Research Article

TLR3 Deficiency in Patients with Herpes Simplex Encephalitis

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Science  14 Sep 2007:
Vol. 317, Issue 5844, pp. 1522-1527
DOI: 10.1126/science.1139522

Abstract

Some Toll and Toll-like receptors (TLRs) provide immunity to experimental infections in animal models, but their contribution to host defense in natural ecosystems is unknown. We report a dominant-negative TLR3 allele in otherwise healthy children with herpes simplex virus 1 (HSV-1) encephalitis. TLR3 is expressed in the central nervous system (CNS), where it is required to control HSV-1, which spreads from the epithelium to the CNS via cranial nerves. TLR3 is also expressed in epithelial and dendritic cells, which apparently use TLR3-independent pathways to prevent further dissemination of HSV-1 and to provide resistance to other pathogens in TLR3-deficient patients. Human TLR3 appears to be redundant in host defense to most microbes but is vital for natural immunity to HSV-1 in the CNS, which suggests that neurotropic viruses have contributed to the evolutionary maintenance of TLR3.

The contribution of Toll and Toll-like receptors to immunity has been studied extensively in the past decade. Toll-deficient Drosophila were shown to be susceptible to experimental infections with certain fungi in 1996 (1), and a Toll-like receptor 4 (TLR4) null mutation in mice resistant to lipopolysaccharide (LPS) but susceptible to certain Gram-negative bacteria was identified in 1998 (2). Mice deficient for individual TLRs have since been generated and shown to have diverse infectious phenotypes, from susceptibility to resistance, depending on the TLR-pathogen combination (3). However, it remains unclear whether TLRs play nonredundant roles—beneficial or detrimental—in natural, as opposed to experimental, infections. This biological question is important, because natural selection acts on a given species in the setting of natural (rather than experimental) ecosystems. The human model is particularly suitable for analyses of the relevance of genes such as those of TLRs to host defense in natural ecosystems (4). Nevertheless, although many studies have suggested that TLR genes are involved in human infectious diseases, this has not been unambiguously demonstrated (5). In particular, no primary immunodeficiency involving TLRs has been identified.

The discovery of inherited interleukin 1 receptor-associated kinase-4 (IRAK-4) deficiency in children with bacterial diseases implicated human TLRs, interleukin-1 receptors (IL-1Rs), or both in host defense (6, 7). However, the narrow range of infections documented in such patients indicates that IRAK-4–dependent, TLR-mediated immunity is redundant for protective immunity to most microbes. In particular, IRAK-4–deficient patients are not susceptible to herpes simplex virus 1 (HSV-1) encephalitis (HSE). In HSE, HSV-1 infects epithelial cells in the oral and nasal mucosa and progresses to the central nervous system (CNS) via the trigeminal or olfactory nerves (8). A genetic etiology of HSE was found in two children who lacked functional UNC-93B (9), an endoplasmic reticulum protein required for TLR3, TLR7, TLR8, and TLR9 signaling (10). Both UNC-93B–and IRAK-4–deficient patients fail to signal through TLR7, TLR8, and TLR9, but unlike IRAK-4–deficient patients (7), UNC-93B–deficient patients display impaired TLR3-dependent interferon-α (IFN-α)-β, and -λ production (9). Moreover, HSV-1 is a double-stranded DNA virus with double-stranded RNA (dsRNA) intermediates (11), and TLR3 recognizes dsRNA (12). Finally, TLR3 is expressed in CNS-resident cells (1315) and peripheral nerves (16). Collectively, these observations suggest that impaired TLR3-dependent induction of IFN-α, -β and -λ might be involved in HSE.

A heterozygous TLR3 mutation in two children with HSE. We investigated two unrelated French children (P1 and P2) with HSE (SOM Text, note 2). UNC-93B deficiency was excluded on genetic and immunological grounds (fig. S1, A to D). Leukocytes and fibroblasts from P1 and P2 harbored the same heterozygous substitution (C→T) in TLR3 at nucleotide position 1660 (c.1660C>T) (Fig. 1, A and B). The two kindreds represent independent mutational events because the two P554S mutations were in different TLR3 haplotypes. The mutation leads to the replacement of a proline (P) by a serine (S) at residue 554 (P554S) (Fig. 1C). P554S has not previously been described (17, 18) and was not found in any of the 1581 unrelated healthy individuals examined (3162 chromosomes), including 241 Europeans. Residue P554 of TLR3 is conserved in the 18 animal species studied (Fig. 1D). The extracellular, ligand-binding domain of TLR3 contains 23 contiguous leucine-rich repeats (LRRs) forming a large, horseshoe-shaped solenoid (Fig. 1E) (19). P554 anchors the TLR3-specific insertion of residues 544 to 554 in LRR20 (Fig. 1E) (19, 20). This region is thought to be critical for dsRNA binding to TLR3 (20) and TLR3 multimerization (19). Three relatives of P1 and two of P2 were also heterozygous for the mutation (Fig. 1A). They were HSV-1 seropositive but had not suffered from HSE, which suggests that the P554S TLR3 mutation conferred an autosomal dominant predisposition to HSE with incomplete clinical penetrance.

Fig. 1.

Heterozygous TLR3 P554S mutation in two unrelated children with HSE. (A) Family pedigrees, with allele segregation in the two families. The patients, in black, are heterozygous for the mutation. The other family members heterozygous for the mutation are indicated by bold vertical lines. (B) Heterozygous c.1660C>T mutation in the patients. The sequence of the polymerase chain reaction products of genomic DNA from leukocytes of a control (C) and P1 (P) is shown. The mutation was confirmed in genomic DNA and cDNA from leukocytes and fibroblasts. (C) Schematic representation of TLR3 gene structure. Human TLR3 has five exons (Roman numerals) encoding a protein (shown in gray) composed of a leader sequence (L), an LRR domain, a transmembrane (TM) domain, and a Toll/interleukin-1 receptor (TIR) domain. The various LRR motifs, the N-terminal cap, and the C-terminal cap of the LRR domain are separated by dotted vertical lines, and the two LRRs with an insertion are indicated by asterisks. The c.1660C>T mutation results in a proline (P) to serine (S) substitution at amino acid position 554 (P554S) in LRR20. (D) LRR20 of TLR3 in humans and the corresponding region in the other 17 species studied, with the insertion indicated. The amino acids conserved in the insertion in all these species are shaded in gray. (E) Two views of the human TLR3 ectodomain (ECD) surface. H539 and N541 (left), implicated in ligand binding, and P554 (right) are shown in magenta. “Ins” refers to the eight residues from W546 to G553 in the TLR3-specific insertion 544 to 554 of the LRR20, and is shown in dark gray. Glycan is shown in yellow, and the C terminus of the TLR3 ECD is at the bottom.

Impaired responsiveness of fibroblasts to poly(I:C) stimulation. We derived dermal fibroblastic cell lines, which selectively express TLR3 (9), from patients and controls. The TLR3 agonist polyinosine-polycytidylic acid [poly(I:C)], which mimics dsRNA (12), induced IFN-β, -λ, and IL-6 in a dose- and time-dependent manner in all control fibroblasts but not in the TLR3-deficient fibrosarcoma P2.1 cell line (SOM Text, note 1) (Fig. 2A and fig. S2A). Primary and simian virus 40 (SV40)–transformed fibroblasts from P1 and P2 displayed only a residual response at high concentrations of poly(I:C) and late time points (Fig. 2A). IL-6 induction was less impaired. The induction of IFN-β and -λ mRNA production by poly(I:C) was markedly weaker in P1 fibroblasts (fig. S2B). Both nuclear factor kappa B (NF-κB) (Fig. 2B) and IFN regulatory factor-3 (IRF-3) (Fig. 2C) activation were impaired in response to poly(I:C) in the patients' fibroblasts, which responded normally to tumor necrosis factor–α (TNF-α) and IL-1β (Fig. 2B and fig. S2C). NF-κBessential modulator (NEMO)–deficient fibroblasts (SOM Text, note 1) did not respond to poly(I:C), IL-1β, or TNF-α (Fig. 2B), and UNC-93B–deficient fibroblasts (9) did not respond to poly (I:C) (Fig. 2C). Finally, all tested relatives carrying the TLR3 mutation, but none of the relatives without this mutation, displayed impaired responses to poly(I:C) (fig. S2D). The cosegregation of genotype and fibroblastic phenotype suggests that heterozygosity for the P554S TLR3 allele confers autosomal dominant hyporesponsiveness to poly(I:C) in fibroblasts.

Fig. 2.

Impaired response to poly(I:C) of fibroblasts and dominant-negative effect of the TLR3 P554S allele in fibroblasts (A) IFN-β, -λ, and IL-6 production in SV40-transformed fibroblasts (SV40 fibroblasts) from a control (C), P1, P2, and a UNC-93B–deficient (UNC-93B–/–) patient upon stimulation with various doses of poly(I:C) for 12 or 24 hours. (B) NF-κB-DNA–binding activity of nuclear extracts from the SV40 fibroblasts of a control (C), P1, P2, and a NEMO-deficient (IP) patient upon TNF-α and IL-1β stimulation for 30 min, or poly(I:C) stimulation for 60 min or 90 min, as assessed by electrophoretic mobility shift assay. The experiment is representative of two. (C) IRF-3 monomers and dimers in total cell extracts from SV40 fibroblasts of a control (C), P1, P2, and a UNC-93B–/– patient, upon poly(I:C) stimulation for 1 or 2 hours, as assessed by Western blotting. (D) TLR3 mRNA levels in SV40 fibroblasts from six controls (C) [mean value indicated by (–)], P1, and P2; β-glucuronidase (GUS) was used for normalization. The experiment shown is representative of two. (E to G) In P2.1 cell lines not transfected (P2.1) or stably transfected with pUNO expression vectors carrying no insert (P2.1-mock), or the C-terminal HA-tagged TLR3 cDNA with the WT sequence (P2.1-TLR3 WT) or with the P554S mutation (P2.1-TLR3 P554S), IFN-λ production (E) was measured after 24 hours stimulation with poly(I:C). The TLR3 cDNA in these cells (F) is shown, with the internal amplification control GAPDH; the experiment shown is representative of three. TLR3 expression in these cells (G) was assessed by Western blotting, using two antibodies to N-terminal TLR3 [anti-TLR3 (N) Ab1 and anti-TLR3 (N) Ab2] and an antibody to C-terminal–tagged HA. The experiment shown is representative of six. The recombinant TLR3 ECD protein was used as a positive control for the antibody. The internal expression control was glyceraldehyde-phosphate dehydrogenase (GAPDH). (H) IFN-λ production, in a control SV40-fibroblast cell line, stably transfected with an empty vector (C-mock), a C-terminal HA-tagged pUNO-TLR3 WT vector (C-TLR3 WT), or an HA-tagged pUNO-TLR3 vector containing the P554S mutation (C-TLR3 P554S) upon stimulation with various doses of poly(I:C) for 12 or 24 hours. In (A), (E) and (H), the production of IFNs and IL-6 was measured by enzyme-linked immunosorbent assay (ELISA). Mean values ±SD were calculated from three independent experiments.

Dominant-negative effect of the P554S TLR3 allele in fibroblasts. TLR3 multimerizes upon binding dsRNA, and several TLR3 mutants are dominant negative (2022), which suggests that the P554S mutation may be dominant negative. TLR3 mRNA is produced in normal quantities (Fig. 2D) in the patients' fibroblasts (fig. S2E), and the wild-type (WT) and P554S TLR3 mRNAs were equally abundant (fig. S2F). Stable transfection of P2.1 cells with C-terminal hemagglutinin (HA)–tagged WT TLR3, but not with P554S TLR3, restored the cell response to poly(I:C), as measured by IFN-β (fig. S2G) and IFN-λ production (Fig. 2E). Both WT and P554S TLR3 mRNAs were detected (Fig. 2F). The P554S TLR3 protein had a lower molecular weight than the WT, as shown by Western blotting with two antibodies that specifically recognize the TLR3 N-terminal ectodomain, but not with an antibody to C-terminal–tagged HA (Fig. 2G). Upon transient transfection of control fibroblasts with various ratios of mock vector and P554S TLR3 allele, the response to poly(I:C) decreased as the proportion of P554S TLR3 allele increased (fig. S2H). Moreover, control fibroblasts stably transfected with the P554S TLR3 allele lost their ability to respond to poly(I:C) (Fig. 2H). These observations were extended to P2.1 recipient cells (SOM Text, note 3). The P554S TLR3 protein is thus C-terminally truncated, loss-of-function for poly(I:C) responsiveness, and dominant negative in dermal fibroblasts and the fibrosarcoma P2.1 cell line, at least for IFN induction.

Impaired IFN-dependent control of viruses in TLR3-deficient fibroblasts. UNC-93B–deficient fibroblasts produce little IFN-β and -λ upon viral stimulation, resulting in high levels of viral replication and cell death (9). We therefore infected TLR3-heterozygous fibroblasts with HSV-1 and another neurotropic virus, vesicular stomatitis virus (VSV)—a highly cytopathic virus and potent IFN inducer in human fibroblasts. IFN-β and -λ production after infection with VSV and HSV-1 was markedly weaker in fibroblasts from the patients than in those from controls (Fig. 3, A and B). Six hours after VSV infection, viral replication rates were higher in P1 cells—as in Stat-1–deficient (23) and UNC-93B–deficient (9) cells—than in controls (Fig. 3C). Cell survival was also markedly lower for the patients than the controls and was similar to that for UNC-93B–and Stat-1–deficient cells after 24 hours of VSV and 96 hours of HSV-1 infection (Fig. 3D). Treatment with IFN-α or IFN-β complemented the phenotype of TLR3- and UNC-93B–deficient, but not Stat-1–deficient, cells (Fig. 3, C and E) in a dose-dependent manner (fig. S3). IFN-λ also partially complemented the phenotype, albeit less effectively than IFN-α or IFN-β (Fig. 3E). Our results thus demonstrate a causal relationship between heterozygosity for the P544S TLR3 mutation, impaired TLR3 signaling, abnormally weak IFN-α/β and -λ production, enhanced viral replication, and higher levels of fibroblast cell death upon viral infection.

Fig. 3.

High levels of viral replication and cell mortality in fibroblasts from the patients and rescue by treatment with IFN-α, -β, -λ. (A and B) IFN-β and -λ production, measured by ELISA, by SV40 fibroblasts from controls (C), P1, and P2 after 24 hours of VSV (A) or HSV-1 (B) stimulation. Mean values ±SD were calculated from six independent experiments with three different controls. (C) VSV titers, estimated on Vero cells, in SV40 fibroblasts from healthy controls (C), P1, a UNC-93B–/– patient, and a Stat1-deficient (Stat1–/–) patient, at various times after VSV infection with or without 18 hours of pretreatment with IFN-α. Mean values ±SD of two independent experiments with two different controls are shown. (D and E) Live cell percentages, estimated by resazurin oxidation/reduction, for SV40 fibroblasts from a healthy control (C), P1, P2, a UNC-93B–/–, and a Stat-1–/– patient, 24 and 96 hours after infection with various multiplicities of infection of VSV and HSV-1. The cells either were not treated (D), or were subjected to pretreatment (E) for 18 hours with recombinant IFN-α, -β or -λ and with IFN-α, -β or -λ present during infection. Mean values ±SD were calculated for three replicates in each experiment; one representative of three experiments with two different controls is shown.

Impaired response to poly(I:C) stimulation in MDDCs, NK, and CD8 T cells. Monocyte-derived dendritic cells (MDDCs) (24) from P1 and the third sibling of P2 (S3-P2), both heterozygous for the TLR3 mutation, responded more weakly than control cells to poly(I:C) but responded normally to LPS and R-848 in terms of IFN-β, IFN-λ, and IL-12p40 production (Fig. 4A) and CD40, CD80, and CD86 up-regulation (fig. S4A). We tested leukocyte subsets ex vivo to gain further insight into HSE pathogenesis. Unlike purified natural killer (NK) cells from controls (25), the patients' NK cells barely responded to poly(I:C) (Fig. 4B) but responded normally to K562 (Fig. 4B and SOM Text, note 4). Nevertheless, the known patients with inherited NK deficiency were not prone to HSE (9, 26). We did not test γ/δ T cells, but unlike CD8 α/β T cells (27) from controls, cells from P2 and her father, both heterozygous for the P554S mutation, responded weakly to poly(I:C) costimulation (fig. S4C) but normally to costimulation with CD28 (fig. S4C). However, the known CD8- and HLA-I–deficient patients did not present HSE (28). Although affected by the TLR3 mutation, the contribution of NK and CD8 T cells to the pathogenesis of HSE in TLR3-heterozygous children is probably modest.

Fig. 4.

Impaired response to poly(I:C) in MDDCs and NK cells but not in blood DCs and keratinocytes; most viruses trigger IFNs in TLR3 heterozygous blood and fibroblasts (A) IFN-β, -λ, and IL-12p40 production, by MDDCs from controls (C), P1, and a sister of P2 (S3-P2) heterozygous for the P554S mutation. Mean values ±SD were calculated from the data for 12 controls. (B) IFN-γ production, in purified NK cells from five controls (C), P1, and P2, upon stimulation with poly(I:C) or K562 for 24 hours in the presence of IL-12. (C) IFN-λ production in MDCs from eight controls (C) [mean value indicated by (–)] and a sister of P2 (S3-P2) heterozygous for the P554S mutation. (D) IFN-α production, in PDCs from seven controls (C) [mean value indicated by (–)] and S3-P2. (E) IL-6 and IFN-λ production by keratinocytes from controls (C) and P2. Mean values ±SD were calculated for two replicates in each experiment, with two different controls. (F) IFN-α production by PBMCs 24 hours after stimulation with intact viruses. Means ±SD were calculated for the controls (C) from data for six healthy individuals, each tested once, for P1 (tested four times for HSV-1 and VSV and once for the other viruses), and for P2 (tested twice for all the viruses). (G) IFN-β and -λ production, 24 hours after stimulation with intact viruses, in fibroblasts from controls, P1, and a UNC-93B–/– patient. Mean values ±SD were calculated from three independent experiments with two different controls. The production of IFNs and IL-6 was measured by ELISA in (A) to (G).

Response of blood DCs and keratinocytes to poly(I:C) stimulation. Like IRAK-4– and UNC-93B–deficient peripheral blood mononuclear cells (PBMCs) (7, 9), the patients' cells responded normally to poly(I:C) in terms of IFN-α, -β and -λ production (fig. S1, A to C, and fig. S5A). The patients' purified myeloid DCs (MDCs) (24) responded normally to poly(I:C) in terms of IFN-λ production (Fig. 4C). Moreover, IFN-α (Fig. 4D) and -λ (fig. S5B) were produced by poly(I:C)-stimulated purified plasmacytoid DCs (PDCs) from patients and controls, although PDCs are not thought to express TLR3 (24). The lack of clinical HSV-1 dissemination, particularly by the blood, in patients with HSE may therefore be due to the induction of IFNs by MDCs and PDCs stimulated with dsRNA or other viral intermediates (29). HSV-1 also does not spread to epithelia during or following HSE (9). Several epithelial cell types, keratinocytes in particular (30), express TLR3 and respond to poly(I:C). TLR3-heterozygous keratinocytes from P2 did not respond to poly(I:C), as shown by measurements of IL-6 secretion (Fig. 4E). However, they responded to poly(I:C), as shown by IFN-λ (Fig. 4E) and IL-8 (fig. S5C) production. The IFN-λ response of the patients' keratinocytes suggested that the sensing of dsRNA and, possibly, other viral intermediates (29) in epithelial cells prevented the epithelial dissemination of HSV-1 in TLR3-heterozygous patients with HSE. The poly(I:C) responsiveness of DCs and keratinocytes probably operated through TLR3-independent pathways (29), although we cannot exclude the possibility of residual TLR3 signaling or a lack of dominance of the P554S TLR3 mutant in such cells.

Most viruses trigger IFNs in TLR3 heterozygous cells. The lack of other severe viral diseases in TLR3-heterozygous and UNC-93B–deficient patients with HSE is intriguing (9, 31). Our demonstration of poly(I:C) responsiveness in keratinocytes and blood DCs is important because most viruses enter the host via the epithelium, and most forms of human viral encephalitis other than HSE and rabies are blood-borne. We then stimulated the patients' blood cells with 11 viruses (7, 9). TLR3-deficient PBMCs displayed normal production of IFN-α, -β and -λ, and other cytokines in response to the viruses tested (Fig. 4F and fig. S5D). Similarly, cells from IRAK-4–deficient patients showed normal or weak but detectable responses to all viruses (7). Cells from UNC-93B–deficient patients showed impaired, but not abolished, responses to several viruses, including HSV-1 (9). We then tested the responses of the patients' fibroblasts to the six viruses that stimulated IFN-β and -λ production in control fibroblasts. Like IRAK-4–deficient fibroblasts (7), both TLR3-deficient and UNC93-B–deficient fibroblasts responded well to four of the viruses, but unlike the IRAK-4–deficient fibroblasts (7), they responded poorly to HSV-1 and VSV (Fig. 4G). The induction of IFN-α, -β, and -λ in blood cells and fibroblasts from TLR3-heterozygous patients, after stimulation with most of the viruses tested, was consistent with the natural resistance of these patients to most viruses other than HSV-1.

Concluding remarks. After autosomal recessive UNC-93B deficiency (9), autosomal dominant TLR3 deficiency is the second genetic etiology of isolated HSE to be identified. Because Stat-1–deficient (32) patients are also prone to HSE (and other infectious diseases), the molecular pathogenesis of HSE primarily involves impaired TLR3-dependent, IFN-α, -β, and -λ responses. Several lines of evidence also indicate that the pathogenic cellular mechanism underlying HSE in TLR3-heterozygous patients involves an intrinsic defect affecting CNS-resident cells: the neurotropic infection of the CNS by HSV-1, the CNS-restricted clinical course of HSE, the widespread and preferential expression of TLR3 in the CNS, the poly(I:C)–inducible production of antiviral IFNs by blood DCs in TLR3 heterozygotes, and the absence of HSE in patients with conventional primary immunodeficiencies. In addition to revealing the pathogenic mechanism and a basis for both molecular diagnosis and genetic counseling, our findings provide further support for the treatment of HSE patients with IFN-α in addition to acyclovir (9). Interestingly, five of the seven TLR3-deficient individuals and one of the three UNC-93B–deficient individuals did not develop HSE after HSV-1 infection. The incomplete clinical penetrance of TLR3 and UNC-93B deficiency is consistent with the typically sporadic, as opposed to familial, occurrence of HSE (8, 9). Multiple factors may affect clinical penetrance, including age at infection with HSV-1, the viral inoculum, and human modifier genes.

The infection of TLR3-deficient mice with HSV-1 has not yet been reported, but mouse TLR3 appears to be largely redundant in antiviral immunity. TLR3-deficient mice are susceptible to encephalomyocarditis virus (EMCV) (33) and mouse cytomegalovirus (MCMV) (34, 35), at least in some experimental conditions and, to a lesser extent, to respiratory syncytial virus (RSV) (36). However, TLR3-deficient mice have normal resistance to lymphocytic choriomeningitis virus (LCMV), VSV, and reovirus (35). Moreover, TLR3-deficient mice are resistant to influenza A virus (37), West Nile virus (38), and phlebovirus (39). Human TLR3 also appears to be largely redundant for antiviral immunity, as the known TLR3- and UNC-93B–deficient patients have had infections with numerous viruses without developing severe disease (9, 31). Nevertheless, human TLR3 is essential for primary immunity to HSV-1 in the CNS, at least in some circumstances. Our study provides conclusive evidence that an individual TLR can play a nonredundant role in host defense in the setting of a natural ecosystem. Given its ability to recognize dsRNA, human TLR3 may have been of evolutionary importance: Most patients with HSE died until the advent of acyclovir in 1981 (8). As naturally occurring mutations in TLR3 may be dominant negative, it is tempting to speculate that HSV-1 and other neurotropic viruses may have exerted direct selective pressure, driving the maintenance of human TLR3.

Supporting Online Material

www.sciencemag.org/cgi/content/full/317/5844/1522/DC1

Materials and Methods

SOM Text

Figs. S1 to S5

References

References and Notes

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