorouracil (5-FU).
To analyze the contribution of donor and competitor cells in transplanted recipients, blood cells were incubated with a combination of the following antibodies: Ly5.1-PE, Ly5.2-FITC, Ly5.2-biotin or Ly5.2 PerCPCy5.5 (antibodies from Becton Dickenson, Ca). If necessary, cells were incubated with a streptavidin PECy5.5 (BD), mixed with propidium iodide (Sigma) and analysed on a LSRI (BD Biosciences) flow cytometer. To analyse the stem- and progenitor cell compartment, bone marrow cells were incubated with biotinylated or Alexa700 conjugated antibodies against the lineage markers CD2, CD3, CD4, CD8, CD34, B220, CD19, Gr-1, and Ter-119. For stem and progenitor cell detection antibodies against cKit, Sca-1, CD48, AnnexinV, CD105, FcγRII/III or CD135 in different combinations (see antibody list for details). Finally FluoroGold (AAT Bioquest Cat#17514) was added for dead cell detection. Cells were then analysed on LSRII or Fortessa1 (BD Biosciences) flow cytometers.
Reactive oxygen species (ROS) detection
ROS was detected by using Chloromethyl-H2DCFDA dye according to the manufacturer’s instructions (Invitrogen Cat#C6827). In brief, bone marrow cells were loaded with 1 μM Chloromethyl-H2DCFDA for 30 min at 37 °C. Loading buffer was then removed, and cells were placed into 37 °C StemPro-34 serum free medium (ThermoFisher Cat#10639011) for a 15-min chase period. After incubation cells were placed on ice and stained with surface antibodies suitable for FACS analysis. Cells were analysed using a LSRII flow cytometer (Becton Dickinson).
E14.5 fetal liver colony forming assays
1 × 104 fetal liver cells were plated as 1 mL cultures in 35 mm Petri dishes in DMEM containing 10% FCS, 0.3% agar and 104 U per mL GM-CSF. IFN-β was added to the cultures in increasing concentrations from 0 to 30 ng per mL. Colony formation was scored after 7 days of incubation at 37 °C, fully humidified with 10% CO2.
RNA was prepared using Trizol (Invitrogen) according to the manufacturer’s instructions and 10 μg was used for first strand cDNA synthesis using SuperScript II (Life Technologies). 0.5 μg of cDNA was then used in a TaqMan PCR reaction with Universal PCR mastermix and murine Mlkl (Mm1244222_n1) and GAPDH (Mm99999915_m1) Taqman probes (ThermoFisher) on an ABI 7900 Fast Real-Time PCR instrument (Applied Biosystems). Mlkl expression relative to GAPDH control was determined using SDS version 2.3 program (Applied Biosystems) and expressed as ΔCT values.
Statistics (mouse and cell-based assays)
Please consult figure legends for description of error bars used. All data points signify independent experimental repeats, and/or biologically independent repeats. All p values were calculated in Microsoft Excel or Prism using an unpaired, two-tailed t-test, assuming unequal variance and not adjusted for multiple comparison. Asterices signify that p ≤ 0.05 (*), p ≤ 0.01(**) or p ≤ 0.005 (***). All comparisons were made between MlkWt/Wt and MlkD139V/D139V groups only (with the exception of data derived from adult mice, which were comparisons between MlkWt/Wt and MlkWt/D139V groups only.
DNA from CRMO probands and their family members (when available) was purified from saliva or blood and prepared for whole-exome sequencing (WES). The samples underwent WES at several different times, enriched using the Agilent SureSelect Human All Exon V4, V5 or V6 + UTR (Agilent Technologies) before sequencing at either Otogenetics, Inc (Atlanta, GA), Beckman Coulter Genomics (Danvers, MA), or at the University of Iowa Genomics Core (Iowa City, IA). The fastq files were quality-checked and processed to vcf format as described73. Variants for all samples were called together using GATK’s Haplotype Caller74 and were recalibrated and hard-filtered in GATK as described73. Variants were annotated with minor allele frequencies (MAFs) from 1000 genomes75, ExAC and gnomAD48 and with information regarding the effect of each variant using SNPSift/SNPEff76. The databases used for annotation were dbNSFP2.977 (for MAFs) and GRCh37.75 for protein effect prediction.
Ancestry was determined for each CRMO proband using the LASER software package78. A vcf file including ten probands at a time was uploaded to the LASER server and the TRACE analysis was selected using the Worldwide panel. For probands with indeterminate ancestry using the Worldwide panel, the European and Asian panels were used. Principal component values for each proband were plotted using R Statistical Software and the code provided in the LASER package.
MLKL variant quantification
1000 Genomes: Vcf files from 1000 genomes were annotated and filtered as described previously79. Values for MLKL variants rs35589326 (S132P), rs34515646 (R146Q), and rs144526386 (G202V) as well as all MLKL coding variants were queried and tabulated for allele and genotype count for participants of all ancestry (n = 2504), and for those of European ancestry (n = 503). Compound heterozygous variants were evident due to the phasing of all variants in the 1000 genomes dataset. CRMO: Allele and genotype counts for all MLKL coding variants were tabulated in probands of European ancestry (n = 101) and for all probands (n = 128). Compound heterozygous variants were identified using parental sequence data. AS: DNA from all subjects in AS cohort were genotyped using the Illumina CoreExome chip following standard protocols at the Australian Translational Genomics Centre, Princess Alexandra Hospital, Brisbane. Bead intensity data was processed and normalized for each sample and genotypes called using the Illumina Genome Studio software. All the samples listed in the table have passed quality control process80. GB: Genotyping was performed in an ISO15189-accredited clinical genomics facility, Australian Translational Genomics Centre (ATGC), Queensland University of Technology. All samples were genotyped by Illumina HumanOmniExpress (OmniExpress) BeadChip81. QUT controls: A collection of healthy control data of verified European ancestry from various cohort studies, complied by the Translational Genomics Group, QUT and typed on an Illumina CoreExome microarray. Includes data from The UK Household Longitudinal Study, led by the Institute for Social and Economic Research at the University of Essex and funded by the Economic and Social Research Council. The survey was conducted by NatCen and the genome-wide scan data were analysed and deposited by the Wellcome Trust Sanger Institute. University of Essex. Institute for Social and Economic Research, N. S. R., Kantar Public. Understanding Society: Waves 1–8, 2009–2017 and Harmonised BHPS: Waves 1–18, 1991–2009. [data collection]. 11th Edition. UK Data Service., (2018).
All genomic data was derived from patients recruited with consent as described previously48,80,81, and with the approval of human ethics review boards of all Institutes that participated in human genetics studies; University of Iowa Carver College of Medicine, Queensland University of Technology, Australian National University, Shanghai Renji Hospital, JiaoTong University of Shanghai, The Hospital for Sick Children and the University of Toronto, University of Sydney, Australian Institute of Sport, University of Freiburg, Princess Alexandra Hospital, Memorial Hermann Texas Medical Centre, The University of Queensland, Oregon Health and Science University), Groupe Française d’Etude Génétique des Spondylarthrites (GFEGS) and the University of Oxford.
Statistical analysis (human data)
Statistical comparisons were performed at the level of allele frequency or the level of compound heterozygote sample frequency using either a Fisher’s exact test or a Chi-Squared test with Yates correction as specified under each table. Compound heterozygous variants were quantified and compared at the individual rather than the allelic level, where individuals with and without qualifying variants were compared at the allelic level.
gnomAD – https://gnomad.broadinstitute.org/
OrthoDB - https://www.orthodb.org
Clustal Omega - https://www.ebi.ac.uk/Tools/msa/clustalo/
WEBLOGO - https://weblogo.berkeley.edu/logo.cgi
Missense Tolerance Ratio (MTR) Gene Viewer - http://biosig.unimelb.edu.au/mtr-viewer
UK biobank - https://www.ukbiobank.ac.uk
Understanding Society - https://www.understandingsociety.ac.uk/
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
The biological tools generated for MLKL during this study are available from the corresponding authors on reasonable request. MLKL gene variants in CRMO can be accessed from Harvard Dataverse, V1 [https://doi.org/10.7910/DVN/BL3SXQ]. The source data underlying Figs. 1a, d, e–g, 2a–f, 3a–k, 4a–f, 5c, d and Supplementary Figs. 1a, b, 2a–h, 3a, c, d–f, 4b, d–j are provided as a Source Data file. Source data are provided with this paper.
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We thank all the following people for their technical assistance; Jiami Han, Cynthia Liu, Jasmine McManus, Janelle Lochland and Emma Tovey (WEHI), Aira Nuguid and Tina Cardamone (APN histopathology – The University of Melbourne). Thomas Boudier (WEHI Centre for Dynamic Imaging). The WEHI Histology Service, WEHI Antibody Facility and WEHI Bioservices. Y. Uchiyama and S. Kakuta who advised the interpretation of the results of TEM and Annette Jacobsen (WEHI) for important insight and discussion. The generation of MlklD139V mice by CRISPR/Cas9 was performed by Andrew Kueh and Marco Herold (WEHI MAGEC laboratory) supported by the Australian Phenomics Network (APN) and the Australian Government through the National Collaborative Research Infrastructure Strategy (NCRIS) program. This work is supported by; Project grant (1105023) and Fellowships (0541951 and 1142669) from the Australian National Health and Medical Research Council (NHMRC) to J.M.H.; Fellowship (1107149) from the NHMRC to J.S.; Program grant (1113577) and Fellowship (1058344) from the NHMRC (W.S.A.); Project grant (1124735) and Fellowships (1105754, 1172929) from the NHMRC (J.M.M.); NIH training grants T32GM008629 and T32GM082729-01 (A.J.C.); R01AR059703 from the National Institute of Arthritis and Musculoskeletal and Skin Diseases (NIAMS) at the National Institutes of Health (P.J.F. and A.G.B.); the Marjorie K. Lamb Professorship (P.J.F.); Grants-in-Aid from Scientific Research (B) 17H04069 from Japan Society for the Promotion of Science, and Scientific Research on Innovative areas 26110003, the Japan Agency for Medical Research and Development (AMED) through AMED-CREST JP20gm1210002 and Private University Research Branding project from a MEXT (H.N.); Victorian International Research Scholarship (Z.L. and M.C.T.). Australia Postgraduate Award (C.A.D.); S.L.M. acknowledges funding from NHMRC grants (1144282, 1142354, and 1099262), The Sylvia and Charles Viertel Foundation, HHMI-Wellcome International Research Scholarship and Glaxosmithkline; Fellowship from the Lorenzo and Pamela Galli Charitable Trust (E.C.J.), NHMRC grants 1107425 and 1045549 and The Sylvia & Charles Viertel Senior Medical Research Fellowship (M.P.); D.B.A. was supported by the Jack Brockhoff Foundation (JBF 4186, 2016) and NHMRC Fellowship (APP1072476); NHMRC IRIISS 9000587 and Victorian Government Operational Infrastructure Support schemes; NHMRC Project and Targeted Research grants 1006769, 512672, and 512381 (M.F.S.); The Department of Industry, Innovation, Science, Research and Tertiary Education Collaborative Research Network and Diabetes Australia (MAB); I.J.M. was supported by the Victorian Cancer Agency, and by generous support from the Felton Bequest; Cancer Australia and Leukemia Foundation Australia priority grant (PdCCRS 1162023) and a Victoria Cancer Agency (VCA) mid-career fellowship (MCRF 15027) to G.B. We gratefully acknowledge the contribution of genotype data by Dr Yorgi Mavros (University of Sydney), Professor Nick Martin (QIMR), Professor Jim Rosenbaum (Oregon Health and Science University), and Professor Maxime Breban and the Groupe Française d’Etude Génétique des Spondylarthrites (GFEGS). We are grateful to Professor BP Wordsworth of the University of Oxford, UK for access to genotype data on ankylosing spondylitis cases collected in studies funded, in part, by Arthritis Research UK (grants 19536 and 18797), by the Wellcome Trust (grant 076113) and by the Oxford Comprehensive Biomedical Research Centre ankylosing spondylitis chronic disease cohort (theme A91202).
J.M.H., S.N.Y., P.E.C., J.M.M., and J.S. contribute to a project developing necroptosis inhibitors in collaboration with Anaxis Pty Ltd. The remaining authors declare no competing interests.
Peer review information Nature Communications thanks Shigekazu Nagata, Andreas Villunger and other, anonymous, reviewers for their contributions to the peer review of this work.
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Hildebrand, J.M., Kauppi, M., Majewski, I.J. et al. A missense mutation in the MLKL brace region promotes lethal neonatal inflammation and hematopoietic dysfunction. Nat Commun 11, 3150 (2020). https://doi.org/10.1038/s41467-020-16819-z
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