Lymphocytic choriomeningitis virus (LCMV) exhibits natural tropism for dendritic cells and represents the prototypic infection that elicits protective CD8+ T cell (cytotoxic T lymphocyte (CTL)) immunity. Here we have harnessed the immunobiology of this arenavirus for vaccine delivery. By using producer cells constitutively synthesizing the viral glycoprotein (GP), it was possible to replace the gene encoding LCMV GP with vaccine antigens to create replication-defective vaccine vectors. These rLCMV vaccines elicited CTL responses that were equivalent to or greater than those elicited by recombinant adenovirus 5 or recombinant vaccinia virus in their magnitude and cytokine profiles, and they exhibited more effective protection in several models. In contrast to recombinant adenovirus 5, rLCMV failed to elicit vector-specific antibody immunity, which facilitated re-administration of the same vector for booster vaccination. In addition, rLCMV elicited T helper type 1 CD4+ T cell responses and protective neutralizing antibodies to vaccine antigens. These features, together with low seroprevalence in humans, suggest that rLCMV may show utility as a vaccine platform against infectious diseases and cancer.
Vaccines represent one of the most successful interventions in modern medicine, having led to the control of many devastating infectious diseases and recently also to the prevention of cervical cancer. Recombinant DNA technology and bioengineering have made it possible to exploit viral vectors for optimized vaccine delivery. Attenuated or replication-incompetent viruses such as modified vaccinia virus Ankara and recombinant adenovirus 5 are genetically modified to express a vaccine antigen of interest.
Many vectors have limitations, and their ability to counter infection by HIV, hepatitis C virus and tuberculosis or treat tumors remains uncertain. The induction of protective and long-lived cytotoxic T lymphocytes (CTLs) is an unmet yet important goal of vaccination against many of these diseases, which have a considerable effect on human health. Poxvirus-based vectors, for example, effectively induce multifunctional CTL responses1, but they exhibit a limited ability to elicit CTL responses of high magnitude2. Conversely, recombinant adenovirus (rAd)-based vaccines stimulate high-frequency responses that tend to be less multifunctional3. Moreover, a significant proportion of the global population carries adenovirus 5–neutralizing antibodies from natural infection, which can affect vector immunogenicity4,5. Even in the absence of preexisting immunity, vaccination with rAd- or poxvirus-based vaccines elicits potent vector-specific antibody immunity, which interferes with homologous boosting5. Thus, there remains a need to develop viral vectors that elicit effective T cell immunity without concomitant induction of antibodies that block vector re-administration.
The prototypic arenavirus lymphocytic choriomeningitis virus (LCMV) contains a bisegmented negative-strand RNA genome encoding the viral proteins glycoprotein (LCMV-GP), nucleoprotein (NP), Z and L in an ambisense strategy6 (Fig. 1a). LCMV-GP mediates receptor binding and cell entry and represents the only target for LCMV-neutralizing antibodies6. LCMV-induced T cell responses are broad and long-lived7, and LCMV infection has been widely studied as a model of CTL-mediated protection. The neutralizing antibody response to LCMV is extraordinarily weak, and convalescent serum fails to prevent re-infection6,8. These characteristics suggested that modified LCMV might serve as a vector for the induction of CTL immunity. Recently, it has become possible to manipulate the LCMV genome by recombinant cDNA technology9,10. Here we report on a molecular strategy for rendering the virus replication incompetent to confer an acceptable safety profile while allowing the incorporation of diverse antigens that can confer protection against infections and cancers.
Generation of replication-defective rLCMV vectors
To generate replication-deficient LCMV (rLCMV) vectors, we hypothesized that the viral GP open reading frame could be replaced by a gene encoding a vaccine antigen (Fig. 1a). We generated rLCMV vectors in which GP was deleted using a four-plasmid co-transfection system previously used to generate wild-type LCMV10. The short (S) and long (L) vector RNA genome segments were expressed intracellularly from plasmid expression vectors under control of an RNA polymerase I promoter and terminator (Fig. 1b). The minimal viral trans-acting factors (NP and L) were co-expressed from an RNA polymerase II promoter in additional plasmids (Fig. 1b). We used these four plasmids for transient transfection of BHK-21 cells stably transfected with an LCMV-GP expression vector ('producer cells'; Fig. 1c). In these cells, the GP-deficient viral genomes were complemented in trans and gave rise to vectors whose RNA could be amplified and expressed in target cells, but they could not give rise to a spreading virus and propagate infection.
To confirm expression of the heterologous gene, we generated an rLCMV with the green fluorescent protein (GFP) reporter gene in place of LCMV-GP (rLCMV-GFP). Infection of normal BHK-21 or 293T cells with rLCMV-GFP yielded individual fluorescent cells that did not increase in number over time, whereas passage of GP-expressing BHK-21 or 293T producer cells yielded expanding fluorescent foci indicative of viral propagation (Fig. 1d and data not shown). This finding suggested that rLCMV particles formed in normal cells were GP deficient and replication incompetent, as expected. The growth curves of rLCMV-GFP confirmed the presence of vector in the supernatants of producer cells but not those of normal cells (Fig. 1e). In C57BL/6 mice inoculated intravenously with rLCMV-GFP, viral RNA copies in spleen declined rapidly and early, and within 21 d, they approached the limit of detection (Fig. 1f). To determine whether this vector induced disease in the central nervous system, we injected an rLCMV vector expressing ovalbumin (rLCMV-OVA) intracerebrally. This vector failed to elicit clinical signs of choriomeningitis, whereas wild-type LCMV uniformly caused fatal disease (Fig. 1g). Mice with a combined genetic deficiency in type I and type II interferon receptors (Ifnar1−/−Ifngr−/−; called 'Ifnagr−/−' here) are uniquely permissive for LCMV, and Ifnagr−/− mice have therefore been used to detect very low-level LCMV replication11. We inoculated Ifnagr−/− mice with rLCMV-GFP and killed them 2, 7 or 21 d later. We sampled spleen, liver, lung, kidney and brain tissues without detecting infectivity at any time point (Supplementary Fig. 1a), which further documented that the rLCMV vectors were replication incompetent in vivo. The rLCMV vector also did not inhibit CTL or antibody responses to vesicular stomatitis virus (VSV; Supplementary Fig. 1b), which indicated that rLCMV vectors did not adversely affect general immunocompetence.
rLCMV vectors elicit potent CD8+ T cell responses
To characterize the immunogenicity of proteins encoded by rLCMV, we injected increasing doses of rLCMV-OVA or rAd vector expressing OVA (rAd-OVA) into C57BL/6 mice and assessed CD8+ T cell frequencies specific for OVA (SIINFEKL epitope) in the peripheral blood after 28 d. At lower vector doses of 3 × 102 or 3 × 104 plaque-forming units (PFU), rLCMV-OVA elicited higher frequencies of specific CD8+ T cells than did rAd-OVA, whereas at higher doses of 3 × 105 or 3 × 107 PFU, the responses were similar (Fig. 2a). A further increase in dose was technically possible only for rAd-OVA and resulted in exhaustion of T cell responses (Fig. 2a, 2.5 × 108 PFU), similar to previous reports12. An rLCMV vector expressing the HLA-A2.1-restricted CD8+ T cell epitope MelanA26–35(27L) (rLCMV–MelanA26–35(27L)) stimulated vigorous responses in HLA-A2.1-transgenic mice (Supplementary Fig. 2), which demonstrated that rLCMV can trigger responses of a clinically relevant specificity. The route of vector administration may affect immune responses. We used an intravenous route of immunization here, but responses of similar magnitude have been observed after intradermal, subcutaneous, intramuscular or intraperitoneal administration of rLCMV vectors (Supplementary Fig. 3 and data not shown). CTL induction by rLCMV-OVA was abolished by ultraviolet irradiation of vector (data not shown), which indicated that its immunogenicity depended on gene expression in vivo.
When rLCMV- and rAd-induced CTL responses were boosted with homologous vector on day 38, rLCMV-OVA elicited significantly higher specific CD8+ T cell frequencies than did rAd-OVA at all doses (Fig. 2b). The relative increase in specific CD8+ T cell frequency after boosting was particularly evident at lower doses but was also observed at standard doses and was higher for rLCMV-OVA than for rAd-OVA (rLCMV-OVA, 2.46-fold ± 0.54-fold; rAd-OVA, 1.58-fold ± 0.33-fold (mean ± s.d. of three experiments); P < 0.001; data not shown). Furthermore, we found that three administrations of rLCMV-OVA at monthly intervals maintained OVA-specific CD8+ T cell frequencies at ∼3–4% of total CD8 T+ cells 276 d after the final immunization (Supplementary Fig. 4a). We established the functionality of such memory cells in an in vivo cytotoxicity assay on day 168 after the third immunization. Transfusion of syngenic splenocytes incubated with the OVA-derived CTL peptide SIINFEKL resulted in almost complete rejection of these cells within 24 h, whereas control cells without peptide persisted in the circulation (Supplementary Fig. 4b). More than 80% of rLCMV-OVA-induced memory CTLs had high expression of the activation marker CD44. About half were KLRG-1+, 40% were positive for the interleukin 7 (IL-7) receptor (CD127+) and 15% were CD62L+ central memory cells 45 d after a single immunization (Supplementary Fig. 2c). By day 196 after boosting, over 90% had become positive for the IL-7 receptor, and the fraction of CD62L+ central memory cells had increased to slightly over 30%.
Unlike antibodies to adenovirus 5 (ref. 5), antibodies to LCMV have a limited capacity to prevent reinfection6,8, a property that could have explained the superior performance of rLCMV-OVA in homologous prime-boost immunizations (Fig. 2b). To test this hypothesis, we passively transferred serum from rLCMV-OVA-immunized mice into naive mice. After subsequent immunization with rLCMV-OVA, the CD8+ T cell response was similar to or only moderately lower than that of control mice that received naive serum (Fig. 2c). In contrast, passive transfer of rAd-OVA-immune serum markedly decreased the specific CD8+ T cell response after rAd-OVA immunization, consistent with previous studies of preexisting immunity to adenovirus 5 (ref. 5). We obtained analogous results with immune serum collected 100 d after the last of three monthly immunizations with rLCMV-OVA or rAd-OVA (Supplementary Fig. 5), which confirmed that antibodies with the capacity to block rLCMV vector immunogenicity were inefficiently induced.
To evaluate the functionality of rLCMV-induced CTLs, we measured OVA-specific interferon-γ (IFN-γ)-secreting CD8+ T cells and CD8+ T cells producing both IFN-γ and tumor necrosis factor-α (TNF-α) in the spleen. We found that rLCMV-OVA elicited responses at higher frequencies than did immunization with rAd-OVA or recombinant vaccinia virus expressing OVA (VACC-OVA, Fig. 2d), which attested to the quality of rLCMV-induced CTLs.
Induction of CD4+ T cells and protective antibodies
To examine CD4+ T cells and antibody responses, we generated an rLCMV vector expressing a defective form of the VSV G envelope glycoprotein (rLCMV-INDG61), in which the immunodominant I-Ab-restricted epitope of LCMV-GP (GP61) was inserted in the ectodomain of the VSV G envelope glycoprotein. We labeled transgenic CD4+ T cells specific for GP61 (SMARTA1 T cells13) with the fluorescent dye CFSE and transferred the cells into naive C57BL/6 recipients. Administration of rLCMV-INDG61 stimulated rapid cell division evident in the dilution of CFSE on 98% of the SMARTA1 CD4+ T cells within 3 d of vaccination (Fig. 3a). Similarly, adoptively transferred GP33-specific CD8+ T cells from T cell receptor (TCR)-transgenic mice underwent rapid cell division after immunization with rLCMV (Supplementary Fig. 6). After initial population expansion, rLCMV-INDG61-activated SMARTA1 T cells slowly decreased in frequency during the observation period of 2 months, similar to CD4+ T cells after infection with wild-type LCMV7,13 (Fig. 3b). When SMARTA1 CD4+ T cells were restimulated 9 d after rLCMV-INDG61 vaccination, >95% of the cells synthesized TNF-α and many also co-expressed IFN-γ (Fig. 3c, left), whereas secretion of IL-4 and IL-10 was minimally detectable (Fig. 3c, right), indicative of T helper type 1 polarization in rLCMV-triggered CD4+ T cell responses13.
Immunization with rLCMV-INDG61 also stimulated a potent neutralizing antibody response to VSV that reached titers of ∼1:10,000 within 4 d (Fig. 3d). Isotype class switching to immunoglobulin G was evident 7 d after vaccination, which reflected efficient CD4+ T cell help. Titers in the range of 1:5,000 were maintained throughout the observation period of 54 d, which demonstrated the durability of this antibody response after rLCMV vaccination. We confirmed the protective capacity of rLCMV-induced antibodies in mice deficient in type I interferon receptors. Immunization with rLCMV-INDG61 protected these mice against challenge with 2 × 106 PFU VSV (>10,000-fold the 50% lethal dose14), whereas non-immune controls rapidly developed terminal myeloencephalitis (Fig. 3e).
Efficacy and longevity of rLCMV-induced CTL responses
We next examined the protective capacity of rLCMV-induced CTL immunity. We vaccinated C57BL/6 mice with rLCMV-OVA, rAd-OVA or VACC-OVA, challenged them with recombinant Listeria monocytogenes expressing OVA (rLM-OVA15) on day 16 after immunization and measured bacterial titers in the liver 3 d later16. Immunization with rLCMV-OVA or rAd-OVA resulted in bacterial titers that were nearly undetectable. In contrast, immunization with VACC-OVA failed to confer protection (Fig. 4a). When we challenged the mice 58 d after a single vaccination or 200 d after prime-boost immunization, we obtained similar results, which confirmed the durability of protection of rLCMV-OVA and rAd-OVA. This protection was produced in a dose-response manner. When we challenged the mice either 18 d after single immunization or 200 d after prime-boost vaccination, rLCMV-OVA afforded antibacterial protection at doses 30- to 1,000-fold lower than those of rAd-OVA (Supplementary Fig. 7a–b).
Next we assessed the cytolytic efficacy of rLCMV-, rAd- and VACC-induced CTLs in solid tissues. RIP-OVA mice express OVA antigen in pancreatic islet cells17 and exhibit central tolerance to OVA, but adoptively transferred OVA-specific TCR-transgenic CD8+ T cells (OT-I cells18) can destroy pancreatic beta cells and cause diabetes if appropriately stimulated by OVA-specific vaccination. We gave RIP-OVA mice 1 × 103 OT-I splenocytes (∼1 × 102 OVA-specific CD8+ T cells) and then immunized the mice with rLCMV-OVA, rAd-OVA or VACC-OVA (Fig. 4b). In two independent experiments, rLCMV-OVA-immunized mice uniformly exhibited loss of glucose control (nine of nine mice), whereas VACC-OVA-immunized mice (one of six mice) and rAd-OVA-immunized mice (none of six mice) remained mostly unaffected. This finding demonstrated that rLCMV was more effective than rAd and VACC in stimulating specific CTLs that destroyed antigen-expressing cells in solid tissue.
To test the capacity of rLCMV vectors to promote CTL-mediated rejection of peripheral solid tumors, we injected B16.F10 melanoma cells expressing the CTL epitope GP33 subcutaneously into the flank of C57BL/6 mice19. Eight days later, tumor masses were palpable, and we treated mice with rLCMV-, rAd- or VACC-based vectors expressing the GP33 epitope (rLCMV-GP33, rAd-GP33 or VACC-GP33, respectively) and used rLCMV-OVA as a negative control. Within 8 d of injection, the tumor masses were significantly smaller in rLCMV-GP33-treated mice than in all other groups (Fig. 4c, top). Further, all 11 rLCMV-GP33-treated mice survived until day 22 (14 d after immunotherapy; termination of the experiment), with tumors shrinking or stabilizing. In contrast, most mice vaccinated with rAd-GP33 or VACC-GP33 or with the rLCMV-OVA control had died or reached the endpoint criteria of tumor volume (Fig. 4c, bottom).
We used a vaccinia virus challenge to assess the ability of rLCMV to confer antiviral protection. We immunized C57BL/6 mice with increasing doses of rLCMV-GP33 or rAd-GP33. Then, 18 d later, we challenged the mice intraperitoneally with the recombinant vaccinia virus VACC-G2 expressing full-length LCMV-GP (containing GP33) and measured VACC-G2 titers in the ovaries 6 d after challenge. Even at the lowest vaccine dose, VACC-G2 titers in rLCMV-GP33-immunized mice were three orders of magnitude lower than those of non-immune control mice (Fig. 4d). Vaccination with rAd-GP33 also conferred protection but required doses of ≥3 × 105 PFU, 1000-fold higher than the minimal protective dose of rLCMV-GP33.
rLCMV vectors target and activate dendritic cells in vivo
The targeting and activation of dendritic cells (DCs) is key for CTL induction20,21, and wild-type LCMV exhibits tropism for DCs22. To understand the mechanism by which rLCMV vectors might elicit adaptive immune responses, we studied the cellular tropism of an rLCMV expressing Cre recombinase (rLCMV-Cre). After injection of rLCMV-Cre into transgenic reporter mice23, Cre-mediated removal of a loxP-flanked transcription stop signal allowed expression of an actin promoter-driven GFP. Flow cytometry of GFP+ cells identified about 5 × 103 rLCMV-Cre-infected DCs per spleen, in contrast to around 200 fluorescent macrophages, T cells and B cells (Fig. 5a). This indicated that rLCMV vectors showed a tropism for DCs, similar to wild-type LCMV22. DCs infected with rLCMV-Cre (GFP+) exhibited higher surface levels of CD86 than did uninfected (GFP−) DCs in the same mice (Fig. 5b; mean fluorescence indices, 15.5 ± 2.7 (GFP+) versus 5.3 ± 0.4 (GFP−); P < 0.001), and the latter were similar to DCs in mice that received rLCMV-OVA control (mean fluorescence index, 4.6 ± 0.2; P = 0.14), which suggested that rLCMV vectors activated mainly infected DCs. To analyze DC activation by rLCMV further, we used the transgenic mouse model ST33 (ref. 21), which expresses GP33 after intracellular expression of Cre. Expression of GP33 in resting ST33 DCs triggers specific CD8+ T cell tolerance, whereas GP33 expression in activated DCs results in CD8+ T cell priming21. Administration of rLCMV-Cre in ST33 mice resulted in 0.8% GP33-specific CD8+ T cells on day 10 and day 27, and this was absent in ST33 mice inoculated with rLCMV-OVA (Fig. 5c). Subsequent challenge with VACC-G2 triggered a rapid population expansion of the GP33-specific CTLs that produced IFN-γ upon in vitro restimulation. These data confirmed that rLCMV not only targeted DCs but also functionally activated them in vivo.
When rLCMV vectors were incubated with human peripheral blood mononuclear cells (PBMCs) in vitro, they infected over 60% of myeloid DCs, plasmacytoid DCs and monocytes, compared with less than 2% of B cells, CD4+ and CD8+ T cells (Supplementary Fig. 8a), which resembled the vector tropism in mice (Fig. 5a). Infection of human myeloid DCs also increased expression of the activation marker CD86 (Supplementary Fig. 8b). Finally, incubation of PBMCs from human melanoma patients with rLCMV–MelanA26–35(27L) in vitro stimulated a substantial HLA-A*0201-restricted MelanA26–35(27L)-specific CD8+ T cell response (Supplementary Fig. 8c), which exceeded the response triggered by MelanA26–35(27L) peptide. These experimental observations indicate that rLCMV will be immunogenic in humans.
The properties of rLCMV suggest that it holds promise as a vector for vaccination and immunotherapy in infectious diseases and cancer. Its desirable features stem mainly from three properties: (i) its ability to target and functionally activate DCs, (ii) its stimulation of potent CD8+ T cell responses and (iii) its relative insensitivity to antibody neutralization and thus its efficacy in homologous prime-boost vaccination. A cardinal aspect of rLCMV immunogenicity is its targeting to DCs, followed by activation of these cells20, which is probably responsible for the potent CTL induction. The ability of rLCMV-immunized mice to respond to homologous boosting reflects the poor induction of neutralizing antibodies, an intrinsic feature of the LCMV envelope glycoprotein8. In addition, the limited number of rLCMV vector particles administered for vaccination here provided relatively low amounts of LCMV-GP, and exposure of the immune system to LCMV-GP was of short duration. The gene encoding LCMV-GP is absent from rLCMV vectors, and the vaccine cannot produce further LCMV-GP in vivo to trigger GP-specific neutralizing antibody responses. Moreover, even antibodies that potently neutralize LCMV in vitro exhibit only a limited capacity to interfere with T cell induction in vivo24. Together these considerations probably explain why even multiple administrations of rLCMV over prolonged periods of time have failed to elicit antibodies that interfere with vector immunogenicity. In addition to the limited interference by preexisting humoral immunity, all the existing evidence suggests that human seroprevalence to LCMV is generally below 5% (refs. 25,26,27,28). In contrast, high-titer protective neutralizing antibody responses are generated to the transgene encoded by the vector, which indicates its likely utility as a vaccine vector in humans. Wild-type LCMV can replicate and cause disease in immunosuppressed transplant recipients29. The lack of rLCMV replication suggests therefore that these vectors will provide a suitable safety profile for further development in humans.
Possible applications for rLCMV include protective vaccines, for example, against HIV, hepatitis C virus, tuberculosis and malaria, as well as cancer immunotherapy. Preliminary data in mice suggest that rLCMV vectors elicit CD8+ T cell responses to HIV antigens at high frequency and functionality (L.F. and G.J.N., unpublished data). Future studies should determine whether rLCMV vectors are particularly advantageous in eliciting CD8+ T cell responses to self antigens on tumors, in which immunotherapy can be compromised by T cell tolerance.
The choice of an optimal vaccine vector depends on both the properties of the vector and the mechanisms of protection for specific diseases. Additional parameters, including ease of storage, large-scale manufacturing, cost effectiveness and the size of the gene payload, can be limiting and remain to be determined for rLCMV. We have generated rLCMV vectors carrying foreign genes up to 2.6 kilobases in size without technical difficulties. If size limits for inserts existed, multiple vectors carrying individual antigens could be combined in a single vaccine, as successfully performed with recombinant adenovirus 5–based vectors30. Given all of these observations, rLCMV represents an attractive vector for stimulating both cellular and humoral immunity. Thus, it provides a platform that may be used to prevent or treat malignant and infectious diseases for which existing vaccination strategies have yet to confer protection.
Generation and titration of rLCMV vectors.
The rLCMV vectors were recovered as described10, with modifications as outlined in Results (use of GP-expressing BHK-21 cells). The GP-expressing 293T and BHK-21 producer cell lines are stable transfectants carrying plasmid M369 that expresses a codon-optimized LCMV-GP cDNA31. Plasmids pol-I-L, pC-L and pC-NP have been reported10. For generation of the various pSv plasmids directing intracellular expression of vector S segments, the respective open reading frames were amplified by PCR and were inserted into pSBsm(–)9 by a cloning strategy previously outlined in detail9. The plasmid pSvINDG61 (for intracellular expression of the rLCMV-INDG61 S segment) was generated by circular mutagenesis PCR on pSr9. By this procedure, cDNA sequence encoding GP amino acids 61–80 (GLNGPDIYKGVYQFKSVEFD) flanked by upstream and downstream glycine residues was inserted into the INDG open reading frame upstream of the sequence encoding amino acid 190. Two types of rLCMV-OVA were generated expressing either full-length OVA (the same as in VACC-OVA) or the StT-OVA-G fusion construct (the same as in rAd-OVA). Both types of rLCMV-OVA were tested in parallel in the majority of experiments. The immune responses were indistinguishable and hence for simplicity the results of the two rLCMV-OVA groups were pooled. The vector rLCMV–MelanA26–35(27L) was generated by incorporation into the S segment of a fusion gene that has been described32 (identical to VACC-MelanA26–35(27L); described below).The vector rLCMV-GP33 was generated by incorporation of a chimeric protein containing the GP33 epitope as described33. The rLCMV vectors were grown and titrated by immunofocus assay8 on 293T-GP cells.
Bacteria, viruses, viral vectors and quantification.
Recombinant L. monocytogenes expressing OVA15, wild-type LCMV (strain clone 13) and VSV serotype Indiana have been described10. The rAd vectors with deletion of E1 were grown and purified as described34. The vector rAd-OVA expresses StT-OVA-G, a truncated OVA open reading frame fused N-terminally to a T77 domain and C-terminally to EGFP. Immunizations with rAd were performed on the basis of particle titers and are expressed in PFU, with the assumption that 1 PFU ≈ 100 particles by approximation. The vector VACC/MelanA26–35(27L) expresses the MelanA26–35(27L) peptide ELAGIGILTV in a fusion construct as reported32. The recombinant vaccinia viruses VACC-G2, expressing LCMV-GP, VACC-GP33 and VACC-OVA, expressing full-length OVA (all WR strain), have been described35,36,37 and were propagated and titrated on BSC40 cells. A TaqMan RT-PCR protocol targeting the gene encoding LCMV-NP (to be described elsewhere) quantified rLCMV S segment copies in the spleen of vaccinated mice.
Mice, animal experiments, immunization and infectious challenge.
SMARTA1 mice13, P14 mice38, HHD mice39, OT-I mice18, RIP-OVA mice17, Z/EG mice23, ST33 mice21, mice deficient in type I interferon receptors14 on a C57BL/6 background, Ifnagr−/− mice11 and C57BL/6 wild-type mice were bred at the Institute for Laboratory Animal Sciences of the University of Zurich, Switzerland. Animal experiments were performed at the University of Geneva, at the University of Zurich and at the University of Bern, with permission by the respective cantonal authorities. Immunization with rLCMV vectors was performed at a dose of 1 × 105 to 3 × 105 PFU given intravenously, and 5 × 108 to 1 × 109 particles of rAd-OVA were given intravenously unless specified otherwise (referred to as 'standard dose' in the text). The vector VACC-OVA was administered intraperitoneally at a dose of 2 × 106 PFU. For challenge with rLM-OVA, 1 × 105 colony-forming units were given intravenously.
Assessment of T cell and antibody responses.
Intracellular cytokine assays and major histocompatibility complex class I tetramer staining were performed as described10,13. Tetramers were from Beckman Coulter and antibodies were from BD Biosciences, eBioscience and Biolegend. Samples were analyzed using FlowJo (TreeStar). VSV-neutralizing antibodies were measured as reported10.
Two groups were compared with t-tests (unpaired, two-tailed), and single values of multiple groups were compared by one-way analysis of variance with Bonferroni's post-test for multiple comparisons or with Dunnett's post-test for comparison against a reference. Time courses of multiple groups were compared by two-way analysis of variance. Statistical analysis was performed with GraphPad Prism software version 4.0b and SPSS version 13.0. P values of less than 0.05 (*) were considered statistically significant, and P values of less than 0.01 (**) were considered highly significant.
Induction of human MelanA26–35(27L)-specific CD8+ T cells.
PBMCs from HLA-A*0201+ patients with melanoma (Surgery Branch, National Cancer Institute) were stimulated with rLCMV–MelanA26–35(27L) in culture medium containing 300 IU ml−1 of IL-2 (Chiron). MelanA26–35(27L)-specific CD8+ T cell frequencies were evaluated by flow cytometry before stimulation and 2 weeks after stimulation.
Infection of DCs and PBMCs from healthy donors.
Procedures for mDC isolation from blood have been described40. Briefly, enriched populations of lymphocytes and monocytes were obtained by counterflow centrifugal elutriation. The mDCs were isolated from elutriated monocytes with the CD1c magnetic bead isolation kit (Miltenyi Biotec). PBMCs were prepared from buffy coats of healthy normal blood donors by gradient centrifugation (Lympholyte; Cedarlane Laboratories Limited).
DCs and PBMCs were cultured in complete medium (RPMI-1640; Gibco) supplemented with 2 mmol l−1 l-glutamine, 1% streptomycin and penicillin, and 10% FCS (Invitrogen Life Technologies). To maintain viability, the medium was further supplemented with 10 ng ml−1 recombinant human GM-CSF (for mDCs) or 2 ng ml−1 IL-2 (for PBMCs; both PeproTech). The vector rLCMV–MelanA26–35(27L) was added immediately after sorting at a multiplicity of infection of 1. Intracellular staining for LCMV-NP was performed 48 h after infection by using phycoerythrin-conjugated VL-4 antibody to LCMV-NP.
We thank H. Hengartner and R. Zinkernagel for critical comments, suggestions, discussions and long-term support; E. Horvath for technical assistance; S.A. Rosenberg and J.R. Wunderlich for samples from patients with melanoma; M. Roederer and K. Foulds for reagents and flow cytometry support; A. Oxenius, R. Spörri and N. Joller for providing access to their flow cytometry facility; A. Pegu, R. Roychoudhuri and C. Cheng for discussions and advice on human DC cultures; D. von Laer (Georg-Speyer-Haus) for plasmid M369 and GP-expressing 293T cells; H. Shen (University of Pennsylvania School of Medicine) for rLM-OVA; M. Groettrup (University of Constance) for VACC-OVA, originally generated by J. Yewdell (National Institute of Allergy and Infectious Diseases); and R. Schirmbeck (University of Ulm) for StT-OVA-G cDNA. L.F. was supported by a fellowship of the Schweizerische Stiftung für medizinisch-biologische Stipendien. A.N.H. is a fellow of GRAKO1121 of the German Research Foundation. M.L. is a Lichtenberg fellow funded by the Volkswagen Foundation. A.B. was supported by a PhD scholarship of the Boehringer Ingelheim Fonds and by a post-doctoral fellowship of the Roche Research Foundation. D.D.P. holds a stipendiary professorship of the Swiss National Science Foundation (PP00A-114913) and was supported by grant 3100A0-104067/1 of the Swiss National Science Foundation.
Supplementary Figures 1–8
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