Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

FMS-Like Tyrosine Kinase 3 Ligand Treatment Does Not Ameliorate Experimental Rapidly Progressive Glomerulonephritis

  • Joanna R. Ghali ,

    Affiliations Centre for Inflammatory Diseases, Department of Medicine, Monash University, Clayton, Victoria, Australia, Department of Nephrology, Monash Health, Clayton, Victoria, Australia

  • Kim M. O’Sullivan,

    Affiliation Centre for Inflammatory Diseases, Department of Medicine, Monash University, Clayton, Victoria, Australia

  • Peter J. Eggenhuizen,

    Affiliation Centre for Inflammatory Diseases, Department of Medicine, Monash University, Clayton, Victoria, Australia

  • Stephen R. Holdsworth,

    Affiliations Centre for Inflammatory Diseases, Department of Medicine, Monash University, Clayton, Victoria, Australia, Department of Nephrology, Monash Health, Clayton, Victoria, Australia

  • A. Richard Kitching

    Affiliations Centre for Inflammatory Diseases, Department of Medicine, Monash University, Clayton, Victoria, Australia, Department of Nephrology, Monash Health, Clayton, Victoria, Australia, Department of Paediatric Nephrology, Monash Health, Clayton, Victoria, Australia

FMS-Like Tyrosine Kinase 3 Ligand Treatment Does Not Ameliorate Experimental Rapidly Progressive Glomerulonephritis

  • Joanna R. Ghali, 
  • Kim M. O’Sullivan, 
  • Peter J. Eggenhuizen, 
  • Stephen R. Holdsworth, 
  • A. Richard Kitching


Fms-like tyrosine kinase 3-ligand (FL) is a growth factor that may expand dendritic cell and regulatory T cell populations. We hypothesised that FL-induced regulatory T cells would protect mice from experimental rapidly progressive glomerulonephritis. To determine if FL was able to enhance regulatory T cell populations, C57BL/6 mice received 10 days of daily intraperitoneal injections of either FL or phosphate buffered saline. To induce accelerated autologous-phase anti-mouse glomerular basement membrane glomerulonephritis, mice were sensitized to sheep globulin 4 days prior to the induction of glomerulonephritis with sheep anti-mouse glomerular basement membrane globulin, and experiments ended 10 days later. FL was administered before, throughout and during the sensitization phase of this glomerulonephritis model. Renal disease and systemic immunity to the nephritogenic antigen were assessed. FL increased regulatory T cell and plasmacytoid dendritic cell proportions within spleen and lymph nodes. FL administration prior to glomerulonephritis did not protect mice from renal injury. When FL was given throughout the model, FL treated mice had reduced survival, with more interstitial neutrophils and glomerular CD11c+ cells than controls. Systemic immune responses showed increased IL-17A production from splenocytes, with more CD11c+ cells, but reduced plasmacytoid dendritic cell proportions in spleen and lymph nodes, despite increased regulatory T cell proportions. Under homeostatic conditions, FL expanded regulatory T cell and plasmacytoid dendritic cell populations, but FL enhanced systemic inflammatory responses and conventional dendritic cell populations when given during experimental glomerulonephritis, suggesting selective attempts to suppress pathogenic immunity by dendritic cell manipulation may be harmful.


Dendritic cells (DCs) are a heterogeneous population of professional antigen presenting cells, derived initially from common myeloid and common lymphoid progenitors in the bone marrow, which terminally differentiate in lymphoid and non-lymphoid tissues. They are broadly characterized into two groups: conventional or classical DCs (cDCs) and plasmacytoid DCs (pDCs) [1, 2]. In the mouse, cDCs include migratory and lymphoid-tissue resident DCs, which express CD11c and MHC II and are further characterized by the expression of other surface markers, including CD11b, CD103 and CD8. pDCs are found in lymph nodes (LN) or circulating within blood, and are CD11clow-intermediate, have low MHC II expression and express other surface markers including B220 and murine pDC antigen 1 (PDCA-1) [35]. pDCs promote the maturation of cDCs, regulate antigen specific CD4+ T cell proliferation, effector T cell (Teff) production of IFNγ and CD4+foxp3+ Treg homeostasis in mucosal lymphoid tissue [6]. Fms-like tyrosine kinase 3 (FLT3) ligand (FL) is a growth factor that differentiates, matures and expands DCs following ligation of the FLT3 receptor expressed on the surface of hematopoietic precursors [7, 8]. It is expressed in steady state conditions to maintain cDC and pDCs, produced by hematopoietic and stromal cells [9]. Mice deficient in FL lack DCs [10].

Exogenous administration of FL to mice expands DCs within the spleen and lymphoid tissues, and increases tissue resident DC populations, including those in the thymus and kidney [1113], as well as expanding regulatory T cell (Tregs) populations [14, 15]. Administration of FL to humans also expands immature myeloid DCs, pDCs and Tregs in peripheral blood, and is being explored as immunotherapy for certain malignancies [1618].

Rapidly progressive glomerulonephritis (RPGN) is characterized by cellular crescents and fibrinoid necrosis of the glomerular tuft. Current therapies are largely non-specific immunosuppressive agents. There is increasing evidence from animal and human studies that Tregs are protective in RPGN [1924]. Therefore, we hypothesized that exogenous FL may protect mice in experimental RPGN by suppressing nephritogenic immunity via expansion of pDCs and Tregs.

Materials and Methods

Experimental design

Male C57BL/6 mice, aged 6–10 weeks were purchased from Monash Animal Research Platform (Monash University) and were housed in specific pathogen free conditions (Monash Medical Centre Animal Facility, Clayton, Victoria, Australia). Studies were performed in accordance with the National Health and Medical Research Council’s Australian code for the care and use of animals for scientific purposes and were approved by the Monash University Animal Ethics Committee B (Ethics Number MMCB12/42). Aged matched mice were randomly assigned to experimental groups, had free access to water and food throughout experiments and were reviewed daily by both the researchers and animal facility staff. Mice were humanely euthanized with carbon dioxide at the completion of experiments or if mice showed any signs of the following: lethargy, persistent recumbency, hunched posture, rough coat or loss of body condition.

FL–Ig (human/human, BioXcell, West Lebanon, NH, USA; as cited in [25, 26]) was delivered as 10μg in 200μL PBS daily intraperitoneal injections for 10 days, as previously published [15]. Control mice received the same volume of PBS at the same times. Initial assessment of the effect of FL vs PBS on naïve mice was made with 4 mice per group. The model of RPGN used was an accelerated autologous phase anti-glomerular basement membrane (GBM) model (n = 6–9 each group; numbers were determined based on prior experience with this model [19]). Mice were sensitized s.c. with 0.5mg normal sheep globulin (in Freund’s complete adjuvant [FCA]) to the right and left tailbase. Four days later, sheep anti-mouse GBM globulin was injected intravenously into the tail-vein and mice were humanely killed after a further 10 days. For delayed type hypersensitivity (DTH), 0.5mg sheep globulin or horse globulin (as a control) was injected into the right and left hind footpads, respectively, and footpad swelling was measured 24hrs later with a micrometer (n = 4 each group). Statistical analysis was performed on Graphpad Prism 6 software. Data are presented as mean (±SEM) or median (range); assessment of 2 groups was performed with a student’s t test or Mann Whitney test for parametric and non-parametric data, respectively. Differences in survival were assessed with a log-rank test. Significant values were defined as P<0.05.

Assessment of functional and histological injury

Mice were placed on metabolic cages to collect urine prior to the end of experiments. Proteinuria was assessed by Bradford’s assay. Serum was collected from mice and urea levels were measured. To assess renal histology, 3μm-thick formalin-fixed, tissue processed, then paraffin embedded kidney sections were stained with Periodic Acid Schiff’s reagent. Forty glomeruli were assessed for glomerular segmental necrosis and crescent formation (primary outcome). CD4+ T cells, macrophages, and neutrophils were detected by immunoperoxidase staining of 6μm-thick, periodate lysine paraformaldehyde-fixed, frozen kidney sections as previously described [27]. Primary antibodies used were: CD4+ T cells (anti-CD4, GK1.5), macrophages (anti-CD68, FA/11), neutrophils (anti-Gr-1, RB6-8C5) with isotype controls being IgG2b, IgG2a and IgG2b, respectively. For leukocyte infiltration, 20 glomeruli and 10 interstitial high-powered fields were assessed.

Assessment of immunity by flow cytometry

Lymph nodes (cervical, axillary, brachial, inguinal, mesenteric and para-aortic, pooled for each animal) and spleens were harvested and single cell suspensions were created. One million cells were stained for flow cytometric analyses using the following antibodies: PDCA-1 (eBioscience, San Diego, CA, USA; Bio927), CD11c (BD Biosciences, North Ryde, NSW, Australia; HL3), CD4 (BD Biosciences; GK1.5), foxp3 (eBioscience; FJK-16s), CD25 (BD Biosciences; PC61). For intracellular cytokine staining, cells were fixed with eBioscience Fixation/Permeabilization concentrate, diluent and staining buffer according to the manufacturer’s protocol. Flow cytometry was performed on BD FACS Canto II and data analysed using FlowJo software (TreeStar, OR, USA).

Assessment of systemic immune responses to sheep globulin

Cultured cell supernatant was collected after stimulating 4 x 106 splenocytes with 100μg sheep globulin in 1mL RPMI-Complete (containing RPMI, 10% foetal calf serum, 50μM 2ME, 10mL penicillin-streptomycin and 5mL of L-glutamine) for 72 hours. IL-17A, IFNγ and IL-4 concentrations were measured by ELISA [28, 29] and other cytokines were measured with the Mouse Inflammation cytometric bead array (BD Biosciences). EliSpot assays for IFNγ (BD Biosciences) and IL-17A (eBioscience) were performed as previously described [30]. Spots were enumerated using an AID EliSpot platereader and software (v4.0, Autoimmun Diagnostika GmbH, Strassberg, Germany). Mouse anti-sheep IgG antibody levels were measured on diluted serum samples by ELISA [31].

Assessment of CD11c+ DCs in the kidney

To assess renal DCs, immunofluorescent staining of frozen kidney sections was performed using an anti-CD11c antibody (BD Biosciences; HL3) and mounted with DAPI mounting media (Molecular Probes). Images were acquired on a Nikon C1 confocal laser scan head attached to a Nikon Ti-E inverted microscope (Nikon, Tokyo, Japan) using 488 and 561nm lasers. Renal DCs were assessed in three areas: within glomeruli, in the periglomerular region (within 3 cells of Bowman’s capsule) or within a high-powered interstitial field. Twenty glomeruli and periglomerular regions and 10 high-powered fields were assessed for each animal, with CD11c+ immunofluorescence for each of these regions being analysed by Image J software (NIH, Bethesda, MD, USA).


Effects of FL on Tregs and DCs

Daily administration of FL for 10 days (Fig 1A) macroscopically increased spleen size and the size of all LN groups. When quantified, there were increased splenic cell numbers, with a trend towards increased cell numbers in pooled LN (Fig 1B). CD11c+ cells were also increased in the spleen and LN after FL administration (Fig 1C and 1D). Proportions of pDCs (CD11c+PDCA-1+/CD11c+ cells) were significantly elevated in the spleen, with a trend towards increase in the LN (Fig 1C and 1E). The proportion of Tregs (CD4+foxp3+/CD4+ cells) in FL treated animals was significantly increased (Fig 1F and 1G).

Fig 1. The effects of 10 days of intraperitoneal FL on DC and Treg populations.

(A) Experimental design, where FL or PBS was administered intraperitoneally to mice for daily for 10 days. (B) Total spleen and pooled LN cell number. (C) Representative FACS plots showing proportions of pDCs (CD11c+PDCA-1+ cells) in the spleen, gating on all CD11c+ leukocytes. (D) Proportions of CD11c+ cells in the spleen and LN. (E) Proportions of pDCs in the spleen and LN. (F) Representative FACS plots showing Tregs in the spleen, gating on lymphocytes, staining for CD4+ and foxp3+ cells. (G) Proportion of Tregs in the spleen and LN. Black bars represent PBS treated mice. White bars represent FL treated mice. n = 4 per group. *P<0.05, **P<0.01, ***P<0.001.

To determine if increased populations of pDCs and Tregs induced by FL protected mice from generating effector T cell responses, PBS or FL was administered to mice for 10 days, then mice were sensitized to sheep globulin. Mice were then culled 4 or 10 days after sensitization (Fig 2A). At 4 and 10 days post-sensitization, the numbers of splenocytes and LN cells were not different between PBS and FL treated mice (Fig 2B and 2C). Four days after sensitization to sheep globulin, the proportion of CD11c+ cells remained elevated in the LN, but not the spleen of FL treated mice (spleen PBS 20.9±2.5 vs FL 19.4±2.6%, P = 0.7; LN PBS 6.6±0.3 vs FL 9.6±0.4%, P<0.005). FL treated mice had higher proportions of pDCs in spleen and LN (Fig 2D), Ten days after sensitization to sheep globulin, FL treated mice had a reduced proportion of CD11c+ cells in the LN (spleen PBS 4.3±2.2 vs FL 2.4±0.1%, P = 0.44; LN PBS 1.2±0.03 vs FL 0.9±0.02%, P<0.001), but there was no longer any detectable difference in pDC proportions (Fig 2E). No significant differences in Treg proportions were identified four days after sheep globulin sensitization between mice that had been treated with PBS or FL (spleen PBS 7.2±0.8 vs FL 8.6±0.3%, P = 0.16; LN PBS 8.6±0.1 vs FL 9.5±0.5%, P = 0.11). Four days after sheep globulin sensitisation, FL mice developed increased dermal DTH to sheep globulin, suggesting elevated pDC populations did not suppress antigen-specific immunity, but rather enhanced effector T cell function (Fig 2F). When mice were challenged with sheep globulin 10 days after sensitization, DTH was present to a similar degree in PBS and FL treated groups (Fig 2G).

Fig 2. FL therapy expands pDCs but increases delayed type hypersensitivity four days after sensitization to sheep globulin.

(A) Experimental design. (B, C) Total spleen and LN cell number 4 and 10 days after sensitization, respectively. (D, E) Proportion of pDCs in the spleen and LN 4 and 10 days post-sensitization to sheep globulin respectively. (F, G) Footpad swelling in mice 4 and 10 days post-sensitization to sheep globulin, respectively. Black bars represent PBS treated mice. White bars represent FL treated mice. n = 4 per group. *P<0.05, **P<0.01.

FL administered prior to the induction of nephritogenic immunity

When FL or PBS was administered for 10 days before the model of RPGN (with treatment ending the day before mice were immunized with sheep globulin), injury was similar in both groups of mice. No significant differences in renal functional injury (proteinuria or urea; Fig 3A and 3B) or histological damage (glomerular crescents or segmental necrosis; Fig 3C3E) were found. While the total number of splenocytes or LN cells was not different between groups, the proportion of splenic CD11c+ cells was reduced in FL treated mice (Fig 3F and 3G), but unaltered in the LN between groups. There was no difference in the proportion of pDCs (Fig 3H), nor was there a difference in the proportion of activated T cells (CD4+CD25+/CD4+ cells) in the spleen and LN between the two groups (spleen PBS 4.4±0.4 vs FL 5.5±0.4%, P = 0.12; LN PBS 34.1±3.6 vs 35.9±2.8%, P = 0.7). With respect to cellular immune responses, FL treated mice had reduced IL-17A levels in sheep globulin stimulated splenocyte supernatant compared to controls, but no differences were found in IFNγ, IL-4 or IL-10 concentrations (Table 1); TNF, IL-12p70 and IL-6 concentrations were below the threshold for detection in both groups. FL treated animals had a trend towards lower serum mouse anti-sheep immunoglobulin titres (Fig 3I). Therefore, although FL did not protect mice when given prior to the induction of crescentic GN, some elements of cellular and humoral immune responses were attenuated by FL therapy, suggesting that FL might alter renal injury if delivered throughout the entire course of this disease model.

Fig 3. FL administered before accelerated autologous phase anti-GBM disease did not protect against nephritis, but altered systemic immunity.

(A) Proteinuria (dotted line represents measured level in non-nephritic WT mice, n = 4). (B) Serum urea (dotted line represents measured level in non-nephritic WT mice, n = 4). (C) Proportions of glomeruli with crescents and (D) glomerular segmental necrosis. (E) Representative images of glomeruli from PBS and FL treated mice taken at high power (400x, PAS stain). (F) Total spleen and LN cell number. (G) Proportion of CD11c+ cells from leukocytes in spleen and LN. (H) Proportion of pDCs in spleen and LN. (I) Serum mouse anti-sheep IgG antibody levels. Black bars represent PBS treated mice. White bars represent FL treated mice. OD, optical density. n = 6 per group. *P<0.05.

Table 1. Cytokine concentrations in stimulated splenocyte supernatant for mice receiving PBS or FL for 10 days prior to commencement of the anti-GBM disease model.

FL treatment beginning at sensitization, continuing throughout the disease model

When FL treatment commenced on the day mice were sensitized to sheep globulin and continued through the course of disease (Fig 4A), more FL treated animals unexpectedly developed signs of renal failure, and met criteria for humane euthanasia, compared to PBS treated controls, occurring after sheep anti-mouse GBM globulin administration during nephritis (Fig 4B); the experiment was terminated early at day 10 of the model. A repeat experiment was performed, with animals being euthanized at day 9 (five days after anti-GBM administration; Fig 5A). Mice in both groups sustained significant functional renal injury (serum urea; PBS 121±16 vs FL 126±10 mmol/L, P = 0.78), with comparable proteinuria and histological damage, marked by widespread glomerular segmental necrosis (Fig 5B–5E). FL treated mice had enhanced interstitial neutrophil recruitment compared to controls (Table 2). Renal CD11c+ cells were increased within glomeruli of FL treated mice, with a trend to increase in periglomerular and interstitial regions (Fig 5F5I).

Fig 4. FL administered throughout accelerated autologous phase anti-GBM disease reduced mouse survival.

(A) Experimental design. (B) Survival following the induction of nephritis. Black bars represent PBS treated mice. White bars represent FL treated mice. n = 9 per group. *P<0.05.

Fig 5. FL therapy throughout accelerated anti-GBM disease did not protect mice from nephritis.

(A) Experimental design. (B) Proteinuria. (C) Percentage of glomerular crescents and (D) glomeruli with segmental necrosis. (E) Representative images of glomeruli from PBS and FL treated mice taken at high power (400x, PAS stain). (F–H) gcs, periglomerular and interstitial hpf CD11c+ immunofluorescence assessed by fluorescent microscopy of renal sections. (I) Representative images of CD11c+ immunofluorescent staining within the interstitial, glomerular and periglomerular regions. Black bars represent PBS treated mice. White bars represent FL treated mice. AU, arbitrary units; gcs, glomerular cross section; hpf, high-powered field. n = 7 per group. *P<0.05.

Table 2. Intrarenal leukocytes in mice treated with PBS or FL throughout anti-GBM disease until day 9.

Systemic inflammatory immune responses were heightened in the FL treated mice, with significantly increased IL-17A production, and a trend towards enhanced IFNγ production by splenocytes (Fig 6A and 6B). IL-6 concentrations were not different between groups (median with range, PBS 0 [0–12] vs FL 0 [0–14], P = 0.29). IL-12p70, TNF and IL-10 concentrations were undetectable in both groups. Within the spleen and LN, cell numbers were similar between groups, but FL treated mice had significantly increased proportions of CD11c+ cells and reduced proportions of pDCs (Fig 6C6F). FL treated mice had elevated proportions of activated (CD4+CD25+) T cells and Tregs (CD4+CD25+foxp3+), with a similar proportion of effector T cells (CD4+CD25+foxp3-) within LN, but in the spleen FL treated mice had fewer activated T cells and Teff (Fig 6G–6J). Therefore, FL administration throughout experimental RPGN promoted maturation of DCs towards a conventional DC phenotype. It did not suppress nephritogenic immunity, but rather FL enhanced systemic immunity and T cell activation.

Fig 6. Cellular pro-inflammatory immune responses were heightened when FL was given during accelerated anti-GBM disease.

(A) IL-17A+ spots and (B) IFNγ+ spots per 1 million stimulated splenocytes, measured by EliSpot. (C) Total spleen and LN cell number. (D, E) Proportion of CD11c+ cells and pDCs in the spleen and LN. (F) Representative FACS plots of splenocytes stained for CD11c and PDCA-1. (G) Proportion of activated T cells (CD4+CD25+/CD4+) in spleen and LN. (H) Representative FACS plots of pooled LN cells stained for CD4, CD25 and foxp3. (I, J) Proportions of Tregs (CD4+CD25+foxp3+/CD4+) and Teff (CD4+CD25+foxp3-/CD4+) in spleen and LN. Black bars represent PBS treated mice. White bars represent FL treated mice. n = 7 per group. *P<0.05, **P<0.01, ***P<0.001, ****P<0.0001.

FL administered before and during the induction of nephritogenic immunity

This model of RPGN relies on planting sheep globulin, a foreign antigen, within the glomerulus of sensitized mice. It was possible that exogenous FL, administered at the time of anti-GBM globulin injection, enhanced the maturation and expansion of cDCs in sensitized mice rather than polarizing precursor DCs towards this phenotype. We sought to determine if FL could induce pDCs and enhance Treg populations in steady state conditions and suppress subsequent antigen-specific responses. Therefore, we administered FL before and during the sensitization period (i.e. when DCs were playing a key role in inducing immunity to sheep globulin) but discontinued it at the time nephritis was induced (Fig 7A).

Fig 7. Effects of FL given during sensitization, but not during the nephritic phase of injury.

(A) Experimental design. (B) Serum urea (dotted line represents measured level in non-nephritic WT mice, n = 4). (C) Proteinuria (dotted line represents measured level in non-nephritic WT mice, n = 4). (D, E) Percentage of glomerular crescents and segmental necrosis. (F) Total spleen and LN cell number. (G) Proportion of Tregs in the spleen and LN. (H) Serum mouse anti-sheep IgG antibody concentrations. Black bars represent PBS treated mice. White bars represent FL treated mice. OD, optical density. n = 7 for PBS group and 9 for FL group. *P<0.05, ***P<0.001.

Compared to controls, FL treated mice showed similar functional injury, with a trend towards fewer glomerular crescents and less segmental necrosis (Fig 7B–7E). There was no difference in splenocyte number between groups, but LN cell numbers were reduced in FL treated mice (Fig 7F). Splenic regulatory T cell populations of FL treated animals were enhanced, but fewer Tregs were present in the LN of FL treated mice (Fig 7G). There were no significant differences in the proportions of CD11c+ cells and pDCs between groups (CD11c+ spleen PBS 1.3±0.3 vs FL 0.8±0.1%, P = 0.11; CD11c+ LN PBS 1.9±0.1 vs FL 1.8±0.3, P = 0.8 and pDCs spleen PBS 1.4±0.6 vs FL 1.3±0.7%, P = 0.91; pDCs LN PBS 4.5 ±1.2 vs FL 5.3±1.2%, P = 0.67). There was no difference in IFNγ, IL-17A, IL-4 or IL-10 concentrations in stimulated splenocyte supernatant (Table 3); IL-6, IL-12p70 and TNF concentrations were undetectable. Serum antigen specific IgG antibodies between groups were not different (Fig 7H). Therefore, FL administration before and during the sensitization phase did not result in enhanced injury as seen when FL was given throughout the nephritis phase, but did not protect mice from effector T cell mediated renal injury.

Table 3. Cytokine concentrations in stimulated splenocyte supernatant for mice receiving PBS or FL before and during sensitization to the nephritogenic antigen in the anti-GBM disease model.


We have shown that FL administered under homeostatic conditions expands Treg and DC populations. DC expansion was not restricted to pDCs, but both cDC and pDC populations were increased. Despite inducing Tregs, FL given prior to autologous phase accelerated anti-GBM GN did not result in significant protection from renal injury, although we found evidence that some elements of systemic immunity were attenuated, with reduced IL-17A production from splenocytes. When FL was given throughout the nephritis model, FL treated mice exhibited excess mortality. This was likely, but not certain, to be due to renal disease. We repeated this model, euthanizing mice earlier to assess renal injury and systemic immune responses prior to mice becoming too unwell. We found similar, but severe, glomerular injury in both groups. However, glomerular CD11c+ DCs and neutrophil recruitment to the renal interstitium was increased in FL treated mice compared to controls, indicating greater pro-inflammatory local immune responses had developed in the FL group. Systemic immune responses were also increased in the FL group, with enhanced Th17 cellular immunity and increased cDC populations in secondary lymphoid organs. Therefore, FL administration throughout RPGN polarized naïve T cells towards an effector rather than a regulatory phenotype.

Despite the persistence of a higher proportion of pDCs after FL had been given for 10 days, mice subsequently sensitized to sheep globulin had enhanced dermal DTH 4 days later. Therefore, despite enhanced Treg populations and pDCs at the time of sensitization, the induction of immunity to sheep globulin enhanced effector T cell responses, indicating effective antigen presentation by the DC populations. When FL was given before and during sensitization, but not during nephritis, renal injury or systemic immune responses were not altered. These findings suggest that when FL was given in steady-state conditions, expanded DC populations and Treg induction were capable of modulating effector T cell responses and cytokine release.

There are variable reports of the effectiveness of FL therapy in experimental autoimmune disease. In the NOD mouse type I diabetes model, pancreatic beta cell destruction was prevented by administering FL prior to the development of pancreatic injury in young, but not in older mice, despite increasing DC and Treg populations in spleen and pancreatic LN [32, 33]. The onset of diabetes was accelerated by FL therapy given to NOD mice with detectable auto-reactive T cells with increased pro-inflammatory cytokine expression [33]. FL attenuated inflammatory bowel disease in the TNFΔARE mouse model, by enhancing Tregs [34].

In models of T cell dependent inflammation or asthma/airways disease induced by foreign antigens, FL therapy has also provided mixed results. Experimental methylated bovine serum albumin induced arthritis was not significantly attenuated by FL treatment [35], whereas treatment with sumatinib (a tyrosine kinase receptor inhibitor directed against the FLT3 receptor) protected mice from joint damage [35, 36]. FL therapy did protect mice from allergic airways inflammation, with evidence for either a Th2 to Th1 shift in immunity [37, 38] or enhanced Treg function and recruitment [39, 40]. Similarly, experience with FL in models of transplantation provides conflicting results. Allogeneic T cell responses were reduced and mouse survival increased when bone marrow recipients were pre-treated with FL in a model of experimental graft vs host disease [15], and when FL treated renal DCs were transferred into mice receiving allogeneic cardiac transplants [13]. However, FL administration to donors prior to liver transplantation expanded myeloid and lymphoid DCs in the grafts, worsened graft survival, with evidence of heightened Th1 immune responses and less apoptosis of alloreactive T cells [41].

In vitro and in vivo studies suggest DC maturity directs their suppressive or inflammatory capacity. In steady state, DCs from mice receiving FL had an immature phenotype and were poor stimulators of T cell proliferation in co-culture ex vivo, but they could induce expansion of regulatory cells [13, 15, 42, 43], without requiring MHCII expression [15]. However, lipopolysaccharide (LPS)-matured FL-induced DCs potently induced naïve T cell proliferation without Treg expansion [13]. Bone marrow derived DCs cultured with FL plus IFNα or LPS had increased surface expression of activation markers and enhanced T cell proliferation compared to bone marrow DCs cultured with FL alone. Therefore, in an inflammatory milieu, FL treated DCs mature and take on a more conventional phenotype [42]. Similarly, compared to FL treated mice receiving peptide immunisation alone, FL treated mice receiving immunisation with peptide and adjuvant (FCA) had enhanced T cell activation and proliferation, and more DCs with a mature phenotype [44]. In the presence of toll like receptor 9 agonists or inactivated influenza virus, pDCs transformed into cells exhibiting a cDC phenotype, with increased IFNα production and the capacity to stimulate T cells in vitro [45]. Transfer of immature FL treated DCs into mice prior to experimental autoimmune encephalitis (EAE) induction (with myelin oligodendrocyte glycoprotein/FCA) resulted in less severe disease than mice pre-treated with TNF and LPS matured FL DCs [46]. When FL therapy was initiated five days prior to EAE induction and continued for a further five days, FL treated mice developed increased disease severity compared to controls [47], whereas treatment of mice with established EAE with a FL inhibitor (CEP-701, which induced apoptosis of mature DCs) resulted in improvement in disease progression [48]. These studies suggest that although FL therapy promotes immature DCs and Tregs in steady state, these DCs can become polarised towards a conventional phenotype in the presence of pro-inflammatory cytokines and proteins. This may explain some of the conflicting reports about the immunomodulatory effects of FL, and why FL was not protective when given during our experimental crescentic GN model, which relies on an adaptive immune response to sheep globulin planted along the GBM in sensitized mice [46].

The current studies have shown that FL administered throughout a murine model of RPGN heightened inflammatory effector T cell immune responses, resulting in reduced animal survival. The pitfalls of FL therapy demonstrated in this work highlight the challenges inherent in manipulating cellular immunity to promote Tregs in immune renal disease.

Author Contributions

Conceived and designed the experiments: JRG ARK. Performed the experiments: JRG KMO PJE. Analyzed the data: JRG. Contributed reagents/materials/analysis tools: SRH ARK. Wrote the paper: JRG SRH ARK.


  1. 1. D'Amico A, Wu L. The early progenitors of mouse dendritic cells and plasmacytoid predendritic cells are within the bone marrow hemopoietic precursors expressing Flt3. J Exp Med. 2003;198(2): 293–303. pmid:12874262
  2. 2. Shortman K, Naik SH. Steady-state and inflammatory dendritic-cell development. Nature reviews Immunology. 2007;7(1): 19–30. pmid:17170756
  3. 3. Merad M, Sathe P, Helft J, Miller J, Mortha A. The dendritic cell lineage: ontogeny and function of dendritic cells and their subsets in the steady state and the inflamed setting. Annual review of immunology. 2013;31: 563–604. pmid:23516985
  4. 4. Rogers NM, Isenberg JS, Thomson AW. Plasmacytoid dendritic cells: no longer an enigma and now key to transplant tolerance? American journal of transplantation: official journal of the American Society of Transplantation and the American Society of Transplant Surgeons. 2013;13(5): 1125–33. pmid:23617754
  5. 5. Colonna M, Trinchieri G, Liu YJ. Plasmacytoid dendritic cells in immunity. Nature immunology. 2004;5(12): 1219–26. pmid:15549123
  6. 6. Takagi H, Fukaya T, Eizumi K, Sato Y, Sato K, Shibazaki A, et al. Plasmacytoid dendritic cells are crucial for the initiation of inflammation and T cell immunity in vivo. Immunity. 2011;35(6): 958–71. pmid:22177923
  7. 7. Shurin MR, Esche C, Lotze MT. FLT3: receptor and ligand. Biology and potential clinical application. Cytokine & growth factor reviews. 1998;9(1): 37–48.
  8. 8. Karsunky H, Merad M, Cozzio A, Weissman IL, Manz MG. Flt3 ligand regulates dendritic cell development from Flt3+ lymphoid and myeloid-committed progenitors to Flt3+ dendritic cells in vivo. J Exp Med. 2003;198(2): 305–13. pmid:12874263
  9. 9. Miloud T, Fiegler N, Suffner J, Hammerling GJ, Garbi N. Organ-specific cellular requirements for in vivo dendritic cell generation. J Immunol. 2012;188(3): 1125–35. pmid:22198954
  10. 10. McKenna HJ, Stocking KL, Miller RE, Brasel K, De Smedt T, Maraskovsky E, et al. Mice lacking flt3 ligand have deficient hematopoiesis affecting hematopoietic progenitor cells, dendritic cells, and natural killer cells. Blood. 2000;95(11): 3489–97. pmid:10828034
  11. 11. Shurin MR, Pandharipande PP, Zorina TD, Haluszczak C, Subbotin VM, Hunter O, et al. FLT3 ligand induces the generation of functionally active dendritic cells in mice. Cellular immunology. 1997;179(2): 174–84. pmid:9268501
  12. 12. Maraskovsky E, Brasel K, Teepe M, Roux ER, Lyman SD, Shortman K, et al. Dramatic increase in the numbers of functionally mature dendritic cells in Flt3 ligand-treated mice: multiple dendritic cell subpopulations identified. J Exp Med. 1996;184(5): 1953–62. pmid:8920882
  13. 13. Coates PT, Duncan FJ, Colvin BL, Wang Z, Zahorchak AF, Shufesky WJ, et al. In vivo-mobilized kidney dendritic cells are functionally immature, subvert alloreactive T-cell responses, and prolong organ allograft survival. Transplantation. 2004;77(7): 1080–9. pmid:15087775
  14. 14. Darrasse-Jeze G, Deroubaix S, Mouquet H, Victora GD, Eisenreich T, Yao KH, et al. Feedback control of regulatory T cell homeostasis by dendritic cells in vivo. J Exp Med. 2009;206(9): 1853–62. pmid:19667061
  15. 15. Swee LK, Bosco N, Malissen B, Ceredig R, Rolink A. Expansion of peripheral naturally occurring T regulatory cells by Fms-like tyrosine kinase 3 ligand treatment. Blood. 2009;113(25): 6277–87. pmid:19211508
  16. 16. Klein O, Ebert LM, Zanker D, Woods K, Tan BS, Fucikova J, et al. Flt3 ligand expands CD4+ FoxP3+ regulatory T cells in human subjects. European journal of immunology. 2013;43(2): 533–9. pmid:23124877
  17. 17. Marroquin CE, Westwood JA, Lapointe R, Mixon A, Wunderlich JR, Caron D, et al. Mobilization of dendritic cell precursors in patients with cancer by flt3 ligand allows the generation of higher yields of cultured dendritic cells. Journal of immunotherapy. 2002;25(3): 278–88. pmid:12000870
  18. 18. Rini BI, Paintal A, Vogelzang NJ, Gajewski TF, Stadler WM. Flt-3 ligand and sequential FL/interleukin-2 in patients with metastatic renal carcinoma: clinical and biologic activity. Journal of immunotherapy. 2002;25(3): 269–77. pmid:12000869
  19. 19. Ooi JD, Snelgrove SL, Engel DR, Hochheiser K, Ludwig-Portugall I, Nozaki Y, et al. Endogenous foxp3(+) T-regulatory cells suppress anti-glomerular basement membrane nephritis. Kidney international. 2011;79(9): 977–86. pmid:21248715
  20. 20. Paust HJ, Ostmann A, Erhardt A, Turner JE, Velden J, Mittrucker HW, et al. Regulatory T cells control the Th1 immune response in murine crescentic glomerulonephritis. Kidney international. 2011;80(2): 154–64. pmid:21525855
  21. 21. Wolf D, Hochegger K, Wolf AM, Rumpold HF, Gastl G, Tilg H, et al. CD4+CD25+ regulatory T cells inhibit experimental anti-glomerular basement membrane glomerulonephritis in mice. Journal of the American Society of Nephrology: JASN. 2005;16(5): 1360–70. pmid:15788479
  22. 22. Salama AD, Chaudhry AN, Holthaus KA, Mosley K, Kalluri R, Sayegh MH, et al. Regulation by CD25+ lymphocytes of autoantigen-specific T-cell responses in Goodpasture's (anti-GBM) disease. Kidney international. 2003;64(5): 1685–94. pmid:14531801
  23. 23. Ligler FS, Westby GR, Hertz BC, Durning CM, Cohen R, Bonner H. Immunoregulatory cell subsets in Goodpasture's syndrome: evidence for selective T suppressor-cell depletion during active autoimmune disease. Journal of clinical immunology. 1983;3(4): 368–74. pmid:6228561
  24. 24. Ostmann A, Paust HJ, Panzer U, Wegscheid C, Kapffer S, Huber S, et al. Regulatory T cell-derived IL-10 ameliorates crescentic GN. Journal of the American Society of Nephrology: JASN. 2013;24(6): 930–42. pmid:23641052
  25. 25. Liao G, O'Keeffe MS, Wang G, van Driel B, de Waal Malefyt R, Reinecker HC, et al. Glucocorticoid-Induced TNF Receptor Family-Related Protein Ligand is Requisite for Optimal Functioning of Regulatory CD4(+) T Cells. Frontiers in immunology. 2014;5: 35. pmid:24550919
  26. 26. Gonzalez IT, Barrientos G, Freitag N, Otto T, Thijssen VL, Moschansky P, et al. Uterine NK cells are critical in shaping DC immunogenic functions compatible with pregnancy progression. PloS one. 2012;7(10): e46755. pmid:23056436
  27. 27. Kitching AR, Turner AL, Wilson GR, Semple T, Odobasic D, Timoshanko JR, et al. IL-12p40 and IL-18 in crescentic glomerulonephritis: IL-12p40 is the key Th1-defining cytokine chain, whereas IL-18 promotes local inflammation and leukocyte recruitment. Journal of the American Society of Nephrology: JASN. 2005;16(7): 2023–33. pmid:15888563
  28. 28. Summers SA, Phoon RK, Ooi JD, Holdsworth SR, Kitching AR. The IL-27 receptor has biphasic effects in crescentic glomerulonephritis mediated through Th1 responses. The American journal of pathology. 2011;178(2): 580–90. pmid:21281790
  29. 29. Kitching AR, Tipping PG, Kurimoto M, Holdsworth SR. IL-18 has IL-12-independent effects in delayed-type hypersensitivity: studies in cell-mediated crescentic glomerulonephritis. J Immunol. 2000;165(8): 4649–57. pmid:11035108
  30. 30. Ooi JD, Chang J, Hickey MJ, Borza DB, Fugger L, Holdsworth SR, et al. The immunodominant myeloperoxidase T-cell epitope induces local cell-mediated injury in antimyeloperoxidase glomerulonephritis. Proceedings of the National Academy of Sciences of the United States of America. 2012;109(39): E2615–24. pmid:22955884
  31. 31. Tipping PG, Kitching AR, Huang XR, Mutch DA, Holdsworth SR. Immune modulation with interleukin-4 and interleukin-10 prevents crescent formation and glomerular injury in experimental glomerulonephritis. European journal of immunology. 1997;27(2): 530–7. pmid:9045927
  32. 32. O'Keeffe M, Brodnicki TC, Fancke B, Vremec D, Morahan G, Maraskovsky E, et al. Fms-like tyrosine kinase 3 ligand administration overcomes a genetically determined dendritic cell deficiency in NOD mice and protects against diabetes development. International immunology. 2005;17(3): 307–14. pmid:15684037
  33. 33. Van Belle TL, Juntti T, Liao J, von Herrath MG. Pre-existing autoimmunity determines type 1 diabetes outcome after Flt3-ligand treatment. Journal of autoimmunity. 2010;34(4): 445–52. pmid:20004555
  34. 34. Collins CB, Aherne CM, McNamee EN, Lebsack MD, Eltzschig H, Jedlicka P, et al. Flt3 ligand expands CD103(+) dendritic cells and FoxP3(+) T regulatory cells, and attenuates Crohn's-like murine ileitis. Gut. 2012;61(8): 1154–62. pmid:22068168
  35. 35. Svensson MN, Andersson SE, Erlandsson MC, Jonsson IM, Ekwall AK, Andersson KM, et al. Fms-like tyrosine kinase 3 ligand controls formation of regulatory T cells in autoimmune arthritis. PloS one. 2013;8(1): e54884. pmid:23349985
  36. 36. Dehlin M, Andersson S, Erlandsson M, Brisslert M, Bokarewa M. Inhibition of fms-like tyrosine kinase 3 alleviates experimental arthritis by reducing formation of dendritic cells and antigen presentation. Journal of leukocyte biology. 2011;90(4): 811–7. pmid:21771900
  37. 37. Agrawal DK, Hopfenspirger MT, Chavez J, Talmadge JE. Flt3 ligand: a novel cytokine prevents allergic asthma in a mouse model. International immunopharmacology. 2001;1(12): 2081–9. pmid:11710537
  38. 38. Edwan JH, Perry G, Talmadge JE, Agrawal DK. Flt-3 ligand reverses late allergic response and airway hyper-responsiveness in a mouse model of allergic inflammation. J Immunol. 2004;172(8): 5016–23. pmid:15067083
  39. 39. McGee HS, Stallworth AL, Agrawal T, Shao Z, Lorence L, Agrawal DK. Fms-like tyrosine kinase 3 ligand decreases T helper type 17 cells and suppressors of cytokine signaling proteins in the lung of house dust mite-sensitized and-challenged mice. American journal of respiratory cell and molecular biology. 2010;43(5): 520–9. pmid:19933379
  40. 40. McGee HS, Edwan JH, Agrawal DK. Flt3-L increases CD4+CD25+Foxp3+ICOS+ cells in the lungs of cockroach-sensitized and-challenged mice. American journal of respiratory cell and molecular biology. 2010;42(3): 331–40. pmid:19448155
  41. 41. Li W, Lu L, Wang Z, Wang L, Fung JJ, Thomson AW, et al. Il-12 antagonism enhances apoptotic death of T cells within hepatic allografts from Flt3 ligand-treated donors and promotes graft acceptance. J Immunol. 2001;166(9): 5619–28. pmid:11313402
  42. 42. Brasel K, De Smedt T, Smith JL, Maliszewski CR. Generation of murine dendritic cells from flt3-ligand-supplemented bone marrow cultures. Blood. 2000;96(9): 3029–39. pmid:11049981
  43. 43. Yamano T, Watanabe S, Hasegawa H, Suzuki T, Abe R, Tahara H, et al. Ex vivo-expanded DCs induce donor-specific central and peripheral tolerance and prolong the acceptance of donor skin grafts. Blood. 2011;117(9): 2640–8. pmid:21220748
  44. 44. Diener KR, Moldenhauer LM, Lyons AB, Brown MP, Hayball JD. Human Flt-3-ligand-mobilized dendritic cells require additional activation to drive effective immune responses. Experimental hematology. 2008;36(1): 51–60. pmid:17949888
  45. 45. O'Keeffe M, Hochrein H, Vremec D, Caminschi I, Miller JL, Anders EM, et al. Mouse plasmacytoid cells: long-lived cells, heterogeneous in surface phenotype and function, that differentiate into CD8(+) dendritic cells only after microbial stimulus. J Exp Med. 2002;196(10): 1307–19. pmid:12438422
  46. 46. Papenfuss TL, Kithcart AP, Powell ND, McClain MA, Gienapp IE, Shawler TM, et al. Disease-modifying capability of murine Flt3-ligand DCs in experimental autoimmune encephalomyelitis. Journal of leukocyte biology. 2007;82(6): 1510–8. pmid:17855499
  47. 47. Greter M, Heppner FL, Lemos MP, Odermatt BM, Goebels N, Laufer T, et al. Dendritic cells permit immune invasion of the CNS in an animal model of multiple sclerosis. Nature medicine. 2005;11(3): 328–34. pmid:15735653
  48. 48. Whartenby KA, Calabresi PA, McCadden E, Nguyen B, Kardian D, Wang T, et al. Inhibition of FLT3 signaling targets DCs to ameliorate autoimmune disease. Proceedings of the National Academy of Sciences of the United States of America. 2005;102(46): 16741–6. pmid:16272221