Genetic mutations account for many devastating early onset immune deficiencies. In contrast, less severe and later onset immune diseases, including in patients with no prior family history, remain poorly understood. Whole exome sequencing in two cohorts of such patients identified a novel heterozygous de novo IKBKB missense mutation (c.607G>A) in two separate kindreds in whom probands presented with immune dysregulation, combined T and B cell deficiency, inflammation, and epithelial defects. IKBKB encodes IKK2, which activates NF-κB signaling. IKK2V203I results in enhanced NF-κB signaling, as well as T and B cell functional defects. IKK2V203 is a highly conserved residue, and to prove causation, we generated an accurate mouse model by introducing the precise orthologous codon change in Ikbkb using CRISPR/Cas9. Mice and humans carrying this missense mutation exhibit remarkably similar cellular and biochemical phenotypes. Accurate mouse models engineered by CRISPR/Cas9 can help characterize novel syndromes arising from de novo germline mutations and yield insight into pathogenesis.
More than 300 single-gene defects that result in immunological disease have been described so far (Picard et al., 2018). Elucidation of Mendelian immune diseases is important for the families affected and, in some cases, provides insights into disease mechanisms that are of broader therapeutic significance for autoimmunity and lymphoproliferative disease (Woyach et al., 2012). Among the known causes are many homozygous and biallelic loss-of-function alleles that result in devastating early onset immunological disease. In addition, there is an emerging catalog of single-gene defects that result in much less severe phenotypes, and some of these syndromes share significant similarities with diseases assumed to be the result of polygenic variation.
Mutations that result in defective NF-κB signaling and transcription are exemplary. NF-κB is a family of transcription factors that regulate gene expression in many tissues and exert important and well-characterized actions on lymphocyte ontogeny, homeostasis, activation, and maintenance of self-tolerance (Zhang et al., 2017). In the resting state, NF-κB molecules are retained in latent form in the cytoplasm by molecules of the IκB family (Baeuerle and Baltimore, 1988). After receptor ligation, signals converge on a complex comprising IKK1, IKK2, and NEMO (encoded by IKBKA, IKBKB, and IKBKG, respectively), which phosphorylates IκBα, targeting it for partial degradation in the proteasome, which liberates NF-κB molecules p65 (RelA), c-Rel, and p50 (Fan and Maniatis, 1991; Salmerón et al., 2001; Häcker and Karin, 2006; Scheidereit, 2006) to the nucleus as transcription factors (Plaksin et al., 1993; Weih et al., 1995; Bohuslav et al., 1998; Hayden and Ghosh, 2004). Many germline NF-κB defects have been identified as causes of immunological disease. In some cases, for example, CARD11, biallelic mutations cause early onset disease, while heterozygous variants cause different phenotypes (Snow et al., 2012; Stepensky et al., 2013). Interestingly, somatic mutations in many of the same NF-κB genes have also been implicated in lymphoproliferative disease (Staudt, 2010).
Now that there is empirical evidence that single-gene variants can cause complex immune phenotypes, it is important that we explore rare and novel variants in cases where disease remains unexplained. De novo mutations are an important cause of severe sporadic disease with immunological and other phenotypes (Vissers et al., 2010; Conley and Casanova, 2014; Flanagan et al., 2014), although in such cases, opportunities for proving causation by segregation analysis are usually limited. In addition, the catalog of variants of unknown significance is large. In both cases, methods for determining function of precise human mutations that might account for a novel syndrome is a high priority. Here, we report how combined phenotyping of patients carrying a de novo gain-of-function mutation in IKBKB, and a mouse engineered to carry the orthologous variant, helped to describe a novel immune syndrome.
Results and discussion
We assembled a cohort of patients with noncongenital immune deficiency, manifesting as either primary antibody deficiency, unexplained T cell deficiency, or various combined defects. From within this cohort we identified a patient who presented with recurrent respiratory tract infections, severe and atypical eczema, dental abnormalities consistent with ectodermal dysplasia (without conical teeth), hidradenitis suppurativa and subcutaneous abscesses, mucocutaneous candidiasis, and premature cataracts. Both parents were alive with no evidence of immune deficiency or dysregulation. The proband had two children (aged 2 and 5 yr), and both suffered with recurrent otitis media and sinusitis, but no inflammation or ectodermal dysplasia. Initial cellular analysis of peripheral blood mononuclear cells (PMBCs) isolated from the proband and both children revealed lymphopenias. One child, from whom blood was available for analysis, and the proband both exhibited T deficiency, and the other exhibited a reduction in total lymphocytes for age. Lymphopenia was a fixed phenotype in the proband, with no significant change over at least 7 yr of observation (Table S1). In addition, she had mild hypogammaglobulinemia and defective specific antibody responses to pneumococcal vaccination.
Whole exome sequencing and analysis of kindred A using methods described previously (Field et al., 2015) identified a novel heterozygous missense mutation in IKBKB (c.607G>A, cDNA.793G>A, g.37639G>A) encoding a valine to isoleucine (V203>I) amino acid substitution (Fig. 1, a and b). No other rare or novel mutations were identified in genes encoding NF-κB proteins. The IKBKB mutation was not found in either parent, and after excluding nonpaternity with high confidence, we concluded that the mutation had arisen de novo in the proband. An identical codon variation was discovered in a separate and geographically remote kindred (Fig. 1, a and b), involving a 33-yr-old male proband with a history of recurrent respiratory infections, otitis media, and tonsillitis since childhood. He was noted to have hypogammaglobulinemia at age 18 yr and subcutaneous abscesses at age 28 yr. Further investigations revealed bronchiectasis (Fig. 1 c) and hepatosplenomegaly (Table S1).
Valine 203 is conserved to at least Drosophila melanogaster (Fig. 1 d), is located within the active site of IKK2 (Fig. 1, e and f), on the second lobe of the kinase domain, which phosphorylates the N-terminal region of IκBα, and leads to activation of NF-κB (Liu et al., 2013). The mutant protein is predicted to assume an unstable conformation, while maintaining the kinase activity, but disrupting the tetrameric interaction of IKK2. The mutated residue is conserved in protein paralogs of IKK2 (Fig. S1 a). In silico analysis predicted the mutation to be damaging (SIFT, 1.0; Polyphen2, 0.99; Mutation Taster, >0.99). This germline mutation has not been reported before (GnomAD, ExAC, dbSNP), but two instances of the same mutation arising as a somatic variant in brain tumors have been reported (Fukumura et al., 2016). Consistent with our findings, this somatic variant was reported to confer gain of function. Thus, we report a novel syndrome of combined immune deficiency arising from germline gain-of-function IKBKB mutations.
Flow cytometric analysis showed that IKK2 protein was expressed at similar levels in patient and control lymphocytes (Fig. S1 b). We proceeded to analysis of the mutant allele. First, we cloned mutant and WT alleles and expressed them in HEK293 cells. After stimulation with TNF, we observed increased and prolonged IκBα phosphorylation, despite similar levels of WT and mutant allele IKK2 expression (Fig. 1 g). Similarly, we observed increased IκBα phosphorylation at baseline and after activation of PBMCs obtained from the proband (Fig. S1, c and d).
IKK2 activates the canonical NF-κB pathway. We examined the effect of the mutation by assessing abundance of phosphorylated p65 in fibroblasts, T and B cells at rest, and after activation (Fig. 1, h and i; and Fig. S2 a). As had been observed for the proximal event (phospho-IκBα), we observed increased phospho-p65, particularly in the T cell compartment, and an increase in abundance of phospho-p65 after activation out to 60 min (Fig. 1 h). Non-stimulated B cells from the patient showed increased phosphorylation of NF-κB to a level similar to that in CD40-stimulated control B cells (Fig. S2, b and c), with an enhanced response to PMA plus ionomycin and CD40 ligand plus IL-4 (Fig. S2, d and e).
We also assessed the transcriptional consequences of enhanced NF-κB activation. First, dendritic cells were induced in vitro from monocyte precursors. NF-κB2 is under transcriptional control by canonical NF-κB signaling, and while baseline expression was similar in patient and control, we observed an increase in patient cells after activation in vitro with TNF (Fig. S1, e and f). To demonstrate transcriptional regulation, we transfected fibroblasts isolated from patient and a healthy control with a construct containing NF-κB–dependent luciferase. We observed a modest increase in NF-κB–dependent transcription in the absence of stimulation and a significant increase relative to control after activation (Fig. 1 i). We performed a similar analysis after transient transfection of HEK293T cells with either WT, IKBKBV203I, IKBKBR272X (a known hypomorphic allele), or IKBKBK171E (a known gain-of-function allele; Fig. 1 j; Kataoka et al., 2015). Even in the absence of stimulation, IKBKBV203I resulted in enhanced luciferase activity compared to the WT allele, and this response was enhanced after TNF stimulation.
Probands in both kindreds exhibited deficiencies of CD4+ and CD8+ T cells, with a significant reduction in naive T cells in both compartments (Fig. 2, a and b; naive CD4+ T cells, A.II.2: 4.19%; B.II.2: 17.4%. Naive CD8+ T cells, A.II.2: 4.93%; B.II.2: 6.9%). Indeed, this deficiency was observed in both αβ and γδ T cells (data not shown). We also observed a significant increase in circulating follicular helper T cells (Tfh cells; Fig. 2, c and d). Consistent with an effector memory T cell (TEM)/TEM CD45RA+ cell (TEMRA) phenotype, patient CD8+ T cells showed increased expression of CD107a, a degranulation marker (Fig. S2 f).
The probands were also found to exhibit a significant deficiency of memory B cells (Freiburg class Ib), defined either as CD19+IgD−CD27+ (Fig. 2, e and f; and Table S1) or CD19+CD38loCD24hi lymphocytes (Fig. S2 g). Transitional B cells were numerically normal, but were universally CD21hiCD10+ (Fig. S2 h). Analysis of IgD+CD19+ B cells revealed a relatively low level of IgM expression, a phenotype often observed as a result of a reduced threshold of B cell receptor activation (Fig. S2 i). We observed a modest reduction in CD86 induction by both naive and memory B cells after activation with bacteria cytidine-phosphate-guanosine (CpG), while induction of CD25, CD83, and CD69 was normal (data not shown). B cells failed to proliferate normally and exhibited a defect in immunoglobulin production after CD40 or CpG stimulation (Fig. 2, g and h).
We purified naive and memory T cells and assessed their responses to activation in vitro. We observed similar proliferation responses by memory T cells (CD45RO+) from proband and controls (Fig. 3 a). In contrast, activation of naive CD4+ T cells from the proband responded with greater proliferation relative to those from unrelated healthy controls. Activation of naive cells was accompanied by increased expression of markers of activation CD25 and CD69 (Fig. 3, a and b). To confirm the enhanced proliferative response in cells from the proband, we stimulated cells with CD3 only (rather than CD2, CD3, and CD28), which normally induces only a small proportion of cells to enter cycle, and observed a substantial proliferative response in cells from the proband, but not in controls (Fig. 3 c). In these proliferation assays, although we observed an enhanced proliferative response, there were far fewer cells present in cultures at time of analysis, consistent with substantial cell death.
We also observed a significant increase in circulating regulatory T cells (T reg cells) in A.II.2, but not in B.II.2, defined as CD25+CD127− and FOXP3+, and effector T reg cells, defined as CD45RA−, FOXP3+CD25+, and CD127− (Fig. 3, d and e). Interestingly, we also observed an increase in FOXP3 expression per cell, which was evident within T reg cells and also in the otherwise low-level FOXP3 expression in CD4+ T cells considered to be conventional T cells by surface phenotype (Fig. 3, f and g).
IKK2V203 is highly conserved across species and in similar proteins (Fig. 1 d and Fig. S1 a), so to investigate the action of this novel germline mutation in vivo, and to confirm its causal action in immune dysregulation, we engineered a G-to-A transversion in codon 203 of mouse Ikbkb using CRISPR/Cas9 (Fig. 4 a). The mutant allele was propagated, and heterozygous and homozygous mice were born at expected Mendelian ratios.
Analysis of isolated splenocytes revealed constitutive IκBα phosphorylation, with evidence of a gene dose effect: phosphorylation was greater in cells with homozygous mutation compared with heterozygotes, both at baseline (Fig. 4 b) and for at least 120 min after stimulation (Fig. 4, c and d). This result, taken together with transfection results, and analysis of cells from the proband, confirms that the p.V2013>I mutation confers gain of function on IKK2. These findings are consistent with previous reported results for the same mutation identified as a somatic mutation in patients with central nervous system B cell lymphoma, where gain of function was demonstrated biochemically (Fukumura et al., 2016).
As characterized in the proband, we observed that mice heterozygous and homozygous for IkbkbV203I exhibited a relative deficiency of T cells (Fig. 4, e and f). T cells were reduced as a proportion of splenocytes. We also observed a reduction in absolute number of T cells within spleens of affected mice, and a reduction in absolute numbers of both CD4+ and CD8+ T cells (Fig. S3), consistent with the human phenotype. In mice, we observed greater reduction in CD8+ T cells (Fig. 4 g).
In humans, we observed specific deficiency of naive T cells. In mice, effector T cells are marked by expression of CD44 and absence of CD62L. This subset was increased in both CD4 and CD8 compartments, again with evidence of a gene dose effect (Fig. 4, h and i). We also observed a significant increase in T cell activation, indicated by up-regulation of CD69 in both CD4 and CD8 compartments (Fig. S3, c and d). This bias toward activation was a fixed phenotype, observed in both young and old mice (Fig. S3, e and f). The proband exhibited an increase in circulating T reg cells. In mutant mice, we found an increase in T reg cells defined either according to CD25+ surface phenotype or Foxp3 expression (Fig. 4, j and k). A similar increase in T reg cells was observed within thymus of mutant mice, suggesting that the defect arises during T reg cell development (Fig. 4 l).
We have identified a novel germline IKBKB allele in patients with a clinical phenotype of cellular abnormalities of lymphopenia combined with immune activation of both CD4+ and CD8+ T cells. In addition, one patient presented with inflammatory disease and possible ectodermal defect. High evolutionary conservation of the affected codon within IKBKB provided us with an opportunity to generate an accurate mouse model of this novel syndrome, which we generated using CRISPR/Cas9 so that they carry the same amino acid substitution in IKK2 identified in our patient. Phenotypic analysis revealed close phenotypic similarities between mouse and humans carrying the mutant protein, with phenotypes in heterozygotes intermediate between normal and homozygotes, providing strong support for the contention that the novel mutation is responsible for a novel syndrome of immune deficiency (Table 1).
In both human and mouse, we observed pathological immune activation, but this finding needs to be reconciled with clinical manifestation of mild immune deficiency. One possible explanation is the increase in thymic T reg cells, observed in the mouse model, and increased FOXP3 expression in the proband. FOXP3 expression is known to be regulated by canonical NF-κB signaling (Isomura et al., 2009; Long et al., 2009). Furthermore, in loss-of-function defects of canonical NF-κB signaling, concurrent defects in both conventional T cells and T reg cells have been observed, which result in at least partial maintenance of homeostasis because deficiencies of T reg cells are offset by defects in conventional T cell activation conferred by the same mutation (Altin et al., 2011). Patient B.II.1, however, had a late-onset combined immunodeficiency alone and presented with normal T reg cells.
Now that de novo mutations have emerged as important causes of sporadic disease, it is necessary to have methods to confirm causation of novel variants. Our results reveal that even when novel mutations are isolated to a single individual as a result of a de novo mutation, confirmation of function can be confirmed by engineering an orthologous mutation to generate a precise model. This is particularly feasible for immunological diseases, because immunity is highly conserved between mouse and human. In the future, this strategy should prove important for investigating therapeutic interventions for personalized therapy.
Our discovery provides another example of a heterozygous missense mutation in an NF-κB pathway gene that presents with less catastrophic phenotypes than homozygous defects in the same genes. Indeed, given the complex circuits of negative and positive regulatory interactions within NF-κB signaling, cellular, biochemical, and clinical manifestations of specific defects are not always predictable, and complete gene deletions arising spontaneously from nonsense mediated decay or by homologous recombination in mice do not necessarily predict the actions of single–amino acid substitutions. Previously, rare homozygous mutations of IKBKB have been reported that result in absence of protein expression and confer severe early onset immune deficiency, in which the cellular phenotype was the opposite of that conferred by the hypermorphic allele reported here, with expansion of naive T cells, which were refractory to activation, and therefore, there was minimal differentiation of memory or effector T cells. These individuals also exhibit a deficiency of T reg cells (Pannicke et al., 2013; Mousallem et al., 2014). Despite the divergence of cellular phenotypes, we can now conclude that both loss-of-function and hypermorphic alleles of IKBKB confer immune deficiency. Similar effects of mutations conferring different biochemical functions have been observed with other genes (Minegishi et al., 2007; Boisson-Dupuis et al., 2012; Haapaniemi et al., 2015). Finally, the relatively mild nature of the phenotype in the patient described here also serves to emphasize that monogenic causes should be considered not only in patients with extreme phenotypes. The corollary is that by elucidating Mendelian versions of less severe phenotypes, we can start to gain insights into the mechanisms of common disease.
Materials and methods
Enrollments and approvals
The family described in this study is part of a larger cohort of primary antibody deficiency kindreds enrolled and recruited through the Australian and New Zealand Antibody Deficiency Allele Study. This study has been approved by human research ethics committees at Australian Capital Territory Health and Australian National University. A Japanese patient was identified from a cohort of Japanese primary immunodeficiency disease. This study was approved by the Ethics Committee of Tokyo Medical and Dental University. All subjects provided written informed consent to participate, in accordance with the Declaration of Helsinki. All animal experiments were approved from the Institutional Animal Ethics Committee of Australian National University in agreement with the code of practice from the National Health and Medical Research Council in Australia.
Flow cytometry and antibodies
The following antibodies were used for human cell analysis: CD19 (SJ25C1), CD27 (L128), CD38 (HB7), CD3 (HIT3A), CD4 (SK3), CD8 (SK1), CCR7 (3D12), CXCR5 (RF8B2), CD24 (ML5), CD69 (FN50), ΥδTCR, and αβTCR (from BD Biosciences); CD45RA (HI100), CD10 (H110a), CD21 (BU32), and CD45RO (UCHLI; from BioLegend); CD86 (from Miltenyi Biotec); anti-IgM (from Dako); anti-IgD (IAG-2), CD25 Foxp3 (2A3), and phospho-p65 (B33B4WP; from eBioscience); and FOXP3 (259D/C7; from BD Biosciences). The following antibodies were used for mouse flow cytometry analysis: B220 (RA3/6B2), FOXP3 (MF23), and CD127 (A7R34; from eBioscience); and CD3 (17A2), CD4 (RM4-5, GK1.5), CD8 (53/6.7), CD44 (IM7), CD62L (MEL-14), and CD25 (PC61; from BioLegend).
Human PBMCs were isolated by density gradient centrifugation on Ficoll-Paque PLUS (GE Healthcare), washed twice in PBS, and maintained in complete RPMI (Sigma-Aldrich) containing 10% FBS, 2 mM l-glutamine (Sigma-Aldrich), and 100 U/ml penicillin and streptomycin (Sigma-Aldrich). For mouse studies, spleens and thymuses were disrupted to generate single-cell suspensions in RPMI/FCS. For human primary fibroblasts, cells were suspended at a density of 5 × 105 cells/ml in DMEM with 10% FBS.
For surface staining, PBMCs, sorted cells, or mouse cell suspensions were washed with PBS containing 5% FBS (FACS buffer) and then incubated for 20 min at 4°C in dark in FACS buffer containing appropriate fluorochrome-labeled antibodies. Each antibody labeling experiment included an Fc-blocking step (anti-CD16/CD32). Intracellular staining was performed according to standard protocols. Cells were fixed (Fixing Buffer; Thermo Fisher Scientific) and then permeabilized with Perm Buffer III according to the manufacturer's instructions (BD Biosciences).
Naive and memory CD4+ or CD8+ T cells were bead sorted (Miltenyi Biotec), and enriched CD4+ or CD8+ cells or PBMCs were cultured with anti-CD3/CD28 expansion beads (Miltenyi Biotec) for 4 or 6 d. Proliferation of cells was then analyzed using Cell Trace Violet Cell Proliferation kit (Invitrogen) according to the manufacturer’s instructions.
For CFSE experiments, PBMCs were labeled with 3 µM CFSE (Thermo Fisher Scientific) for 5 min at room temperature. CFSE-labeled cells were plated at 0.5–1.0 × 106 cells/ml in triplicate (200 µl/well) in 96-well flat-bottom plates and left unstimulated or stimulated for 7 d with CD40L (1 µg/ml) and CpG (1 µg/ml) for B cell proliferation assay. After staining with fluorochrome-conjugated antibodies, CFSE dilution peaks of CD19+ B cells were analyzed by flow cytometry as a measure of cell division.
CD107a expression analysis
PBMCs were stimulated with staphylococcal enterotoxin B (1 µg/ml) or anti-CD3/CD28 beads in the presence of PE-anti-CD107a (BD Biosciences) and monensin (1 µg/ml) for 6 h and stained for CD8. Cells were analyzed using flow cytometry.
In vitro immunoglobulin production and secretion
PBMCs were stimulated with mitogens (IL-21, 10 ng/ml; CD40L, 2 µg/ml; CpG, 1 µg/ml), and cultured for 11 d. Immunoglobulin levels were evaluated by in-house ELISA assay.
Fibroblasts from a healthy control and the patient were transfected with 5 µg NF-κB–dependent firefly luciferase reporter plasmid (pNiFty-Luc) and 0.1 µg of Renilla Luciferase plasmid (pRLC). 20 h after transfection, a portion of the cells were stimulated with 5 ng/ml IL-1B for 4 h. Relative NF-κB activation was measured using Dual-Glo Luciferase Assay System (Promega) and Glomax plate reader (Promega), and it was calculated by normalizing the relative ratio of firefly to Renilla.
Also, the pFN21A expression vector containing WT or mutant IKBKB, together with Igkcona-Luc (provided by S. Yamaoka, Tokyo Medical and Dental University, Tokyo, Japan) and pRL-TK (Promega), were transfected into the HEK293T cells. At 24 h after transfection, the cells were treated with TNF-α (20 ng/ml) for 4 h and subjected to luciferase reporter assay. The luciferase assays were performed as described above.
Genotyping and Sanger sequencing
Genomic DNA was isolated either from saliva using Oragene-DNA OG-500 kit (DNAgenoTek) or from blood using the QIAamp DNA Blood kit (QIAGEN) according to the manufacturer’s instructions. Genomic DNA was then amplified with primers via a thermocycler. The presence of candidate mutations was then confirmed by Sanger sequencing using Big Dye Terminator v1.1 Sequencing kit (Applied Biosystems), and the amplimers were sent to Biomolecular Resource Facility (Australian National University, Canberra, Australia) to be analyzed by 3730 DNA Analyzer (Applied Biosystems).
Whole exome capture sequencing
For whole exome sequencing, input DNA was extracted from whole blood, analyzed for integrity, and then fragmented by nebulization. DNA library preparation was performed with the Illumina paired-end sample prep kit (Illumina) and followed by exome enrichment (TruSeq Exome Enrichment kit; Illumina). Libraries were sequenced as paired-end reads (100-bp runs) on an Illumina HiSeq 2500.
Analysis comprised alignment of sequences to the human reference sequence GRCh37, using a Burrows-Wheeler aligner (Li and Durbin, 2009). Raw single-nucleotide variants (SNVs) were called against the reference with SAMTools (Li et al., 2009). Common exome variants and deep SNVs were excluded, and coding and splicing variants were captured by alignment with the Ensembl Exomic database. Non-synonymous substitutions were filtered using ANNOVAR. For novel SNVs, prediction of functional effect were done using SIFT (Kumar et al., 2009), PolyPhen-2 (Adzhubei et al., 2010), and Mutation Taster (Schwarz et al., 2014). Filtering of variants for novelty was performed according to the sum of scores for mouse mutant phenotype in the homologous mouse gene, Mendelian disease associations (OMIM), pathway analysis (gene ontology), immune system expression (Immgen), and PolyPhen-2 score. After filtering and ranking variants, heterozygous IKBKB variant was investigated further.
Whole exome sequencing data were deposited in the Sequence Read Archive website, accession ID SAMN10107916.
Mutant and WT IKBKB mammalian expression constructs pcDNA 3.1(−)/myc-His were obtained from Biomatik, and pFN21A expression vector containing IKBKB was purchased from the Promega corporation. The WT and mutant vectors were transfected into HEK293 with Lipofectamine (Invitrogen) and then incubated for 24 h at 37°C with 5% CO2. Transfectants were stimulated with TNF-α for indicated time.
Total protein was extracted from cell line, PBMCs, or mouse spleen cells using radioimmunoprecipitation assay buffer with protease inhibitor cocktail (Roche) and a Halt phosphatase inhibitor (Pierce Net). 25 µg of protein was loaded on a 10% Bolt Bis-Tris PLUS gel (Thermo Fisher Scientific). After separation, proteins were wet-blotted on polyvinylidene fluoride membrane (Bio Rad). Blots were performed with antibodies to phospho-IκBα (Cell Signaling), total IκBα (Cell Signaling), phospho-P100 (Cell Signaling), B-actin (Cell Signaling), and GAPDH (Abcam). Horseradish peroxide–conjugated secondary antibodies were detected with Amersham ELC Western blotting system (GE Healthcare); band intensity was quantitated with Fujifilm multigauge software and normalized to a loading control.
CRISPR/Cas9 mouse construction
Single-guide RNA (sgRNA) design and cloning
For SpCas9 editing, two sgRNAs were designed to ensure a protospacer adjacent motif sequence as close as possible to the desired nucleotide change and to ensure Cas9 endonuclease would generate a double strand break close to the nucleotide of interest, yielding the following sgRNAs: guide 1, 5′-CTCCAGTAGTCAACGGTCACGG-3′ and guide 2, 5′-TACTGGAGCTTCGGCACCCTGG-3′. No significant off-target effects were detected by in silico analysis (CCTop software; Stemmer et al., 2015). A single-stranded oligonucleotide (ssODN) template was chemically synthetized as a 4 nM ultramer oligonucleotide from IDT with the following sequence: ssOdn1 5′-ACCTTGGAAGGTGTGTCTGGGCTGAGGGGAGAAGGCATGAGGCTTGACTCTCCCCTGTTCCCTAGCAGAGGTGAAAGAAGGCAGTGCCTATGGGAGCCAGTCAGTGGAGCAGGAGGCAGAGAAGCTGTGTCCACCCCCTGAGCCTCCAGGAGGGCTCTGCCACGGGCA-3′. For sgRNA synthesis, a 455-bp vector was designed including a U6 promoter with a sgRNA, TracRNA scaffold, and a termination signal. The sgRNA was chemically synthetized as a gBlocks gene fragment (IDT), adapted from Mali et al. (2013). The sequences are as follows: for guide 1, 5′-TGTACAAAAAAGCAGGCTTTAAAGGAACCAATTCAGTCGACTGGATCCGGTACCAAGGTCGGGCAGGAAGAGGGCCTATTTCCCATGATTCCTTCATATTTGCATATACGATACAAGGCTGTTAGAGAGATAATTAGAATTAATTTGACTGTAAACACAAAGATATTAGTACAAAATACGTGACGTAGAAAGTAATAATTTCTTGGGTAGTTTGCAGTTTTAAAATTATGTTTTAAAATGGACTATCATATGCTTACCGTAACTTGAAAGTATTTCGATTTCTTGGCTTTATATATCTTGTGGAAAGGACGAAACACCGCTCCAGTAGTCAACGGTCAGTTTTAGAGCTAGAAATAGCAAGTTAAAATAAGGCTAGTCCGTTATCAACTTGAAAAAGTGGCACCGAGTCGGTGCTTTTTTTCTAGACCCAGCTTTCTTGTACAAAGTTGGCATTA-3′; and guide 2, 5′-TGTACAAAAAAGCAGGCTTTAAAGGAACCAATTCAGTCGACTGGATCCGGTACCAAGGTCGGGCAGGAAGAGGGCCTATTTCCCATGATTCCTTCATATTTGCATATACGATACAAGGCTGTTAGAGAGATAATTAGAATTAATTTGACTGTAAACACAAAGATATTAGTACAAAATACGTGACGTAGAAAGTAATAATTTCTTGGGTAGTTTGCAGTTTTAAAATTATGTTTTAAAATGGACTATCATATGCTTACCGTAACTTGAAAGTATTTCGATTTCTTGGCTTTATATATCTTGTGGAAAGGACGAAACACCGTACTGGAGCTTCGGCACCCGTTTTAGAGCTAGAAATAGCAAGTTAAAATAAGGCTAGTCCGTTATCAACTTGAAAAAGTGGCACCGAGTCGGTGCTTTTTTTCTAGACCCAGCTTTCTTGTACAAAGTTGGCATTA-3′. 100 ng of synthetized gBlock gene fragment was Topo TA–cloned into a pCR2.1TOPO vector (Thermo Fisher Scientific), and the cloned fragments were Ampicillin-selected according to the manufacturer’s instructions. The vector was transformed into Escherichia coli (Thermo Fisher Scientific).
Mouse husbandry and zygotes microinjection
C57BL6/Ncrl and Swiss Webster CFW/crl recipient mice (Charles River) were maintained at the Australian Phenomics Facility under specific pathogen–free conditions. 5-wk-old C57BL/6Ncrl females were superovulated then mated with 20-wk-old C57BL/6Ncrl stud males. Fertilized zygotes were collected from the oviduct and maintained under M16 medium (M7292; Sigma-Aldrich) overlaid with mineral oil. A mix of 50 ng/µl of SpCas9 protein (PNA Bio), Ikbk-purified gBlocks plasmids (guide 1, 5 ng/µl and guide 2, 5 ng/µl), and 100 ng/µl of ssODN suspended into nuclease-free water (Thermo Fisher Scientific) were coinjected into the mouse zygotes. Pronuclear injections were performed in a M2 medium (M7167; Sigma-Aldrich) overlaid with mineral oil under a DMi8 (Leica) inverted microscope apparatus associated with mechanical micromanipulators and a microinjection apparatus. Microinjected zygotes were cultured overnight at 37°C in a 5% CO2 incubator and then surgically transferred at two-cell stage into the ampulla of CFW/crl pseudo-pregnant females.
DNA extraction was performed on ear punches lysed in Tris-EDTA-Tween lysis buffer (50 mM Tris HCl, pH 8.0, 0.125 mM EDTA, and 2% Tween 20, plus proteinase K) and incubated at 56°C for 1 h before the DNA was denatured at 95°C for 10 min. Genotyping primers were as follows: SF, 5′-TTCCTCTCCTCACACCCAAG-3′ and 5′-ATTGAACAAGAGTGGTCGCC-3′. The Sanger sequencing was performed in the Biomolecular Resource facilities at the Australian National University.
The structure data of the human IKK2 protein (PDB code: 4KIK) was used. The structures of the mutants, p.K171E and p.V203I, of IKK2 protein were built with the Molecular Operating Environment software (2013.08; Chemical Computing Group Inc.), and the structural figures were prepared.
Student’s t test, ANOVA, and χ2 tests were used to determine the statistical significance, which was set at the 95% confidence level.
Online supplemental material
Table S1 summarizes clinical results for patients. Fig. S1 shows conservation and function of IKK2 mutation. Fig. S2 shows human lymphocyte function and phenotype. Fig. S3 shows T cell phenotype in IkbkbV203I mice.
The authors thank Anastasia Wilson, Ann-Maree Hatch, Yafei Zhang, Wesley Lam, Yuichi Shiraisih, Kenichi Chiba, Hiroko Tanaka, and Hideki Muramatsu for their technical assistance in the conduct of the study. We thank our colleagues at the Centre for Personalised Immunology and Dr. Bodo Grimbacher from Freiburg University for helpful discussions and feedback on the study. We are grateful to our patients and their families for their willing participation in the research.
The study was funded by National Health and Medical Research Council grants 1107464 (to M.C. Cook), 1079648 (to C.G. Vinuesa and M.C. Cook), and 1113577 (to C.G. Vinuesa and M.C. Cook); The Bev and Alan Harvey Bequest; Japan Society for the Promotion of Science grants KAKENHI JP16H05355 (to S. Okada), 16K15528 (to S. Okada), JP26461570 (to H. Kanegane), and JP17K10099 (to H. Kanegane); and the Practical Research Project for Rare/Intractable Diseases from the Japan Agency for Medical Research and Development.
The authors declare no competing financial interests.
Author contributions: C. Cardinez, B. Miraghazadeh, K. Tanita, A. Hoshino, and E. da Silva performed cellular and biochemical phenotyping experiments. S. Okada performed the luciferase reporter assays. R. Chand performed flow cytometry. T. Asano and M. Tsumura performed additional immunological studies. K. Yoshida, Y. Okuno, S. Miyano, and S. Ogawa performed whole exome sequencing. M. Yamazaki provided clinical samples and data. Z. Kato and H. Ohnishi undertook structural analysis. T.D. Andrews and M.A. Field performed bioinformatic analysis. G. Burgio generated the CRISPR/Cas9 mouse strain. T. Morio, C.G. Vinuesa, H. Kanegane, and M.C. Cook supervised the study. C. Cardinez, B. Miraghazadeh, K. Tanita, S. Kojima, H. Kanegane, and M.C. Cook wrote the manuscript.
C. Cardinez, B. Miraghazadeh, and K. Tanita contributed equally to this paper.