The dendritic cell receptor DNGR-1 controls endocytic handling of necrotic cell antigens to favor cross-priming of CTLs in virus-infected mice

DNGR-1 (CLEC9A) is a receptor for necrotic cells required by DCs to cross-prime CTLs against dead cell antigens in mice. It is currently unknown how DNGR-1 couples dead cell recognition to cross-priming. Here we found that DNGR-1 did not mediate DC activation by dead cells but rather diverted necrotic cell cargo into a recycling endosomal compartment, favoring cross-presentation to CD8⁺ T cells. DNGR-1 regulated cross-priming in non-infectious settings such as immunization with antigen-bearing dead cells, as well as in highly immunogenic situations such as infection with herpes simplex virus type 1. Together, these results suggest that DNGR-1 is a dedicated receptor for cross-presentation of cell-associated antigens. Our work thus underscores the importance of cross-priming in immunity and indicates that antigenicity and adjuvanticity can be decoded by distinct innate immune receptors. The identification of specialized receptors that regulate antigenicity of virus-infected cells reveals determinants of antiviral immunity that might underlie the human response to infection and vaccination.

DCs are central players in the establishment and maintenance of self-tolerance, as well as in the induction of immunity against invading microorganisms (1, 2). In mice and humans, distinct subsets of DCs can be variably defined by phenotype, ontogeny, and function (3–5). They include the CD8α⁺ DC subset found in mouse lymphoid organs and the related CD103⁺ DC subset in non-lymphoid tissues, both of which are selectively lost in animals lacking the transcription factor BATF3 (6, 7). Cells bearing a similar phenotype have recently been described in humans, humanized mice, and sheep, indicating cross-species conservation of the CD8α⁺ DC family (8–12). This extended family has distinct functional properties, most notably a remarkable efficiency at capturing material from dead or dying cells, as well as processing exogenous antigens for cross-presentation on MHC class I (8–11, 13–16). These two features allow CD8α⁺-like DC to cross-present cell-associated antigens (17, 18) and trigger CTL responses against infectious agents or tumors (6, 19–24). In addition to priming CD8⁺ T cells, CD8α⁺ DCs have been implicated in the establishment of cross-tolerance to tissue-specific cell-associated antigens (18, 25–27).

The ability of CD8α⁺-like DCs to either cross-prime or cross-tolerize CD8⁺ T cells against cell-associated antigens implies that they can decode the context in which they encounter dead cells. In the case of infection, priming may be favored by signals from pattern recognition receptors (PRRs) that recognize bacterial or viral signatures associated with the dying infected cell (28, 29). In the case of uninfected cells such as tumors or allografts, it has been argued that the type of cell death dictates immunogenicity versus tolerogenicity, with necrosis and some forms of apoptosis favoring the former (30–32). This notion implies that CD8α⁺-like DCs possess receptors that couple innate sensing of necrotic cells to the induction of adaptive immunity. In this regard, we have identified DNGR-1, also known as CLEC9A, as a receptor for necrotic cells that favors cross-priming of CTLs to dead cell–associated antigens in mice (33). DNGR-1 is selectively expressed at high levels by mouse CD8α⁺ DCs (34, 35) and CD103⁺ DCs (36) and by their human equivalents (9, 37) and recognizes an intracellular ligand that is only exposed after cell death (33). Notably, loss-of-function experiments in the mouse showed that DNGR-1 is not required for dead cell uptake but plays a non-redundant role in priming CD8⁺ T cells against antigens contained within necrotic cells (33). However, it is currently unknown how DNGR-1 couples dead cell recognition to cross-priming and whether it only controls immunity to cell-associated antigens or is also involved in cross-tolerance.

DNGR-1 is a type II transmembrane C-type lectin receptor (CLR) bearing an extracellular C-type lectin-like domain (CTLD) and a cytoplasmic tail with a hemi–immunoreceptor tyrosine-based activation motif (hemITAM) motif that promotes signaling via spleen tyrosine kinase (Syk) (34, 37). The related CLR, Dectin-1, contains a similar hemITAM motif and functions as an activatory receptor in myeloid cells, promoting NF-κB activation and proinflammatory cytokine production in response to engagement by agonist ligands (38, 39). Reflecting the structural similarity between the two receptors, DNGR-1 has been proposed to also act as an activatory CLR (37). Therefore, it is plausible that interaction of DNGR-1 with its ligand on dead cells leads to activation of CD8α⁺ DCs, thereby enhancing their ability to prime naive CD8⁺ T cells. Consistent with this notion, the function of DNGR-1 in cross-priming to dead cell–associated antigens is dependent on the integrity of the DNGR-1 hemITAM motif and requires Syk kinase (33).

Here, we analyze the role of DNGR-1 in immunity to dead cells and the ability of the receptor to function as a DC activatory receptor. We find that DNGR-1 specifically controls cross-priming, but not cross-tolerance, to cell-associated antigens. However, contrary to expectations, we found that DNGR-1 does not mediate activation of DCs by dead cells. Rather, we show that DNGR-1 has a dedicated function in endocytic handling of necrotic cargo that results in diversion from a degradative fate and favors MHC class I cross-presentation to CD8⁺ T cells. Consistent with that notion, we show that DNGR-1 deficiency impairs CTL priming even in highly immunogenic situations such as upon infection with herpes simplex virus (HSV) type 1. Thus, DNGR-1 is a dedicated DC receptor for cross-presentation of dead cell–associated antigens that can impact CTL responses to virus infection in mice and may therefore regulate immunity in humans.

DNGR-1–dependent cross-priming of CTLs against dead cell–associated antigens. The conclusion that DNGR-1 is required for efficient cross-priming of naive CD8⁺ T cells against antigens borne by dead cells rests on the observation of decreased expansion of antigen-specific CD8⁺ T cells and impaired development of CTL activity when antigen-bearing dead cells are injected i.v. into DNGR-1–deficient (Clec9a^gfp/gfp) mice (33). To confirm that this protocol results in immunity, we injected mice with UV-treated secondary necrotic OVA-expressing mouse embryonic fibroblasts (OVA-MEFs) i.v. and then challenged them with an OVA-expressing tumor. Groups that had received the necrotic OVA-MEFs were completely protected from tumor growth, in contrast to untreated mice (Figure 1A). In addition, as cross-priming but not cross-tolerance to dead cell–associated antigens requires CD4⁺ T cell help (23, 40, 41), we compared OVA-specific CD8⁺ T cell expansion in WT versus IAα^–/– mice after i.v. injection with UV-treated OVA-MEFs. The percentage of OVA-specific CD8⁺ T cells was severely reduced in IAα^–/– mice and, in agreement with our previous observations, was also significantly lower in DNGR-1–deficient mice (Figure 1B). Even when precursor frequencies of antigen-specific CD8⁺ T cells were artificially increased by adoptive transfer of TCR-transgenic CD8⁺ T cells (OT-I), i.v. injection of necrotic OVA-MEFs promoted more robust clonal expansion of OVA-specific T cells in WT mice than in DNGR-1–null mice as measured by CFSE dilution and by total cell counts (Figure 1C). Overall, these results confirm and extend our previous observations that immunization with necrotic cells carrying a foreign antigen results in bona fide cross-priming of CTLs, which is partially dependent on DNGR-1.

Figure 1

DNGR-1 is required for cross-priming but not for cross-tolerance to dead cell–associated antigens. (A) WT mice were left untreated or were injected with UV-treated H-2^bm1 OVA-expressing MEFs i.v. One week later mice received B16-OVA cells i.v., and the number of tumors per lung was determined after 18 days. Data are representative of 2 independent experiments (n = 6/group, each dot represents 1 mouse). (B) WT (n = 16), DNGR-1–deficient (n = 11), or IAα^–/– (n = 6) mice were injected with UV-treated H-2^bm1 OVA–expressing MEFs, and the percentage of H2-K^b-OVA tetramer⁺ cells among CD8⁺ T cells in blood was determined 7 days after injection. Data were pooled from 2 independent experiments; each dot represents 1 mouse. (C) WT or DNGR-1–deficient mice received CFSE-labeled CD45.1⁺ OT-I cells, followed by immunization with UV-treated OVA-MEFs 1 day later. Spleens were analyzed 5 days after immunization for OT-I proliferation. CFSE dilution (left panel) and total number of divided cells (right panel) are shown; each dot represents 1 mouse. (D) DNGR-1–sufficient or DNGR-1–deficient RIP-mOVA mice received CFSE-labeled CD45.1⁺ OT-I cells. Renal LNs were analyzed 3 days after injection for OT-I proliferation quantified by CFSE dilution (left panel) and total number of divided cells (right panel); each dot represents 1 mouse. *P < 0.05, **P < 0.01, ***P < 0.001, unpaired Student’s t test and 1-way ANOVA (Tukey’s post-test).

Cross-tolerance of CD8⁺ T cells against dead cell–associated antigens is DNGR-1 independent. To test whether DNGR-1 might additionally be involved in promoting cross-tolerance to cell-associated antigens, we crossed DNGR-1–deficient mice with RIP-mOVA transgenic mice, which express membrane-bound OVA under the control of the rat insulin promoter (42). In these mice, the cross-presentation of endogenous OVA, presumably from dead or dying cells, promotes proliferation and subsequent deletion of adoptively transferred OT-I T cells (42, 43). Notably, and in contrast to mice receiving an inoculum of necrotic cells (Figure 1B), the proliferation of OT-I cells in renal LNs of RIP-mOVA mice was comparable in the DNGR-1–sufficient and –deficient backgrounds, indicating that DNGR-1 is not required for the process culminating in cross-tolerization to cell-associated antigens (Figure 1D). Together these results suggest that DNGR-1 plays a specific and non-redundant role in cross-priming, but not in cross-tolerance, against dead cell–associated antigens in vivo.

Activation of CD8α⁺ DCs by dead cells is DNGR-1 independent. The above results could be interpreted to mean that necrotic cells promote the activation of CD8α⁺ DCs in part by acting through DNGR-1. As a first approach to assess this possibility, we cultured WT and DNGR-1–deficient CD8α⁺-like DCs (derived from Flt3L cultures of BM cells; ref. 44) with necrotic cells and monitored DC maturation and production of inflammatory cytokines. In comparison to a positive control stimulus, CpG, stimulation with dead cells induced only limited upregulation of co-stimulatory markers (CD86, CD80, CD40) and low levels of secreted IL-12/23p40 but not other proinflammatory cytokines (data not shown and Supplemental Figure 1A; supplemental material available online with this article; doi: 10.1172/JCI60644DS1). However, these responses were comparable in cultures of DNGR-1–deficient and WT DCs (Supplemental Figure 1A). Additional microarray analysis of the transcriptome of DNGR-1–deficient and WT DCs cultured with dead cells failed to reveal any DNGR-1 dependence in the transcriptional response to the corpses (Supplemental Figure 2). Finally, we injected dead cells into mice and monitored the activation of CD8α⁺ DCs but failed to detect any differences between WT and DNGR-1–deficient animals (Supplemental Figure 1B). Thus, CD8α⁺ DC activation by dead cells appears DNGR-1 independent.

In a separate approach, we carried out experiments with BM-derived DCs or macrophages (from GM-CSF or M-CSF BM cultures, respectively) ectopically expressing DNGR-1. These experiments also failed to reveal gain of function at the level of myeloid cell activation upon coculture with dead cells (Supplemental Figure 3). In marked contrast, overexpression of DNGR-1 in Syk-expressing B3Z (B3Z.Syk) cells, a Syk-transduced T cell–derived cell line containing a reporter for NFAT, or in LK cells, a B cell–derived cell line, allowed NFAT activation and led to IL-2 and TNF-α production after stimulation with UV-treated dead cells (Supplemental Figure 4). This response was absent in B3Z.Syk cells expressing a Y7F mutant DNGR-1 (33), indicating that it was hemITAM dependent (Supplemental Figure 4). These results demonstrate that recognition of dead cells by DNGR-1 can induce gene expression and cell activation via hemITAM signaling. However, this response was observed in lymphoid-derived cells ectopically expressing DNGR-1 but absent in myeloid cells constitutively expressing or overexpressing DNGR-1.

DNGR-1 does not act as a myeloid activatory CLR. The inability of DNGR-1 to trigger myeloid cell activation in response to dead cells could result from nullification by simultaneous engagement of inhibitory receptors by the corpses (45). To selectively trigger only DNGR-1, we tried receptor cross-linking with mAbs but failed to detect signs of CD8α⁺ DC activation (Supplemental Figure 5), as reported by others (46). Therefore, we adopted an approach used for human DNGR-1 (37) and generated a chimeric receptor comprising the cytoplasmic tail of mouse DNGR-1 fused to the transmembrane domain and extracellular domain of mouse Dectin-1 (Figure 2A). The chimera can be uniquely triggered using a pure β-glucan, curdlan (39), thereby circumventing the need for a specific DNGR-1 agonist and obviating the possibility of additional receptor engagement by dead cells.

Figure 2

DNGR-1 does not behave as a myeloid activatory receptor. BM cells from Dectin-1–deficient mice were retrovirally transduced with a vector encoding for Dectin-1 or for a chimeric receptor (Chimera) bearing the cytoplasmic tail of DNGR-1 (WT) or 3 mutant versions thereof (Y7F, A3D, and I6G) fused to the transmembrane, stalk region, and CTLD of Dectin-1. All constructs were followed by an IRES-GFP sequence, which allowed sorting based on GFP levels to normalize for Dectin-1 or chimera surface expression. (A) Schematic representation of the chimeric DNGR-1/Dectin-1 receptors. Asterisks denote the mutated residues. (B) Expression of Dectin-1 or the different chimeras by GFP⁺ GMCSF-BMDCs purified by cell sorting as determined by staining with an anti–Dectin-1 antibody before overnight stimulation. (C) Purified GFP⁺ DCs as in B were cultured overnight in the presence of increasing amounts of curdlan (0, 30, and 100 μg/ml). Concentrations of TNF-α, IL-2, and IL-10 in the supernatant after culture are shown. Results are mean ± sem and representative of at least 3 independent experiments. ND, not detected.

In order to test for proper folding and signaling capacity of the chimeric receptor, we first expressed it in B3Z.Syk cells. Surface expression of the receptors was monitored with an anti–Dectin-1 mAb and was comparable in chimera- and Dectin-1–expressing cells (Supplemental Figure 6A). In addition, curdlan stimulation promoted NFAT activation and IL-2 and TNF-α secretion by B3Z.Syk cells transduced with retroviral vectors encoding either Dectin-1 or the chimeric receptor, but not by cells transduced with an empty vector or a vector encoding a chimeric receptor with a tyrosine to phenylalanine mutation (Y7F) in the hemITAM (Supplemental Figure 6, A and C). Similar results were obtained with LK cells (Supplemental Figure 6B), indicating that the chimeric receptor is able to recognize curdlan and signal for cytokine production with efficiency comparable to that of WT Dectin-1 in lymphoid cells.

We next compared Dectin-1–deficient GM-CSF–grown BMDCs retrovirally transduced to express either Dectin-1 or the chimeric receptor. The retroviral constructs also encoded GFP, which allowed us to sort the transduced cells based on different GFP levels and compare only those with matching levels of surface receptor expression (Figure 2B). Curdlan promoted robust production of TNF-α, IL-2, or IL-10 by DCs transduced with Dectin-1–encoding retrovirus but not by DCs transduced with empty control retrovirus encoding only GFP (Figure 2C). In stark contrast, curdlan-induced cytokine production was undetectable or greatly reduced in DCs expressing the chimeric receptor (Figure 2C). A control stimulus, CpG, induced comparable levels of cytokine production by all 3 populations of transduced DCs (Supplemental Figure 7). Similar results were obtained when we used a different chimeric receptor consisting of both the cytoplasmic tail and the transmembrane domain of mouse DNGR-1 fused to the extracellular domain of Dectin-1 (Supplemental Figure 8). These results suggest that, compared with that of Dectin-1, the tail of DNGR-1 is markedly deficient in its ability to signal for cytokine production in myeloid cells.

This conclusion appears to be in contrast to that in a previous report in which RAW264.7 macrophages transduced with an analogous chimeric receptor of human DNGR-1 and mouse Dectin-1 secreted significantly more TNF-α than control cells upon stimulation with zymosan particles (37). Importantly, curdlan specifically triggers Dectin-1, while zymosan can trigger other PRRs such as TLR2 and Dectin-2. It is therefore conceivable that binding of the particles to the chimeric receptor facilitated their recognition by other zymosan-specific receptors, which in turn signaled for TNF-α secretion. To address these possibilities, we procured the cells used in that study (37) and compared their response to zymosan versus curdlan. All cells expressed comparable levels of surface receptor and bound zymosan particles with similar efficiency (Supplemental Figure 9). As reported (37), zymosan induced increased TNF-α production in cells overexpressing either the chimera or Dectin-1 when compared with control cells transduced with an empty vector (Supplemental Figure 9). However, curdlan led to enhanced TNF-α production only in Dectin-1–transduced cells and not in cells expressing the chimera (Supplemental Figure 9). These results are concordant with our earlier conclusion that signaling by the cytoplasmic tail of DNGR-1 by itself is markedly inefficient at promoting activation of myeloid cells.

Examination of the data revealed a very low level of curdlan-induced cytokines in DCs expressing the Dectin-1/DNGR-1 chimera but not in cells transduced with empty vector (Figure 2C and Supplemental Figure 8). This appeared to depend on weak signaling by the receptor, as it was not seen with the Y7F mutant (Figure 2C), despite equivalent surface expression of all chimeras (Figure 2B). A DEDG sequence immediately upstream of the hemITAM tyrosine and shared by Dectin-1 and CLEC-2 but not by DNGR-1 has been shown to contribute to signaling by CLEC-2 (47). In DNGR-1 from all species, the glycine was replaced by an isoleucine and, in mouse but not human DNGR-1, it was preceded by two rather than three acidic residues (Figure 2A). We mutated these residues in the Dectin-1/DNGR-1 chimeras to determine whether restoration of a Dectin-1–like DEDG sequence could potentiate the weak signaling by DNGR-1. All chimeras were expressed at similar levels in Dectin-1–deficient BMDCs and signaled to NFAT with comparable efficiency when expressed in B3Z.Syk cells (Figure 2B and Supplemental Figure 6C). However, restoration of the tri-acidic motif had no effect on DC activation by curdlan (Figure 2C). In contrast, the I6G mutant chimeras were able to signal for DC activation as measured by production of TNF-α or IL-2 in response to curdlan, albeit less efficiently than WT Dectin-1 (Figure 2C). We conclude that the DNGR-1 hemITAM can potentially signal to induce myeloid cell activation but this ability is constrained by the presence of an isoleucine residue immediately upstream of the tyrosine.

DNGR-1 deficiency does not impact the adjuvanticity of dead cells. Despite the failure to lead to overt DC activation, weak DNGR-1 signaling could still mediate a subtle change in CD8α⁺ DCs that would lead to an improved ability to stimulate T cells in response to dead cells and account for the role of the receptor in cross-priming. To test for such an effect, we pulsed CD8α⁺-like Flt3L-derived BMDCs with a limiting concentration of OVA peptide (SIINFEKL) and subsequently allowed them to interact with necrotic MEFs (lacking OVA) before adding naive CFSE-labeled OT-I cells and measuring T cell proliferation. Notably, the expansion of OT-I cells was clearly improved as a function of the ratio of dead cells to DCs (Figure 3A), confirming that dead cell–derived signals improve the stimulatory ability of CD8α⁺ DCs for naive CD8⁺ T cells. However, this “adjuvant” effect of dead cells was independent of DNGR-1, as it was seen equally with WT and DNGR-1–deficient DCs (Figure 3A). These results suggest that DNGR-1 does not play a role in DC activation by dead cells even when the latter is measured with a T cell assay that presumably integrates known and unknown parameters of DC activation.

Figure 3

DNGR-1 regulates MHC class I cross-presentation but not MHC class II presentation of dead cell–associated antigens. (A) The adjuvanticity of dead cells is independent of DNGR-1. Purified CD8α⁺-like Flt3L-BMDCs from WT or DNGR-1–deficient (Clec9a^gfp/gfp) mice were pulsed with 1 pM SIINFEKL peptide, washed, and cultured with UV-treated H-2^bm1 MEFs and CFSE-labeled OT-I T cells. OT-I proliferation was quantified after 3 days. (B and C) DNGR-1 regulates cross-presentation of dead cell–associated antigens. Purified CD8α⁺-like Flt3L-BMDCs from WT or DNGR-1–deficient mice were cultured with UV-treated OVA-MEFs or latex beads coated with OVA (OVA beads). Proliferation of CFSE-labeled OT-I (B) or OT-II (C) T cells was quantified on day 3 or 5 (respectively) of coculture with DCs. (D) Purified CD8α⁺-like Flt3L-BMDCs from WT, DNGR-1–deficient, or Tap1^–/– mice were cultured with UV-treated OVA-MEFs and B3Z cells. NFAT reporter activity in B3Z cells was measured using a colorimetric assay after 24 hours of coculture. Results are mean ± sd and representative of at least 3 independent experiments. *P < 0.05, **P < 0.01, unpaired Student’s t test.

DNGR-1 regulates cross-presentation of dead cell–associated antigens. To reconcile the lack of DC activatory potential with the demonstrable effect of DNGR-1 on cross-priming to dead cell–derived antigens, we hypothesized that DNGR-1 might instead regulate antigen cross-presentation. We therefore assessed the ability of DNGR-1–deficient CD8α⁺ DCs to stimulate antigen-specific CD8⁺ and CD4⁺ T cells in vitro when antigen was offered in different forms. As reported (33), DNGR-1–deficient DCs were impaired in their ability to support proliferation and clonal expansion of OT-I CD8⁺ T cells when antigen was given in the form of necrotic OVA-MEFs but not when it was offered as a conjugate with latex beads (Figure 3B). In contrast, I-A^b–restricted OVA_323–339–specific OT-II CD4⁺ T cells proliferated and expanded equally after priming by WT and DNGR-1–deficient DCs (Figure 3C). Thus, DNGR-1 deficiency appears to affect the ability of CD8α⁺ DCs to prime CD8⁺ T cells but not CD4⁺ T cells in vitro, consistent with the hypothesis that DNGR-1 controls cross-presentation of dead cell–associated antigens on MHC class I molecules rather than DC activation by cell corpses. Direct assessment of SIINFEKL:H-2K^b complexes by mAb staining (48) was not feasible because of sensitivity issues (data not shown), and therefore we measured presentation indirectly by using MHC class I (H-2^b)–restricted OVA_257–264–specific B3Z cells, which respond to antigen without requiring co-stimulation (49). B3Z cells were cocultured with CD8α⁺-like DCs presenting antigens derived from dead cells, and NFAT reporter activity was assessed after 24 hours (Figure 3D). NFAT reporter activity was lower in B3Z cells cultured with DNGR-1–deficient DCs than those cultured with WT DCs (Figure 3D). To test the dependence on the transporter associated with antigen processing (TAP), we also included Tap1^–/– DCs in the analysis. The decreased reporter activity in B3Z cells cultured with these DCs confirmed the involvement of TAP during the generation of dead cell–derived peptides for MHC class I loading (Figure 3D). Therefore, DNGR-1 appears to be necessary for efficient cross-presentation of dead cell–associated antigens in a processing pathway that is largely TAP dependent.

DNGR-1 diverts phagocytosed dead cell cargo to a non-degradative recycling endosome compartment. To explain the above results, we tested whether DNGR-1 specifically functions by diverting necrotic cargo to a subcellular compartment that favors cross-presentation, as suggested for another CLR, the mannose receptor (50). We first asked whether DNGR-1 is directed to early endosomal compartments associated with antigen cross-presentation. Consistent with that hypothesis, anti–DNGR-1 mAb bound to the surface of CD8α⁺ DCs was selectively delivered to vesicles positive for EEA-1, Rab27a, or Rab5a, which mark such compartments (50, 51). Indeed, 75% of DNGR-1⁺ endosomes colocalized with EEA-1 at 30 minutes and with Rab27a or Rab5a at 60–90 minutes after internalization (Figure 4A). We then examined the fate of necrotic cargo taken up by CD8α⁺-like DCs. We found that DNGR-1⁺ vesicles containing dead cell–derived cargo colocalized with Rab5a. Indeed, at 60 minutes of coculture of WT DCs with Alexa Fluor 647–labeled necrotic MEFs, we detected Rab5a in approximately 60% of vesicles with dead cell–derived material (Figure 4B). This percentage decreased to approximately 20% at 240 minutes of coculture, indicating that the nature of DNGR-1⁺ vesicles changes at later time points after phagocytosis. Interestingly, co-localization of cargo with Rab5a was significantly reduced in DNGR-1–deficient DCs (Figure 4B), suggesting that DNGR-1 may actively determine the intracellular route along which the cargo is directed.

Figure 4

DNGR-1 diverts cargo to the early/recycling endosomal pool. (A) Purified splenic CD8α⁺ DCs from WT mice were cultured for 30 minutes (EEA-1) or for 90 minutes (Rab5a and Rab27a) with Alexa Fluor 488–coupled anti–DNGR-1 Ab. Cells were fixed and stained for confocal microscopy. Distribution of internalized anti–DNGR-1 Ab⁺ vesicles relative to EEA-1⁺, Rab5a⁺, or Rab27a⁺ vesicles was quantified as percentage of vesicles positive for anti–DNGR-1 antibody also positive for endosomal markers in 15 cells per condition. (B and C) Purified CD8α⁺-like Flt3L-BMDCs from WT or DNGR-1–deficient mice were cultured with UV-treated Alexa Fluor 647–labeled H-2^bm1 MEFs. Cells were fixed after 60 or 240 minutes and stained for confocal microscopy. Distribution of cargo derived from dead cells relative to Rab5a (B) and Rab11 (C) was quantified as percentage of total vesicles positive for endosomal markers containing dead cell cargo in 15 cells per condition. Scale bars: 5 μm. Results are representative of 2 independent experiments. *P < 0.05, **P < 0.01, unpaired Student’s t test.

In order to further characterize the nature of the compartment in which cargo associates with DNGR-1, we tested co-localization with Rab11, a marker for recycling endosomes, which have also been implicated in antigen cross-presentation (52). At 60 minutes after uptake, neither WT nor DNGR-1–deficient DCs contained more than 10% of cargo-positive vesicles that were also Rab11⁺ (Figure 4C). However, at 240 minutes, approximately 50% of cargo-containing vesicles costained for Rab11 in WT DCs. This co-localization with the recycling endosomal marker was significantly reduced in DCs lacking DNGR-1 (Figure 4C). Together, these data suggest that a proportion of phagocytosed dead cell–derived material associates with DNGR-1 and is diverted to the recycling endosomal route, thereby facilitating cross-presentation.

DNGR-1 is non-redundant for CTL responses to virus infection. If the major role of DNGR-1 were to activate DCs in response to contact with dead cells, its involvement in cross-priming should dissipate when the antigens are derived from virus-infected cells. The latter produce virus nucleic acids that engage PRRs and thereby should overwhelmingly drive DC activation, overriding any putative DNGR-1 contribution. If, on the other hand, the major role of DNGR-1 is to divert cargo to a compartment that facilitates cross-presentation, as argued above, the activity of DNGR-1 should still be apparent even in highly immunogenic conditions such as upon virus infection.

To first test this notion in vitro, we used an OVA-expressing “suicide” cytopathic Semliki Forest virus (SFV) that infects cells and replicates to produce double-stranded RNA but no progeny virions (28, 53). Phagocytosis of dead or dying SFV-OVA–infected cells by CD8α⁺ DCs leads to TLR3-dependent activation of the cells and drives robust cross-priming against OVA (28). Indeed, coculture of SFV-OVA–infected H-2^bm1 MEFs with H-2^b CD8α⁺-like DCs led to marked CD40 and CD86 upregulation, as well as IL-6 and TNF-α production, all of which were markedly reduced in the absence of TLR3 (Figure 5A). Consistent with this defect in activation and/or an additional effect of TLR3 on cross-presentation, Tlr3^–/– CD8α⁺ DCs were also impaired in their ability to drive OT-I expansion in response to SFV-OVA–infected cells (Figure 5B). Notably, neither upregulation of DC maturation markers nor the level of cytokines produced was affected by DNGR-1 deficiency (Figure 5A). However, the expansion of OT-I T cells primed by DNGR-1–deficient DCs was still significantly decreased (Figure 5B).

Figure 5

SFV-OVA–infected cells induce TLR3-dependent DC activation and DNGR-1–dependent cross-presentation. Purified CD8α⁺-like Flt3L-BMDCs from WT, DNGR-1–deficient, or Tlr3^–/– mice were cultured with SFV-OVA–infected H-2^bm1 MEFs (infected cells) at the indicated ratios in the absence (A) or presence (B) of CFSE-labeled OT-I T cells. (A) Concentration of IL-6 and TNF-α in the supernatant (upper panels) and MFI of CD86 and CD40 surface expression (lower panels) after overnight culture. As a positive control, DCs were cultured in the presence of CpG (500 ng/ml). Results are mean ± sem and representative of 2 independent experiments. (B) OT-I proliferation was quantified after 3 days. Results are mean ± sem and representative of at least 3 independent experiments. *P < 0.05, **P < 0.01, unpaired Student’s t test.

To extend these findings to the context of real virus infection in vivo, we chose a model of cytopathic HSV-1 virus infection of the lung and measured CTL responses in the draining mediastinal LNs by MHC pentamer staining and by restimulating the cells and performing intracellular staining for IFN-γ (Supplemental Figure 10). By either measure, CTL responses to the dominant HSV-1 glycoprotein B (gB) epitope in C57BL/6 mice were markedly reduced in Batf3^–/– mice, indicating a major contribution of the CD8α⁺ DC family to CD8⁺ T cell priming (Figure 6A). Remarkably, a reduction of around 30%–80% in the CTL response to gB was also observed in DNGR-1–deficient animals, when measured as number or frequency of gB-specific CTLs (Figure 6A) or by examination of gB peptide–specific IFN-γ production by CD8⁺ T cells (Figure 6B). In contrast, there was no defect in anti–HSV-1 antibody titers in DNGR-1–deficient mice (Supplemental Figure 11), indicating that DNGR-1 selectively regulates CTL priming. Importantly, no reduction in HSV-1–specific CTL numbers or frequency was seen when DNGR-1–deficient mice were infected via the i.v. route (Supplemental Figure 12). This is likely because cross-priming is dispensable in that setting and establishes that there is no intrinsic defect in the priming of anti–HSV-1 CD8⁺ T cells in DNGR-1–deficient mice. Thus, DNGR-1 selectively contributes to priming of virus-specific CTLs in a model of lung cytopathic HSV-1 infection, presumably through its ability to regulate cross-presentation of antigens within dying infected cells.

Figure 6

DNGR-1 contributes to the CTL response to HSV-1 lung infection. WT, DNGR-1–deficient, or Batf3^–/– mice were infected with HSV-1 i.n. Mediastinal LNs were harvested 7 days later, and CTL responses were measured directly ex vivo or after in vitro restimulation. (A) Left panel: H-2K^b-gB pentamer⁺ cells as a percentage of CD8⁺CD44⁺ T lymphocytes. Right panel: Number of H-2K^b-gB pentamer⁺CD8⁺CD44⁺ T cells. (B) IFN-γ⁺ cells as a percentage of CD8⁺CD44⁺ T lymphocytes after restimulation with gB_498–505 peptide for 6 hours. Data were pooled from 3 independent experiments, with each dot representing 1 mouse; naive WT, n = 5; WT, n = 13; DNGR-1–deficient, n = 13, Batf3^–/–, n = 8 mice. *P < 0.05, **P < 0.01, ***P < 0.001, 1-way ANOVA (Tukey’s post-test).

Antigens expressed by dead or dying cells can be made visible to the adaptive immune system, inducing either activation or inactivation of existing lymphocyte repertoires in many experimental models. However, the mechanisms by which innate recognition of cell death is translated into adaptive immunity or tolerance are not fully understood. CD8α⁺ DCs and the related CD103⁺ lineage are thought to be the major DC subsets mediating cross-priming and cross-tolerance to cell-associated antigens (3, 54, 55). We have shown previously that CD8α⁺ DCs utilize DNGR-1 to recognize a preformed signal exposed in necrotic cells and that ablation or blockade of the receptor reduces their ability to stimulate CTL responses against dead cell–associated antigens in vitro and in vivo (33). Those data and the previously reported function of DNGR-1 as a myeloid activatory CLR (36) suggested that DNGR-1 promotes cross-priming by activating DCs in response to contact with dead cells. Surprisingly, here we failed to find a role for DNGR-1 in promoting DC activation, which is probably regulated by other receptors (32). Rather, we suggest that the receptor acts to regulate the intracellular trafficking of internalized dead cell material, diverting it from a lysosomal proteolytic fate to a non-degradative recycling endosomal compartment that favors antigen extraction for TAP-dependent cross-presentation on MHC class I. We further show that the dedicated function of DNGR-1 in cross-presentation of dead cell–derived antigens contributes in a non-redundant manner to the overall CTL response to HSV-1 lung infection, indicating that it can be a key component of the immune response to cytopathic viruses.

The primacy of the CD8α⁺ DC family in cross-priming to dead cell–associated antigens has been put in question by a recent report suggesting that CD11c⁺CD169⁺ subcapsular sinus macrophages are the primary LN APC cross-presenting necrotic cell–derived antigens upon subcutaneous immunization with dead cells (56). Contrary to that report, we found that the CTL response to dead cell–associated antigens remains dependent on DNGR-1 and BATF3 even after subcutaneous immunization (S. Zelenay, B.U. Schraml, and C. Reis e Sousa, unpublished observations). A likely explanation for the discrepancy is that CD169 can be highly expressed by CD8α⁺ DCs and CD103⁺ DCs and can therefore inadvertently serve as a marker for DCs rather than subcapsular sinus macrophages, especially given the high levels of CD11c expressed by the latter (B.U. Schraml, S. Zelenay, and C. Reis e Sousa, unpublished observations). Thus, cross-priming to dead cell–associated antigens remains dependent on DNGR-1 expressed by CD8α⁺ DC family members irrespective of administration route.

Coupling of recognition of dead cells to production of proinflammatory cytokines was previously reported for macrophage-inducible C-type lectin (Mincle) (57). This ITAM-coupled receptor drives production of TNF-α and MIP-2 and thereby mediates recruitment of neutrophils into the damaged tissue. Mincle and other innate immune receptors, which signal for cellular activation upon recognition of microbial or endogenous ligands, are widely expressed among immune cells. In contrast, DNGR-1 is selectively expressed at high levels by the CD8α⁺ DC subset, with lower levels of expression on plasmacytoid DCs (34). Moreover, the expression of DNGR-1 on CD8α⁺ DCs is not increased in vivo upon LPS administration in contrast to that of many CLRs with activating functions in myeloid cells (58). Therefore, DNGR-1 exhibits several properties that appear to be unique within the family of C-type lectins that function as innate immune receptors. One additional unique feature underscored in the present study is the apparent separation of cell death sensing from proinflammatory signaling.

Our conclusion that DNGR-1 does not act by promoting CD8α⁺ DC activation in response to cell corpses is supported by multiple lines of investigation. First, coculture with dead cells fails to promote DNGR-1–dependent cytokine production or DC maturation. This is the case when testing CD8α⁺-like FLT3L BMDCs constitutively expressing DNGR-1 or GM-CSF–derived BMDCs and BM-derived macrophages ectopically expressing high levels of DNGR-1. Second, using DNGR-1/Dectin-1 receptor chimeras, we found that, unlike Dectin-1, DNGR-1 signaling only weakly induces production of proinflammatory cytokines by DCs. The chimera approach allows us to stimulate cells with a pure Dectin-1 agonist, avoiding the potential co-engagement of multiple agonistic and antagonistic receptors when using dead cells as a stimulus. Notably, the inability of DNGR-1 to signal for cytokine expression can be attributed to specific sequence features of its intracellular tail. Thus, a chimeric receptor consisting of Dectin-1 with the cytoplasmic tail of DNGR-1 was unable to signal for cytokine production, but conversion of a single isoleucine at position 6 into glycine markedly improved stimulatory potential. Third, DC activation triggered by phagocytosis of virus-infected cells was greatly diminished by loss of TLR3 but comparable in WT and DNGR-1–deficient DCs. This finding suggests that, independent of any ability to activate DCs autonomously, DNGR-1 also does not act synergistically with TLR to promote DC activation and further invalidates a model in which DNGR-1 acts by delivering infected cell cargo to TLR3-accessible endosomal compartments. Fourth, loss of DNGR-1 did not affect the ability of CD8α⁺ DCs to stimulate CD4⁺ T cells against dead cell–associated antigens or to stimulate CD8⁺ T cells in response to preprocessed antigen plus necrotic cells as “adjuvants.”

Interestingly, DNGR-1 could drive activation in T and B cell–derived cell lines, but not in myeloid cells, such as Flt3L BMDCs, GM-CSF BMDCs, BM-derived macrophages, or RAW264.7 macrophages. GM-CSF BMDCs, in particular, are especially amenable to activation by the Dectin-1/Syk pathway, in part because of high expression of CARD9, which permits coupling to NF-κB (59). These data suggest that signaling downstream of Syk-coupled CLR, in particular to NF-κB, is not only cell context dependent (59) but is also controlled in a CLR-specific manner. Further studies will be required to determine the molecular basis of this regulation, which leaves open the possibility that DNGR-1 may still trigger a specific type of CD8α⁺ DC activation in some circumstances that are not mimicked by our present analyses. Nevertheless, collectively, our results do not support the notion that DNGR-1 is a receptor whose primary function is to activate DCs in response to contact with necrotic cells.

Surprisingly, our data highlight an underappreciated aspect of CLR function in regulating endocytic traffic and the retrieval and cross-presentation of dead cell–associated antigens. We have previously demonstrated that DNGR-1⁺ vesicles in CD8α⁺ DCs do not colocalize with a tracer that accumulates in lysosomes (33). We now find that the receptor and associated dead cell–derived cargo localize to vesicles bearing markers of early endosomes and the recycling endocytic route, indicating that DNGR-1 is confined to the recycling endosome pool. Mannose receptor–mediated uptake and transport of soluble OVA to Rab5a-positive vesicles has been previously reported to favor cross-presentation of OVA-derived peptides (50), and the recycling endosomal compartment is the most favorable point in the endosomal pathway for cross-presentation (60). This may be because recycling endosomes are poorly degradative relative to other endosomal compartments and/or because the recycling pathway intersects with a specialized intracellular compartment where acidification is limited by production of NOX2-dependent reactive oxygen species (61). In either case, the limited acidity and proteolytic activity allowed for preservation of intact antigens and translocation into the cytosol for TAP-dependent cross-presentation (61–64). In contrast, generation of peptides for presentation on MHC class II molecules does not require sequestration from degradation, and the presentation of dead cell–associated antigens to CD4⁺ T cells was not impaired in the absence of DNGR-1. DNGR-1 seems, therefore, to specifically direct dead cell–derived cargo toward a compartment where antigens can be preserved and retrieved for cross-presentation. As such, DNGR-1 may be a useful subcellular marker for identifying and characterizing the elusive “cross-presentation compartment” in CD8α⁺ DCs. Of course, our data do not exclude the possibility that DNGR-1 may additionally control the process of cross-presentation, for example, by promoting fusion with the ER–Golgi intermediate compartment (65) or by facilitating translocation of ligand to the cytosol, as recently shown for another myeloid CLR, the mannose receptor (66). Consistent with that notion, the Y7F hemITAM mutant DNGR-1 still localized to the recycling endosomal compartment even though it was impaired in its ability to promote cross-presentation of dead cell–associated antigens (unpublished observation). Further dissection of the role of DNGR-1 in the regulation of cross-presentation will be greatly facilitated by the identification of the DNGR-1 ligand (67).

Our findings indicate that DNGR-1 regulates cross-priming to dead cell–associated antigens by controlling the antigenicity rather than the adjuvanticity of dead cells. Similarly, it has previously been argued that recognition of HMGB-1 by TLR4 might primarily serve to regulate the ability of DCs to cross-present dead cell antigens (68). If DNGR-1 is involved in regulating cross-presentation rather than DC activation, it might seem odd that its function is apparent only in cross-priming conditions and not in a model of cross-tolerance to cell-associated antigens. This could simply reflect that, during physiological cell death in tissues such as pancreas, the dying cells are cleared before loss of membrane integrity occurs. As the ligands for DNGR-1 are intracellular (33), normal clearance of apoptotic cells during homeostatic conditions may not allow for engagement of the receptor. Even if apoptotic cells are sampled by CD8α⁺ DCs, digestion of the corpse with consequent ligand exposure is likely to occur only in late, degradative endocytic compartments from which, as shown here, DNGR-1 is excluded. Thus, we believe that DNGR-1 involvement is only likely to become apparent in a pathological setting rather than during steady-state physiological cell turnover.

To test for such involvement, we resorted to a model of cytopathic lung infection with HSV-1. Lung contains a prominent population of CD103⁺ DCs (69) that expresses DNGR-1 at high levels (36) and corresponds to the migratory DCs previously shown to ferry antigen to draining LNs following virus infection (21, 70). In addition, DNGR-1–expressing CD8α⁺ DCs in the draining mediastinal LNs can also be prominent APCs for virus-specific CD8⁺ T cells following lung infection (21). Therefore, the CD8α⁺ DC family is likely to be important in inducing CTL responses to respiratory viruses. Consistent with that notion, we found that the CTL response to HSV-1 antigens was markedly reduced in Batf3-deficient mice, which lack CD103⁺ and CD8α⁺ DCs. Importantly, this response was also reduced by an average of 50% in DNGR-1–deficient mice. HSV-1 lung infection is cleared independently of lymphocytes (71), and therefore, we did not see any increase in virus accumulation in the lungs of DNGR-1– or Batf3-deficient mice (data not shown). However, in a different model of vaccinia virus infection, DNGR-1 deficiency clearly impacted virus clearance (72). While we do not know whether the DNGR-1–dependent component reflects cross-priming by the CD8α⁺ DC family or the activity of other cells (e.g., plasmacytoid DCs, which express low levels of the receptor), these findings nevertheless indicate that DNGR-1 can play a key role in the CTL response even under highly immunogenic situations such as virus infection. Our observations therefore suggest a novel and non-redundant point of control in immunity to infection, in which some DC receptors mark dead cells as cargo that contains antigens worthy of cross-presentation, whereas other receptors detect signs of infection in the corpses. As shown here, the former are necessary for cell-associated antigen processing and presentation. In contrast, the latter correspond to typical PRRs, which contribute to effective antigen processing and additionally provide DCs with the activation signals necessary for producing co-stimulatory and other factors that promote effector T cell development. Manipulation of the pathways involved in dead cell sensing and antigen extraction may have wide implications for the design of vaccines designed to elicit CTLs in infectious disease or cancer immunotherapy. In addition, the identification of specialized receptors that regulate antigenicity of virus-infected cells reveals previously unappreciated determinants of antiviral immunity that might underlie the human response to infection and vaccination.

View Supplemental data

Work in the C. Reis e Sousa laboratory is funded by Cancer Research UK and a prize from Fondation Bettencourt-Schueller. S. Zelenay, A.M. Keller, and B.U. Schraml were supported by EMBO long-term fellowships and by a Marie Curie Intra-European Fellowship to S. Zelenay. P.G. Whitney was supported by an Overseas Biomedical Fellowship from the National Health and Medical Research Council of Australia. D. Sancho is a recipient of a Ramón y Cajal fellowship from the Spanish Ministry of Innovation and Science. We thank Gordon Brown for RAW264.7 macrophages expressing the human DNGR-1/mouse Dectin-1 chimeric receptor and Philip East for microarray analysis. We are grateful to members of the Cancer Research UK Immunobiology Laboratory for assistance and helpful discussions.

Address correspondence to: Caetano Reis e Sousa, Immunobiology Laboratory, Cancer Research UK, London Research Institute, Lincoln’s Inn Fields Laboratories, 44 Lincoln’s Inn Fields, London WC2A 3LY, United Kingdom. Phone: 44.20.7269.2832; Fax: 44.20.7269.2833; E-mail: [email protected].

Conflict of interest: The authors have declared that no conflict of interest exists.

Reference information: J Clin Invest. 2012;122(5):1615–1627. doi:10.1172/JCI60644.

See the related articles at The DC receptor DNGR-1 mediates cross-priming of CTLs during vaccinia virus infection in mice and Cross-presenting CD103⁺ dendritic cells are protected from influenza virus infection.

1. Steinman RM. Lasker Basic Medical Research Award. Dendritic cells: versatile controllers of the immune system. Nat Med. 2007;13(10):1155–1159.
   View this article via: PubMed CrossRef Google Scholar
2. Steinman RM. Dendritic cells in vivo: a key target for a new vaccine science. Immunity. 2008;29(3):319–324.
   View this article via: PubMed CrossRef Google Scholar
3. Villadangos JA, Schnorrer P. Intrinsic and cooperative antigen-presenting functions of dendritic-cell subsets in vivo. Nat Rev Immunol. 2007;7(7):543–555.
   View this article via: PubMed CrossRef Google Scholar
4. Heath WR, Carbone FR. Dendritic cell subsets in primary and secondary T cell responses at body surfaces. Nat Immunol. 2009;10(12):1237–1244.
   View this article via: PubMed CrossRef Google Scholar
5. Merad M, Manz MG. Dendritic cell homeostasis. Blood. 2009;113(15):3418–3427.
   View this article via: PubMed CrossRef Google Scholar
6. Hildner K, et al. Batf3 deficiency reveals a critical role for CD8alpha+ dendritic cells in cytotoxic T cell immunity. Science. 2008;322(5904):1097–1100.
   View this article via: PubMed CrossRef Google Scholar
7. Edelson BT, et al. Peripheral CD103+ dendritic cells form a unified subset developmentally related to CD8alpha+ conventional dendritic cells. J Exp Med. 2010;207(4):823–836.
   View this article via: PubMed CrossRef Google Scholar
8. Jongbloed SL, et al. Human CD141+ (BDCA-3)+ dendritic cells (DCs) represent a unique myeloid DC subset that cross-presents necrotic cell antigens. J Exp Med. 2010;207(6):1247–1260.
   View this article via: PubMed CrossRef Google Scholar
9. Poulin LF, et al. Characterization of human DNGR-1+ BDCA3+ leukocytes as putative equivalents of mouse CD8alpha+ dendritic cells. J Exp Med. 2010;207(6):1261–1271.
   View this article via: PubMed CrossRef Google Scholar
10. Bachem A, et al. Superior antigen cross-presentation and XCR1 expression define human CD11c+CD141+ cells as homologues of mouse CD8+ dendritic cells. J Exp Med. 2010;207(6):1273–1281.
    View this article via: PubMed CrossRef Google Scholar
11. Crozat K, et al. The XC chemokine receptor 1 is a conserved selective marker of mammalian cells homologous to mouse CD8alpha+ dendritic cells. J Exp Med. 2010;207(6):1283–1292.
    View this article via: PubMed CrossRef Google Scholar
12. Contreras V, et al. Existence of CD8alpha-like dendritic cells with a conserved functional specialization and a common molecular signature in distant mammalian species. J Immunol. 2010;185(6):3313–3325.
    View this article via: PubMed CrossRef Google Scholar
13. Schulz O, Reis e Sousa C. Cross-presentation of cell-associated antigens by CD8alpha+ dendritic cells is attributable to their ability to internalize dead cells. Immunology. 2002;107(2):183–189.
    View this article via: PubMed CrossRef Google Scholar
14. Iyoda T, et al. The CD8+ dendritic cell subset selectively endocytoses dying cells in culture and in vivo. J Exp Med. 2002;195(10):1289–1302.
    View this article via: PubMed CrossRef Google Scholar
15. Schnorrer P, et al. The dominant role of CD8+ dendritic cells in cross-presentation is not dictated by antigen capture. Proc Natl Acad Sci U S A. 2006;103(28):10729–10734.
    View this article via: PubMed CrossRef Google Scholar
16. Dudziak D, et al. Differential antigen processing by dendritic cell subsets in vivo. Science. 2007;315(5808):107–111.
    View this article via: PubMed CrossRef Google Scholar
17. den Haan JM, Lehar SM, Bevan MJ. CD8(+) but not CD8(–) dendritic cells cross-prime cytotoxic T cells in vivo. J Exp Med. 2000;192(12):1685–1696.
    View this article via: PubMed CrossRef Google Scholar
18. Belz GT, et al. The CD8alpha(+) dendritic cell is responsible for inducing peripheral self-tolerance to tissue-associated antigens. J Exp Med. 2002;196(8):1099–1104.
    View this article via: PubMed CrossRef Google Scholar
19. Allan RS, et al. Epidermal viral immunity induced by CD8alpha+ dendritic cells but not by Langerhans cells. Science. 2003;301(5641):1925–1928.
    View this article via: PubMed CrossRef Google Scholar
20. Belz GT, et al. Cutting edge: conventional CD8 alpha+ dendritic cells are generally involved in priming CTL immunity to viruses. J Immunol. 2004;172(4):1996–2000.
    View this article via: PubMed Google Scholar
21. Belz GT, et al. Distinct migrating and nonmigrating dendritic cell populations are involved in MHC class I-restricted antigen presentation after lung infection with virus. Proc Natl Acad Sci U S A. 2004;101(23):8670–8675.
    View this article via: PubMed CrossRef Google Scholar
22. Allan RS, et al. Migratory dendritic cells transfer antigen to a lymph node-resident dendritic cell population for efficient CTL priming. Immunity. 2006;25(1):153–162.
    View this article via: PubMed CrossRef Google Scholar
23. Bennett SR, Carbone FR, Karamalis F, Miller JF, Heath WR. Induction of a CD8+ cytotoxic T lymphocyte response by cross-priming requires cognate CD4+ T cell help. J Exp Med. 1997;186(1):65–70.
    View this article via: PubMed CrossRef Google Scholar
24. Bedoui S, et al. Cross-presentation of viral and self antigens by skin-derived CD103+ dendritic cells. Nat Immunol. 2009;10(5):488–495.
    View this article via: PubMed CrossRef Google Scholar
25. Ferguson TA, Herndon J, Elzey B, Griffith TS, Schoenberger S, Green DR. Uptake of apoptotic antigen-coupled cells by lymphoid dendritic cells and cross-priming of CD8(+) T cells produce active immune unresponsiveness. J Immunol. 2002;168(11):5589–5595.
    View this article via: PubMed Google Scholar
26. Luckashenak N, et al. Constitutive crosspresentation of tissue antigens by dendritic cells controls CD8+ T cell tolerance in vivo. Immunity. 2008;28(4):521–532.
    View this article via: PubMed CrossRef Google Scholar
27. Qiu CH, Miyake Y, Kaise H, Kitamura H, Ohara O, Tanaka M. Novel subset of CD8{alpha}+ dendritic cells localized in the marginal zone is responsible for tolerance to cell-associated antigens. J Immunol. 2009;182(7):4127–4136.
    View this article via: PubMed CrossRef Google Scholar
28. Schulz O, et al. Toll-like receptor 3 promotes cross-priming to virus-infected cells. Nature. 2005;433(7028):887–892.
    View this article via: PubMed CrossRef Google Scholar
29. Torchinsky MB, Garaude J, Martin AP, Blander JM. Innate immune recognition of infected apoptotic cells directs T(H)17 cell differentiation. Nature. 2009;458(7234):78–82.
    View this article via: PubMed CrossRef Google Scholar
30. Matzinger P. The danger model: a renewed sense of self. Science. 2002;296(5566):301–305.
    View this article via: PubMed CrossRef Google Scholar
31. Kroemer G, Zitvogel L. Death, danger, and immunity: an infernal trio. Immunol Rev. 2007;220:5–7.
    View this article via: PubMed CrossRef Google Scholar
32. Green DR, Ferguson T, Zitvogel L, Kroemer G. Immunogenic and tolerogenic cell death. Nat Rev Immunol. 2009;9(5):353–363.
    View this article via: PubMed CrossRef Google Scholar
33. Sancho D, et al. Identification of a dendritic cell receptor that couples sensing of necrosis to immunity. Nature. 2009;458(7240):899–903.
    View this article via: PubMed CrossRef Google Scholar
34. Sancho D, et al. Tumor therapy in mice via antigen targeting to a novel, DC-restricted C-type lectin. J Clin Invest. 2008;118(6):2098–2110.
    View this article via: JCI PubMed CrossRef Google Scholar
35. Caminschi I, et al. The dendritic cell subtype-restricted C-type lectin Clec9A is a target for vaccine enhancement. Blood. 2008;112(8):3264–3273.
    View this article via: PubMed CrossRef Google Scholar
36. Poulin LF, et al. DNGR-1 is a specific and universal marker of mouse and human Batf3-dependent dendritic cells in lymphoid and non-lymphoid tissues [published online ahead of print March 22, 2012]. Blood . doi:10.1182/blood-2012-01-406967.
37. Huysamen C, Willment JA, Dennehy KM, Brown GD. CLEC9A is a novel activation C-type lectin-like receptor expressed on BDCA3+ dendritic cells and a subset of monocytes. J Biol Chem. 2008;283(24):16693–16701.
    View this article via: PubMed CrossRef Google Scholar
38. Gross O, et al. Card9 controls a non-TLR signalling pathway for innate anti-fungal immunity. Nature. 2006;442(7103):651–656.
    View this article via: PubMed CrossRef Google Scholar
39. LeibundGut-Landmann S, et al. Syk- and CARD9-dependent coupling of innate immunity to the induction of T helper cells that produce interleukin 17. Nat Immunol. 2007;8(6):630–638.
    View this article via: PubMed CrossRef Google Scholar
40. Kurts C, et al. CD4+ T cell help impairs CD8+ T cell deletion induced by cross-presentation of self-antigens and favors autoimmunity. J Exp Med. 1997;186(12):2057–2062.
    View this article via: PubMed CrossRef Google Scholar
41. Griffith TS, et al. Apoptotic cells induce tolerance by generating helpless CD8+ T cells that produce TRAIL. J Immunol. 2007;178(5):2679–2687.
    View this article via: PubMed Google Scholar
42. Kurts C, Heath WR, Carbone FR, Allison J, Miller JF, Kosaka H. Constitutive class I-restricted exogenous presentation of self antigens in vivo. J Exp Med. 1996;184(3):923–930.
    View this article via: PubMed CrossRef Google Scholar
43. Kurts C, Kosaka H, Carbone FR, Miller JF, Heath WR. Class I-restricted cross-presentation of exogenous self-antigens leads to deletion of autoreactive CD8(+) T cells. J Exp Med. 1997;186(2):239–245.
    View this article via: PubMed CrossRef Google Scholar
44. Naik SH, et al. Cutting edge: generation of splenic CD8+ and CD8- dendritic cell equivalents in Fms-like tyrosine kinase 3 ligand bone marrow cultures. J Immunol. 2005;174(11):6592–6597.
    View this article via: PubMed Google Scholar
45. Chen GY, Tang J, Zheng P, Liu Y. CD24 and Siglec-10 selectively repress tissue damage-induced immune responses. Science. 2009;323(5922):1722–1725.
    View this article via: PubMed CrossRef Google Scholar
46. Lahoud MH, et al. Targeting antigen to mouse dendritic cells via Clec9A induces potent CD4 T cell responses biased toward a follicular helper phenotype. J Immunol. 2011;187(2):842–850.
    View this article via: PubMed CrossRef Google Scholar
47. Fuller GL, et al. The C-type lectin receptors CLEC-2 and Dectin-1, but not DC-SIGN, signal via a novel YXXL-dependent signaling cascade. J Biol Chem. 2007;282(17):12397–12409.
    View this article via: PubMed CrossRef Google Scholar
48. Porgador A, Yewdell JW, Deng Y, Bennink JR, Germain RN. Localization, quantitation, and in situ detection of specific peptide-MHC class I complexes using a monoclonal antibody. Immunity. 1997;6(6):715–726.
    View this article via: PubMed CrossRef Google Scholar
49. Karttunen J, Sanderson S, Shastri N. Detection of rare antigen-presenting cells by the lacZ T-cell activation assay suggests an expression cloning strategy for T-cell antigens. Proc Natl Acad Sci U S A. 1992;89(13):6020–6024.
    View this article via: PubMed CrossRef Google Scholar
50. Burgdorf S, Kautz A, Bohnert V, Knolle PA, Kurts C. Distinct pathways of antigen uptake and intracellular routing in CD4 and CD8 T cell activation. Science. 2007;316(5824):612–616.
    View this article via: PubMed CrossRef Google Scholar
51. Jancic C, et al. Rab27a regulates phagosomal pH and NADPH oxidase recruitment to dendritic cell phagosomes. Nat Cell Biol. 2007;9(4):367–378.
    View this article via: PubMed CrossRef Google Scholar
52. Kutomi G, et al. Targeting to static endosome is required for efficient cross-presentation of endoplasmic reticulum-resident oxygen-regulated protein 150-peptide complexes. J Immunol. 2009;183(9):5861–5869.
    View this article via: PubMed CrossRef Google Scholar
53. Smerdou C, Liljestrom P. Two-helper RNA system for production of recombinant Semliki forest virus particles. J Virol. 1999;73(2):1092–1098.
    View this article via: PubMed Google Scholar
54. Segura E, Villadangos JA. Antigen presentation by dendritic cells in vivo. Curr Opin Immunol. 2009;21(1):105–110.
    View this article via: PubMed CrossRef Google Scholar
55. Helft J, Ginhoux F, Bogunovic M, Merad M. Origin and functional heterogeneity of non-lymphoid tissue dendritic cells in mice. Immunol Rev. 2010;234(1):55–75.
    View this article via: PubMed CrossRef Google Scholar
56. Asano K, et al. CD169-positive macrophages dominate antitumor immunity by crosspresenting dead cell-associated antigens. Immunity. 2011;34(1):85–95.
    View this article via: PubMed Google Scholar
57. Yamasaki S, Ishikawa E, Sakuma M, Hara H, Ogata K, Saito T. Mincle is an ITAM-coupled activating receptor that senses damaged cells. Nat Immunol. 2008;9(10):1179–1188.
    View this article via: PubMed CrossRef Google Scholar
58. Joffre OP, Sancho D, Zelenay S, Keller AM, Reis e Sousa C. Efficient and versatile manipulation of the peripheral CD4+ T-cell compartment by antigen targeting to DNGR-1/CLEC9A. Eur J Immunol. 2010;40(5):1255–1265.
    View this article via: PubMed CrossRef Google Scholar
59. Goodridge HS, et al. Differential use of CARD9 by dectin-1 in macrophages and dendritic cells. J Immunol. 2009;182(2):1146–1154.
    View this article via: PubMed Google Scholar
60. Belizaire R, Unanue ER. Targeting proteins to distinct subcellular compartments reveals unique requirements for MHC class I and II presentation. Proc Natl Acad Sci U S A. 2009;106(41):17463–17468.
    View this article via: CrossRef PubMed Google Scholar
61. Savina A, et al. NOX2 controls phagosomal pH to regulate antigen processing during crosspresentation by dendritic cells. Cell. 2006;126(1):205–218.
    View this article via: CrossRef PubMed Google Scholar
62. Accapezzato D, et al. Chloroquine enhances human CD8+ T cell responses against soluble antigens in vivo. J Exp Med. 2005;202(6):817–828.
    View this article via: PubMed CrossRef Google Scholar
63. Delamarre L, Couture R, Mellman I, Trombetta ES. Enhancing immunogenicity by limiting susceptibility to lysosomal proteolysis. J Exp Med. 2006;203(9):2049–2055.
    View this article via: PubMed CrossRef Google Scholar
64. Delamarre L, Pack M, Chang H, Mellman I, Trombetta ES. Differential lysosomal proteolysis in antigen-presenting cells determines antigen fate. Science. 2005;307(5715):1630–1634.
    View this article via: PubMed CrossRef Google Scholar
65. Cebrian I, et al. Sec22b regulates phagosomal maturation and antigen crosspresentation by dendritic cells. Cell. 2011;147(6):1355–1368.
    View this article via: PubMed CrossRef Google Scholar
66. Zehner M, et al. Mannose receptor polyubiquitination regulates endosomal recruitment of p97 and cytosolic antigen translocation for cross-presentation. Proc Natl Acad Sci U S A. 2011;108(24):9933–9938.
    View this article via: PubMed CrossRef Google Scholar
67. Ahrens S, et al. F-actin is an evolutionarily-conserved damage-associated pattern recognized by DNGR-1, a receptor for dead cells. Immunity. In press.
68. Apetoh L, et al. Toll-like receptor 4-dependent contribution of the immune system to anticancer chemotherapy and radiotherapy. Nat Med. 2007;13(9):1050–1059.
    View this article via: PubMed CrossRef Google Scholar
69. Ginhoux F, et al. The origin and development of nonlymphoid tissue CD103+ DCs. J Exp Med. 2009;206(13):3115–3130.
    View this article via: PubMed CrossRef Google Scholar
70. GeurtsvanKessel CH, et al. Clearance of influenza virus from the lung depends on migratory langerin+CD11b- but not plasmacytoid dendritic cells. J Exp Med. 2008;205(7):1621–1634.
    View this article via: PubMed CrossRef Google Scholar
71. Reading PC, Whitney PG, Barr DP, Smyth MJ, Brooks AG. NK cells contribute to the early clearance of HSV-1 from the lung but cannot control replication in the central nervous system following intranasal infection. Eur J Immunol. 2006;36(4):897–905.
    View this article via: PubMed CrossRef Google Scholar
72. Iborra S, Izquierdo HM, Martínez-López M, Blanco-Menéndez N, Reis e Sousa C, Sancho D. The DC receptor DNRG1 mediates cross-priming of CTLs during vaccinia virus infection in mice. J Clin Invest. 2012;122(5):1628–1643.
    View this article via: JCI Google Scholar
73. Inaba K, et al. Generation of large numbers of dendritic cells from mouse bone marrow cultures supplemented with granulocyte/macrophage colony-stimulating factor. J Exp Med. 1992;176(6):1693–1702.
    View this article via: PubMed CrossRef Google Scholar
74. Kappler J, White J, Wegmann D, Mustain E, Marrack P. Antigen presentation by Ia+ B cell hybridomas to H-2-restricted T cell hybridomas. Proc Natl Acad Sci U S A. 1982;79(11):3604–3607.
    View this article via: PubMed CrossRef Google Scholar