Introduction
Varicella zoster virus (VZV) is a neurotropic
alphaherpesvirus exclusively infecting humans, in whom it causes two distinct pathologies: varicella (chickenpox) upon primary infection and herpes zoster (shingles) following reactivation [
1]. VZV spreads via inhalation of infectious droplets and infects mononuclear cells in the tonsils, leading to viremia through infected T cells and dissemination to the skin to replicate and cause the characteristic vesicular eruptions known as varicella [
1]. Importantly, VZV establishes latency in sensory neuronal ganglia, from which it can reactivate and spread to the skin as zoster or to the central nervous system (CNS), manifesting as meningitis, encephalitis, cerebellitis, or vasculopathy with stroke [
2,
3]. About 20% of patients hospitalized with chickenpox experience neurological complications [
4], suggesting a correlation between impaired systemic control of the infection and development of severe varicella with dissemination to the CNS. Knowledge on the pathogenesis of VZV infection and immunity remains incomplete, and although implementation of a VZV vaccine with the Oka strain in certain countries has resulted in reduced frequency of VZV cases, this infectious disease remains a worldwide health problem [
5].
VZV is an enveloped DNA virus, which can infect epithelial cells, peripheral blood mononuclear cells (PBMCs), and neurons [
1,
6]. The genome of VZV comprises 71 known
open reading frames (
ORF)
s, of which the
VZV latency-associated transcript (
VLT) is the only viral gene known to be transcribed during latency, together with a
VLT-ORF63 fusion transcript [
7,
8]. Unrelated clinical VZV isolates exhibit only little variability in virulence [
9], suggesting that defective host immunity is the major determinant of disease severity rather than differences between virus strains. The precise determinants of protective immunity toward VZV are incompletely understood, in part because VZV is a strictly human pathogen, and limited data are available from humanized mice studies [
10]. Studies regarding inborn errors of immunity (IEI) that cause increased susceptibility to VZV are therefore of particular importance. From these studies, it is clear that cellular immunity mediated by natural killer (NK) cells and T cells plays a particularly important role during VZV infection, as individuals with IEI affecting NK and T cell function may present with severe and disseminated VZV infections [
11‐
13]. Moreover, genetic defects in the interferon-γ-receptor 1 (IFNGR1) and tyrosine kinase (TYK) 2 interfere with macrophage function and were found to predispose to disseminated infection with mycobacteria and VZV [
14,
15]. Finally, genetic defects in the innate cytosolic DNA sensor RNA polymerase III (POL III) were identified and demonstrated to cause selectively increased susceptibility to VZV CNS infection and pneumonitis in otherwise healthy children and adults [
16‐
18].
The innate immune system utilizes pattern recognition receptors (PRRs) to detect pathogen-associated molecular patterns (PAMPs) in order to mount protective immune responses. This includes the production of cytokines and interferons (IFN)s, the latter exhibiting antiviral activity through their ability to induce IFN-stimulated genes (ISGs) [
19]. Different classes of PRRs are involved in the recognition of virus infections, including membrane-associated Toll-like receptors (TLR)s, cytosolic RNA-sensing retinoic acid-inducible gene 1 (RIG-I)-like receptors, and finally cytosolic DNA sensors [
19]. Within the group of DNA sensors, TLR9 detects unmethylated DNA, RNA polymerase III (POL III) recognizes AT-rich DNA, while absent in melanoma (AIM)2, gamma-interferon-inducible protein 16 (IFI16) and cyclic GMP-AMP synthase (cGAS) senses double-stranded (ds) DNA in a sequence-independent manner [
20,
21]. Among these, cGAS has emerged as the main cytosolic DNA sensor, signaling through the adaptor molecule Stimulator of Interferon Genes (STING) to induce mainly type 1 IFN responses, but also to contribute to nuclear factor kappa B (NF-κB) activation [
22].
Recent reports have described the occurrence of hemophagocytic lymphohistiocytosis (HLH) during VZV infection in the setting of IEI [
23]. HLH is a rare but life-threatening clinical syndrome characterized by uncontrolled activation of immune cells and severe systemic inflammation [
24]. Familial (or primary) HLH (fHLH) is a genetic disorder most often caused by autosomal recessive loss of function mutations in genes that disrupt the cytotoxic activity of NK and CD8 + T cells, including
PRF1,
UNC13D,
STX11,
STXBP2,
RAB27A,
LYST,
AP3B1,
SH2D1A, and
BIRC4 [
25]. While autosomal recessive primary HLH presents early in childhood, hypomorphic mutations in HLH genes are generally associated with fHLH onset in adulthood [
26]. Sporadic (or secondary) HLH develops without a known underlying genetic cause but rather presents in association with malignancies, autoimmune or autoinflammatory diseases, or is triggered by infections [
27,
28]. Interestingly, both familial and sporadic HLH might present with an infectious trigger, and herpesviruses are the most common causes of virus-induced HLH, with Epstein-Barr-virus (EBV) and cytomegalovirus (CMV) accounting for more than 50% of virus-associated HLH [
27]. Similarly, VZV can trigger HLH upon primary infection or reactivation, although this is mostly reported in patients with underlying immunosuppression or fHLH [
23,
29‐
31].
Here, we describe a patient with severe clinical manifestations of VZV infection and HLH, whom we studied in great detail in order to understand the underlying genetic and immunological pathogenesis. We hypothesize that severe VZV disease in some otherwise healthy individuals may be caused by monogenic IEI, not necessarily displaying complete clinical penetrance. Based on the current knowledge on VZV infection pathogenesis, innate and adaptive immune circuits, and HLH-associated molecules, we searched whole exome sequencing (WES) data for rare gene variants that may underlie susceptibility to severe VZV infection and/or HLH. In this patient, we identified a monoallelic variant in the gene encoding the ubiquitin ligase autocrine motility factor receptor (AMFR) which regulates cGAS-STING signaling through STING poly-ubiquitination. This finding was functionally validated in the by showing reduced STING activation and IFN responses as well as increased VZV replication in patient PBMCs and fibroblasts from the patient compared to controls. We propose that defects in AMFR, which impair cGAS-STING-mediated sensing of foreign DNA, confer enhanced susceptibility to severe disseminated VZV infection and risk of secondary hyperinflammation.
Methods
Patient Material
Whole blood was collected at hospitalization in EDTA-stabilized tubes for DNA purification and after recovery in lithium heparin tubes for peripheral blood mononuclear cell (PBMC) isolation. PBMCs were isolated by Ficoll density gradient centrifugation using SepMate PBMC isolation tubes (STEMCELL Technologies, no. 85460) and frozen down in liquid nitrogen. Control PBMCs were purified from healthy donors after obtaining written consent. Genomic DNA was purified using QIAamp DNA Blood Mini Kit (Qiagen, no. 51104) according to the manufacturer’s instructions.
WES was conducted on genomic DNA from the patient using KAPA HTP library preparation and Nimblegen SeqCap EZ MedExome Plus kits and analyzed with Nextseq version2 chemistry (2 × 150 basepairs) (Ilumina). Single nucleotide polymorphisms were called relative to hg19. Variant call files were uploaded to Ingenuity Variant Analysis (IVA) software (Qiagen) and filtered according to rarity (gnomAD frequency < 0.1%) and predicted deleteriousness (Combined Annotation Depletion Dependent (CADD) score > 15 and CADD score > mutation significance cutoff (MSC) score). De novo variants were also included. In addition, variants were filtered based on their biological relevance using gene lists, including all genes related to known IEI according to the IUIS Guidelines [
32] and broad biological filters in IVA related to VZV, HLH, PID, and immune response.
Sanger Sequencing of AMFR
Genomic AMFR DNA from the patient and the patient’s mother, father, younger sister, and younger brother were amplified by PCR using Phusion Hot Start II DNA polymerase (Thermo Fischer Scientific, no. F-594S) and the following primers: AMFR forward: 5′AAGCTGCTGCTCCATTATCCG-3′ and AMFR reverse 5′-TACCAGCATCAGAGGTAGACCA-3′. The genotype of amplified AMFR was confirmed using Sanger sequencing with AMFR forward primer.
In Vitro Stimulations of PBMCs
Patient and control PBMCs were thawed and seeded in RPMI supplemented with 10% heat-inactivated fetal bovine serum and 1% penicillin/streptomycin (cRPMI) at a density of 5 × 105 cells/well for infection experiments and 1 × 106 cells/well for stimulation with 2′3′-cGAMP and dsDNA and incubated overnight at 37 °C and 5% CO2. Cells were infected with 50 HAU of Sendai virus (SeV) (Cantell strain, Charles River), 3 MOI of HSV1 (KOS Strain), or 0.2 MOI of cell-free (CF) VZV debris (rOKa strain) or CF debris mock). Following 24 h of infection, supernatants were harvested for mesoscale, and cells were lysed for RNA isolation. In addition, PBMCs were stimulated with 100 µg/mL of 2′3′-cGAMP (InvivoGen) or 2 µg/mL of transfected ht (herring testes) dsDNA for 3 h following cell lysis for Western blotting or stimulated with 50 µg/mL high molecular weight poly(I:C) (InvivoGen, USA) or 5 µg/mL CpG ODN2395 (InvivoGen, USA) for 6 h before being lysed for downstream RT-qPCR analysis.
Fibroblast Experiments
A skin biopsy from P1 was taken under local anesthesia after the clinical symptoms had disappeared, with the written consent of P1 and his parents. Dermal fibroblasts were subcultured at the Department of Clinical Genetics, Aarhus University Hospital (Aarhus, Denmark). Normal human dermal fibroblasts (NHDF) were obtained from Promocell (Heidelberg, Germany). Primary fibroblasts were grown in DMEM with 10% FBS and 1% penicillin–streptomycin.
VZV Infection
Primary fibroblasts were seeded at a density of 60,000 cells/well in 24-well plates. The following day, growth media was removed, and cell-free VZV rOka strain debris was added to the cells in 0.6 mL Hank’s Balanced Salt Solution (Gibco, Montana, USA) at MOI 1. The plate was centrifuged at 250 × g for 10 min after which the virus adsorbed for 4 h at 37 °C. The virus media was removed, and the cells were washed once in PBS before the addition of 0.5 mL 10% DMEM. At 48 hpi, the supernatant was removed, and the cells were washed once in PBS before lysing for downstream RT-qPCR measurement of viral ORF expression.
RT-qPCR
Total RNA was purified using Nucleospin 96 RNA core kit (Macherey–Nagel, Germany). For two-step RT-qPCR, the RNA was reverse transcribed into cDNA using Iscript™ gDNA Clear cDNA Synthesis Kit (Bio-Rad, USA). qPCR was then performed with either TaqMan Fast Advanced Master Mix (Applied Biosystems, USA) or Brilliant III Ultra-Fast SYBR Green qPCR Master Mix (Agilent, USA). For one-step RT-qPCR, the TaqMan RNA to CT One Step Kit (Applied Biosystems, USA) was used. Relative mRNA was calculated using the 2−ΔΔCq method.
RT-qPCR Primers
The following TaqMan primers were used (Thermo Fisher Scientific, USA): AMFR (Hs01031688_m1), IFNB1 (Hs01077958_s1), MX1 (Hs00895608_m1), CXCL10 (Hs00171042_m1), TBP (Hs00427620_m1), GAPDH (Hs02758991_g1), and 18S (Hs03928985_g1).
The following PCR-primers were used for SYBR Green qPCR: ORF63 forward: 5′-GCGCCGGCATGATATACC-3′, ORF63 reverse: 5′-GACACGAGCCAAACCATTGTA-3′; ORF40 forward: 5′-ACTTGGTAACCGCCCTTGTG-3′; ORF40 reverse: 5′-CGGGCTACATCATCCATTCC-3′, ORF9 forward: 5′-GGGAGCAGGCGCAATTG-3′, ORF9 reverse: 5′-TTTGGTGCAGTGCTGAAGGA-3′. WPRE forward: 5′-GGCACTGACAATTCCGTGGT-3′, WPRE reverse: 5′-AGGGACGTAGCAGAAGGACG-3′, ALB forward: 5′-GCTGTCATCTCTTGTGGGCTGT-3′, and ALB reverse: 5′-ACTCATGGGAGCTGCTGGTTC-3′, PPIB forward: 5′-CAACGCAGGCAAAGACACCAAC-3′, PPIB reverse: 5′-GGTTTATCCCGGCTGTCTGTCTTG-3′.
Western Blotting
For PMBC stimulations, cells were washed twice with PBS and lysed in RIPA buffer (Thermo Fischer Scientific, no. 89901) supplemented with Halt Protease and Phosphatase Inhibitor Cocktail (Thermo Fischer Scientific, no. 78440) and Benzonase Nuclease (Sigma-Aldrich, no. E1014-25KU). Protein concentrations were measured using Pierce BCA Protein Assay Kit (Thermo Scientific, no. 23227), and cell lysates were denatured at 95 °C for 5 min with 50 mM DTT (Sigma-Aldrich, no. 43816-10ML) and 4 × Laemmli buffer (Bio-Rad, no. 1610747). Samples were subjected to SDS gel electrophoresis and transferred to a PVDF membrane using the Transfer-Blot Turbo systems. The membrane was blocked in 5% skimmed milk in PBS-T or TBS-T for 1 h, followed by incubation overnight at 4 °C with primary antibodies against STING (cell signaling, no. 13647S, 1:1000), phospho-STING (cell signaling, no. 19781S, 1:1000), TBK1 (cell signaling, no. 3013S 1:1000), phospho-TBK1 (cell signaling, no. 5483S, 1:1000), IRF3 (cell signaling, no. 11904S, 1:1000), phospho-IRF3 (cell signaling, no. 4947S, 1:1000), ISG15 (cell signaling, no. 2758S, 1:1000), Vinculin (cell signaling, no. 13901S, 1:2000), AMFR (Proteintech, no. 16674–1-ap), GFP (Santa Cruz no. sc-8334, 1:500), FLAG-Tag (cell signaling, no. 17793S, 1:500), Myc-Tag (cell signaling, no. 2278S, 1:1000) or HA-Tag (cell signaling, no. 3724S, 1:1000). Primary antibodies were visualized using secondary horseradish-peroxidase-coupled anti-rabbit or anti-mouse antibodies (Jackson ImmunoResearch no. 715–036-150, no. 711–035-152) at 1:10.000 on ChemiDoc gel imaging system (Bio-Rad).
Mesoscale Measurements of Cytokines and Interferons in Supernatants
Expression of IFNs (IFNα2, IFNβ, IFNλ1, and IFNγ) and proinflammatory cytokines (IL-1β and TNFα) was measured in cell culture supernatants using U-PLEX assays (Meso Scale Diagnostics, USA) according to manufacturer’s protocols on a Meso Quickplex SQ 120 instrument.
STING Immunoprecipitation
HEK293T cells were seeded at a density of 2.5 × 106 cells in a 6-cm Petri dish and following overnight incubation, transfected with 1 µg of the following plasmids: pcDNA3/FLAG-STING, pRK5/HA-K27-ubiquitin, and pcDNA3/Myc-AMFR WT or pcDNA3/Myc-AMFR R594C. Controls transfected only with FLAG-STING, HA-K27-Ubiquitin, and pcDNA3-empty vector (No AMFR control), or HA-K27-Ubiquitin, AMFR WT, and FLAG-Empty vector (No STING control) were included. Cells were lysed 24 h post transfection in Pierce IP lysis buffer (Thermo Fischer Scientific, no. 8788) supplemented with 1 × protease inhibitor cocktail (Roche, no. 05.892.970.001) and 1 × PhosSTOP cocktail (Roche, no. 04.906.837.001) for 1 h at 4 °C with rotation and centrifuged for 10 min at 1400 × g at 4 °C. Lysates were then incubated with FLAG M2 Dynabeads (Sigma, no. M8823) for 1.5 h at room temperature, washed 3 times in TBS with 0.05% Tween20 and phosphatase inhibitors (TBS-T +) and incubated with 3XFLAG peptide (Sigma-Aldrich) for 15 min at room temperature to elute STING. Then, eluents were denatured by boiling for 5 min at 95 °C in the presence of 1% sodium dodecyl sulfate (SDS) after which samples were diluted in lysis buffer with protease-, phosphatase-, and deubiquitylating enzyme inhibitors (Merck, no. 662141) and incubated overnight at 4 °C with FLAG M2 Dynabeads. Finally, samples were washed three times in TBS-T and FLAG-STING eluted by boiling the samples in Laemmli concentrate sample buffer (Sigma, no. S3401-10VL) at 95 °C for 10 min. Lastly, samples were immunoblotted for expression of FLAG-STING, Myc-AMFR, and HA-Ubiquitin.
IFNB Luciferase Reporter Gene Assay
HEK293T cells with stable STING expression were plated on 96-well plates (20–30.000 cells per well) and transfected with 30 ng constructs harboring IFNB-promoter firefly luciferase reporter genes, and 15 ng β-actin-promoter-driven Renilla luciferase together with the indicated amounts of the AMFR WT and AMFR R594C. At 18 h post-transfection, the cells were stimulated with 2′3′-cGAMP or left untreated. After 8 h of stimulation, the cells were lysed, and the Firefly and Renilla luciferase signals were developed with a Dual-Glo luciferase assay (Promega) and read on a Luminoskan Ascent (Labsystems) according to the manufacturer’s instructions.
ImageStream
The co-localization of STING–ER and STING–Golgi, was determined by ImageStream using the ImageStream MK II Imaging Flow Cytometer (Amnis). The cells transfected with the indicated plasmids for 24 h were fixed using 4% formalin for 20 min at room temperature and then pre-permeabilized with 0.2% Triton X-100 for 6 min. The cells were incubated with primary antibodies for 1 h on ice and then incubated with the Alexa-Fluor-labeled secondary antibodies for 1 h. After every step, the cells were washed with 1 × PBS three times. Finally, the cells were resuspended in 1 × PBS with 2 mM EDTA and 3% BSA. An original magnification of × 60 was used for all samples. The images of 7000–10,000 single cells with different channels were acquired in the ImageStream, and the data were analyzed through IDEAS software v6.2 (Amnis Corporation). The antibodies used were mouse anti‐STING (1:300), rabbit anti-PDI (1:50), and rabbit anti-GM130 (1:3000). After gating of focused, single and positive cells with the defined fluorescent markers, the colocalization of STING–PDI (ER marker) and STING–GM130 (Golgi marker) was analyzed through the Bright Detail Similarity feature for the corresponding channels. The accuracy of the cell populations gated as representing colocalization was controlled by visual inspection of individual pictures in the gated cell populations.
Lentiviral Reconstitution of Patient PBMCs
Third-generation lentiviral vectors were produced as previously described [
33]. Briefly, HEK293T cells were transfected with 11.25 µg pMD.2G, 9 µg pRSV-Rev, 39 µg pMDLg/pRRE, and 39 µg lentiviral transfer vector for T175 bottles using a standard polyethylenimine transfection protocol. Five hours after transfection, the medium was changed. Forty-eight hours after transfection, viral supernatants were harvested, filtered, and ultracentrifuged at 25,000 rcf for 2 h using a sucrose gradient (sucrose, 20% w/v) before titration by quantification of the number of lentiviral integrations in HEK293T as previously described [
33]. For the reconstitution, patient and control PBMCs were thawed and seeded as described above. At the time of seeding, the cells were stimulated with 150 1.5 µg/ml PHA (Fisher Scientific, USA) for 72 h before transduction with MOI 10 of lentiviral particles. Seventy-two hours after transduction cells were stimulated with 2′3′-cGAMP as previously described, followed by cell lysis for Western blotting.
Statistics
For statistical testing, Prism 9.2 (GraphPad Software, USA) was used. All tests were two-tailed and an adjusted alpha < 0.05 was considered statistically significant. Correction for multiple comparisons was carried out as specified in the figure legends.
Ethics
The patient, family, and healthy controls were included following oral and written consent in accordance with The Helsinki Declaration and national ethics guidelines and after approval from the Danish National Committee on Health Ethics (no. 1–10-72–275-15), the Data Protection Agency, and Institutional Review Board.
Discussion
The major finding of the present study is the description of a novel predisposition to severe viral infection involving abnormal AMFR-mediated polyubiquitination and decreased activation of STING in a child with a cellular phenotype showing impaired VZV-induced type I IFN responses and increased VZV replication and a clinical presentation with severe VZV infection and HLH. To our knowledge, this is the first report of a defect in STING signaling in humans causing increased susceptibility to viral infection.
Following the initial discovery of STING [
37] and the subsequent discovery of cGAS [
38], the cGAS-STING pathway is now appreciated as the major driver of the antiviral IFN response. Other DNA sensors, including RNA POL III, have been identified by many independent groups, but their respective roles in innate immunity are not fully clarified and may be dependent on cell type and cellular context [
16,
39,
40]. cGAS recognizes foreign and host-derived dsDNA in a sequence-independent manner and catalyzes the formation of 2′3′-cGAMP that serves as a second messenger to the ER-bound adaptor protein STING [
41,
42], which traffics to the Golgi, where it recruits TBK1, thus leading to phosphorylation of STING on serine 366, and this in turn leads to recruitment of IRF3 [
43]. This positions IRF3 for phosphorylation by TBK1 allowing IRF3 dimerization, nuclear translocation, and induction of IFN-β gene expression [
44]. The role of ubiquitination in STING biology is well documented and includes multiple types of ubiquitin linkage [
45]. For instance, K63 ubiquitination by TRIM56, TRIM32, and Mul1 is important for the activation of signaling [
46‐
48] and is targeted by HSV1 to facilitate CNS infection [
49]. Moreover, K48 ubiquitination by RNF5 and RNF90 has been reported to promote STING degradation and downregulate signaling [
50,
51]. Finally, K27-linked ubiquitination of STING by AMFR promotes STING ER-to-Golgi trafficking [
35], which is a rate-limiting step in STING signaling [
52] and promotes activation of the pathway and antiviral defense [
35].
AMFR/g78 is an E3 protein ubiquitin ligase embedded in the ER membrane, important for the degradation of misfolded proteins in the ER-associated degradation response (ERAD). Upon microbial DNA challenge, AMFR catalyzes K27-linked polyubiquitination of STING, and this ubiquitin chain creates an anchoring platform for recruiting and activating TBK1, resulting in IRF3 phosphorylation and IFN-β induction [
35]. Moreover, AMFR is also involved in regulating cholesterol biosynthesis which may impact ER membrane fluidity and STING trafficking from ER to Golgi, thereby influencing IFN activation and ISG responses [
53]. Indeed, previous research has shown that STING signaling is linked to cholesterol metabolic pathways and cellular cholesterol content. Specifically, reprogramming of lipid metabolism leading to altered cholesterol synthesis via the mevalonate pathway can influence the threshold for type-I IFN production through STING activation [
54]. The missense variant causing an amino acid substitution from arginine to cysteine is localized at the well-preserved position 594 within the G2BR domain, which is responsible for binding to the E2 ubiquitin-conjugating enzyme UBE2G, thus facilitating interaction between the RING domain and E2 enzyme and subsequently ubiquitin transfer. Deletion of the G2BR domain was reported to abolish the ERAD function of AMFR [
55], and a pathogenic variant in this domain would therefore be expected to cause disturbed AMFR-mediated functions, most notably defective ubiquitination and activation of STING [
35]. Indeed, we found that the cGAS-STING pathway is impaired in patient PBMCs stimulated by 2′3-cGAMP or dsDNA when measuring pSTING, pTBK-1, and ISG15, as well as decreased response to HSV1 despite the integrity of TLR3 and TLR9 signaling pathways in the patient. We were able to attribute this directly to decreased STING ubiquitination in cells expressing AMFR R549C as compared to cells expressing AMFR WT. Moreover, we demonstrate that the AMFR R549C variant interferes with AMFR WT in a partially dominant-negative manner with dose–response kinetics, although we cannot formally exclude a contribution from haploinsufficiency.
The effect of the AMFR variant may be through interaction with endogenous WT AMFR expressed from the other allele, thus eventually resulting in limiting amounts of AMFR for full STING activation. Alternatively, mutant AMFR may bind to STING and by competition cause dysregulation/insufficient activation of a fraction of cellular STING available for activation. At the molecular level, structural biology may provide some hypotheses. The R595C mutation in the patient AMFR variant is located in the E2 ubiquitin-conjugating enzyme binding domain responsible for interaction with the E2 ligase UBE2G2/UPC7 [
56] and is part of a stretch of positively charged residues on positions 594–596. Therefore, we speculate that the R595C mutation impairs the recruitment of the E2 ubiquitin ligase to AMFR. Since AMFR is part of a larger protein complex including, for instance, INSIGR1, some likely mechanisms for the dominant negative effect include (i) more than one AMFR molecule is involved in each AMFR-containing complex, and the patient variant, therefore, leads to impaired recruitment of the E2 ligase to the complexes containing WT:mutant and mutant:mutant AMFR; (ii) there is only one AMFR molecule per complex, but other proteins in the complex are rate-limiting, and complexes containing mutant AMFR, therefore, compete for these proteins, hence exerting dominant negative activity toward complexes containing WT AMFR. Altogether, elucidation of the exact nature of the mechanism of the dominant negative activity required further investigation.
Finally, we establish the causal relationship between genotype and phenotype by demonstrating the reconstitution of the cellular phenotype (cGAS-STING signaling) in patient PBMCs complemented with WT AMFR. Whether the AMFR-STING defect is relatively specific to VZV and HSV1, or alternatively involves other DNA viruses remains to be resolved, but our finding of normal responses to SeV may indicate a defect mainly related to infection by DNA viruses. Collectively, the precise role of cGAS STING-mediated DNA sensing and IFN induction in humans remains to be determined.
The existence of defective innate DNA sensing predisposing to VZV infection, possibly through impaired signaling in response to the presence of viral cytosolic DNA, is similar to the previously reported IEI affecting another cytosolic DNA sensor RNA polymerase III, which has been described in children and adults with severe VZV CNS encephalitis, vasculopathy, and recurrent VZV meningoencephalitis [
16‐
18]. Therefore, defective DNA sensing may be a common theme in VZV predisposition and might act in a partially cell-type-dependent manner. In the case of POL III deficiency, with CNS involvement constituting a prominent feature, we hypothesized that a particularly important role of POL III in recognizing the AT-rich VZV genome may be at play in certain cell types, such as neuronal cells, in which cGAS expression is low/absent [
16,
17]. On the other hand, one study identified an important role of STING in mounting type I and type III IFN responses to VZV in human dermal fibroblasts and HaCaT keratinocytes with potential implications for varicella pathogenesis and suggesting an important role of cGAS-STING in the skin [
57]. Recently, the cGAS-STING DNA sensing pathway was demonstrated to be required for IFN induction and VZV restriction during VZV infection in THP1 cells, and the VZV protein ORF9 was reported to antagonize cGAS-STING signaling and IFN production [
58]. The observation that POL III dominates as a VZV sensor in mononuclear cells might in fact explain why we do not observe significantly decreased IFN induction in PBMCs in response to VZV and only could measure a modest increase in VZV replication in this cell type from the patient. The pattern of inheritance appears to be autosomal dominant with incomplete penetrance since the mother and two younger siblings also carry the AMFR R594C variant and so far have not experienced severe VZV infection. However, PBMCs from the mother of the patient also exhibit decreased phosphorylation of IRF3 (although less pronounced than in the patient), as well as significantly reduced IFNα/β responses to VZV infection together with increased VZV replication. The data suggest a milder cellular phenotype in the mother. However, since fibroblasts from the mother were not available, we were unable to make a precise comparison of antiviral responses in different cell types between patient, mother, and healthy controls. Indeed, fibroblast which produces more vivid antiviral responses than PBMCs may more precisely reflect the physiological situation in vivo. Moreover, it also has to be kept in mind that VZV infection models in primary human cells combined with the difficulty of measuring intracellular signaling pathways by a slowly replicating virus (i.e., not a potent agonist added at one given time) that can only be used in relatively low titers can be variable and is unlikely to give a completely straight biochemical picture in vitro regarding cellular responses. Incomplete penetrance is a frequent observation in IEI and may be due to influences from other genetic variants, differences in allele expression (for monoallelic variants), differences in viral load, or other immunomodulatory external factors. In order to hopefully avoid future severe illness in the siblings, they have been vaccinated against VZV by the live attenuated VZV vaccine.
As to the possible link between this variant causing increased VZV replication and severe VZV infection to the development of HLH, this remains insufficiently understood. However, some previous observations in the literature may suggest a possible pathophysiological mechanism. Among cases of secondary HLH, viral infection is the most common trigger [
59], and more recently, it has been suggested that monoallelic variants in known HLH genes, or less penetrant other gene variants associated with IEI, may underlie HLH [
26,
60]. This may be the case for other IEI affecting innate immunity as exemplified by a previous study demonstrating disseminated VZV and HLH in a patient with GATA2 defect [
23]. In this context, enhanced viral replication and an increased load of PAMPs may increase the risk of developing a hyperinflammatory state. Further, we cannot exclude that dysregulated STING activation as described in our patient may lead to hyperinflammation during a high viral burden. We suggest that the variant may not have a very strong direct disease-causing effect but rather lowers the threshold for virus-induced inflammation and HLH. The link between STING-signaling and reduced threshold for HLH is further underpinned by a recent study implicating the well-established HLH-disposing gene
UNC13D in STING regulation [
61]. Collectively, these complex cellular interactions between pathogen/PAMP and the immune system that may trigger a cytokine storm and HLH cannot be sufficiently mimicked and studied in an in vitro system. Based on the present report, we would encourage others with the relevant expertise to investigate this matter in a physiological context, which would however require modified animals, since VZV is strictly a human pathogen.
Previously, Goldbach-Mansky and associates described a vascular and pulmonary syndrome in patients with gain-of-function variants in the STING-encoding gene
STING1 (formerly known as
TMEM173) and suggested the name STING-associated vasculopathy with onset in infancy (SAVI) for this autoinflammatory interferonopathy [
62]. The authors identified three different mutations in exon 5 of
STING1 in these six patients and observed constitutive STAT1 phosphorylation and increased constitutive and inducible type I IFN expression in patient cells [
62]. Since then, several other publications have described additional patients and extended the clinical phenotype [
63,
64]. Moreover, other IEIs also affecting IFN production, such as STAT2 deficiency, translate into partially overlapping clinical manifestations together with the interferonopathy signature [
65,
66]. However, despite the description of numerous IEIs affecting pathogen and PAMP receptors and their downstream IFN-inducing signaling pathways causing susceptibility to severe viral infections, defects in the cGAS-STING pathway in humans have not been previously reported. The clinical and cellular phenotype described here is significantly different from the one ascribed to SAVI, and notably, we did not observe increased IFN nor ISG levels in vitro under the given conditions examining patient cells harvested after acute illness. However, we cannot entirely exclude that elevated ISGs may have been present in the circulation of the patient during the acute episode, and thus we cannot rule out a degree of autoinflammation/interferonopathy caused by the AMFR variant and possibly associated to the development of VZV-triggered HLH in the patient.
In conclusion, we suggest a novel genetic etiology of severe VZV disease in childhood, also representing the first IEI related to a defect in the STING-cGAS pathway. The present work contributes information on the question of the role of DNA sensors in host defense in human immunology. Together with our previous work on POL III, the available data suggest that POL III and cGAS-STING may each play non-redundant roles in VZV immunity in humans, depending on the cell type and tissue involved. Collectively, the precise role of cGAS STING-mediated DNA sensing and IFN induction in humans remains to be further studied. Identification of human IEIs involving these molecules remains a powerful tool for establishing the contributions of relevant immune signaling pathways in humans and for gaining valuable insights into how dysregulated cGAS-STING signaling may lead to human disease, ranging from autoinflammatory interferonopathy to severe viral infection.
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