Abstract
The initiation of the mucosal immune response in Peyer’s patch (PP) relies on the sampling, processing, and efficient presentation of foreign antigens by dendritic cells (DCs). Among PP DCs, CD11b+ conventional DCs (cDCs) and lysozyme-expressing DCs (LysoDCs) have distinct progenitors and functions but share many cell surface markers. This has previously led to confusion between these two subsets. In addition, another PP DC subset, termed double-negative (DN), remains poorly characterized. Here we show that both DN and CD11b+ cDCs belong to a unique SIRPα+ cDC subset. At steady state, cDCs and TIM-4+ macrophages are mainly located in T-cell zones, i.e., interfollicular regions, whereas a majority of subepithelial phagocytes are monocyte-derived cells, namely, LysoDCs and TIM-4− macrophages. Finally, oral administration of a Toll-like receptor 7 ligand induces at least three TNF-dependent events: (i) migration of dome-associated villus cDCs in interfollicular regions, (ii) increase of CD8α+ interfollicular cDC number, and (iii) activation of both CD11b+ and CD8α+ interfollicular cDCs. The latter is marked by a genetic reprograming leading to the upregulation of type I interferon-stimulated and of both immuno-stimulatory and -inhibitory gene expression.
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Introduction
Among antigen-presenting cells, dendritic cells (DCs) are the most efficient at initiating antigen-specific responses, inducing differentiation of both naive CD4+ and CD8+ T cells.1 DCs have a remarkable pattern of functional specialization overtime, also called maturation. It includes specific mechanisms to control antigen uptake, processing, and presentation.2, 3 In their immature state, DCs detect and capture incoming pathogens. Then, upon stimulation, they begin a complex process of differentiation that involves a profound genetic reprograming.4, 5 This leads to important phenotypic, morphological, and functional changes required for their migration to lymph node T-cell zones as well as for antigen presentation and priming of naive T cells to mount an appropriate adaptive immune response.
To give rise to protective immunity, mucosal vaccines require the use of adjuvants that override the natural bias of the mucosal immune system toward the induction of tolerance. Knowing how these adjuvants are able to modify DC behavior in vivo is crucial to a better understanding of the mucosal immune response initiation, especially in primary inductive sites such as Peyer’s patches (PPs) of the small intestine. Nevertheless, there is still little information about the alteration induced by adjuvants on PP DC populations. Cholera toxin is a powerful mucosal adjuvant that induces the migration of cells expressing CD11c, a marker of mouse gut DCs and macrophages,6 into the follicle-associated epithelium (FAE) followed by the migration of microsphere-loaded CD11c+ phagocytes in interfollicular regions (IFRs) enriched in T cells.7, 8 Several Toll-like receptor (TLR) ligands also induce CD11c+ cell migration into the FAE.7, 9, 10, 11 Finally, R848, a TLR7 agonist, induces an increase of CD103+ cells, presumably DCs, in the IFR of rat PP.12 However, these CD11c+ or CD103+ cells have not been characterized further and could correspond to different subsets of DC or macrophages.
Mouse common DC precursor (CDP)-derived DCs, also termed conventional DC (cDCs), encompass indeed two major subsets that have been initially characterized by the expression of either CD8α (cDC1) or CD11b (cDC2), in addition to CD11c and major histocompatibility complex class II (MHCII).13 CD8α+ cDCs have been well described in different tissues including PPs where they are located in the IFRs.14, 15, 16 Unlike CD8α+ cDCs, CD11b+ cDCs remain poorly characterized depending on the examined tissue. This is mainly due to the overlap of their surface markers (i.e., CD11c, CD11b, and MHCII) with macrophages.6 Thus, we recently showed that PP CD11chiCD11b+ mononuclear phagocytes comprise CD11b+ cDCs but also lysozyme-expressing DCs (LysoDCs) and macrophages (LysoMacs) that, unlike CD11b+ cDC, are both CX3CR1+ monocyte-derived cells.17 Unlike LysoDCs, LysoMacs display CD4 at their surface and encompass two subsets based on the expression of the apoptotic cell receptor TIM-4. TIM-4+ LysoMacs are mainly located in the T-cell zone of PP, i.e., the IFR, and in the lower part of the follicle, whereas TIM-4− LysoMacs are located in the upper part of the follicle and in the subepithelial dome (SED).17 Particulate antigens and pathogenic bacteria that have been transported through M-cells of the FAE are mainly internalized in the SED by TIM-4− LysoMacs and LysoDCs, which both display strong innate antiviral and antibacterial gene signatures.17, 18, 19 In addition, LysoDC dendrites can directly sample luminal antigens through M-cell-specific transcellular pores by a mechanism independent of CX3CR1 expression.17, 18 LysoDC and LysoMac recruitment is independent of microbiota colonization.17 Finally, unlike LysoMacs, LysoDCs display a rapid renewal rate, strongly express genes of the MHCII presentation pathway and prime naive helper T cells for interferon-γ production in vitro.17
If phenotypic distinction between PP CD11b+ cDCs and monocyte-derived DCs has recently been solved,17 confusion still remains concerning their location and functions. Moreover, PP CD11b+ cDCs encompass both dome cDCs and dome-associated villus (DAV) cDCs.17 Finally, PPs contain another cDC subset termed double-negative DCs (DN DCs), as it neither expresses CD11b nor CD8α.14, 15 Both CD11b+ and DN cDCs express Clec4a4 and SIRPα, whereas CD8α+ cDCs do not.17 Moreover, the transcription factor Batf3, which is required for the differentiation of CD8α+ cDCs, is dispensable for CD11b+ and DN cDCs.17 Finally, CD8α+ cDCs prime naive helper T cells to secrete interferon-γ, whereas CD11b+ and DN cDCs do not.17 Thus, DN DCs may be more closely related to CD11b+ than to CD8α+ cDCs.
Here we have studied into details the genetic relationship, the distribution, and location of the different dome cDC subsets and investigated their activation transcriptional profile upon oral delivery of R848 as a model of mucosal adjuvant. We also show that, upon stimulation, DAV cDCs migrate to the T-cell zone of PPs, i.e., the IFR.
Results
DN and CD11b+ dome cDCs belong to a unique SIRPα+ cDC subset
We established a flow cytometry gating strategy to sort CD8α+, DN, and CD11b+ dome cDCs and study their genetic relationship. CD11chi monocyte-derived cells, i.e., LysoDCs and LysoMacs, express BST2, whereas cDCs do not.17 Among cDCs, DN and CD11b+ cDCs express SIRPα, whereas CD8α+ cDCs do not. Thus, CD11chiMHCII+ cells were first gated into three populations based on the expression of BST2 and SIRPα: LysoDCs/LysoMacs (SIRPαhiBST2+), DN/CD11b+ cDCs (SIRPα+BST2−), and CD8α+ cDCs (SIRPα−BST2−; Figure 1a). Then, SIRPα+BST2− cells were further separated into three subsets based on CD11b differential expression:17 dome DN (CD11b−), dome CD11b+ (CD11bint), and DAV CD11b+ (CD11bhi) cDCs (Figure 1a). In addition, LysoMacs were separated into TIM-4− and TIM-4+ subsets. Triplicates of TIM-4− and TIM-4+ LysoMacs, CD8α+ and DN dome cDCs, and quintuplicate of CD11b+ dome cDCs were analyzed by mouse whole-genome microarray. Generated data were combined with those of LysoDCs and CD11b+ dome cDCs previously obtained,17 and the transcriptional proximity between CD11chi phagocytes was determined by hierarchical clustering (Figure 1b). Two main clusters were observed: one composed by cDCs and the other by monocyte-derived cells. Among the latter, LysoDCs clustered apart from TIM-4− and TIM-4+ LysoMacs, whereas among cDCs, DN and CD11b+ cDCs clustered together apart from CD8α+ cDCs. We also performed a principal component analysis. The first principal component separated cells according to their origin, i.e., monocyte vs. CDP-derived cells (Figure 1c). Genes contributing to this axis included typical cDC markers (e.g., Itgae, Flt3, Btla, Id2, and Ccr7; Supplementary Table S1 online) on one side, and monocyte and macrophage markers on the other (e.g., Mertk, Mafb, Tcfec, Cx3cr1; Supplementary Table S1). The second principal component separated mainly SIRPα+ (DN and CD11b+ cDCs, LysoDCs, and LysoMacs) from SIRPα− (CD8α+ cDCs) phagocytes and contributing genes were either associated with the CD8α+ cDC subset (e.g., Clec9a, Xcr1, Tlr3, Tlr11, Cd8a, Cadm1, and Irf8; Supplementary Table S1) or the CD11b+ cDC subset (e.g., Clec4a4, Sirpa, Sirpb1, Csf1r, and Il22ra2; Supplementary Table S1). Principal component analysis failed to discriminate DN from CD11b+ cDCs confirming their close genetic relatedness (Figure 1c). In line with these results, the genes encoding the key transcriptional factors IRF4 and IRF8 involved either in CD11b+ or CD8a+ cDC subset commitment were either expressed or not by DN cDCs, respectively (Supplementary Figure S1A). Only 230 differentially expressed genes (DEGs) were found between DN and CD11b+ cDCs, whereas 1,098 DEGs distinguished the latter from CD8α+ cDCs. The top 20 of CD11b+ vs. DN cDC upregulated genes comprised typical DC maturation transcripts encoding molecules involved in migration to T-cell zones (lymph node homing chemokine receptor CCR7) and in attraction (chemokines CCL17 and CCL22) and stimulation (the cystine/glutamate antiporter SLC7A11 and the proinflammatory cytokine interleukin-6) of effector cells (Supplementary Figure S1B). In addition, the genes encoding for fascin1 (Fscn1), which is an actin-bundling protein involved in DC migration upon maturation,20 and for the transcription factor STAT4, which is induced upon DC maturation,21 were also upregulated in CD11b+ cDCs (Supplementary Figure S1A). Thus, DN and CD11b+ dome cDCs were likely different homeostatic maturation stages of PP SIRPα+ cDCs. To strengthen this hypothesis, we performed a multiple gene set enrichment analysis using the recently developed BubbleGUM software.22 Gene signatures were obtained from mouse and cross-species studies performed by several laboratories (Supplementary Table S2).4, 5, 23, 24, 25, 26, 27, 28, 29 First, we corroborated the monocytic and CDP origin of LysoDCs/LysoMacs and DN/CD11b+/CD8α+ DCs, respectively (Figure 1d, pink boxes). Second, we confirmed that both LysoDCs and CD11b+ cDCs were enriched for a CD11b+/cDC2 cDC gene signature as compared to LysoMacs, whereas there was a lack of enrichment for this signature between CD11b+ cDCs and LysoDCs (Figure 1d, blue boxes). Third, we confirmed that both DN and CD11b+ belonged to the CD11b+/cDC2 lineage (Figure 1d, orange boxes). Finally, BubbleGUM analysis supported that DN and CD11b+ cDCs differed by their maturation state as underlined by the enrichment of the latter for migratory/activated cDC gene signatures (Figure 1d, green box). The strongest enrichment score was obtained for the migratory cDC signature, which includes key DC maturation genes such as Stat4, Socs2, Fscn1, Ccr7, and Ccl22 (Figure 1d, right panel). These data establish a close genetic relationship between DN and CD11b+ cDCs, and suggest that DN cDCs likely represent an immature stage of CD11b+ cDCs.
SIRPα+ dome cDCs form a continuum of cells ranging from CD11chiSIRPα+ BST2−CD11b−MHCIIlo CD24hi EpCAMlo JAM-Aint to CD11chi SIRPα+ BST2− CD11bint MHCIIhi CD24int EpCAMintJAM-Ahi
A hallmark of DC maturation is the increased surface display of MHCII molecules for antigen presentation.3 Interestingly, based on MHCII and CD11b expression, SIRPα+ dome cDCs formed a continuum of cells ranging from CD11b−MHCIIlo to CD11bintMHCIIhi (Figure 1a and 2a). This suggests that transitional states exist between DN (CD11b−MHCIIlo) and CD11b+ (CD11bintMHCIIhi) cDCs. In order to study these transitional states, we divided SIRPα+ cDCs into four putative differentiation stages (Figure 2a). We selected three cell surface markers, namely, EpCAM, JAM-A, and CD24, based on differential gene expression between DN and CD11b+ cDCs and antibody availability (Figure 2b). We observed a progressive increase of CD11b, MHCII, EpCAM, and JAM-A surface expression from the first (I, CD11b−MHCIIlo cells, DN cDCs) to the last cell population (IV, CD11bintMHCIIhi cells, CD11b+ cDCs), whereas CD24 expression decreased along the same path (Figure 2c). To assess whether DN cDCs could indeed express CD11b, we checked the phenotype of isolated DN cDCs after an overnight culture. Both DN and CD11b+ cDCs increased their surface levels of MHCII after culture and as expected, nearly half of DN cDCs acquired surface expression of CD11b (Figure 2d). We also observed that DN cDCs incorporated the marker of proliferation EdU slightly but significantly faster than CD11b+ cDCs in vivo, suggesting that they were the first to be replaced by progenitors (Figure 2e; Supplementary Figure S1C).
Altogether, these results suggest that DN and CD11b+ cDCs likely represent the two extremities of a PP SIRPα+ cDC developmental path (see Figure 2f for a differentiation model of SIRPα+ dome cDCs).
CD11chiCD11bhi cells of the SED are mainly LysoDCs and LysoMacs
Unlike Ccr7, the gene encoding CCR6, which is a chemokine receptor expressed by immature DCs,30 was expressed at higher levels in DN than in CD11b+ cDCs (Supplementary Figure S1A). CCL20, the ligand of CCR6, is secreted by the FAE in the SED,14, 31 whereas CCL19 and CCL21, the ligands of CCR7, are expressed in the IFR.32, 33, 34 In agreement with these chemokine locations, CCR6 messenger RNA has been detected throughout the follicle and the SED but not in the IFR, whereas CCR7 messenger RNA expression has only been reported in the IFR.14 This suggests that DN and CD11b+ cDCs could be attracted to the SED and the IFR, respectively. Nevertheless, CD11c+CD11b+ cells are known to be mainly located in the SED but not in the IFR.14, 19, 31 However, when we examined into more details the phenotype of these subepithelial CD11c+CD11b+ cells, most of them also expressed lysozyme and CX3CR1, indicating that they were LysoDCs or TIM-4− LysoMacs but not CD11b+ cDCs (Figure 3a). In addition and in agreement with previous reports,14, 19, 31 we only detected rare CD11c+CD11b+ cells in the IFR (Figure 3b). However, the relative ratio of PP mononuclear phagocyte subsets obtained after tissue dissociation of C57BL/6 mouse PP indicated that CD11b+ cDCs were the main subset (Figure 3c). Thus, we were unable to detect the main dome cDC subset by microscopy using CD11b as a marker. We also observed that CX3CR1+ cells of the IFR were not stained with CD11b (Figure 3b), indicating that the expression of CD11b at the surface of TIM-4+ LysoMacs, which represent most CX3CR1+ cells of the IFR (Figure 3d), was too low to be detected by microscopy. Altogether, these data suggest that some phagocytes positive for CD11b by flow cytometry may not be detectable by microscopy with this marker. LysoDCs and CD11b+ DAV cDCs expressed indeed more CD11b than TIM-4+ LysoMacs and CD11b+ dome cDCs by flow cytometry (Figure 3e; Supplementary Figure S2A). Thus, we established a flow cytometry-correlated minimal threshold of detection of the marker CD11b by microscopy (Figure 3e; Supplementary Figure S2A). In agreement with this threshold, LysoDCs, CD11c+CX3CR1− DAV cDCs, CD11c+CX3CR1+ DAV macrophages, and some but not all TIM-4− LysoMacs were stained for CD11b (Supplementary Figure S2A,B). Thus, at steady state, the only PP cDCs detectable by microscopy with CD11b were DAV cDCs. Of note, there was a good correlation between the surface expression of CD11b and its gene expression levels in the different dome phagocyte subsets (Supplementary Figure S2C). Altogether, these data indicate that CD11chiCD11bhi cells of the SED are mostly constituted of LysoDCs and TIM-4− LysoMacs, and raise the question of CD11b+ cDC main location.
CD11b+ dome cDCs are mainly located in the IFR
We sought out to determine the location of CD11b+ dome cDCs using alternative markers. We previously noticed that, although the antibody against lysozyme specifically labels LysoDCs and LysoMacs, green fluorescent protein (GFP) staining of lys-EGFP mice allows the visualization of another subset of CD11chi cells undetectable with the anti-lysozyme antibody.19 We observed that these CD11chiGFP+Lysozyme− cells represented half of the CD11b+ dome cDCs (Figure 4a). In contrast, in Cx3cr1-GFP−/+ mice, nearly all CD11chiMHCII+GFP+ cells expressed lysozyme and were LysoDCs and LysoMacs (Figure 4a). By microscopy, while most GFP+ cells of the IFR of Cx3cr1-GFP−/+ mice were TIM-4+ LysoMacs, many GFP+ cells of the IFR of lys-EGFP mice did not express lysozyme nor TIM-4, indicating that they correspond to the GFP+CD11b+ cDCs detected by flow cytometry (Figure 4b). As expected, these GFP+lysozyme− cells expressed SIRPα and CD11c (Figure 4c). Thus, at least part of CD11b+ dome cDCs was located in the T-cell zone of PPs. In addition to these CD11chiGFP+lysozyme− cells, another important population of CD11chiSIRPα+GFP−lysozyme− cells resided in the IFR (Figure 4c). Moreover, CCR7 staining was observed in cDCs (CD11c+ CX3CR1−cells) of the IFR but not of the SED (Figure 4d; Supplementary Figure S3). As CD8α+ dome cDCs did not express SIRPα (Figure 1a) and DN cDCs expressed less Ccr7 and more Ccr6 than CD11b+ cDCs (Supplementary Figure S1A), CD11chiSIRPα+CCR7+GFP−lysozyme− cells of the IFR were likely CD11b+ cDCs, whereas CD11chiSIRPα+CCR7−GFP−lysozyme− cells of the SED were likely DN cDCs. We quantified the number of cells for each subset on cryostat sections (Figure 4e). Two-third of the total SED phagocyte population was monocyte-derived cells. On the contrary, nearly three quarters (almost half SIRPα+ and a quarter SIRPα−) of the total IFR phagocyte population were cDCs. The IFR contained, however, the specific population of macrophages termed TIM-4+ LysoMacs.
In agreement with these results, when Zbtb46-GFP mice were analyzed for cDC location, most of them (CD11chiGFP+MerTK− cells) were located in the IFR and serosal regions, whereas only a few were in the SED with, however, an enrichment toward crypts and base of domes (Supplementary Figure S4A–C). On the contrary, monocyte-derived cells (CD11chiGFP−MerTK+ cells) were enriched in the SED, especially in its upper part (Supplementary Figure S4A). In general, cDCs appeared smaller and less dendritic than monocyte-derived cells. As expected, cDCs of the SED were stained for SIRPα but not CD11b, which was only observed on monocyte-derived cells (Supplementary Figure S4B,C). Like LysoDCs, few cDCs resided in the FAE, sometimes in close contact with LysoDCs (Supplementary Figure S4B,C). In the IFR, the major part of cDCs expressed SIRPα (Supplementary Figure S4C).
In conclusion, the SED, the key site of antigen uptake, is dominated by monocyte-derived cells, whereas the IFR, the major site of antigen presentation, is outnumbered by cDCs (see Figure 10 for a summary model).
TLR7 ligand stimulation induces an increase of CD8α+ interfollicular cDC number and migration of DAV cDCs in the IFR
We studied the behavior of PP cDCs upon a perturbation of homeostasis through detection of an activation signal in vivo. R848 is a TLR7 agonist known to drastically alter intestinal DC distribution, migration, and activation, including those of PPs.12 Alteration induced by R848 did not strongly interfere with our PP phagocyte gating strategy (Supplementary Figure S5A). We observed that the absolute number of CD8α+ cDCs doubled 9 h after R848 gavage of C57BL/6 mice, whereas those of DN and CD11b+ dome cDCs remained stable (Figure 5a). Accordingly, the proportion of CD8α+ cDCs among PP cDCs increased from 16.5±2.1 to 25.1±5.3% (Figure 5b).
Surprisingly, although villus cDCs are known to massively and rapidly migrate to the mesenteric lymph nodes (MLNs) upon R848 treatment,12 we did not observe any loss of DAV cDCs after tissue dissociation (Figure 5a,b). In parallel, we observed a strong recruitment of CD11chiCX3CR1−CD11bhi cDCs in the IFR (Figure 5c to be compared with Figure 3b). In order to determine whether these newly recruited interfollicular cDCs were coming from DAV, we investigated the expression of CD101, which gene was expressed by CD11b+ cDCs of the villus but not of the dome (Figure 5d). At steady state, CD101 was expressed by DAV but not by interfollicular cDCs (Figure 5e; Supplementary Figure S6). However, CD11c+CX3CR1−CD101+ cDCs were massively recruited in the IFR upon R848 treatment, whereas there were very few left in DAV as compared to untreated PP (Figure 5f; Supplementary Figure S6). There was an anatomic continuity between the base of DAV and the IFR, and we observed the appearance of CD11c+CX3CR1−CD101+ cDCs at the base of DAV and in DAV crypts from 5 h of R848 treatment onwards (Figure 5g). This indicates that the recruitment of cDCs from DAV to the IFR occurred through migration across the base and the crypts of DAV. Interestingly, CCR7 expression was upregulated in DAV cDCs (Supplementary Figure S5B) and appeared in DAV crypt-located CD11c+CX3CR1− cDCs (Figure 5h; Supplementary Figure S3). Altogether, these data indicate that, following R848 treatment, the IFR is a site of DAV cDC migration.
TLR7 ligand induces the activation of both CD11b+ and CD8α+ interfollicular cDCs.
R848 treatment induced an alteration of CD8α+ cDC phenotype with an increase of MHCII and a slight decrease of CD11c surface expression (Figure 6a). Although less pronounced, a similar activation profile was observed for CD11b+ dome cDCs.
At steady state, PP CD8α+ cDCs can be detected using CD205.14 We confirmed that CD205 was expressed by all CD8α+ cDCs but not or weakly by SIRPα+ cDCs (Figure 6b). However, upon R848 gavage, one-third of CD11b+ dome cDCs but very few DN dome cDCs acquired CD205. Moreover, expression of CD205 on CD11b+ dome cDCs was correlated with their state of activation (Figure 6b). This confirmed the immature status of DN as compared to CD11b+ cDCs. By confocal microscopy, CD205 was absent from the SED of R848-treated mice, indicating that R848 did not induce the recruitment of CD8α+ and activated CD205+CD11b+ cDCs in the SED (Figure 6c). However, CD205 was strongly expressed in the IFR of R848-fed mice, indicating that both activated CD8α+ cDCs and CD11b+ cDCs reside in the IFR (Figure 6d). The activated status of interfollicular cDCs was further confirmed by the strong increase of the staining for CCR7, the activation marker CD83, and the co-stimulatory molecule CD86 in the IFR of R848-treated mice (Supplementary Figures S3 and S7A,B).
R848-induced PP cDC stimulation is indirect and mediated at least in part through a TNF-dependent mechanism
TLR7 messenger RNA and protein were detected in PP monocyte-derived cells (LysoDCs and LysoMacs) and pDCs but not in cDCs (Figure 7a,b). Migration and activation of PP cDCs is thus likely to be indirect. We previously showed that LysoDCs and LysoMacs produce and secrete TNF upon R848 stimulation in vitro.17 Moreover, Yrlid et al.12 have shown that R848-induced migration of villus DCs to the MLN is dependent on TNF. We thus investigated the role of TNF in PP cDC migration and activation processes. As previously reported, migration of villus DCs to the MLN was impaired when TNF signaling was neutralized (Figure 7c). In PP, TNF inhibition prevented the increase of CD8α+ cDC number and strongly decreased interfollicular cDC activation (Figure 7d,e). In addition, the recruitment of CD101+ DAV cDC in the IFR was blocked by anti-TNF treatment (Figure 7e). Therefore, both migration and to some extent activation of dome and DAV cDCs were dependent on TNF.
The genetic reprograming of R848-activated interfollicular cDCs converges toward steady-state PP monocyte-derived cell transcriptional profiles and induces the expression of both immuno-stimulatory and -inhibitory molecules
As activated cDCs display a distinct phenotypical pattern (Figure 6a), quintuplicates of activated CD8α+ cDCs and triplicates of activated CD11b+ cDCs were isolated and submitted to mouse whole-genome microarray analysis. Generated data were combined with those of phagocytes from unstimulated mice. CD8α+ cDCs were much more impacted by R848 treatment than CD11b+ cDCs with 1,052 DEGs as compared to 356 DEGs for CD11b+ cDCs (Figure 8a). Fifty-three DEGs between activated and resting cDCs belonged to the core gene signature associated with activated DCs as defined by Vu Manh et al.5 (Supplementary Table S3). A striking feature was the induction and repression in both cDC subsets of interferon-stimulated and -inhibited genes, respectively. (Figure 8a). A set of chemokine genes was induced in stimulated cDCs (Ccl19 for CD8α+ cDCs; Ccl8, Cxcl9, and Cxcl10 for CD11b+ cDCs; and Ccl5 and Ccl22 for both subsets; Figure 8a,b). CCL22 was indeed strongly expressed in the IFR of R848-fed mice (Supplementary Figure S7C). Il15 was the main cytokine gene to be upregulated in both subsets upon stimulation (Figure 8a). Interestingly, genes involved in cell migration were drastically downregulated in both activated cDC subsets at the notable exception of Ccr7 and of the two integrin genes Itga4 and Itgb1, which proteins (CD49d and CD29) form the integrin complex VLA4 (Figure 8a,b). In agreement with these data, CCR7 and CD49d were strongly expressed in interfollicular cDCs (Figures 5h and 8c; Supplementary Figure S3).
Activation tended to attenuate cDC subset identity as both R848-activated CD11b+ and CD8α+ cDCs clustered together apart from their resting counterparts (Figure 8d). Accordingly, genes encoding key general cDC markers (e.g., CD11c, CD103, and c-Kit) or markers of CD11b+ (e.g., CD11b, CLEC4A4, and M-CSFR) and CD8α+ (e.g., XCR1, CLEC9A, and TLR3) cDCs were strongly downregulated in activated as compared to resting state (Figure 8a; Supplementary Figure S8A). Although still detectable, we indeed observed a decrease of XCR1 molecules at the surface of activated CD8α+ cDCs (Supplementary Figure S8B). As the expression of Sirpa and Cd8a was not or weakly altered (Supplementary Figure S8A), they represent key markers to distinguish PP SIRPα− (CD8α+) from SIRPα+ (DN/CD11b+) cDCs whatever their state of activation. Upon activation, CD101 was not induced in CD11b+ dome cDCs, thus confirming the DAV origin of CD101+ interfollicular cDCs in R848-fed mice (Supplementary Figure S8C).
In principal component analysis, the second principal component separated resting from activated cDCs (Figure 8e). Interestingly, steady-state PP monocyte-derived cells (i.e., LysoDCs and LysoMacs) segregated with activated cDCs on this axis, suggesting that the former displayed a constitutive activated state. Accordingly, there was a main contribution to this axis of interferon-stimulated genes (e.g., GBP family of genes, Irf7, Rsad2, Zbp1, Oasl1, Oasl2, and Vcam1; Supplementary Table S4) expressed by steady-state PP monocyte-derived cells.17 Sixty-three upregulated genes in resting PP monocyte-derived cells as compared to resting cDCs became upregulated in activated cDCs as compared to resting cDCs (Supplementary Table S3), confirming this shift of activated cDCs toward a genetic program already imprinted in steady-state PP monocyte-derived cells.
BubbleGUM analysis (Figure 9a; Supplementary Table S2) confirmed the enrichment of type I interferon-stimulated genes in resting LysoDCs and LysoMacs (green boxes) and in activated PP cDCs (blue box) as compared to resting cDCs. As expected, cDC migration and activation gene signatures were enriched in activated as compared to resting PP cDCs (orange box, Figure 9a). Surprisingly, in addition to genes linked to the activation of the immune response, those related to its control were also enriched in activated PP cDCs as compared to their resting counterparts (Figure 9a, black box). In order to confirm this early upregulation of immunomodulatory molecules in R848-treated mice, we investigated the expression of two major T-cell activation suppressors, PD-L1 and PD-L2, which transcripts were strongly upregulated in CD8α+ cDCs (Figure 9b). These two molecules were indeed strongly induced in interfollicular cDCs of 9 h R848-fed mice (Figure 9c,d). These data indicate that activated interfollicular cDCs have a contrasted pattern of gene expression that could lead to either stimulation or inhibition of T-cell activation.
Discussion
In this study, we determined the genetic relationship and the location of cDC subsets in PP and analyzed their alteration upon a TLR7 agonist stimulation in vivo. We previously showed that DN and CD11b+ dome cDCs are Batf3-independent and share some surface receptors such as SIRPα and Clec4a4.17 Here we extended these findings by showing that they belong to a unique SIRPα+ cDC subset. Thus, our whole-genome expression analysis shows that they cluster together apart from CD8α+ cDCs, and that DN cDCs could correspond to a more immature differentiation state of SIRPα+ cDCs than CD11b+ cDCs. In agreement with this transcriptional analysis, we identified putative transitional states between DN and CD11b+ cDCs with progressive surface acquisition of MHCII, CD11b, EpCAM, and JAM-A.
Although it has been known for a long time that CD11c+CD11b+ cells are located in the SED,14, 35, 36 the accurate identity of these phagocytes remained obscure, especially because three different dome phagocyte subsets with distinct origin express both integrins.17 The expression levels of CD11b differ between these phagocyte subsets17 and we show here that those that are actually detectable by microscopy in the SED with CD11b correspond to LysoDCs and some TIM-4− LysoMacs but not CD11b+ cDCs. Accordingly, the main phagocyte populations of the SED are constituted of LysoDCs and TIM-4− LysoMacs (Figure 10). In turn, CD11b+ cDCs are mainly located in the IFR, although some of them may be present in the SED, especially at its base. Recently, Reboldi et al.37 have reported that efficient IgA class switching of PP B cells requires their interaction with CD11chiMHCII+CD11b+ cells in the SED. However, whether these CD11chiMHCII+CD11b+ phagocytes correspond to CD11b+ cDCs, LysoDCs, or LysoMacs remains to be established. Comparison of the ratio of the different subsets obtained by flow cytometry with the ratio of the subsets that can be well defined with markers by microscopy suggests that DN cDCs are mainly located in the SED in agreement with their high and low expression of Ccr6 and Ccr7, respectively as compared to CD11b+ dome cDCs. We indeed found that cDCs of the IFR express CCR7, whereas those of the SED do not. Interestingly, CD11b+CD11c+ cells of the SED are known to be sensitive to CCL9 inhibition but not CCR6 deficiency,31 which is in agreement with the fact that LysoDCs and LysoMacs do not express Ccr6 but Ccr1.17 However, CCR6 may be required to recruit DN cDCs in the SED and the FAE, especially upon infection.38
R848 induces an indirect TNF-mediated activation of PP cDCs, which tends to attenuate each subset specificity while promoting common activation features, as previously observed on spleen cDCs after viral infection.5 Thus, key marker genes of each cDC subset are downregulated upon activation. Nevertheless, SIRPα expression stability during activation or during homeostatic maturation confirms that it is a much better marker of cDC2 than CD11b. Upon activation, cDCs acquire the expression of innate defense genes that otherwise belong to the signature of PP monocyte-derived cells. This strongly supports the role of SED-located LysoDCs and TIM-4− LysoMacs as the main constitutive first line of defense of PP. CD8α+ cDCs also rapidly acquire the expression of inhibitors of the T-cell response, such as PD-L1 and PD-L2, indicating that the immune response initiation is probably tightly regulated. This could also represent a way to favor naive T-cell priming rather than resident effector T-cell reactivation, as only some of the latter express the PD-L1 and PD-L2 receptor PD-1.39
Upon stimulation, SED DCs are believed to migrate from the SED to the IFR enriched in T cells in order to induce a mucosal adaptive immune response. This is supported by the fact that microsphere-loaded CD11c+ cells normally located in the SED are observed in the IFR after cholera toxin or Salmonella Typhimurium feeding.8 In addition, systemic injection of soluble Toxoplasma gondii tachyzoite antigen induces a loss of CD11c+CD11b+ cells in the SED and a concomitant recruitment of CD11c+CD11b+ cells in the IFR.14 Finally, the number of CD103+ cells supposed to be cDCs has been shown to increase in the IFR of R848-fed rats.12 Here we confirmed that cDC number rises in the IFR of mice upon R848 gavage and that all activated cDCs reside in the IFR as illustrated by their CD205, CD83, CD86, CD49d, CCL22, and CCR7 expression in this region. However, we also showed that this is at least in part due to CD8α+ interfollicular cDC number increase and to DAV cDC recruitment (Figure 10). The latter migration could allow in a single place a simultaneous comparison of antigens that have been sampled either in DAV or in SED. Taking into account that uptake of pathogens and toxins is largely favored in the FAE as compared to villus epithelium,18, 19, 40, 41 such mechanism of antigen screening could help the mucosal immune system to distinguish innocuous from hazardous matters. It has now to be determined whether other stimuli than R848 induce similar migratory activities of DAV cDCs. If so, the current model of PP phagocyte activation will have to be refined and identity of migrating phagocytes to the IFR carefully assessed.
Methods
Antibodies. Antibodies used are listed in Supplementary Information.
Animals. Six- to ten-week-old C57BL/6 mice were from Charles River Laboratories (Saint-Germain-Nuelles, France). Lys-EGFP and Cx3cr1-GFP and Zbtb46-GFP mice have been previously described.42, 43, 44 All experiments were done in agreement with French and European guidelines for animal care.
Chemical treatments. Mice were injected intraperitoneal with EdU (Thermo Fisher Scientific Inc., Waltham, MA). For R848 in vivo experiments, mice were fed with 10 μg of R848 (Invivogen, San Diego, CA, USA). An amount of 330 μg rat anti-TNF-blocking antibody (clone MP6-XT22; BioLegend, San Diego, CA) or of isotype control (clone RTK2071) was given to mice intraperitoneal 30 h before R848.
PP cell extraction. PPs were digested for 40 min at room temperature with collagenase/DNase as previously described.45 All subsequent procedures were at 0–4 °C. CD11c+ cells were sorted using anti-CD11c microbeads and an AutoMACS magnetic cell separator according to the manufacturer’s instructions (Miltenyi Biotec, Bergisch Gladbach, Germany).
Flow cytometry and cell sorting. CD11c+ cells were preincubated on ice for 10 min with the 2.4G2 antibody to block Fc receptors, stained for surface markers, and then permeabilized for lysozyme labeling according to the manufacturer’s protocol (Intracellular staining kit; BD Biosciences, San Jose, CA). Cell viability was evaluated using Fixable Viability Dye eFluor 506 (eBiosciences, Thermo Fisher Scientific Inc.). Multiparameter flow cytometry and cell sorting were performed using a FACS LSRII and a FACSAria III (BD Biosciences), respectively. Data were analyzed with the BD FACSDiva software (BD Biosciences).
In vitro DC culture. Sorted PP DN and CD11b+ DC subsets (5 × 103 cells) were immediately fixed (control) or cultured overnight in RPMI-1640 supplemented with 10% fetal calf serum, 1% granulocyte–macrophage colony-stimulating factor, 10% macrophage colony-stimulating factor, 1% penicillin/streptomycin, 10 mM HEPES, 1 mM sodium pyruvate, 1 mM glutamine, 1 mM non-essential amino-acids, and 50 mM 2-ME. CD11b and MHCII surface expression were determined by flow cytometry as above.
RNA isolation and microarray analysis. The total RNA of PP-sorted phagocytes from three to five independent experiments was extracted with a RNAeasy PLUS micro kit (Qiagen, Hilden, Germany). Quantity, quality, and absence of genomic DNA contamination were assessed with a Bioanalyser (Agilent Technologies, Santa Clara, CA). Microarray experiments were performed by the Plateforme Biopuces of Strasbourg, France (http://www.igbmc.fr/technologies/5/team/54/) using the GeneChip Mouse Gene 1.0 ST array (Affymetrix, Thermo Fisher Scientific Inc.). Quality controls and normalization of array data were performed as previously described.45
Immunofluorescence staining and confocal microscopy. PPs of mice fed or not with R848 for 9 and 16 h were fixed with Antigenfix (Diapath, Martinengo, Italy) for 1 h, washed and processed as previously described.18 PP sections from anti-TNF-treated mice were first incubated with the Fab fragment of donkey anti-rat IgG (Jackson ImmunoResearch, West Grove, PA) to prevent the detection of rat anti-TNF with anti-rat secondary antibodies. Slides were observed with a Zeiss LSM 780 confocal microscope (Carl Zeiss, Oberkochen, Germany). Images were analyzed using Adobe Photoshop CS6 (Adobe systems, San Jose, CA).
Statistical analysis. Results were compared with GraphPad Prism 6 software (GraphPad Software, La Jolla, CA) using unpaired t-test with Welch’s correction.
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Acknowledgements
We thank the CIML histology, cytometry, and mouse house core facilities; Violaine Alunni and Christelle Thibault from the “Plateforme Biopuces et sequençage de l’IGBMC” (Strasbourg, France) for performing the microarray experiments; M. Barad for cell-sorting experiments; C. Jones, T. Soos, and C. Arendt for helpful discussions. We acknowledge the PICSL imaging facility of the CIML (ImagImm), member of the national infrastructure France-BioImaging supported by the French National Research Agency (ANR-10-INBS-04). This work was supported by institutional grants from INSERM, CNRS, and Aix-Marseille University to the CIML and by the I2HD collaborative project developed jointly by CIML and SANOFI. CDS was supported by the FRM fellowship FDT20160434982.
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The microarray data have been deposited to the NCBI GEO under accession numbers GSE94380 and GSE65514.
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J.B. and H.L. designed the study. C.D.S., C.W., R.B. and J.B. performed all experiments. C.D.S., J.B. and H.L. analyzed and interpreted the data. H.L. wrote the manuscript. J.P.G., J.B. and C.D.S. contributed to the design of the study and revised the manuscript. L.C. performed cryostat sectioning. M.M., E.P. and M.D. analyzed the microarray data and gave feedback on the manuscript.
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Bonnardel, J., Da Silva, C., Wagner, C. et al. Distribution, location, and transcriptional profile of Peyer’s patch conventional DC subsets at steady state and under TLR7 ligand stimulation. Mucosal Immunol 10, 1412–1430 (2017). https://doi.org/10.1038/mi.2017.30
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DOI: https://doi.org/10.1038/mi.2017.30