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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptNIH Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
Nat Immunol. Author manuscript; available in PMC Sep 17, 2009.
Published in final edited form as:
Published online May 11, 2008. doi:  10.1038/ni.1615
PMCID: PMC2746085
NIHMSID: NIHMS140534

FMS-like tyrosine kinase 3 is required for dendritic cell development in peripheral lymphoid tissues

Abstract

Dendritic cell (DC) development begins in the bone marrow but is not completed until after immature progenitors reach their sites of residence in lymphoid organs. The hematopoietic growth factors regulating these processes are poorly understood. Here we examine the effects of FMS-like tyrosine kinase 3 (Flt3) signaling on macrophage DC progenitors (MDP) in the bone marrow and on peripheral DCs. We find that the MDP compartment is responsive to super–physiologic levels of Flt3 ligand (Flt3L) but is not dependent on Flt3 for its homeostatic maintenance in vivo. In contrast, Flt3 is essential in regulation of homeostatic DC development in the spleen where it is required to maintain normal numbers of DCs by controlling their division in the periphery.

Introduction

Dendritic cells (DC) are a heterogeneous group of specialized antigen presenting cells that maintain peripheral tolerance and induce adaptive immune responses1,2. Three major groups of DCs have been defined: antigen-presenting conventional DCs (cDCs) found in lymphoid organs such as spleen; type I interferon secreting plasmacytoid DC (pDC); and migratory DC (mDC) such as epidermal Langerhans cells or dermal DC which capture antigens and deliver them to T cells in lymphoid organs3,4.

cDCs, some tissue macrophages, and monocytes originate from a common precursor designated as macrophage DC progenitor (MDP)5,6. Others have uncovered a common DC precursor (CDP) that is restricted to cDC and pDC development but the macrophage potential of CDP and its precise relationship to MDP was not determined7,8. Nevertheless, MDP, CDP or their progeny enter the circulation and are rapidly cleared due to migration into lymphoid tissues where they undergo a limited number of cell divisions while differentiating into DCs9. DC proliferation in the spleen contributes to maintaining the size of the peripheral DC pool and can also prolong antigen presentation9-11. Little is known about how DC proliferation in the periphery is regulated, and among the known DC growth factors, only lymphotoxin-β has been implicated in helping maintain CD8 cDC homeostasis by regulating cell division in the periphery10.

Flt3 (Flk2, CD135) is broadly expressed on early hematopoietic precursors in the bone marrow12. Consistent with this expression pattern, Flt3 ligand (Flt3L, Flk2L) injection increases the numbers of early myeloid and lymphoid progenitors, but not committed T or B cell precursors and this is accompanied by increases in peripheral DCs13,14, granulocytes, monocytes, and polymorphonuclear neutrophils (PMN) leading to the conclusion that the effect of Flt3L is BM restricted12. In addition, inhibition of Flt3-mediated signals results in reduced numbers of peripheral DC15,16. However, addition of Flt3L to cultured DC precursors has only modest effects on their proliferative expansion and the effects of Flt3L on DC precursors and peripheral DC were not examined in vivo5,7,8. Here we report on the role of Flt3 on DC development in the bone marrow and in peripheral lymphoid organs and show that it is an important regulator of homeostatic DC division in the periphery in vivo.

Results

BM-resident DC progenitors

Bone marrow derived DC (BMDC) precursors, or MDP do not express lineage markers (Lin = CD3CD19NK1.1I-Ab−CD11cB220Ter119CD11bGr-1) and were originally identified by expression of Kit (CD117), CX3CR1 promoter driven transgenic GFP, making analysis in mutant mouse strains cumbersome5. MDPs can also give rise to monocytes and some tissue macrophages5,6. Recently defined common dendritic cell precursors (CDP) (LinKitintFlt3+CSF1R+) give rise to pDC and cDC in vivo7,8. To further define DC progenitors we purified Lin cells expressing CSF1R and analyzed their developmental potential in vitro and in vivo (Fig. 1).

Figure 1
Identification of cDC progenitors. (a) Flow cytometry of Lineage-negative (Lin = CD3CD19B220NK1.1CD11cCD11bTer119Gr-1) BM (top) and spleen (bottom) cells analyzed for the ...

We found that ~8 % of all LinSca-1 cells express CSF1R in the bone marrow (absolute number: 7.2 × 104 ± 0.3 per 2 femura, n = 7) (Fig. 1a). This fraction is rapidly proliferating (35 ± 4 % of the cells are in S or G2 phase of cell cycle [n = 4]) (Supplementary Fig. 1 online) and does not include early self-renewing hematopoietic precursors (Sca-1+ cells) (Fig. 1a). LinCSF1R+ cells respond to GM-CSF in vitro by giving rise to DCs, which are Gr-1MHCII+CD11c± (Supplementary Fig. 2 online) but fail to respond to CSF1, or erythropoietin with or without IL-3 (Fig. 1b). Although the majority of the cells in GM-CSF treated cultures were DCs there was little expansion (3-fold) indicating that this progenitor population undergoes only a limited number of cell divisions prior to differentiation in response to GM-CSF (LinKit+CSF1R cells expanded 18-fold). Consistent with the work of others, in vitro colony formation in response to Flt3L was undetectable (7 and Fig. 1b). We conclude that LinCSF1R+ cells are devoid of early and late erythroid progenitor cells and that they produce DCs in response to GM-CSF in vitro. In contrast, LinCSF1R cells respond to GM-CSF in vitro by giving rise to cells with diverse phenotypes (Fig. 1b, Supplementary Fig. 2 online).

In adoptive transfer experiments purified LinCSF1R+ cells (Supplementary Fig. 3 online) gave rise exclusively to spleen CD8+ CD8 cDC and SIGNR1+ marginal zone macrophages but not pDC, PMN, red pulp macrophages (F4/80+) or metallophilic macrophages (Ser-4+) irrespective of Kit expression (Fig. 1c and Supplementary Fig. 4 online). In contrast LinKit+CSF1R cells gave rise to all other myeloid cell types (not shown). No donor-derived cells were detected in the BM of recipients suggesting that LinCSF1R+ cells cannot migrate back to their site of origin (not shown).

MDP were originally defined as Lin cells expressing a CX3CR1 promoter driven GFP transgene, Kit5, and CSF1R6 (Fig. 1d). LinCX3CR1+ cells contain Kit+ and Kit cells and both populations have identical DC potential in adoptive transfer experiments in vivo (Fig. 1e), thus LinCX3CR1+Kit+ and LinCX3CR1+Kit cells are MDPs (Fig. 1d). LinCX3CR1+ cells are heterogenous in expression of CSF1R (44%, 21% Kit+ and 23% Kit) (Fig. 1d) but all LinCSF1R+ cells are CX3CR1+ (data not shown). 75% of LinCSF1R+ cells (36% Kit+ and 39% Kit) express Flt3 (Fig. 1d), and when separated on the basis of Flt3 expression cDC progenitor potential is concentrated in Flt3+ cells in vivo (data not shown). LinCSF1R+Flt3 cells fail to give rise to any other cell type (data not shown). CDP7 (LinKitintFlt3+CSF1R+) represents <39 % of LinCSF1R+ cells and is therefore included in MDP (Fig. 1d). We conclude that BM derived LinCSF1R+ cells give rise to cDCs in vivo and that when analyzing Flt3 mutant mice (see below) the LinCSF1R+ phenotype is sufficient to define MDPs.

Granulocyte monocyte progenitors (GMP), common myeloid progenitors (CMP) and common lymphoid progenitors (CLP) all harbor cDC progenitor activity21,22. To determine how MDPs relate to these other progenitor fractions we analyzed LinKit+CX3CR1+ 5 and LinCSF1R+ MDPs for expression of CD34 and FcγRII/III (CD16/32) (Supplementary Fig. 5 online). We found that both MDPs overlap with GMP and CMP, and due to the restricted in vivo developmental potential of MDP we conclude that GMP and CMP are mixed progenitor populations that contain MDPs23.

Flt3L effects on MDPs

To determine how Flt3L impacts DC development we examined the effects of its administration on bone marrow and peripheral DCs. Following administration of Flt3L, expression of its receptor, Flt3, was down-regulated on MDPs and on spleen cDC indicating a rapid response to Flt3L in all DC compartments (Fig. 2a, and data not shown). MDPs (LinCSF1R+ (Fig. 2b) or LinKit+CX3CR1+ cells in CX3CR1-GFP transgenic mice (Supplementary Fig. 6 online) were increased by a factor of ~10, whereas GMP and CMP only increased by a factor of ~5, and MEP, a megakaryocytic and erythroid prone progenitor cell was unaffected (12 and Supplementary Fig. 6 and Supplementary Fig. 7 online). However, Flt3L treatment did not alter the developmental potential of MDPs on a per cell basis as measured by adoptive transfer experiments where MDPs from Flt3L treated and untreated mice had the same ability to give rise to cDCs (Fig. 2c). We conclude that Flt3L increases the numbers of MDPs but does not alter their ability to give rise to DCs.

Figure 2
Effects of Flt3 ligand (Flt3L) stimulation. (a) Flow cytometry of spleen cells (top) gated on CD3CD19NK1.1Ter119 and BM cells (bottom) gated on Lin (CD3CD19B220NK1.1CD11b ...

In the spleen, absolute numbers of cDC, pDC, PMN, monocytes, and red pulp macrophages were increased in response to Flt3L (Fig. 2a,b). To determine whether Flt3L injection also alters the numbers of DC precursors in spleen we performed adoptive transfer experiments with mixtures of Flt3L treated and untreated DC–depleted splenocytes (Fig. 2d). Donor populations were depleted of DC, thus, de novo generated cDC developed from intrasplenic precursors. The relative increase in DC from the Flt3L treated spleens suggests that DC progenitors are mobilized to the spleen after Flt3L treatment (Fig. 2d).

Reduced numbers of cDC and pDC in Flt3−/− mice

To further investigate the role of Flt3 in DC development we examined Flt3 deficient mice (Flt3−/− mice17). Absence of Flt3 led to reduced numbers of pDC (Fig. 3a,b) and cDC (Fig. 3c), more pronounced in younger mice24,25, but MDP (Fig. 3j) and spleen pre-cDC19 (Fig. 3h and Supplementary Fig. 7 online) numbers remained unaltered. The reduction in cDC and pDC was not due to a general defect in myeloid cells since monocytes, PMN, Ser-4+ metallophilic and SIGNR-1+ marginal zone macrophages were not significantly altered (Fig. 3d-f, Supplementary Fig. 8 online). Surprisingly no further reductions in pDC or cDC were observed in double mutant mice lacking Flt3 and granulocyte-macrophage colony-stimulating factor receptor (GM-CSFR) (Supplementary Fig. 9 online). Thus, GM-CSFR is not required for DC development in vivo even in the absence of Flt3. We conclude that there is a specific DC defect in the spleen of Flt3−/− mice.

Figure 3
Myeloid compartments in Flt3−/− mice. (a) Representative flow data showing reduced numbers of cDC, pDC in Flt3−/− mice. Spleen cells from 4 week old mice were gated on CD3CD19NK1.1Ter119 ...

Flt3 in DC homeostasis

To determine whether the DC defect in Flt3−/− mice is cell intrinsic we compared BM chimeras in which Flt3−/− or wild-type cells were engrafted in wild-type mice and analyzed 4 months later (Fig. 4a). Recipients showed comparable levels of Flt3−/− and wild-type hematopoetic stem cell (HSC) engraftment as determined by flow cytometry (LinKit+Sca-1+ [KSL] cells, data not shown) and similar numbers of PMN, red pulp–macrophages (RP-Mp), and monocytes (Mono) but there were decreased numbers of Flt3−/− pDCs and cDCs (Fig. 4a). We conclude that the DC deficiency in Flt3−/− mice is cell intrinsic.

Figure 4
DC development in Flt3−/− bone marrow chimeras. (a) Absolute numbers of wild-type (closed squares) and Flt3−/− (open squares) spleen PMN, RP–macrophages, monocytes, pDC, and cDC in bone marrow chimeras 4 months ...

To directly compare the developmental potential of mutant and wild-type progenitors we constructed mixed BM chimeras and analyzed them after 1.5 months (Fig. 4b and Supplementary Fig. 10 online). In the bone marrow, HSCs and MDPs were reconstituted to comparable levels and in the periphery, PMN and monocyte reconstitution was 47% and 37%, respectively (Fig. 4b). In contrast, Flt3−/− contribution to both subsets of DCs, RP-Mp and as reported previously, T and B lymphocytes was very low, indicating specific defects in the generation of these lineages in the absence of Flt3 (17 and Fig. 4b). The defects in DCs were more pronounced than MDPs suggesting the existence of a Flt3 dependent checkpoint for DC development beyond the MDP stage (Fig. 4b).

To further investigate the possible role of Flt3 in peripheral DC homeostasis we parabiosed Flt3−/− with wild-type mice and compared them to parabiosed congenic wild-type mice (Fig. 4c and Supplementary Fig. 11 online). In contrast to controls, only 2 % of the cDC in the spleen of the wild-type parabiotic partner were of Flt3−/− origin and a disproportionate number of wild-type cDCs were found in the Flt3−/− spleen when compared to wild-type vs. wild-type controls (WT into WT: 15 %; WT into Flt3−/− : 64 %) (Fig. 4c and Supplementary Fig. 11 online). To determine whether the imbalance in Flt3−/− vs. wild-type parabionts was due to reduced DC progenitor potential or to decreased numbers of progenitors we transplanted a mixture of purified MDPs from wild-type and Flt3−/− mice into irradiated recipients. 11 days after transfer the majority of cDC were of wild-type origin suggesting that Flt3−/− MDPs had a decreased potential to develop into cDCs (Fig. 5a). To determine whether this difference in DC differentiation potential between wild-type and Flt3−/− MDPs was Flt3L dependent we transferred the mixture of the two types of MDPs into Flt3L−/− mice. In contrast to the wild-type recipient, the ratio of wild-type and Flt3−/− cDCs in spleen of Flt3L−/− recipients reflected the input ratio of MDPs (Fig. 5a). The same result was obtained by transplantation of peripheral blood (PB) cells containing circulating cDC precursors (Fig. 5a). Thus, in the absence of Flt3L, wild-type and Flt3 mutant MDPs and PB-resident cDC precursors have the same potential to develop into cDCs. We conclude that Flt3 is an important mediator of DC development after the MDP and circulating cDC precursor stage.

Figure 5
Flt3 in peripheral expansion. (a) Adoptive transfer of mixed BM LinCSF1R+ (MDP, left) or white blood cells (WBC, right) from wild-type and Flt3−/− mice into mildly irradiated wild-type (top) or Flt3L−/− (bottom) ...

To analyze proliferation of Flt3-deficient and -proficient cells in the same microenvironment we generated BM chimeras and measured BrdU incorporation into MDP and cDC after a pulse of 2 hours (Fig. 5b,c). There was no difference in BrdU uptake in MDP, confirming Flt3-independent generation. In contrast, Flt3−/− cDC incorporated less BrdU than Flt3+ cDC, suggesting that in situ cDC proliferation depends on Flt3 (Fig. 5b,c). After a BrdU pulse of 4 days Flt3−/− cDC incorporated ~10 % less BrdU than wild-type cells, but pDC show no difference in BrdU incorporation compared to wild-type pDC, suggesting that a distinct mechanism underlies paucity of pDC in Flt3−/− mice (Fig. 5c).

To determine whether a defect in cell division in the periphery contributes to the DC defect in the absence of Flt3 we transferred mixtures of CFSE labeled Flt3−/− and wild-type MDPs into irradiated recipients and measured cell division by CFSE dilution. We found that Flt3−/− cells divided less than wild-type cells in the spleen suggesting that Flt3 regulates DC cell division in the periphery (Fig. 5d). To examine the effects of Flt3 on peripheral DC division directly we injected CFSE labeled spleen and LN cells into un-irradiated wild-type and Flt3L−/− mice and measured cDC proliferation by dye dilution. DC proliferation was readily detected in wild-type mice but difficult to document in Flt3L−/− recipients (Fig. 5e). We conclude that Flt3 regulates DC division in the periphery in the steady state.

Discussion

We have shown that mice deficient in Flt3 show abnormalities in lymphoid tissue resident cDC and pDC. The effects of Flt3 deficiency are most evident in the periphery where this receptor is essential for homeostatic expansion of DC progenitors in lymphoid organs.

In contrast to migratory DCs such as Langerhans cells which are derived from Gr–1+ monocytes26, lymphoid tissue resident cDC are derived from hematopoietic precursors, which have been called MDP or CDP5,7,8. MDP were initially defined by expression of a CX3CR1 driven GFP transgene, and could only be studied in mice bearing this marker5. We have established that MDPs can also be identified by expression of CSF1R and absence of lineage markers including CD11c and CD11b (LinCSF1R+). MDP are rapidly dividing cells exclusively found in the BM multipotent progenitor compartment (Sca-1) and make up to 0.2 % of the nucleated cells in the marrow. They are restricted to the BM suggesting that they are a non–circulating population, a finding, which is also supported by lack of transfer in parabiosed mice. The original LinKit+CX3CR1 expressing MDP include the LinCSF1R+ MDP and have equivalent developmental potential in vivo. However, LinCSF1R+ MDP include Kit+ and Kit cells, which have identical differentiation potential. Despite homogenous expression of CSF1R, MDP like CDP fail to proliferate in response to CSF1 in vitro which may be secondary to their isolation using anti-CSF1R antibodies7. In vivo, MDP are developmentally restricted in that they do not give rise to granulocytes, erythroid cells, pDC, red pulp (F4/80+), or metallophilic macrophages (Ser 4+), but they do have the potential to produce cDCs and SIGNR1+ marginal zone macrophages when injected intravenously. CDPs are LinCSF1R+ cells which are further defined by being KitintFlt3+. These cells constitute a fraction of the MDPs. In contrast to MDP (5 and this study), CDP give rise to cDC and pDC in vivo7. However, CDP-derived pDC constituted small numbers of graft-derived cells, which were increased by Flt3L treatment of the recipients7. We failed to detect MDP-derived pDC over 0.6% (±0.9 [n = 20]) after injection into irradiated recipients but this may have been due to the fractional contribution of CDP to the overall number of MDP. Moreover, in our experiments, presence of small numbers of PDCA1+ cells was always accompanied by presence of small numbers of PMN (1.3 % ± 3.5 [n = 20]), a cell type not analyzed in previous studies, suggesting alternative possibility that CDP were contaminated with small numbers of multipotent progenitors. Thus, we conclude that the developmental potential of MDP is restricted to cDC and marginal zone macrophages. We find that like CDPs, MDPs express Flt3, and that Kit appears to be dispensable for MDP isolation. In conclusion, CDPs overlap with LinCSF1R+ MDPs as do GMP, and CMP, which may account for the observation that DC progenitors are found in both of these hematopoietic precursor populations21,23,27.

Like many other hematopoietic progenitors in the bone marrow including ST-HSCs, CLPs, CMPs, and GMPs, MDPs express Flt312,28,29. All of these cells expand in response to exogenous Flt3L, but we find that the effects of Flt3L on MDPs is more pronounced than on any other defined progenitor12,30. Nevertheless, deletion of Flt3L has only modest effects on bone marrow cellularity and does not alter the relative frequency of myeloid progenitors29,31. The only prominent hematopoetic developmental defect in Flt3L−/− mice is in pro- and pre-B cell development29. Flt3 deletion shows even milder effects with no significant alteration in bone marrow cellularity, but Flt3−/− progenitors have a reduced ability to competitively reconstitute the T and myeloid cell lineages in mixed bone marrow adoptive transfer experiments 17. Consistent with these findings Flt3L alone is not sufficient to support robust growth of MDP in vitro 5,7 and the numbers of MDPs were unaffected by absence of Flt3. Thus, the MDP compartment is increased in response to superphysiologic levels of Flt3L, but its maintenance is independent of Flt3 in vivo.

Small number of DC progenitors rapidly transit from bone marrow to spleen and lymph nodes via the blood as relatively immature progenitors that do not express surface MHCII or CD11c32. These cells undergo several rounds of cell division while differentiating into cDCs that continue to express Flt39,10,12,15. Inhibition of Flt3-mediated signals results in reduction of DC numbers in vivo, possibly due to increased apoptosis16.

DC division in lymphoid organs is limited, and the peripheral cDC compartment must be continually replenished from blood borne precursors9. Peripheral lymphoid organ DC homeostasis is therefore dependent on the rate of DC progenitor input from blood, cell division and cell death9. Our experiments show that Flt3L can regulate two aspects of peripheral DC homeostasis, progenitor migration and cDC division. The enhanced migration of DC progenitors to spleen in response to Flt3L is consistent with enhanced migration of monocyte and PMN progenitors and the expansion of these cells in the bone marrow12,14. Little is known about the regulation of cDC division in peripheral lymphoid organs. Among the known DC growth factors only lymphotoxin–β has been implicated in helping maintain the homeostasis of the CD8 subset of cDC in spleen by regulating cell division in the periphery10. Our adoptive transfer experiments show that in the absence of Flt3 cDCs are impaired in their ability to undergo homeostatic division and therefore Flt3 is a pivotal growth factor in maintenance of cDC homeostasis in the periphery in steady-state.

In summary, committed DC progenitors in the bone marrow do not require Flt3-mediated signals for their generation, but they expand and emigrate from the bone marrow in response to superphysiologic doses of Flt3L in vivo. In contrast, Flt3 is required for DC homeostasis and the effect is on a novel peripheral checkpoint that regulates cDC division.

Methods

Mice, parabiosis, Flt3L injection

Flt3−/− mice were generated and kindly provided by Ihor Lemischka17, Csf2ra−/− mice were generated and kindly provided by Lorraine Robb and Glenn Begley18. C57BL/6 (B6), B6C57BL/6 Pep3b CD45.1+ (SJL), and CD45.1+CD45.2+ F1 mice were obtained from Jackson Lab or bred at Rockefeller University. Parabiotic mice were produced as described9. Briefly, mice were anesthesized (2.5 % Avertin, Fluka) and shaved. Skin incisions were made in the adjacent sides of two mice from hip to elbow and the ligaments sutured together with chromic gut (Ethicon). Subsequently, the skin of the mice was clipped with with 9 mm stainless steel wound clips to close the skin incisions. Mice were kept on antibiotic and ibuprofen (0.16 mg/l) throughout the following 3 weeks. Flt3L injections: 10 μg rhFlt3L (Amgen) was daily injected subcutaneously in 100 μl PBS. All mice were maintained under specific pathogen free conditions and mouse protocols were approved by the Rockefeller University Animal Care and Use Committee.

Cell preparations, flow cytometry, immunohistology

Spleen and thymus were gently dispersed between frosted slides, and digested for 30 min at 37 °C in PBS with 5 % FCS containing collagenase D (typeII, Roche) at a final concentration of 0.4 U/ml. Cell numbers were determined on a cell analyzer (Calibur, BD), using counting beads (Caltag) and determination of absolute leukocyte numbers was performed according to the manufacturers instructions using Ter119 antibody. Medium density spleen cells (MDP, 1.076-1.084 g/cm3, Optiprep, Sigma) were prepared as described19. Cell preparation for flow cytometry: Before staining with specific antibodies, unspecific binding sites were blocked using total rat Ig (Jackson Lab) and purified FcγRII/III antibody (93, eBioscience). All stainings were performed at 4 °C in PBS with 5% FCS. Immunohistology: Cryosections were fixed in 100% ethanol at -20 °C, unspecific binding sites were blocked with purified FcγRII/III antibody and streptavidine / biotin blocking kit (Vector Laboratories), and stained in PBS with 5% FCS. Following reagents were used for stainings (flow cytometry and immunohistology): CD3 (2C11), CD11c (HL3), CD45RA (14.8), CD43 (S7), SIRPα (P84) (all Pharmingen), CD8 (53–6.7), CD19 (1D3), CD45R (RA3-6B2), CD11b (M1/70), Gr-1 (RB6-8C5), Ter119 (Ter119), Kit (2B8), Sca-1 (D7), CSF1R (AFS98), FcγRII/III (93), CD34 (RAM34), Flt3 (A2F10), I-Ab (MS/114.15.2), F4/80 (BM8), CD45.1 (A20), CD45.2 (104) (all eBioscience), PDCA1 (JFOS-1C2.4.1) (Myltenyi), and CD169 (Ser-4), SIGNR1 (22D1) were self generated and kindly provided by Chae Gyu Park (Rockefeller University). Secondary steps: Streptavidin-Allophycocyanine from Pharmingen, Streptavidine-Pacific Orange, 4′,6-Diamidino-2-Phenylindole (DAPI), anti-fluoresceine-Alexa488 from Molecular Probes, Streptavidin-Phycoerythrine carbocyanine 5.5 from Caltag, anti-hamster Carbocyanine 3 from Jackson Lab.

Methyl cellulose colony assay, liquid cultures

105 total BM cells or 103 isolated progenitors were plated in methyl cellulose containing medium (StemCell Technologies M3334) supplemented with erythropoietin (10 ng/ml), or erythropoietin and IL-3 (50 ng/ml). Erythroid colonies were counted after 48 hours (erythropoietin) or 7 days (erythropoietin and IL-3) as previously described20. Briefly, cultures were overlayed with an equal volume of 0.4 % benzidine in 12 % acetic acid, and scored according to blue staining of colonies. BFU-E colonies contained at least one benzidine+ erythroid cell, and CFU-E colonies were uniformly benzidine+. 2 × 105 sorted total BM cells or 103 isolated progenitors were plated in methyl cellulose containing medium (StemCell Technologies M3231) supplemented with GM-CSF (10 ng/ml), CSF1 (10 ng/ml), or Flt3L (100 ng/ml). Colony formation was assessed after 7 days. For liquid cultures, 2 × 105 total BM cells or 5 × 104 sorted cells were cultured in 1 ml medium supplemented with GM-CSF (10 ng/ml). At day 3 medium was exchanged, and at day 6 cultures were analyzed.

BrdU labeling and detection, CFSE labeling, cell cycle analysis

Mice were injected with BrdU (1mg, i.p.). 2 hours or 4 days later mice were sacrificed and BrdU incorporation was analyzed according to manufacturers instructions (BD). Briefly, cell surface antigens were stained with indicated antibodies, fixed, and permeabilized. BrdU epitopes were exposed by DNAse I digestion for 1 hour at 37 °C and detected using anti-BrdU monoclonal antibody (3D4, BD). For CFSE labeling cells were stained in 5 μM Carboxy Fluoroscein Succinimidyl Ester (CFSE, Molecular Probes) in PBS with 0.1 % FCS at a concentration of 107 cells/ml for 10 minutes at 37 °C. The reaction was quenched by adding an equal volume of 100 % FCS followed by washing 3 times in PBS with 5 % FCS to ensure removal of CFSE. For cell cycle analysis cells were sorted and incubated in 80 % PBS 20 % water 0.1 % TritonX-100 (Sigma) 50 mg/ml propidium iodide (Sigma) and 10 μg/ml RNAse A (Roche) over night at room temperature in the dark. Analysis was performed on a FACS Calibur using doublet discrimination mode.

Cell transfer experiments

Recipient mice were conditioned as indicated (lethal irradiation: 550cGy + 500cGy 3 hours between irradiations, sublethal irradiation: 600cGy) and cell suspensions were injected intravenously approximately 3h after irradiation. Mice were fed antibiotic–supplemented food (TestDiet, Richmond, IN) and given water ad libidum. Following numbers of cell sorter purified progenitors were injected and yielded the given numbers of cDC: Fig. 1c LinCSF1R+Kit input: 3.9 × 105 yield: 750 cDC, LinCSF1R+Kit+ input: 2.7 × 105 yield: 2200 cDC (14 days); Fig. 1e CX3CR1-GFP+Kit+ input: 2.1 × 105 yield: 7300 cDC CX3CR1-GFP+Kit input: 7.2 × 105 yield: 2500 cDC (14 days); CSF1R+Kit input: 4.3 × 105 yield: 2100 cDC; Fig. 2c MDP w/o Flt3L treatment input: 105 yield: 8910, 5730 cDC, Flt3L treatment input: 3 × 105 yield: 18800, 22600 cDC (9 days). Single and mixed bone marrow chimeras were produced by injecting LinKit+ cells from Flt3−/− or WT or Flt3−/− : WT (CD45.2 : CD45.1) mice into lethally irradiated wild-type recipients (SJL, CD45.1 or SJL×B6 F1, CD45.1+CD45.2+).

Supplementary Material

supp info

Acknowledgments

We thank Amgen for the generous gift of rhFlt3L. We are very thankful to Ihor Lemischka for providing Flt3−/− mice, and to Lorraine Robb and Glenn Begley for providing GM-CSFR-deficient (Csf2ra−/−) mice. We thank Chae Gyu Park for providing CD169 and SIGNR1 monoclonal antibodies. We wish to thank R. Steinman and A. Kamphorst for critical reading of the manuscript, and Mayte Suarez–Farinas for help with statistical analysis.

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