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. 2018 May 29;8:8259. doi: 10.1038/s41598-018-25646-8

Leukocyte mono-immunoglobulin-like receptor 8 (LMIR8)/CLM-6 is an FcRγ-coupled receptor selectively expressed in mouse tissue plasmacytoid dendritic cells

Ayako Kaitani 1,2, Kumi Izawa 1,2, Akie Maehara 1,2, Masamichi Isobe 1,2, Ayako Takamori 1, Toshihiro Matsukawa 2,3, Mariko Takahashi 2, Yoshinori Yamanishi 2,4, Toshihiko Oki 2, Hiromichi Yamada 1,5, Masakazu Nagamine 1, Shino Uchida 1,6, Koichiro Uchida 1, Tomoaki Ando 1, Keiko Maeda 1, Nobuhiro Nakano 1, Toshiaki Shimizu 1,5, Toshiyuki Takai 7, Hideoki Ogawa 1, Ko Okumura 1, Toshio Kitamura 2,✉, Jiro Kitaura 1,2,✉
PMCID: PMC5974347  PMID: 29844322

Abstract

Plasmacytoid dendritic cells (pDCs) produce large amounts of type-I interferon (IFN) in response to viral infection or self nucleic acids. Leukocyte mono-immunoglobulin-like receptor 8 (LMIR8), also called CMRF-35-like molecule-6 (CLM-6), is a putative activating receptor among mouse LMIR/CLM/CD300 members; however, the expression and function of LMIR8 remain unclear. Here, we characterize mouse LMIR8 as a pDC receptor. Analysis of Flag-tagged LMIR8-transduced bone marrow (BM)-derived mast cells demonstrated that LMIR8 can transmit an activating signal by interacting with immunoreceptor tyrosine-based activating motif (ITAM)-containing FcRγ. Flow cytometric analysis using a specific antibody for LMIR8 showed that LMIR8 expression was restricted to mouse pDCs residing in BM, spleen, or lymph node. FcRγ deficiency dampened surface expression of LMIR8 in mouse pDCs. Notably, LMIR8 was detected only in pDCs, irrespective of TLR9 stimulation, suggesting that LMIR8 is a suitable marker for pDCs in mouse tissues; LMIR8 is weakly expressed in Flt3 ligand-induced BM-derived pDCs (BMpDCs). Crosslinking of transduced LMIR8 in BMpDCs with anti-LMIR8 antibody did not induce IFN-α production, but rather suppressed TLR9-mediated production of IFN-α. Taken together, these observations indicate that LMIR8 is an FcRγ-coupled receptor selectively expressed in mouse tissue pDCs, which might suppress pDC activation through the recognition of its ligands.

Introduction

Paired activating and inhibitory receptor families positively or negatively regulate immune cell activation1,2. Examples include CD300, also called leukocyte mono-immunoglobulin-like receptor (LMIR), CMRF-35-like molecule (CLM), and myeloid-associated immunoglobulin-like receptor (MAIR)3–8. CD300/LMIR/CLM members harbor highly homologous immunoglobulin-like domains in their extracellular regions; CD300a/LMIR1/CLM-8 and CD300f/LMIR3/CLM-1 are inhibitory receptors that contain the immunoreceptor tyrosine-based inhibitory motif (ITIM) in the cytoplasmic region, while other members are putative activating receptors that are coupled with immunoreceptor tyrosine-based activating motif (ITAM)-bearing adaptor proteins such as FcRγ and DNAX activating protein 12 (DAP12)3–9. Lipids or lipid-binding proteins have been identified as ligands for several CD300/LMIR members in mice and humans9–17. Accumulated studies using CD300a−/−, CD300b−/−, or CD300f−/− mice implicate CD300 molecules in the pathogenesis of inflammatory diseases, autoimmune diseases, and infectious diseases9–12,18–20.

Plasmacytoid dendritic cells (pDCs) are a unique subset that specializes in the production of type I interferons (IFNs). pDCs recognize viruses and self nucleic acids through Toll-like receptor 7 (TLR7) and TLR9, which are located in endosomal compartments, resulting in the secretion of proinflammatory cytokines and chemokines, via the myeloid differentiation primary response protein 88 (MYD88)-nuclear factor-κB (NF-κB) pathway, and type I interferons (IFNs), via the MYD88-interferon regulatory factor 7 (IRF7) pathways. pDCs can also function as antigen-presenting cells. Accordingly, pDCs participate not only in anti-viral innate immunity but also in adaptive immunity involving autoimmunity21–25. Surface markers of pDCs in mice include CD11c, B220, Ly-6C, bone marrow (BM) stromal antigen 2 (BST2), and sialic acid-binding immunoglobulin-like lectin H (Siglec-H)21–24. Human pDCs selectively express blood dendritic cell antigen-2 (BDCA2) and immunoglobulin-like transcript 7 (ILT7)21–24. Cell surface receptors expressed by pDCs are known to regulate the amplitude of type I IFN production. Notably, high avidity crosslinking of pDC receptors (e.g., BDCA2, ILT7, and NKp44 in humans and Siglec-H and BST2 in mice), interacting with FcRγ or DAP12, attenuates TLR7/9-mediated production of IFN-α or proinflammatory cytokines21–33. However, the relevant molecular mechanisms remain unclear.

In the present study, we analyzed the expression and function of mouse LMIR8/CLM-6, demonstrating that LMIR8, an FcRγ-coupled receptor, is selectively expressed in pDCs. In addition, we found that LMIR8 engagement induces cytokine production of BM-derived mast cells (BMMCs) transduced with LMIR8, while it suppresses the TLR9-mediated production of IFN-α in Flt3 ligand-induced BM-derived pDCs (BMpDCs) transduced with LMIR8. Although expression and function of human CD300a/CD300c in pDCs were previously reported34,35, this is the first demonstration of a possible specialized role of LMIR8 in mouse pDCs.

Results

Mouse LMIR8/CLM-6 is an N-glycosylated surface receptor that is likely expressed in hematopoietic cells

We cloned a full-length cDNA for LMIR8/CLM-6 from a C57BL/6 J mouse BM cDNA library. LMIR8 protein is composed of an N-terminal signal peptide, an extracellular region, a transmembrane domain with a positively charged residue lysine, and a short cytoplasmic tail without signaling motifs such as ITAM and ITIM. LMIR8 contains an immunoglobulin-like domain in the extracellular region that shares 70% identity of amino acid sequences with that of the inhibitory receptor LMIR1 (CLM-8/CD300a) (Fig. 1a)3–5. The existence of a positively charged residue lysine in the transmembrane domain of LMIR8 led us to postulate that like other activating LMIR members, LMIR8 might interact with an adaptor protein bearing a negatively charged residue in the transmembrane domain. We then examined expression profiles of LMIR8 in mouse tissues. Reverse transcription polymerase chain reaction (RT-PCR) analysis showed that LMIR8 expression was detectable in BM, spleen, or thymus (Fig. 1b and Supplementary Fig. S1), suggesting that LMIR8 is expressed in hematopoietic cells. Accordingly, we transduced Flag-tagged LMIR8 or mock into the pro-B cell line Ba/F3. Staining of these transfectants with anti-Flag antibody (Ab) displayed surface expression of Flag-tagged LMIR8 in the transduced Ba/F3 cells, but not in mock transfectants, confirming that LMIR8 is a surface receptor (Fig. 1c). As revealed by Western blot analysis using anti-Flag Ab, Flag-tagged LMIR8 protein expression in Ba/F3 cell transfectants was detected as several protein bands (44–46, 29–30, 27–28, or 26 kDa), whereas the same protein was recognized as two bands with lower molecular weights (23–24 or 21 kDa) by pre-treatment with N-Glycosidase F (Fig. 1d and Supplementary Fig. S1). These results indicate that LMIR8 is an N-glycosylated protein, which was supported by the existence of a putative N-glycosylation site within the extracellular domain of LMIR8. Thus, LMIR8 is an N-glycosylated surface receptor that is likely expressed in hematopoietic cells.

Figure 1.

Figure 1

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Mouse LMIR8 is an N-glycosylated surface receptor. (a) The phylogenetic tree of LMIR1/CLM-8, LMIR2/CLM-4, and LMIR8/CLM-6 is shown based on homology with the immunoglobulin-like domain. Percentages of identity in amino acid sequences of the immunoglobulin-like domain are depicted. (b) RT-PCR analysis of LMIR8 or β-actin (control) expression in murine tissues is indicated. (c) Ba/F3 cells transduced with Flag-tagged LMIR8 or mock were stained with mouse anti-Flag Ab or a control Ab followed by PE-conjugated anti-mouse IgG goat F(ab’)2 Ab. (d) Lysates of Ba/F3 cells transduced with either Flag-tagged LMIR8 or mock were immunoprecipitated with mouse anti-Flag Ab. The precipitates treated with or without μM N-glycosidase F were immunoblotted with rabbit anti-Flag Ab. (b–d) One representative of three independent experiments is shown.

LMIR8 transmits an activating signal in transduced BMMCs

To test if LMIR8 acts as an activating receptor, Flag-tagged LMIR8 or mock was transduced into BMMCs that express ITAM-containing adaptor proteins such as FcRγ. Equivalent levels of FcεRI and c-Kit were exhibited by these transfectants (Fig. 2a). We confirmed that Flag-tagged LMIR8 was expressed in the transduced BMMCs, but not in mock transfectants (Fig. 2a). When these two BMMC transfectants were stimulated with plate-coated anti-Flag Ab or a control Ab, we found significant cytokine (IL-6 and TNF-α) production of Flag-tagged LMIR8-transduced BMMCs in response to stimulation with plate-coated Flag Ab, but not with a control Ab (Fig. 2b). In contrast, the same stimulation did not induce cytokine production of mock-transduced BMMC (Fig. 2b). Stimulation with phorbol 12-myristate 13-acetate (PMA) led to comparable levels of cytokine production between the two types of BMMC transfectants (Fig. 2b). Thus, LMIR8 engagement induced cytokine production in the transduced BMMC transfectants. Consistent with this, stimulation with anti-Flag Ab caused remarkable activation of extracellular signal-regulated kinase (ERK) in Flag-tagged LMIR8-transduced BMMCs, but not in mock transfectants (Fig. 2c and Supplementary Fig. S2). These results indicate that LMIR8 can act as an activation receptor in the transduced BMMC transfectants.

Figure 2.

Figure 2

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LMIR8 transmits an activating signal in transduced BMMCs. (a) BMMCs transduced with Flag-tagged LMIR8 or mock were stained with FITC-conjugated anti-FcεRIα Ab and PE-conjugated anti-c-Kit Ab or with mouse anti-Flag Ab or a control Ab followed by PE-conjugated anti-mouse IgG goat F(ab’)2 Ab. (b) BMMCs transduced with Flag-tagged LMIR8 or mock were stimulated with plate-coated anti-Flag Ab or a control Ab or with 100 nM PMA or PBS as a control. IL-6 or TNF-α released into the culture supernatants were measured by ELISA. (c) BMMCs transduced with Flag-tagged LMIR8 or mock were stimulated with anti-LMIR8 Ab for 3 or 15 min. Cell lysates were subjected to immunoblotting with anti-phospho-p44/42 MAPK (pERK1/2) Ab or anti-ERK1/2 Ab. (a,c) One representative of three independent experiments is shown. (b) All data points correspond to the mean ± S.D. of three independent experiments. Statistically significant differences are shown. *p < 0.01 (Student’s t-test).

FcRγ is required for maintaining maximum surface expression of and transmitting an activation signal by the transduced LMIR8 in BMMC transfectants

To test if FcRγ is an adaptor protein of LMIR8, wild-type (WT) or FcRγ−/− BMMCs were transduced with Flag-tagged LMIR8. We found that FcRγ deficiency dampened surface expression of FcεRI as expected but did not influence surface expression levels of c-Kit (upper panels in Fig. 3a)6. Notably, the loss of FcRγ substantially, but not completely, lowered surface expression levels of Flag-tagged LMIR8 in the BMMC transfectants (lower panels in Fig. 3a). Possibly related to this, the loss of FcRγ abolished the production of pro-inflammatory cytokines (IL-6 and TNF-α) triggered by Flag-tagged LMIR8 crosslinking with anti-Flag Ab in the BMMC transfectants, presumably in part due to the lowered surface expression of Flag-tagged LMIR8 in the FcRγ-deficient BMMC transfectants (Fig. 3b). We confirmed that FcRγ deficiency did not significantly affect PMA-induced cytokine production of BMMCs transduced with Flag-tagged LMIR8 (Fig. 3b). In addition, FcRγ deficiency dampened Flag-tagged LMIR8-mediated ERK activation of the transduced BMMCs (Fig. 3c and Supplementary Fig. S3). Although it was clear that FcRγ was required for maintaining maximum surface expression of the transduced LMIR8, we asked if FcRγ was indispensable for transmitting an activation signal mediated by the transduced LMIR8 in BMMC transfectants. To this end, FcRγ−/− BMMCs were transduced with Flag-tagged LMIR8 together with FcRγ WT, FcRγ mutant in which tyrosine residues within the ITAM of FcRγ were replaced with phenylalanine residues, or mock. Notably, FcRγ−/− BMMCs transduced with FcRγ WT or FcRγ mutant exhibited comparable levels of the transduced Flag-tagged LMIR8 as well as FcεRI on the cell surfaces (Fig. 3d). We confirmed that the loss of FcRγ dampened FcεRI expression and remarkably lowered Flag-tagged LMIR8 expression in the BMMCs transfectants (Fig. 3d). Comparable levels of c-Kit expression were observed in these three transfectants (Fig. 3d). Then, BMMC transfectants were stimulated with plate-coated anti-Flag Ab or a control Ab. The results show that stimulation with anti-Flag Ab, but not with a control Ab, induced significant cytokine production in the transfectants expressing FcRγ WT (Fig. 3e). It should be noted that FcRγ mutant-expressing transfectants did not induce cytokine production at all in response to stimulation with anti-Flag Ab (Fig. 3e). These results indicate that the ITAM of FcRγ was indispensable for delivering an activating signal of LMIR8 in the BMMC transfectants. Co-immunoprecipitation experiments verified that LMIR8 could physically interact with FcRγ in the transiently transfected 293 T cells (Fig. 3f and Supplementary Fig. S3). Collectively, FcRγ was required for maintaining maximum surface expression of and transmitting an activation signal through the transduced LMIR8 in BMMC transfectants.

Figure 3.

Figure 3

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The role of FcRγ in the transduced Flag-taggedLMIR8 in BMMC transfectants. (a,d) WT or FcRγ−/− BMMCs transduced with Flag-tagged LMIR8 (a) or FcRγ−/− BMMCs transduced with FcRγ WT, FcRγ Mt, or mock (d) were stained with FITC-conjugated anti-FcεRIα Ab and PE-conjugated anti-c-Kit Ab (upper panel) or with mouse anti-Flag Ab or a control Ab followed by PE-conjugated anti-mouse IgG goat F(ab’)2 Ab (lower panel). (b,e) WT or FcRγ−/− BMMCs transduced with Flag-tagged LMIR8 (b) or FcRγ−/− BMMCs transduced with FcRγ WT, FcRγ Mt, or mock (e) were stimulated with plate-coated anti-Flag Ab or a control Ab or with 100 nM PMA or PBS as a control. IL-6 or TNF-α released into the culture supernatants were measured by ELISA. (c) WT or FcRγ−/− BMMCs transduced with Flag-tagged LMIR8 were stimulated with anti-Flag Ab for 3 or 15 min. Cell lysates were subjected to immunoblotting with anti-phospho-p44/42 MAPK (pERK1/2) Ab or anti-ERK1/2 Ab. (f) Lysates of 293 T cells transiently expressing Myc-tagged LMIR8 or mock together with Flag-tagged FcRγ or mock were immunoprecipitated with anti-Myc Ab or mouse anti-Flag Ab, and then immunoblotted with rabbit anti-Flag Ab or anti-Myc Ab. (a,c,d,f) One representative of three independent experiments is shown. (b,e) All data points correspond to the mean ± S.D. of three independent experiments. Statistically significant differences are shown. *p < 0.01 (Student’s t-test).

LMIR8 is selectively expressed in mouse tissue pDCs

To analyze the expression profiles of LMIR8 in hematopoietic cells, we generated a monoclonal Ab for LMIR8. Like anti-Flag Ab, this Ab detected surface expression of the transduced Flag-tagged LMIR8 in Ba/F3 cells (Fig. 4a). By contrast, anti-LMIR8 Ab did not recognize Flag-tagged mouse LMIR1 (CLM-8), LMIR2 (CLM-4), LMIR3 (CLM-1), LMIR4 (CLM-5), LMIR5 (CLM-7), LMIR7 (CLM-3), or mock on the surface of the transduced Ba/F3 cells3–8, although we found surface expression of each LMIR member tested by using anti-Flag Ab (Fig. 4a). Thus, we confirmed the specificity of a newly generated monoclonal Ab for LMIR8. We then stained BM cells with anti-LMIR8 Ab and performed flow cytometric analysis. When FSClowSSClow or FSChighSSChigh BM cells were gated, we found that LMIR8 were not expressed in CD3+ T cells, CD19+ B cells, NK1.1+ NK cells, or CD11b+ myeloid cells (Fig. 4b,c). Notably, LMIR8 was expressed in a subpopulation of FSCintSSCint BM cells, which expressed Siglec-H, BST-2, B220, and CD11c (Fig. 4d). In addition, we found that CD11c+B220+ or BST2+Siglec-H+ BM cells corresponding to pDCs expressed high levels of LMIR8 (Fig. 4e,f)21–24. In addition, LMIR8 was highly expressed in BST2+Siglec-H+ pDCs in both spleen and lymph node (Fig. 4g,h). It should be noted that LMIR8 was only weakly expressed in Flt3 ligand-induced BMpDCs (Fig. 4i). Neither BM-derived myeloid dendritic cells (BMmDCs), BM-derived macrophages (BMΦ), nor BMMCs expressed LMIR8 (Fig. 4i). Collectively, these results indicate that LMIR8 was selectively expressed in pDCs in mouse tissues.

Figure 4.

Figure 4

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LMIR8 is highly expressed in pDCs. (a) Ba/F3 cells transduced with Flag-tagged LMIR1, LMIR2, LMIR3, LMIR4, LMIR5, LMIR7, LMIR8, or mock were stained with mouse anti-Flag Ab or a control Ab followed by PE-conjugated anti-mouse IgG goat F(ab’)2 Ab (upper panel) or with biotinylated anti-LMIR8 Ab or biotinylated rat IgG2a Ab followed by PE-conjugated streptavidin. (b–h) Single cell suspensions were prepared from BM (b–f), spleen (g), or lymph node (h). (b–d) Cells were stained with biotinylated anti-LMIR8 Ab or biotin rat IgG2a Ab followed by PE-conjugated streptavidin and FITC-conjugated Abs as indicated. FSClowSSClow populations (b), FSChighSSChigh populations (c), or FSCintSSCint populations (d) were gated. (e–h), BM cells (e,f), spleen cells (g), or lymph node cells (h) were stained with FITC-conjugated anti-CD11c Ab and APC-conjugated anti-B220 Ab (e) or with FITC-conjugated anti-BST2 Ab and APC-conjugated anti-Siglec-H Ab (f–h), and then with biotinylated anti-LMIR8 Ab or biotinylated rat IgG2a Ab followed by PE-conjugated streptavidin. CD11c+B220+ (e) or BST2+Siglec-H+ (f–h) cell populations were gated and analyzed for LMIR8 expression. (i) Flt3 ligand-induced BMpDCs, BMmDCs, BMMΦ, or BMMCs were stained with biotinylated anti-LMIR8 Ab or biotinylated rat IgG2a Ab followed by PE-conjugated streptavidin. One representative of four independent experiments is shown.

FcRγ-coupled LMIR8 is a suitable marker for pDC

We then asked if stimulation with this anti-LMIR8 Ab induces LMIR8-dependent cytokine production in transduced BMMCs. The results showed that similar to anti-Flag Ab, plate-coated anti-LMIR8 Ab, but not with control Ab, stimulated IL-6 production at both mRNA and protein levels in Flag-tagged LMIR8-transduced BMMCs (Fig. 5a and Supplementary Fig. S4a). In addition, LMIR8 engagement enhanced lipopolysaccharide (LPS)-stimulated IL-6 production in Flag-tagged LMIR8-transduced BMMCs, indicating that LMIR8 cooperates with TLR4 to upregulate cytokine production in transduced BMMCs (Supplementary Fig. S4b). Thus, LMIR8 can transmit an activating signal in transduced BMMCs. To test if FcRγ is an adaptor protein for LMIR8 in pDC, WT or FcRγ−/− BM cells were stained with anti-LMIR8 Ab, demonstrating that the loss of FcRγ dampened surface expression of LMIR8 in BM pDCs (Fig. 5b). Thus, FcRγ was indispensable for surface expression of LMIR8 in pDC. We next asked if stimulation with a TLR9 agonist affected surface expression of LMIR8 in pDCs. In vivo administration of a TLR9 agonist, CpG oligodeoxynucleotide (ODN) D19, induced expression of BST2, a surface marker for PDC in steady state, in CD19+ B cells or CD11b+ myeloid cells in BM, although we found no expression of BST2 in these cell populations before stimulation (Fig. 5c)36. By contrast, neither CD19+ B cells nor CD11b+ myeloid cells in BM expressed detectable levels of LMIR8 irrespective of in vivo administration of a TLR9 agonist (Fig. 5c). The same stimulation slightly upregulated expression of BST-2, but not of LMIR8, in Siglec-H+ pDCs in BM (Fig. 5c). These results indicate that LMIR8 is a suitable marker for pDC in tissues.

Figure 5.

Figure 5

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FcRγ-coupled LMIR8 is a suitable marker for PDC. (a) BMMCs transduced with Flag-tagged LMIR8 or mock were stimulated with plate-coated anti-LMIR8 Ab or a control Ab or with 100 nM PMA or PBS as a control. IL-6 released into the culture supernatants were measured by ELISA. All data points correspond to the mean ± S.D. of three independent experiments. Statistically significant differences are shown. *p < 0.01 (Student’s t-test). (b) BM cells from WT or FcRγ−/− mice were stained with FITC-conjugated anti-CD11c Ab and biotinylated anti-LMIR8 Ab or biotinylated rat IgG2a Ab followed by PE-conjugated streptavidin. (c) BM cells from WT mice before or 24 h after an intravenous injection of 12.5 μg of CpG ODN D19 were stained with either FITC-conjugated anti-Siglec-H Ab, anti-CD19 Ab, or anti-CD11b Ab and biotinylated anti-LMIR8 Ab or biotinylated rat IgG2a Ab followed by PE-conjugated streptavidin. Siglec-H+ (left panel), CD19+ (middle panel), or CD11b+ (right panel) cell populations were gated and analyzed for LMIR8 expression. One representative of four independent experiments is shown.

LMIR8 engagement with anti-LMIR8 Ab inhibits the TLR9-mediated IFN-α production in transduced pDCs

Then, we examined the effect of LMIR8 engagement with anti-LMIR8 Ab on the activation of pDCs. Since BMpDCs expressed lower levels of LMIR8 than did pDC in tissues, BMpDCs were transduced with Flag-tagged LMIR8 or mock. Staining of these transfectants with anti-LMIR8 Ab displayed high levels of LMIR8 in Flag-tagged LMIT8-transduced BMpDCs (Fig. 6a). Neither plate-coated anti-LMIR8 Ab nor a control Ab induced significant levels of IFN-α in Flag-tagged LMIT8-transduced BMpDCs (Fig. 6b). By contrast, stimulation with a TLR9 agonist, CpG ODN 1585, induced significant production of IFN-α; however, we found that co-stimulation with anti-LMIR8 Ab, but not with a control Ab, substantially decreased IFN-α production (Fig. 6b). Similarly, co-stimulation with anti-Flag Ab decreased TLR9-meditaed IFN-α production (Fig. 6c). These results indicated that LMIR8 signals inhibit TLR9-mediated IFN-α production in transduced pDCs. However, similar co-stimulation with anti-LMIR8 Ab failed to do so in Flt3 ligand-induced BMpDCs or in pDCs sorted from BM or spleen, which expressed lower levels of LMIR8 than did the LMIR8-transduced pDCs. In any case, the signals triggered by LMIR8 engagement downregulated TLR9-mediated pDC activation.

Figure 6.

Figure 6

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LMIR8 engagement with anti-LMIR8 Ab inhibits the TLR9-mediated cytokine production in transduced pDCs. (a) WT BMpDCs transduced with Flag-tagged LMIR8 or mock were stained with FITC-conjugated anti-CD11c Ab and APC-conjugated anti-B220 Ab or with biotinylated anti-LMIR8 Ab or biotinylated rat IgG2a Ab followed by PE-conjugated streptavidin. One representative of three independent experiments is shown. (b,c) Flag-tagged LMIR8-transduced WT BMpDCs were stimulated with plate-coated anti-LMIR8 Ab or a control Ab (b) or with anti-Flag Ab or a control Ab (c) in the presence or absence of 5 μM CpG ODN 1585 or PBS as a control. IFN-α released into the culture supernatants were measured by ELISA. All data points correspond to the mean ± S.D. of three independent experiments. Statistically significant differences are shown. *p < 0.01 (Student’s t-test).

Ceramide, sphingomyelin, phosphatidylserine, and phosphatidylethanolamine are not ligands for LMIR8

To identify LMIR8 ligands, we performed functional reporter assays9. We transduced a chimera receptor, in which the extracellular domain of LMIR8 was fused to the transmembrane domain of LMIR3 followed by an intracellular domain of human CD3ζ containing an ITAM, into the parental reporter cells 2B4-GFP, where GFP expression would be induced by the activation of nuclear factor of activated T-cells (NFAT)9,37,38, to generate the new reporter cells LMIR8-2B4-GFP. If an extracellular domain of the chimera receptor were engaged by LMIR8 ligands, GFP expression would be induced in LMIR8-2B4-GFP cells. We confirmed that plate-coated anti-LMIR8 Ab induced GFP expression in LMIR8-2B4-GFP cells, but not in 2B4-GFP cells (Fig. 7). We then asked if lipids, including ceramide, sphingomyelin, phosphatidylserine, or phosphatidylethanolamine, which are ligands for several LMIR/CD300 members, acted as ligands for LMIR89–17. However, GFP expression was not induced by any plate-coated lipids tested (Fig. 7). The ligands for LMIR8 remain to be identified.

Figure 7.

Figure 7

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Ceramide, sphingomyelin, phosphatidylserine, and phosphatidylethanolamine are not ligands for LMIR8. Flow cytometry of GFP expression of 2B4-LMIR8-GFP cells or 2B4-GFP cells that were incubated for 24 h on plates coated with indicated lipids or with anti-LMIR8 Ab. PC, PS, PE, SM, or SPC indicates phosphatidylcholine, phosphatidylserine, phosphatidylethanolamine, sphingomyelin, or sphingosylphosphocholine. One representative of three independent experiments is shown.

Discussion

In the present study, we generated a specific Ab for LMIR8 and demonstrated that LMIR8 is exclusively expressed in CD11c+B220+Siglec-H+BST2+ pDCs in mouse tissues. In accordance with a previous report showing that BST2 is expressed in pDCs and plasma cells in steady state, while its expression is induced in many cell types following IFN-inducing stimulation36, our results confirm that BST2 is unsuitable as a PDC marker, in particular under inflammatory conditions. In addition, given that Siglec-H is expressed not only in pDCs but also in specialized macrophage subsets in the spleen, lymph nodes, or brain39,40, LMIR8 may be a more suitable marker for pDC; LMIR8 expression in cell types other than pDCs was neither detected nor induced under the inflammatory conditions tested. Unlike Siglec-H expression which is down-regulated upon activation41, LMIR8 expression remained significantly uninfluenced by stimulation with a TLR9 agonist in pDCs. However, it should be noted that Flt3 ligand-induced BMpDCs expressed extremely lower levels of LMIR8 than did pDCs in tissues. Accordingly, LMIR8 or Siglec-H appeared to be expressed in pDCs in different stages of differentiation21,22. In any case, we provide evidence that LMIR8 is a novel and suitable marker for mouse pDCs in tissues. Since the transcription factor E2-2 binds to a large proportion of pDC-enriched genes22,42, it is possible that E2-2 also regulates expression of LMIR8. Crossing mice expressing Cre recombinase under the control of the LMIR8 promoter with mice carrying the floxed target gene might make it possible to analyze the protein of interest expressed in pDCs in vivo.

On the basis of our results regarding LMIR8-transduced BMMCs, it is plausible to assume that LMIR8 functions as an activating receptor in the BMMC transfectants; FcRγ is required for both maintaining maximum surface expression of and delivering activating signals through the transduced LMIR8. Consistent with this, FcRγ was indispensable for surface expression of endogenous LMIR8 in mouse pDCs. However, this is in sharp contrast to the finding that FcRγ is not required for the surface expression of FcRγ-coupled LMIR7 in mast cells and macrophages8. It is important to note that LMIR8 engagement inhibited the production of IFN-α in LMIR8-transduced BMpDCs in response to a TLR9 agonist, which supports previous studies pointing to several surface receptors that interact with ITAM-containing adaptor proteins as a negative regulator of TLR7/9 signaling; engagement of FcRγ-coupled BDCA2 or ILT7 or DAP12-coupled NKp44 in human pDCs or of DAP12-coupled Siglec-H in mouse pDCs attenuates TLR7/9-mediated activation of pDCs21–33. Although we do not know the relevant mechanisms, different localization of internalized FcRγ-coupled LMIR8 bound by anti-LMIR8 Ab and TLR9 in endosomes might explain this phenomenon22–24. In addition, a recent finding that the CD2-associated adaptor protein (CD2AP)/SH2 domain-containing inositol phosphatase 1 (SHIP1) complex positively regulates BDCA2 and/or FcRγ signaling in humans pDCs to inhibit the E3 ubiquitin ligase Cbl22,23,43 led us to speculate that the similar regulation of signaling might be involved in FcRγ-coupled LMIR8-mediated inhibition of TLR9 signaling in mice. Because human pDCs have significant surface expression of CD300a, but not of other CD300 members including CD300c15,35, a previous report showing that engagement of human CD300a and CD300c with their cross-linking antibody reduced TNF-α production and increased IFN-α production in human pDCs might reflect the function of human CD300a34. This indicates that the regulation of pDC activation by CD300 members is different between mice and humans. Moreover, we need to examine the effect of LMIR8 engagement with physiological ligands, which remain to be identified, on TLR7/9 signaling in mouse pDCs to fully understand the role of LMIR8 in pDC activation. Because ceramide and sphingolipids have been identified as ligands for several CD300/LMIR members9–17, it is possible that LMIR8, a pDC receptor, recognizes specific viral components, including lipids, which directly regulate immune responses to certain viral infections. Further studies to analyze LMIR8-deficient mice in viral infection models or in autoimmune disease models as well as to identify ligands for LMIR8 will further our understanding of the physiological functions of LMIR8 in mouse pDCs to develop therapeutic strategies against pDCs-associated diseases.

In conclusion, LMIR8 is an FcRγ-coupled receptor that is selectively expressed in pDCs. Our results suggest that LMIR8 signals might negatively regulate the activation of pDCs in response to viral infections or to self nucleic acids, implicating LMIR8 in innate immunity or autoimmunity.

Methods

Antibodies and Other Reagents

Rat anti-LMIR8 monoclonal IgG2a Ab was generated by ACTGen, Inc. Mouse anti-Flag IgG1 Ab (M2), rabbit anti-Flag Ab, and mouse IgG1 Ab (MOPC21) were purchased from Sigma-Aldrich. Mouse anti-Myc Ab (9E10) was from Roche Diagnostics. R-phycoerythrin (PE)-conjugated anti-c-Kit, fluorescein isothiocyanate (FITC)-conjugated anti-FcεRIα, CD3, CD19, CD11b, Siglec-H, BST2, B220, CD11c, NK1.1, or F4/80 antibodies, PE-Cy7-conjugated anti-B220 Ab, and peridinin chlorophyll protein complex (PerCP)-conjugated anti-Siglec-H Ab were from BioLegend. PE-conjugated anti-mouse IgG goat F(ab’)2 Ab was from Beckman Coulter. Rat IgG2a Ab and PE-conjugated streptavidin were from eBioscience. Anti-ERK 1/2 Ab was from Santa Cruz Biotechnology. Anti-phospho-p44/42 MAPK (EER1/2) was from Cell Signaling Technology. Anti-LMIR8 Ab or rat IgG2a Ab was biotinylated with sulfo-NHS-LC-biotin (Pierce, Thermo Fisher Scientific) according to the manufacturer’s instructions. Cytokines were obtained from R&D Systems. Peptide-N-Glycosidase F (PNGase F) was from New England Biolabs. CpG oligodeoxynucleotide (ODN) 1585 or D19 (Hokkaido System Science Co.) was used for in vitro or in vivo experiments, respectively. Sphingosine, sphingomyelin (SM), and sphingosylphosphorylcholine (SPC) were from BIOMOL; C-24 ceramide was from Toronto Research Chemicals, Inc.; lipid A, lysophosphatidylcholine (lysolecithin), and cholesterol were from Avanti Polar Lipids, Inc.; 1,2-Dipalmitoyl-sn-glycero-3-phosphocholine (PC), 1,2-Dipalmitoyl-sn-glycero-3-phosphoserine (PS), and 1,2-Dipalmitoyl-sn-glycero-3-phosphoethanolamine (PE) were from Echelon Biosciences Inc. All other reagents were from Sigma-Aldrich unless stated otherwise.

Mice and cells

Cell lines Ba/F3, 2B4-GFP (a kind gift from Takashi Saito, RIKEN Research Center for Allergy and Immunology, Yokohama, Japan), and HEK 293 T were used6,9,37,38. C57BL/6 J WT and FcRγ−/− mice44 were used at 8–10 weeks of age. Mouse tissues were removed from C57BL/6 J mice for RNA extraction. BM, spleen, and lymph node cells were purified from mice and used as previously described6–8. All procedures were approved by an institutional review committee of the University of Tokyo and Juntendo University. BMMCs were generated from BM cells in the presence of 10 ng/mL IL-3 as described. BMΦ, BMmDCs, and BMpDCs were generated from BM cells in the presence of 10 ng/mL M-CSF, 20 ng/mL GM-CSF, and 50 ng/mL Flt3-ligand, respectively, as described6–8,45.

Ethics statement

All animal experiments were approved by the ethical committee of the University of Tokyo (approval no 20–8) and Juntendo University (approval no 290108). All the methods were carried out in accordance with the approved guidelines and regulations.

Gene Expression Analysis

Expression of LMIR8 was analyzed by reverse transcriptase-polymerase chain reaction (RT-PCR) as previously described6–8. Total RNAs were extracted from each tissue or transduced BMMCs with TRIzol reagents (Invitrogen) and reverse-transcribed by using High Capacity cDNA Reverse Transcription Kits (Applied Biosystems). A fragment of LMIR8 was amplified with primers 5′-TTCAGATATGCATGGAGGCCATT-3′ and 5′-TGATACCGTTCCCAGGGCGT-3′. For normalization, a fragment of β-actin was amplified with 5′-CATCACTATTGGCAACGAGC-3′ and 5′-ACGCAGCTCAGTAACAGTCC-3′. Relative expression levels of mouse IL-6 among samples were measured by real-time RT-PCR as described8. The following primers were used: 5′-GCCAGAGTCCTTCAGAGAGATACA-3′ (forward) and 5′-CTTGGTCCTTAGCCACTCCTTC-3′ (reverse) for IL-6 and 5′-GAAGTGTGACGTTGACATCC-3′ (forward) and 5′-GTACTTGCGCTCAGGAGGAG-3′ (reverse) for β-actin. Relative gene expression levels were calculated using standard curves generated by serial dilutions of cDNA and normalized to β-actin expression levels. Product quality was checked by melting curve analysis via LightCycler software (Roche Diagnostics).

Plasmid Constructs

On the basis of the sequence data, the cDNAs of mouse LMIR8 (GenBankTM accession number XM_017314637.1) and FcRγ (GenBankTM accession number NM_010185) were isolated by PCR from a BM cDNA library derived from C57BL/6J mice and their sequences were confirmed. A cDNA fragment of LMIR8 lacking the signal sequence was tagged with a Flag or Myc epitope at the N-terminus to generate Flag- or Myc-tagged LMIR8. A signaling lymphocyte-activating molecule (SLAM) signal sequence (a gift from Hisashi Arase, Osaka University, Osaka, Japan)46 and Flag- or Myc-tagged LMIR8 were subcloned into a pMXs-IRES-puror (pMXs-IP)47 retroviral vector to generate pMXs-FLAG- or Myc-LMIR8-IP. A cDNA fragment of FcRγ lacking the signal sequence was tagged with a Flag epitope at the N-terminus to generate Flag-tagged FcRγ. A SLAM signal sequence and Flag-tagged FcRγ were subcloned into a pMXs-IRES-blasticidin (pMXs-IB) to generate pMXs-Flag-FcRγ-IB6–8,47. To generate the Flag-tagged FcRγ (Y82F-Y93F) mutant (Flag-FcRγ-Mt), two-step PCR mutagenesis was performed by using pMXs-Flag-FcRγ-IB as a template. A SLAM signal sequence and Flag-tagged FcRγ-Mt were subcloned into pMXs-IB to generate pMXs-Flag-FcRγ-Mt-IB. To generate a chimera receptor LMIR8-CD3ζ, SLAM signal sequence-Flag-LMIR8, excluding transmembrane and intracellular domains, was fused to the transmembrane domain of LMIR3 and an intracellular domain of human CD3ζ (Naoki Matsumoto, University of Tokyo, Tokyo, Japan). LMIR8-CD3ζ was subcloned into pMXs-IP to generate pMXs-Flag-LMIR8-CD3ζ-IP9,14,15. All constructs were verified by DNA sequencing.

Transfection and Infection

Retroviral transfection was performed as previously described47,48. Briefly, retroviruses were generated by transient transfection of PLAT-E packaging cells. Cells were infected with retroviruses in the presence of 10 μg/mL Polybrene and selected with puromycin and/or blasticidin.

Flow Cytometry

Flow cytometric analysis of the stained cells was performed with a FACSCalibur (BD Biosciences) equipped with CellQuest software and FlowJo software (Tree Star) as previously described6–9. For detection of LMIR8, cells were incubated with 10 μg/mL biotinylated anti-LMIR8 Ab or biotinylated rat IgG2a Ab before incubation with PE-conjugated streptavidin. For detection of Flag (Flag-tagged receptor), cells were incubated with 10 μg/mL anti-Flag Ab or mouse IgG1 Ab before incubation with PE-conjugated anti-mouse IgG goat F(ab’)2 Ab.

Cell stimulation and measurement of cytokines

Plates were coated overnight with 20 μg/mL of each Ab. BMMCs transfectants expressing Flag-tagged LMIR8 or mock were stimulated with plate-coated mouse ant-Flag Ab or mouse IgG1 as a control, plate-coated rat anti-LMIR8 Ab or rat IgG2a as a control with or without 1000 ng/ml LPS, or with 100 nM PMA for 24 h. BMpDCs were stimulated with 5 mM CpG ODN 1585 for 24 h on plate-coated rat anti-LMIR8 Ab or rat IgG2a as a control. The concentrations of cytokines/chemokines in the supernatants were measured using enzyme-linked immunosorbent (ELISA) kits for IL-6 and TNF-α (R&D Systems) or using the Procarta cytokine assay kit (Affymetrix) for IFN-α. Alternatively, lipids dissolved in methanol (10 μg/mL) or methanol only as a control were added to plates and air-dried for the reporter assay9. 2B4-GFP or LMIR8-2B4-GFP cells were cultured for 24 h on plates coated with the indicated lipids or vehicle or with anti-LMIR8 Ab.

Biochemistry

BMMCs expressing FLAG-tagged LMIR8 or mock were stimulated by plate-coated anti-Flag Ab or mouse IgG1 Ab as a control, for the indicated time. Equal amounts of cell lysates were immunoblotted with anti-phospho-ERK1/2 Ab or anti-ERK1/2 Ab. Equal amounts of HEK 293 T cells transiently expressing Myc-tagged LMIR8 or mock together with Flag-tagged FcRγ or mock were immunoprecipitated with anti-Myc Ab, and were immunoblotted with rabbit anti-Flag Ab or anti-Myc Ab. Alternatively, the same cell lysates were immunoprecipitated with mouse anti-Flag Ab, and were immunoblotted with rabbit anti-Flag Ab. Immunoprecipitation and Western blotting were done as previously described6–8.

Statistical Analysis

Data are shown as the mean ± S.D., and statistical significance was determined by Student’s t test with *p < 0.01 taken as statistically significant.

Electronic supplementary material

Supplemental information (390.3KB, pdf)

Acknowledgements

We thank Dr. Hisashi Arase (Osaka University) and Dr. Naoki Matsumoto (University of Tokyo) for providing plasmids. We also thank Dr. Takashi Saito for providing cell lines. This study was supported by grants from the Ministry of Education, Science, Technology, Sports and Culture, Japan (JSPS KAKENHI Grant Number 23390257 and 26293231).

Author Contributions

A.K. performed all the experiments and participated in writing the manuscript. K.I., A.M., M.I., A.T., T.M., M.T., Y.Y., T.O., H.Y., M.N., S.U., K.U., T.A., K.M. and N.N. assisted with the experiments. T.T. provided mice. T.S., H.O., and K.O. analyzed the data. T.K. and J.K. conceived the project, analyzed the data, and actively participated in manuscript writing.

Competing Interests

The authors declare no competing interests.

Footnotes

Electronic supplementary material

Supplementary information accompanies this paper at 10.1038/s41598-018-25646-8.

Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Contributor Information

Toshio Kitamura, Email: kitamura@ims.u-tokyo.ac.jp.

Jiro Kitaura, Email: j-kitaura@juntendo.ac.jp.

References

  • 1.Colonna M. TREMs in the immune system and beyond. Nat Rev Immunol. 2003;3:445–453. doi: 10.1038/nri1106. [DOI] [PubMed] [Google Scholar]
  • 2.Ravetch JV, Lanier LL. Immune inhibitory receptors. Science. 2000;290:84–89. doi: 10.1126/science.290.5489.84. [DOI] [PubMed] [Google Scholar]
  • 3.Chung DH, et al. CMRF-35-like molecule-1, a novel mouse myeloid receptor, can inhibit osteoclast formation. J Immunol. 2003;171:6541–6548. doi: 10.4049/jimmunol.171.12.6541. [DOI] [PubMed] [Google Scholar]
  • 4.Yotsumoto K, et al. Paired activating and inhibitory immunoglobulin-like receptors, MAIR-I and MAIR-II, regulate mast cell and macrophage activation. J Exp Med. 2003;198:223–233. doi: 10.1084/jem.20021825. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 5.Kumagai H, et al. Identification and characterization of a new pair of immunoglobulin-like receptors LMIR1 and 2 derived from murine bone marrow derived mast cells. Biochem Biophys Res Commun. 2003;307:719–729. doi: 10.1016/S0006-291X(03)01245-2. [DOI] [PubMed] [Google Scholar]
  • 6.Izawa K, et al. Functional analysis of activating receptor LMIR4 as a counterpart of inhibitory receptor LMIR3. J Biol Chem. 2007;282:17997–18008. doi: 10.1074/jbc.M701100200. [DOI] [PubMed] [Google Scholar]
  • 7.Yamanishi Y, et al. Analysis of mouse LMIR5/CLM-7 as an activating receptor: differential regulation of LMIR5/CLM-7 in mouse versus human cells. Blood. 2008;111:688–698. doi: 10.1182/blood-2007-04-085787. [DOI] [PubMed] [Google Scholar]
  • 8.Enomoto Y, et al. Characterization of leukocyte mono-immunoglobulin-like receptor 7 (LMIR7)/CLM-3 as an activating receptor: its similarities to and differences from LMIR4/CLM-5. J Biol Chem. 2010;285:35274–35283. doi: 10.1074/jbc.M110.137166. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 9.Izawa K, et al. The Receptor LMIR3 Negatively Regulates Mast Cell Activation and Allergic Responses by Binding to Extracellular Ceramide. Immunity. 2012;37:827–839. doi: 10.1016/j.immuni.2012.08.018. [DOI] [PubMed] [Google Scholar]
  • 10.Yamanishi Y, et al. TIM1 is an endogenous ligand for LMIR5/CD300b: LMIR5 deficiency ameliorates mouse kidney ischemia/reperfusion injury. J Exp Med. 2010;207:1501–1511. doi: 10.1084/jem.20090581. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 11.Nakahashi-Oda C, et al. Apoptotic cells suppress mast cell inflammatory responses via the CD300a immunoreceptor. J Exp Med. 2012;209:1493–1503. doi: 10.1084/jem.20120096. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 12.Tian L, et al. p85α recruitment by the CD300f phosphatidylserine receptor mediates apoptotic cell clearance required for autoimmunity suppression. Nat Commun. 2014;5:3146. doi: 10.1038/ncomms4146. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 13.Cannon JP, O’Driscoll M, Litman GW. Specific lipid recognition is a general feature of CD300 and TREM molecules. Immunogenetics. 2011;64:39–47. doi: 10.1007/s00251-011-0562-4. [DOI] [PubMed] [Google Scholar]
  • 14.Izawa K, et al. Sphingomyelin and ceramide are physiological ligands for human LMIR3/CD300f, inhibiting FcεRI-mediated mast cell activation. J Allergy Clin Immunol. 2014;133:270–273. doi: 10.1016/j.jaci.2013.08.008. [DOI] [PubMed] [Google Scholar]
  • 15.Takahashi M, et al. Human CD300C delivers an Fc receptor-γ-dependent activating signal in mast cells and monocytes and differs from CD300A in ligand recognition. J Biol Chem. 2013;288:7662–7675. doi: 10.1074/jbc.M112.434746. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 16.Murakami Y, et al. CD300b regulates the phagocytosis of apoptotic cells via phosphatidylserine recognition. Cell Death Differ. 2014;21:1746–1757. doi: 10.1038/cdd.2014.86. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 17.Simhadri VR, et al. Human CD300a binds to phosphatidylethanolamine and phosphatidylserine, and modulates the phagocytosis of dead cells. Blood. 2012;119:2799–2809. doi: 10.1182/blood-2011-08-372425. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 18.Matsukawa T, et al. Ceramide-CD300f binding suppresses experimental colitis by inhibiting ATP-mediated mast cell activation. Gut. 2016;65:777–787. doi: 10.1136/gutjnl-2014-308900. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 19.Shiba E, et al. Ceramide-CD300f binding inhibits lipopolysaccharide-induced skin inflammation. J Biol Chem. 2017;292:2924–2932. doi: 10.1074/jbc.M116.768366. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 20.Izawa K, et al. Disrupting ceramide-CD300f interaction prevents septic peritonitis by stimulating neutrophil recruitment. Sci Rep. 2017;7:4298. doi: 10.1038/s41598-017-04647-z. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 21.Swiecki M, Colonna M. Unraveling the functions of plasmacytoid dendritic cells during viral infections, autoimmunity, and tolerance. Immunol Rev. 2010;234:142–162. doi: 10.1111/j.0105-2896.2009.00881.x. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 22.Swiecki M, Colonna M. The multifaceted biology of plasmacytoid dendritic cells. Nat Rev Immunol. 2015;15:471–485. doi: 10.1038/nri3865. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 23.Hirsch I, Janovec V, Stranska R, Bendriss-Vermare N. Cross Talk between Inhibitory Immunoreceptor Tyrosine-Based Activation Motif-Signaling and Toll-Like Receptor Pathways in Macrophages and Dendritic Cells. Front Immunol. 2017;8:394. doi: 10.3389/fimmu.2017.00394. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 24.Gilliet M, Cao W, Liu YJ. Plasmacytoid dendritic cells: sensing nucleic acids in viral infection and autoimmune diseases. Nat Rev Immunol. 2008;8:594–606. doi: 10.1038/nri2358. [DOI] [PubMed] [Google Scholar]
  • 25.Kawai T, Akira S. Toll-like receptors and their crosstalk with other innate receptors in infection and immunity. Immunity. 2011;34:637–650. doi: 10.1016/j.immuni.2011.05.006. [DOI] [PubMed] [Google Scholar]
  • 26.Blasius AL, Colonna M. Sampling and signaling in plasmacytoid dendritic cells: the potential roles of Siglec-H. Trends Immunol. 2006;27:255–260. doi: 10.1016/j.it.2006.04.005. [DOI] [PubMed] [Google Scholar]
  • 27.Cao W, et al. Plasmacytoid dendritic cell-specific receptor ILT7-Fc epsilonRI gamma inhibits Toll-like receptor-induced interferon production. J Exp Med. 2006;203:1399–1405. doi: 10.1084/jem.20052454. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 28.Cao W, et al. Regulation of TLR7/9 responses in plasmacytoid dendritic cells by BST2 and ILT7 receptor interaction. J Exp Med. 2009;206:1603–1614. doi: 10.1084/jem.20090547. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 29.Fuchs A, Cella M, Kondo T, Colonna M. Paradoxic inhibition of human natural interferon-producing cells by the activating receptor NKp44. Blood. 2005;106:2076–2082. doi: 10.1182/blood-2004-12-4802. [DOI] [PubMed] [Google Scholar]
  • 30.Florentin J, et al. HCV glycoprotein E2 is a novel BDCA-2 ligand and acts as an inhibitor of IFN production by plasmacytoid dendritic cells. Blood. 2012;120:4544–4551. doi: 10.1182/blood-2012-02-413286. [DOI] [PubMed] [Google Scholar]
  • 31.Rosental B, et al. Proliferating cell nuclear antigen is a novel inhibitory ligand for the natural cytotoxicity receptor NKp44. J Immunol. 2011;187:5693–5702. doi: 10.4049/jimmunol.1102267. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 32.Blasius A, et al. A cell-surface molecule selectively expressed on murine natural interferon-producing cells that blocks secretion of interferon-alpha. Blood. 2004;103:4201–4206. doi: 10.1182/blood-2003-09-3108. [DOI] [PubMed] [Google Scholar]
  • 33.Blasius AL, Cella M, Maldonado J, Takai T, Colonna M. Siglec-H is an IPC-specific receptor that modulates type I IFN secretion through DAP12. Blood. 2006;107:2474–2476. doi: 10.1182/blood-2005-09-3746. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 34.Ju X, Zenke M, Hart DN, Clark GJ. CD300a/c regulate type I interferon and TNF-alpha secretion by human plasmacytoid dendritic cells stimulated with TLR7 and TLR9 ligands. Blood. 2008;112:1184–1194. doi: 10.1182/blood-2007-12-127951. [DOI] [PubMed] [Google Scholar]
  • 35.Zenarruzabeitia O, et al. The expression and function of human CD300 receptors on blood circulating mononuclear cells are distinct in neonates and adults. Sci Rep. 2016;6:32693. doi: 10.1038/srep32693. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 36.Blasius AL, et al. Bone marrow stromal cell antigen 2 is a specific marker of type I IFN-producing cells in the naive mouse, but a promiscuous cell surface antigen following IFN stimulation. J Immunol. 2006;177:3260–3265. doi: 10.4049/jimmunol.177.5.3260. [DOI] [PubMed] [Google Scholar]
  • 37.Ohtsuka M, et al. NFAM1, an immunoreceptor tyrosine-based activation motif-bearing molecule that regulates B cell development and signaling. Proc Natl Acad Sci USA. 2004;101:8126–8131. doi: 10.1073/pnas.0401119101. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 38.Yamasaki S, et al. Mincle is an ITAM-coupled activating receptor that senses damaged cells. Nat Immunol. 2008;9:1179–1188. doi: 10.1038/ni.1651. [DOI] [PubMed] [Google Scholar]
  • 39.Zhang J, et al. Characterization of Siglec-H as a novel endocytic receptor expressed on murine plasmacytoid dendritic cell precursors. Blood. 2006;107:3600–3608. doi: 10.1182/blood-2005-09-3842. [DOI] [PubMed] [Google Scholar]
  • 40.Kopatz J, et al. Siglec-h on activated microglia for recognition and engulfment of glioma cells. Glia. 2013;61:1122–1133. doi: 10.1002/glia.22501. [DOI] [PubMed] [Google Scholar]
  • 41.Puttur F, et al. Absence of Siglec-H in MCMV infection elevates interferon alpha production but does not enhance viral clearance. PLoS Pathog. 2013;9:e1003648. doi: 10.1371/journal.ppat.1003648. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 42.Cisse B, et al. Transcription factor E2-2 is an essential and specific regulator of plasmacytoid dendritic cell development. Cell. 2008;135:37–48. doi: 10.1016/j.cell.2008.09.016. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 43.Bao M, et al. CD2AP/SHIP1 complex positively regulates plasmacytoid dendritic cell receptor signaling by inhibiting the E3 ubiquitin ligase Cbl. J Immunol. 2012;189:786–792. doi: 10.4049/jimmunol.1200887. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 44.Takai T, Li M, Sylvestre D, Clynes R, Ravetch JV. FcR gamma chain deletion results in pleiotrophic effector cell defects. Cell. 1994;76:519–529. doi: 10.1016/0092-8674(94)90115-5. [DOI] [PubMed] [Google Scholar]
  • 45.Kitaura J, et al. Evidence that IgE molecules mediate a spectrum of effects on mast cell survival and activation via aggregation of the FcepsilonRI. Proc Natl Acad Sci USA. 2003;100:12911–12916. doi: 10.1073/pnas.1735525100. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 46.Shiratori I, Ogasawara K, Saito T, Lanier LL, Arase H. Activation of natural killer cells and dendritic cells upon recognition of a novel CD99-like ligand by paired immunoglobulin-like type 2 receptor. J Exp Med. 2004;199:525–533. doi: 10.1084/jem.20031885. [DOI] [PMC free article] [PubMed] [Google Scholar]
  • 47.Kitamura T, et al. Retrovirus-mediated gene transfer and expression cloning: powerful tools in functional genomics. Exp Hematol. 2003;31:1007–1014. doi: 10.1016/S0301-472X(03)00260-1. [DOI] [PubMed] [Google Scholar]
  • 48.Morita S, Kojima T, Kitamura T. Plat-E: an efficient and stable system for transient packaging of retroviruses. Gene Ther. 2007;7:1063–1066. doi: 10.1038/sj.gt.3301206. [DOI] [PubMed] [Google Scholar]

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