Yellow fever vaccine YF-17D activates multiple dendritic cell subsets via TLR2, 7, 8, and 9 to stimulate polyvalent immunity

To determine whether YF-17D activates DCs, we first cultured human monocyte-derived DCs [mDCs] with YF-17D (Fig. 1). UV irradiated or heated YF-17D was used as a negative control. These mDCs had a dose-dependent response to YF-17D with increasing multiplicities of infection (MOIs) of virus leading to greater induction of proinflammatory cytokines, including IL-6, TNF-α, MCP-1, and IP-10 (Fig. 1 A). YF-17D also induced both IL-12p40 and IL-12p70 from mDCs, although the amounts induced were lower than with LPS, and induction of IL-12p70 was only apparent when an additional CD40 ligand signal was provided (in the form of a fibroblast cell line, expressing the CD40 ligand signal), consistent with numerous previous studies (e.g., reference 45 and Fig. S1). Stimulation of DCs with CD40 ligand–expressing fibroblasts alone resulted in little or no IL-12p70. Furthermore, YF-17D was also an efficient inducer of the costimulatory molecules CD80 and CD86 (Fig. 1 B). Both UV irradiation and heat treatment for 1 h at 56°C of YF-17D impaired its ability to stimulate cytokines or induce costimulatory molecules on mDCs, although the effects of UV irradiation varied with the cytokine being examined. Thus, there was only a modest effect of UV irradiation on production of IL-10 (Fig. 1) and IL-12p40 (Fig. 2). Therefore, it is possible that induction of IL-10 (Fig. 1) and IL-12p40 (Fig. 2) by YF-17D is not critically dependent on viral replication, and that nonreplicating virions, or non-RNA components such as viral proteins, may mediate this.

To evaluate whether YF-17D infects DCs, human mDCs were exposed to YF-17D and the intracellular expression of nonstructural proteins NS4A and NS4B and evaluated 48 h after infection. As shown by intracellular FACS staining in Fig. S2 and consistent with similar, recently published observations (50), a significant proportion of DCs contain intracellular NS4A and NS4B. Interestingly, enhanced induction of the DC activation marker CD86, relative to mock-infected DCs, appears to occur in all DCs (Fig. S2). Therefore, although productive viral infection induces robust activation of DCs, DCs that are not productively infected also appear to be activated, perhaps as a result of viral entry or surface binding to a PRR or bystander activation.

Plasmacytoid DCs (pDCs) play a key role in many viral infections by producing IFNα, which in turn activates other immune cells and induces an antiviral program in cells. To determine if YF-17D can activate pDCs, pDCs were isolated from human blood and cultured with the virus. Cell culture supernatants were assayed for IFNα. pDCs produced high levels of IFNα in response to an MOI of 1 of the virus and this cytokine production was greatly inhibited by heating the virus to 56°C for 1 h (Fig. 1 C). UV irradiation did not have as much of an effect on reducing the activation of the pDCs.

Given that YF-17D induced potent activation of DCs, we sought to determine the innate immune receptors through which YF-17D mediated its effects. For these studies, we used mouse DCs based on the inherent advantages in using animals deficient in specific genes that might provide insights into mechanism. Splenic CD11c^high DCs from Flt3 ligand–treated mice were cultured in vitro with YF-17D, and 6 h later, the induction costimulatory molecules were evaluated by FACS. As with human DCs, YF-17D induced CD86, CD80, and CD40 on splenic DCs (unpublished data). As previous studies suggest that several viruses can activate DCs via TLRs, we assessed the capacity of YF-17D to activate DCs from various TLR-deficient mice strains.

MyD88 is an adaptor protein that is associated with all TLRs, except TLR3 (36, 51, 52) and that mediates the signal transduction from TLRs. Thus, as a first measure of whether any TLRs are involved in the response to YF-17D, CD11c⁺ DCs from MyD88^−/− mice or wild-type mice were cultured in the presence of live or inactivated virus. As shown in Fig. 2 A, there was a profound impairment in the induction of IL-12p40 and IL-6 by YF-17D in MyD88^−/− DCs, relative to control DCs from wild-type mice. Furthermore, inactivation of the virus by UV irradiation or heating to 56°C for 1 h largely abrogates its ability to induce the cytokine response from the wild-type cells. In the case of murine DCs, we could not detect significant numbers of infected cells, either by FACS analysis of the intracellular expression of nonstructural proteins NS4A and NS4B, or by a PCR-based assay (unpublished data). The reasons for the differences in infection between human (Fig. S2) and murine DCs are not clear. Despite the apparent lack of productive infection of murine DCs, clearly YF-17D does induce robust cytokine production from such cells. The likely explanation for this might be viral entry or surface binding to a PRR.

In addition to MyD88, at least three other adaptor proteins (TIRAP, TRIF, and TRAM) have been described previously (51–57). TIRAP appears only to be associated with TLR2 and 4 (52, 55), whereas TRIF is only associated with TLR3 and 4 (53–56). We cultured splenic CD11c^high DCs from TIRAP^−/− mice with YF-17D. As shown in Fig. 2 B, there was a very significant diminution of both IL-12p40 and IL-6 in response to YF-17D in TIRAP^−/−, relative to wild-type controls. Thus, YF-17D activates DCs through at least two different TLR adaptor proteins, MyD88 and TIRAP.

Next, we determined precisely which TLRs were activated by YF-17D. DCs from wild-type mice, TLR2^−/−, TLR4^−/−, TLR7^−/−, and TLR9^−/− mice were cultured in vitro with YF-17D (Fig. 2, C–F). No difference in IL-12p40 and IL-6 production was observed between the TLR4^−/− and wild-type cultures. This indicates that TLR4 does not play a role in the response to YF-17D. In contrast, TLR2 does play a role, as TLR2^−/− DCs had a greatly impaired production of IL-12p40 and IL-6. This is consistent with recent reports that certain viruses such as measles (58), HCV (59, 60), and LCMV (61) also signal through TLR2. Furthermore, TLR7 also appears to be important as DCs from TLR7^−/− mice display impaired production of IL-12p40 (Fig. 2 F), consistent with the fact that YF-17D is a single-stranded RNA virus and previous observations that TLR7 is a receptor for single-stranded RNA (33–35, 40). However, we could not detect a consistent effect on IL-6 production in TLR 7^−/− mice (unpublished data). The reason for this is at present unclear.

Until recently, TLR9 has been shown to respond only to particular unmethylated CpG DNA motifs found in certain bacteria and viruses (29). Given that YF-17D is an RNA virus, we expected to exclude a role for TLR9 in the vaccine response. Surprisingly, TLR9^−/− DCs had a clear diminution in both IL-12p40 and IL-6, although the induction of these cytokines by YF-17D in this strain and its littermate was weaker than with the other strains, likely due their mixed C57BL/6 × 129 genetic backgrounds. A possible explanation for TLR9 signaling by YF-17D was that there was contaminating DNA from the SW480 cells used to grow the virus. To address this issue, YF-17D or control CpG DNA were pretreated with DNase buffer and with preincubations for 30 min in ice, or at 37°C, or at 37°C in the presence of DNase. pDCs were cultured with these various stimuli and supernatants were assayed for IFN-α (Fig. S3). Incubation at 37°C had no effect on YF-17D and CpG DNA relative to the stimuli on ice (unpublished data). DNase treatment substantially reduced cytokine output from cultures treated with DNase digested CpG DNA, but had no effect on YF-17D, suggesting that the contaminant cellular DNA likely did not play a role in the effects of YF-17D on DCs. This observation is consistent with the recent finding that Newcastle Disease virus, another single-stranded RNA virus, also activates DCs through both TLR7 and TLR9 (62). In addition, as demonstrated recently, certain metabolites such as the hemozoin of malaria parasites may signal through TLR9 (63). Thus, TLR9 may sense not only unmethylated, CpG-rich DNA, but also other microbial or viral components.

In addition to TLR7, TLR8 has also been shown to respond to certain single-stranded RNA viruses such as HIV, human parechovirus 1, and Cocksackie virus B (34, 64, 65). To determine whether YF-17D also signals through TLR8, HEK293 cells stably transfected with human TLR8 and an NFκB-luciferase reporter were cultured with YF-17D or the synthetic TLR7/8 agonist 3M-003. Cell lysates were measured for luciferase activity as a measure of NFκB activation downstream of TLR8 (Fig. 3). After 1 d of culture, an 11-fold increase in luciferase activity was measured from the cells treated with 3M-003, but there was only a modest increase in activity from YF. However, on the second day of culture (after the virus had a chance to begin replication), YF produced an 18-fold increase in luciferase activity. The very slight decrease in the response induced by 3M-003 is likely a reflection of the earlier effect of the compound through the NFκB promoter and decay of the NFκB response, and not decay of the compound itself. The comparatively delayed response by the virus is more likely to be explained by the kinetics of cellular infection and subsequent synthesis of viral components required to stimulate the TLR8–NFκB pathway. Thus, YF-17D appears to activate DCs via multiple TLRs.

Given that YF-17D activates multiple DC subsets via distinct TLRs, we sought to determine the quality of the adaptive immune responses stimulated by this vaccine. We first wanted to ascertain whether DCs were activated at all in vivo. YF-17D or control TLR ligands were injected subcutaneously and, 1 d later, the draining lymph nodes were isolated and the phenotype and activation status of DCs was evaluated by flow cytometry. The costimulatory molecules CD86 and CD40 in addition to the MHC class I molecule I-A^b were all clearly up-regulated when compared with the PBS injection at equivalent levels to that induced by LPS (Fig. 4), although we were unable to detect any substantial up-regulation of CD80.

It has been shown previously that most TLR ligands induce robust Th1 responses (66, 67), but several studies suggest that signaling via TLR 2 results in very weak induction of IL-12p70 in DCs and a bias toward the Th2 or T regulatory pathway (44–49, 68–71). Because YF-17D signaled through TLR2, 7, 8 and 9, it was important to characterize the quality of the T cell response after the DC activation in vivo. For this purpose, we obtained YF-Ova8, which expresses a cytotoxic T lymphocyte epitope derived from chicken ovalbumin (SIINFEKL) (15). These recombinant viruses replicated comparably to the YF-17D vaccine strain in cell culture (unpublished data) and stably expressed the SIINFEKL peptide, and infected cells presented the antigen in the context of MHC class I. YF-Ova8 was injected subcutaneously into Thy1.1⁺ mice that had received 2.5 × 10⁶ OT-I transgenic T cells (Thy 1.2⁺) 1 d earlier; 5 d after vaccination, the cells in the draining lymph nodes were either analyzed directly by flow cytometry or restimulated in vitro with SIINFEKL for T cell proliferation assays and cytokine analysis of cell culture supernatants. YF-Ova8 induced clonal expansion of antigen-specific CD8⁺ T cells, as indicated by the increased frequency of CD8⁺ Thy 1.2⁺ cells (Fig. 5 A). 5 d after vaccination, the draining lymph nodes were isolated, and single cell suspensions were prepared and cultured in vitro with SIINFEKL peptide or in media. 72 h later, the induction of Th1 and Th2 cytokines, IFN-γ (Fig. 5 B) and IL-4, IL-5, IL-13, and IL-10 (Fig. 5 C), in culture was evaluated by ELISA and by intracellular flow cytometry. As indicated in Fig. 5 B, YF-Ova8 induced the production of IFN-γ by CD8⁺ T cells. This cytokine production was largely specific to the SIINFEKL peptide as indicated by much higher frequency of CD8⁺IFN-γ⁺ cells in response to YF-Ova8 relative to immunization with nonrecombinant YF-17D (Fig. 5 B). However, there were still nanograms/ml amounts produced (Fig. 5 B) by cells incubated with media alone (presumably as a result of viral carry over) and the ensuing T cell responses to endogenous YF-17D proteins. In contrast with IFN-γ, the production of the Th2 cytokines IL-4, IL-5, IL-13, and IL-10 did not appear to be specific to OVA, as restimulation with SIINFEKL did not increase their production. This is likely a result of the fact that the OT-1 CD8⁺ transgenic T cells may have an intrinsic bias to secrete IFN-γ and their relatively high frequency in this adoptive transfer system would result in much higher levels of IFN-γ (but not IL-4, IL-5, or IL-13) being secreted. In contrast, the endogenous YF-17D proteins may stimulate specific T cells that produce a mixed Th1/Th2 profile; thus, the bulk of the Th2 cytokines detected in this system may well be produced by such T cells and, thus, be produced independently of SIINFEKL stimulation (Fig. 5 C).

We next sought to determine the contribution that individual TLRs made to the quality of the T cell response induced by YF-17D. Based on previous findings that MyD88^−/− mice show a selective defect in Th1 responses (66), one possibility was that YF-17D signaling through TLRs only resulted in a Th1 response and that the Th2 responses were mediated by some other innate immune receptors. Alternatively, signaling via TLR2 might mediate Th2 or T regulatory responses (44–49, 68–71). To distinguish between these possibilities, wild-type or MyD88^−/− mice were injected subcutaneously with either YF-17D or with supernatant from mock-infected SW-480 cells. 5 or 10 d later, the draining lymph nodes were removed and single cell suspensions from these lymph nodes were cultured in vitro either in media alone or with a mixture of CD4⁺ T cell epitopes and CD8⁺ T cell epitopes that had been previously identified (72). The CD4⁺ T cell epitope is an I-A^b–restricted epitope from the viral envelope protein (residues 231–247 from the envelope protein, LVEFEPPHAATIRVL), whereas the CD8⁺ T cell epitopes are comprised of one subdominant H-2D^b–restricted epitope (residues 1–15 from the E1 envelope protein, AHCIGITDRDFIEGV), and another H-2K^b–restricted dominant epitope mapped to the NS3 protein (residues 261–275 from the NS3 protein, VIDAMCHATLTYRML) (72). After 3 d, the supernatants were assayed for cytokines (IFN-γ, IL-4, IL-5) and intracellular staining of CD8⁺, CD4⁺, and IFN-γ on the cells was performed. As shown in Fig. 6 A, in wild-type mice, YF-17D induced high levels of IFN-γ. This induction occurred even when the cells were cultured in media alone, likely reflecting carry over of viral components that served as antigen for in vitro restimulation. In MyD88^−/− mice, however, there was a profound reduction in IFN-γ levels (Fig. 6 A). These trends were reflected in the intracellular staining assays for IFN-γ⁺ cells shown in Fig. 6 B. Similar trends were also observed with CD4⁺IFN-γ⁺ cells (Fig. 6 C). Thus, as described previously (66), MyD88 appears to be critical for the induction of Th1 and Tc1 responses. Also, in agreement with previous findings, MyD88^−/− mice displayed enhanced induction of IL-4 and IL-5 (unpublished data).

Next, we evaluated immune responses in TLR2^−/− mice. The experiments were performed exactly as described in the previous paragraph with MyD88^−/− mice. In brief, we immunized wild-type or TLR2^−/− mice subcutaneously with either YF-17D or with supernatant from mock-infected SW-480 cells. 5 or 10 d later, the draining lymph nodes were removed, and single cell suspensions from these lymph nodes were cultured in vitro, either in media alone or with a mixture of CD4⁺ T cell epitopes and CD8⁺ T cell epitopes, which had been previously identified as described in the previous paragraph (72). After 3 d, the supernatants were assayed for cytokines (IFN-γ, IL-4, IL-5) and intracellular staining of CD8⁺, CD4⁺, and IFN-γ on the cells was performed. As shown in Fig. 7 A, the frequency of CD8⁺IFN-γ⁺ T cells in wild-type mice at day 10 is 1.05%. However, at this time point, the TLR2^−/− mice contained 3.63%. A similar trend was observed at day 5. Furthermore, in the case of CD4⁺IFN-γ⁺ T cells (Fig. 7 B), at day 5 after immunization, the response in TLR2^−/− mice appeared to be markedly higher than in wild-type mice. However, by day 10, the CD4⁺IFN-γ⁺ response appeared to have subsided, and no differences were apparent. This suggests that signaling through TLR 2 may exert an inhibitory effect on the induction of CD4⁺IFN-γ⁺ or CD8⁺ IFN-γ⁺ cells in response to YF-17D. These results are consistent with the enhanced secretion of IFN-γ in TLR2 knockout splenocytes, relative to wild-type splenocytes as evaluated by ELISA (Fig. S4). These results are consistent with previous findings that TLR2 signaling induces Th2 or T regulatory responses (26, 44–49, 68–71). Interestingly, in the case of the Th2 cytokines IL-4 and IL-5, there appeared to be a modest decrease in TLR 2^−/− mice (unpublished data). Collectively, these data suggest that TLR2 might regulate the induction of Th1/Th2 balance in response to YF-17D.

The data presented here, together with that reported recently by Barba-Spaeth et al. (50), offer some insights into the mechanism of action of YF-17D, one of the most effective vaccines available. In particular, our data suggest that YF-17D activates DCs via multiple TLRs, including TLR2, 7, 8 and 9, and that signaling via distinct TLRs exerts differential effects on the quality of the antigen-specific T cell response induced by YF-17D. Whether other TLRs, particularly TLR3, which is a receptor for double-stranded RNA (36), are also involved in YF-17D recognition is at present unclear.

The biological significance of activation of several TLRs is highlighted by two intriguing aspects of the data. First, the absence of a single TLR appears to result in a significant impairment of IL-12p40 and IL-6 (Fig. 2). This is surprising because it might have been expected that other TLRs would compensate for this deficiency. One explanation for this observation is that the TLRs signal in a synergistic manner, and that YF-17D contains suboptimal amounts of individual TLR ligands, which by themselves stimulate suboptimal responses, but which can signal in concert, to produce a synergistic effect. This hypothesis is consistent with two recent reports that suggest that selected TLR combinations can indeed synergistically trigger a Th1 polarizing program in human DCs (73, 74). In the case of YF-17D, whether such synergy might occur by triggering multiple TLRs on a single DC subset, by triggering multiple TLRs on distinct DC subsets, or by both mechanisms is yet to be determined. A second intriguing aspect to the data is that signaling via distinct TLRs appear to differentially bias the Th1/Th2 balance. Thus, eliminating signaling via MyD88 impairs Th1 responses, whereas eliminating TLR2 signaling enhances Th1 responses (Figs. 5 and 6). This is consistent with emerging data that distinct TLRs may differentially affect the Th1/Th2 balance (44–49, 68–71). Therefore, vaccines that target multiple TLRs might facilitate both immune synergy as well as polyvalent immune responses to generate broad-based protective immunity. In this context, a recent study suggests that conjugating HIV Gag protein to a TLR7/8 agonist results in activation of both myeloid and pDCs, and enhances the magnitude and quality of Th1 and CD8⁺ T cell responses in nonhuman primates (75).

The question of which types of immune responses offer protection against challenge with the pathogenic strain of yellow fever virus is of considerable interest. This was not addressed in the present study, primarily because yellow fever appears to be rather host (primate) restricted and mice are not very susceptible. Even immunosuppressed mice appear to be relatively poor hosts. In fact, several investigators appear to have used nonhuman primates for their experiments with yellow fever and chimeric yellow fever viruses (6–15). However, it is known that YF-17D does kill mice after intracerebral challenge (9), but the relevance of such a model to yellow fever infection in humans is questionable. These issues notwithstanding, one might speculate on which types of responses confer protection against yellow fever. Though neutralizing antibody titers are thought to be important, a role for cytotoxic T cell responses has also been suggested (5). However, what influence the Th1/Th2 balance might have on protection is unknown. Because Th1 versus Th2 cytokines are thought to favor the development of cytotoxic T cells versus antibodies, respectively, it is conceivable that both Th1 and Th2 responses are important for protection. Thus, intracerebral infection of MyD88 knockout mice or TLR2 knockout mice might have both resulted in impaired survival of the hosts as a result of perturbed Th1/Th2 balances.

Finally, it is also important to address the question of precisely which viral components act through which innate immune receptors. In this context, it is important to note that live viral vaccines contain not only viral proteins and nucleic acids, but also cellular contaminants derived from the cell lines in which the vaccines were grown. Such cellular contaminants (Janeway's “dirty little secrets” [reference 76] or Matzinger's “danger signals” [reference 77]), may well play important roles in the induction and modulation of vaccine induced immune responses. Thus, the chicken embryos and cell lines in which YF-17D are grown are potential sources of these dirty little secrets or danger signals. In this context, avian retroviral proteins, ovalbumin, and chicken DNA are all found in YF-17D preparations for human use (78). It is thus likely that these factors and other nonviral components of the YF-17D vaccine, such as heat shock proteins and uric acid, contribute to the induction of an immune response. Both heat shock proteins and uric acid are released from stressed cells and are potent activators of DCs and monocytes (for review see reference 79). Thus, future vaccinologists should not only concern themselves with using the right combination of adjuvants but also having vaccine preparations that are “clean,” but which recapitulate the immunogenicity of the “dirty” vaccines. Furthermore, whatever the source of the molecules that stimulate a given TLR or PRR, clearly further work is required to determine the specific combinations of PRRs (the correct “code” of innate immune buttons) that promote a particular facet of the immune response, such Th1/Th2 balance, neutralizing antibody responses, long-lived antibody-producing cells that home to mucosal tissues and continuously secrete high-affinity neutralizing antibody, and long-lived memory T cells.

In conclusion, the present data enhance our understanding of the molecular mechanisms of action of YF-17D and highlight the potential of vaccination strategies that use combinations of different TLR ligands to stimulate polyvalent and synergistic immune responses. The present approach of determining the TLRs that YF-17D signals through could be used to deconstruct the immunological basis for the efficacy of other successful vaccines. It is likely that many of these vaccines, which consist of live attenuated viruses or bacteria, may well signal through multiple TLRs, as well as other non-TLRs such as RIG-1 (62). Conversely, it conceivable that “poor” vaccines, which require repetitive boosts to generate robust protective responses, do not trigger TLRs at all or even inhibit TLR signaling. A common method used in the construction of many developing vaccines is to use a single adjuvant, such as CpG DNA, in combination with an antigen. However, such vaccines maybe limited in the quantity and quality of the immune response generated and, therefore, may not provide the most effective prevention or treatment possible. Thus, future vaccine strategies aimed at incorporating multiple TLR ligands and antigens into delivery systems such as nanoparticles, which can target specific DC subsets in vivo, is likely to be of great benefit in conferring the degree of immunogenicity and protection mediated by our best vaccines such as the yellow fever vaccine YF-17D.

Mutant mice (MyD88^−/−, TIRAP^−/−, TLR2^−/−, TLR4^−/−, TLR7^−/−) were provided by S. Akira (Osaka University, Osaka, Japan) and were either in the C57BL/6 background or in a mixed C57BL/6 × 129 background (backcrossed at least five times to C57BL/6). C3H/HeJ and C3H/HeN were purchased from The Jackson Laboratory and Taconic Farms, respectively. Spleens from TLR 9^−/− mice on the mixed C57BL/6 × 129 background were provided by R. Medzhitov (Yale University School of Medicine, New Haven, CT). In each case, the appropriate littermate control was used. All mutant mice and controls were sex- and age-matched and between 6 and 16 wk old. For adoptive transfer studies, OT-1 TCR transgenic mice and B6.PL mice were purchased from The Jackson Laboratory and bred at the Yerkes Vivarium. B6.PL recipients were injected i.v. with 2.5 × 10⁶ OT-1 TCR transgenic T cells. All animal studies were approved by the Institutional Animal Care and Use Committee of Emory University.

YF-17D subpassaged from YF-VAX (Aventis Pasteur) in SW-480 cells was a gift from R. Ahmed (Emory University, Atlanta, GA), and YF-Ova8 (encoding the SIINFEKL peptide) and YF-FL were gifts from R. Andino (University of California, San Francisco, CA) (15). Viruses were passaged in SW-480 cells in DMEM + 10% FBS + penicillin/streptomycin. Cell culture supernatants were collected ∼6 d after infection when ∼20% cytopathic effect was noted. Supernatants were clarified by centrifugation twice at 750 g for a total of 20 min. This crude virus stock was purified further, as follows: sucrose purified virus was generated by centrifuging the virus through a PBS + 35% sucrose + 10 μM Tris cushion at 100,000 g for 2 h. The viral pellet was resuspended in PBS and frozen at −80°C in aliquots. Viral titers were calculated by plaque assay using Vero cells. Virus was inactivated by either incubating at 56°C for 1 h or UV irradiated with 120 mJ/cm² for 5 min.

Purified E. coli was a gift from T. van Dyke (Boston University, Boston, MA). CpG A (ODN 2336) and CpG B (ODN 2006) DNA was purchased from Coley Pharmaceutical. Pam-3-cys was obtained from EMC Microcollections. 3M-003, a proprietary TLR7/8 agonist was a gift from K. Gorden (3M Corporation, St. Paul, MN).

CD11c⁺ DCs were purified from the spleens of Flt-3L–injected mice. Mice were injected with 20 μg Flt-3L per day for nine consecutive days. On the 10th day, spleens were digested with Collagenase, Type IV (1 mg/ml; Worthington Biochemical) in complete DMEM + 2% FBS for 30 min at 37°C. Cells were washed 2× with PBS + EDTA + FBS and cell cultures of >95% CD11c⁺ DC purity were established after enrichment of splenocytes with CD11c⁺ microbeads (Miltenyi Biotec).

Human mDCs were generated from apheresis samples of healthy donors. PBMCs were plated at 10 × 10⁶ cells/well in six-well plates. After 2 h, nonadherent cells were removed and the adherent monocytes were cultured in RPMI 1640 + 10% FBS + 50 μg/ml GM-CSF + 10 μg/ml IL-4 (PeproTech) for 6 d. After this time, the nonadherent DCs were collected, washed, and used for experiments. Human pDCs were enriched from PBMCs using BDCA-2 microbeads (Miltenyi Biotec).

The mDCs, pDCs, and mouse CD11c⁺ DCs were plated at 10⁶ cells/ml in 48-well culture dishes and incubated with the stimuli under humid conditions at 5% CO₂ and 37°C. The human DCs were cultured in RPMI 1640 + 10% FBS + pen/strep. Human IL-3 (PeproTech) was added for the pDCs. Mouse DCs were cultured in complete DMEM + 10% FBS. Costimulatory molecule expression was analyzed by flow cytometry after 48 h for human DCs. Alternatively, the supernatants were analyzed after 48 h for cytokines.

Cells were washed in staining medium and stained for surface CD86 for 30 min, 0°C. Subsequently cells were washed twice then fixed and permeabilized using a BD Biosciences cytofix/perm reagent kit following the manufacturer's instructions. A rabbit polyclonal antisera that recognizes the nonstructural proteins NS4A and NS4B (C. Rice, The Rockefeller University, New York, NY) was used to detect intracellular virus (30 min, 0°C). Next, the cells were washed twice to remove unbound antibody and stained with allophycocyanin-labeled anti–rabbit secondary antibody for an additional 30 min at 0°C followed by washing. Data was acquired on FACSCalibur and analyzed using Flowjo analysis software.

C57BL/6 mice were injected subcutaneous with either PBS alone, 50 μg Pam-3-cys, 25 μg E. coli LPS, 50 μg CpG B, 2 μg 3M-003, or 10⁶ PFU YF-17D. After 1 d, the draining popliteal and inguinal lymph nodes were dissected and the DCs were isolated with collagenase, type IV digestion. The cells were stained and analyzed by flow cytometry for costimulatory molecule expression. B6.PL (Thy 1.1⁺) mice reconstituted with OT-1 TCR transgenic T cells (Thy 1.2⁺) were injected subcutaneously with 50 μg of MHC class I–restricted OVA peptide (SIINFEKL; OVA257-264; BioSynthesis) with 25 μg E. coli LPS or 10⁶ PFU of YF-FL or YF-Ova8. After 4 d, the cells from the draining popliteal and inguinal lymph nodes were subjected to assays as described in the T cell assays section.

Infection assays were performed as described previously by Barba-Spaeth et al. (50). In brief, DCs were washed in RPMI 1640 and cultured with YF-17D for 1 h at 37°C. The infection was quenched with 5% pooled human serum and the cells were washed extensively to remove excess virus. After 1 h of infection, DCs were resuspended in conditioned media and incubated for 24 h before monitoring for infection. Surface staining was done in serum containing media at 4°C. Antibodies were obtained from BD Biosciences. Cytoperm/CytoFix Kit (BD Biosciences) was used for fixation and permeabilization. C12 is a rabbit polyclonal antisera that recognizes the nonstructural proteins NS4A and NS4B, and was a gift from C. Rice (50). Secondary antibodies used were PE (Jackson ImmunoResearch Laboratories) or allophycocyanin (Invitrogen).

Isolated lymph node cells from injected mice were either stained directly ex vivo and analyzed by flow cytometry for T cell clonal expansion, or restimulated in vitro. Cells were plated at 5 × 10⁵ cells/well in 96-well plates and cultured in complete DMEM + 10% FBS alone or with various concentrations of MHC class I–restricted OVA SIINFEKL peptide, or an I-A^b–restricted epitope from the viral envelope protein (residues 231–247 from the envelope protein, LVEFEPPHAATIRVL), or an H-2D^b–restricted epitope (residues 1–15 from the E1 envelope protein, AHCIGITDRDFIEGV), or an H-2K^b–restricted dominant epitope mapped to the NS3 protein (residues 261–275 from the NS3 protein, VIDAMCHATLTYRML) (72), or a combination of these epitopes. On the third day, the wells for in vitro proliferation assays had 1 μCi of [³H]thymidine added to them. On the fourth day, supernatants were collected for cytokine measurement, or the cultures were frozen at −20°C to lyse the cells for the measurement of thymidine incorporation.

For the mouse cytokines, the following kits were used: IL-4 and IFN-γ were obtained from eBioscience; IL-5, IL-6, IL-10, and IL-12p40 were obtained from BD Biosciences; and IL-13 was obtained from R&D Systems. Human IL-6, TNF-α, IL-10, IP-10, and MCP-1 were all measured using kits obtained from BD Bioscience. IFN-α was measured with the kit obtained from Biosource.

The HEK293 cells stably transfected with human TLR8 and an NFκB driven luciferase reporter were a gift from 3M Pharmaceuticals. Cells were plated at 4 × 10⁴ cells per well in 96-well plates with DMEM + 10% FBS + pen/strep in the evening. 18 h later, the cells were stimulated with 10 μM of 3M-003, 4 × 10³ PFU of YF-17D, or left in media alone. After 24 or 48 h of stimulation, the luciferase activity of the cells was assayed using the Luciferase Assay System (Promega).

YF-17D induces IL-12p40 and IL-12p70 in both human mDCs (Fig. S1, A and B) and murine splenic CD11c+ DCs (Fig. S1 C). In Fig. S2, YF-17D productively infects human mDCs. Immature human mDCs were exposed to YF-17D, and 48 h later the DCs were harvested stained for intracellular flow cytometric analysis of NS4A and NS4B. Fig. S3 shows that cellular DNA does not contribute to the immune stimulatory effects of YF-17D. Fig. S4 depicts TLR2 exerting an inhibitory effect on Th1 responses induced by IFN-γ.

We would like to thank A. Krieg and members of our lab for discussion and comments on the manuscript.

This work was supported by grants from the National Institutes of Health, nos. U19 AI057266, R01 AI048638, R01 AI056499, R01 DK057665, R21 AI056957, and U54 AI057157.

The authors have no conflicting financial interests.