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Hedgehog/GLI1 activation leads to leukemic transformation of myelodysplastic syndrome in vivo and GLI1 inhibition results in antitumor activity

Abstract

Myelodysplastic syndromes (MDSs) are stem cell disorders with risk of transformation to acute myeloid leukemia (AML). Gene expression profiling reveals transcriptional expression of GLI1, of Hedgehog (Hh) signaling, in poor-risk MDS/AML. Using a murine model of MDS we demonstrated that constitutive Hh/Gli1 activation accelerated leukemic transformation and decreased overall survival. Hh/Gli1 activation resulted in clonal expansion of phenotypically defined granulocyte macrophage progenitors (GMPs) and acquisition of self-renewal potential in a non-self-renewing progenitor compartment. Transcriptome analysis of GMPs revealed enrichment in gene signatures of self-renewal pathways, operating via direct Gli1 activation. Using human cell lines we demonstrated that in addition to canonical Hh signaling, GLI1 is activated in a Smoothened-independent manner. GLI1 knockdown or inhibition with GANT61 resulted in decreased proliferation and clonogenic potential. Our data suggest that GLI1 activation is frequent in MDS during disease progression and inhibition of GLI1 is an attractive therapeutic target for a subset of patients.

Introduction

Myelodysplastic syndromes (MDSs) are clonal hematopoietic stem cell (HSC) disorders characterized by ineffective hematopoiesis manifested by peripheral blood cytopenias and bone marrow hypocellularity [1, 2]. Although low-risk MDS generally carries a good prognosis, clinical outcomes considerably deteriorate upon progression to secondary acute myeloid leukemia (sAML) with a dismal median survival of <6 months [3, 4]. Several mechanisms, including the acquisition of structural chromosomal changes, point mutations, and the distortion of epigenetic signatures are associated with leukemic transformation of MDS [5,6,7]. However, the cellular pathways involved in this process have not been clearly defined. Consequently, with the exception of lenalidomide in 5q− syndrome, targeted therapies proven to be effective in other human malignancies are not currently available for patients with MDS. Approved therapeutic options are limited to hypomethylating (HMA) and immunomodulatory agents, but these are not curative and only marginally prolong survival in a subset of patients [8]. More aggressive approaches like induction chemotherapy and allogeneic bone marrow transplantation are frequently limited in this group of patients due to excessive toxicity and/or low efficacy [9, 10].

The Hedgehog (Hh) signaling pathway is active during embryogenesis and silenced in most adult tissues. Abnormal pathway activation has been demonstrated in a variety of solid and hematologic malignancies [11]. Hh signaling is initiated by binding of one of the three ligands to the cell surface receptor Patched (PTCH) that normally inhibits the protein Smoothened (SMO), and is further transmitted via a protein complex that includes Suppressor of Fused and downstream zinc-finger Gli transcription factors (TFs). GLI1 functions exclusively as an activator, GLI3 is a repressor, and GLI2 can operate as either activator or repressor [12, 13]. In addition to canonical Hh signaling, the activity of GLI1 can be modulated by other pathways frequently involved in human tumorigenesis, including Wnt, Notch, RAS-MEK, and transforming growth factor-β (TGF-β) [14,15,16,17].

Hh signaling plays a pivotal role in the development and progression of various hematologic malignancies [18,19,20,21]. Most recently we established that GLI2 expression is an independent predictor of poor outcome in FLT3-ITD-mutated AML, and Hh activation leads to accelerated progression and leukemic transformation of FLT3-ITD-driven indolent myeloproliferative disease in mice [18]. Only limited data exist on Hh signaling in MDS and very little is known about the role of pathway activation in disease development and progression [22]. Hh inhibitors have been shown to be effective in preclinical studies in MDS and AML, and preliminary data from ongoing clinical trials using SMO inhibitors demonstrate promising antitumor activity [23, 24]. However, optimal Hh-targeting strategies remain to be determined.

Here we examine the clinical impact of aberrant Hh signaling in MDS and further explore the mechanism of Hh-driven disease progression and leukemic transformation using the Nup98-HoxD13 (NHD13) animal model of MDS. We have found that constitutive activation of Hh signaling results in accelerated leukemic transformation via acquisition of self-renewal in phenotypically defined granulocyte macrophage progenitors (GMPs). We have also demonstrated that the inhibition of Hh pathway at the level of GLI1 rather than upstream SMO may be a more effective targeted therapeutic approach in MDS and sAML.

Results

Hh signaling is silenced in normal hematopoietic stem and progenitor cells and aberrantly activated in a subset of MDS patients

Hh signaling activation results in transcriptional activation of GLI1. To determine the activity of Hh signaling pathway in normal and malignant hematopoiesis we analyzed the expression of GLI1 using publicly available expression datasets. GLI1 was found to be significantly upregulated in MDS (Figure S1), poor-risk AML (Fig. 1a), and AML with complex cytogenetics (Fig. 1b). These subtypes of AML frequently arise from antecedent hematological disorders like MDS. Moreover, high GLI1 expression correlated with shorter overall survival (median survival 24.1 vs. 16.3 months, p = 0.03) (Fig. 1c). Further analysis revealed that GLI1 was overexpressed in CD34+ cells in a subset of MDS patients but not by normal CD34+ hematopoietic stem and progenitor cells (HSPCs) (Fig. 1d). To determine whether Hh pathway activation marked the disease progression and leukemic transformation, we analyzed the expression of Hh targets using serial bone marrow samples. While the expression of GLI1 and PTCH1 was absent in CD34+ cells from healthy controls and low-risk MDS patients, the pathway activation coincided with the progression to AML in 4/6 (67%) patients (Fig. 1e).

Fig. 1
figure1

The Hedgehog signaling pathway is activated in human disease. Analysis of GLI1 expression using publicly available expression datasets in a AML based on risk category and b AML based on cytogenetics (TCGA). c Overall survival based on GLI1 expression in TCGA AML cohort (GLI1 high: GLI1 > mean expression; GLI1 low: GLI1 < mean expression), p value calculated using log-rank test. d The expression of GLI1 in CD34+ HSPC from a subset of MDS patients compared to healthy controls (GSE 58831). e GLI1 and PTCH1 expression in longitudinal MDS samples as the time of diagnosis and upon progression to AML. Dot plots represent individual values; mean and standard deviation are shown as whisker plots mean and standard deviation

Hh pathway activation results in accelerated leukemic transformation of NHD13 mouse MDS

Recurrent chromosomal abnormalities have been identified in MDS and AML, including the translocation of chromosome 2 and 11 leading to fusion of the NHD13 genes. Transgenic mice expressing the NHD13 fusion protein develop highly penetrant and reproducible myelodysplasia and progression to leukemia with the median survival of 14 months [25]. To determine the role of aberrant Hh signaling in MDS progression, we crossed transgenic NHD13 mice with mice expressing the constitutively active Smo mutant SmoM2 fused to yellow fluorescent protein (YFP) [25, 26]. Conditional expression of SmoM2 within the hematopoietic system was achieved with Mx1Cre expression and treatment with poly(I:C) (Fig. 2a). SmoM2-driven expression of Hh signaling was confirmed by the presence of YFP-positive hematopoietic cells and the expression of GLI1, which was observed in NHD13/SmoM2 and SmoM2 mice and remained undetectable in NHD13 and wild-type (WT) animals (Figure S2a, b).

Fig. 2
figure2

Constitutive Hh activation in NHD13 mice results in rapidly progressing acute leukemia. a Schematic of transgenic mouse model with constitutive activation of mutant Smoothened (SmoM2) in NHD13 mice. b Overall survival of NHD13/SmoM2 mice compared to NHD13, SmoM2, and WT controls. c WBC and spleen size of NHD13/SmoM2, NHD13, SmoM2, and WT controls. Dot plots represent individual values; mean and standard deviation are shown as whisker plots

We and others have previously shown that the expression of SmoM2 has no effect on hematopoiesis and HSPCs [18, 27, 28]. In contrast, activation of Hh signaling in NHD13/SmoM2 mice resulted in significantly shorter median survival compared to NHD13 mice (3 vs. 13 months, p < 0.0001) (Fig. 2b). The white blood cell count and the mean spleen weight were significantly increased in NHD13/SmoM2 compared to NHD13, SmoM2, or WT mice (p < 0.05 and <0.0001, respectively) (Fig. 2c). Peripheral blood at 6–8 weeks post poly(I:C) injection showed significant myeloid skewing in NHD13 mice, which was even more pronounced in NHD13/SmoM2 animals (Figure S2c). The analysis of complete peripheral blood count showed significant anemia and leukocytosis (Figure S2d). These findings were consistent with the observed increased penetrance of combined NHD13/SmoM2 transgenes toward myeloid leukemia compared to NHD13 alone (58% vs. 42%). Immunophenotyping of peripheral blood, bone marrow, and spleen showed the emergence of an immature myeloid population (Mac1+Gr1dim) and significant expansion of leukemic blasts in NHD13/SmoM2 animals (Fig. 3a, b, S3c). Histologically, peripheral blood, bone marrow, and spleen were infiltrated by morphologically immature cells (Fig. 3a). Necropsy of NHD13/SmoM2 animals revealed multiple sites of extramedullary involvement by aggressive leukemia (Figure S3a, b).

Fig. 3
figure3

NHD13/SmoM2 mice showed significant expansion of immature myeloid blasts in blood, bone marrow, and spleen. a Wright-Giemsa stain of peripheral blood, and hematoxylin and eosin staining of the bone marrow and spleen sections showed expansion of immature hematopoietic progenitors. b Flow cytometry of peripheral blood, bone marrow, and spleen showed significant increase in the myeloid progenitor cell population (Mac1+/Gr1dim) in NHD13/SmoM2 mice. The flow cytometry plots depict representative animals. Dot plots demonstrate individual animals; mean and standard deviation are shown as whisker plots

Hh signaling results in expansion of immature myeloid cells and gain of aberrant self-renewal potential in GMPs

Bone marrow cellularity was significantly increased in NHD13/SmoM2 animals compared to NHD13 controls (Fig. 4a). To better characterize the HSPC compartment we utilized multiparameter flow cytometry. Since multiple groups have demonstrated no differences in HSPC frequencies between WT and SmoM2 animals [18], we studied NHD13/SmoM2 and NHD13 animals and found similar frequencies of LinSca1+cKit+, LinCD34+FcγR multipotent progenitors, and LinCD34FcγR+ common myeloid progenitors (Fig. 4b). However, LinCD34+FcγR+ GMPs were significantly expanded in NHD13/SmoM2 mice (p < 0.05) (Fig. 4b, S4a). Additionally, whole bone marrow cells from NHD13/SmoM2 showed significantly higher in vitro clonogenic potential; colonies showed morphologic characteristics of Colony Forming Unit-Granulocyte/Macrophage (CFU-GM) consistent with myeloid differentiation (Fig. 4c). In order to define the long-term leukemia-initiating potential in vivo we transplanted total bone marrow from NHD13/SmoM2 mice to congenic recipients after sublethal irradiation (Figure S4b). The recipient mice developed rapidly progressing leukemia with leukocytosis, splenomegaly, expansion of Mac1+Gr1dim leukemic blasts, and median survival of 2 months (Figure S4c, d). Furthermore, the expansion of GMPs was maintained (Figure S4e). To determine whether Hh activation resulted in aberrant self-renewal of the GMP compartment, we serially transplanted GMPs from NHD13/SmoM2 and NHD13 mice (Fig. 4d). NHD13 GMPs showed only transient engraftment (n = 3), characteristic of non-self-renewing progenitors. In contrast, NHD13/SmoM2 GMPs robustly engrafted and significantly expanded over time, and all recipient animals (n = 3) developed aggressive leukemia within 2–3 months. Engraftment potential was also maintained during secondary transplantation, and all secondary recipients succumbed to leukemia (Fig. 4d). These findings suggest that the activation of Hh signaling in NHD13 animals results in acquisition of aberrant self-renewal in normally non-self-renewing progenitors leading to the development of lethal AML.

Fig. 4
figure4

Granulocyte macrophage progenitors (GMPs) are expanded in NHD13/SmoM2 mice and acquire self-renewal potential. a Bone marrow cellularity presented as number of nucleated cells per femur, vertical lines represent mean values. b Absolute GMP number per femur in NHD13/SmoM2 mice and NHD13 littermate controls. c Colony formation assay using total nucleated bone marrow cells from NHD13/SmoM2 (n = 4), NHD13 (n = 3), and WT animals (n = 3). Box plots represent mean and standard deviation. d Self-renewal potential of GMP was assessed in vivo. A total of 0.5 × 106 FACS-sorted GMPs from NHD13/SmoM2 and NHD13 controls were transplanted into congenic recipients (3 mice per group). Percent engraftment in peripheral blood over time after primary and secondary transplantation; mean and standard deviation are shown

Hh signaling activates self-renewal program in differentiated progenitors in MDS

To delineate the mechanisms leading to aberrant self-renewal in GMPs, we compared the transcriptional profile of GMPs isolated from NHD13/SmoM2 and NHD13 mice. Gene expression clustering showed a distinct transcriptional pattern between NHD13/SmoM2 and NHD13 cells (Figure S5a). We used Gene Set Enrichment Analysis (GSEA) to determine the key biological pathways involved in oncogenic transformation. As expected, we confirmed activation of the transcription signature of Hh signaling (Figure S5b). Additionally, the transcriptional programs characteristic of other developmental pathways such as Wnt and TGF-β were enriched in NHD13/SmoM2 GMPs (Fig. 5a). Both pathways are well known to drive cancer stem cells self-renewal [14, 17]. Interestingly, also a transcription signature of EWS/FLI1-driven model of myeloid leukemia was significantly enriched for in NHD13/SmoM2 GMPs (Fig. 5b). Analogous to our model, EWS/FLI1 expression in murine HSPC resulted in expansion of immature myeloid progenitors with aberrantly activated self-renewal potential [29]. Interestingly, GLI1 has been reported as a direct transcriptional target of EWS/FLI1 [30,31,32]. Our data suggest that aberrant Hh signaling in NHD13 GMPs leads to activation of a self-renewal program via transcriptional activation of GLI1. Moreover, the transcriptional program activated by GLI1 resembles the transcriptional characteristics of other developmental pathways suggesting its key role as an oncogenic TF.

Fig. 5
figure5

Self-renewal gene signature is enhanced in NHD13/SmoM2 GMPs. a Gene set enrichment analysis (GSEA) of the GMPs revealed the enrichment in expression signature consistent with activation of Wnt and TGF-β signaling—developmental pathways frequently dysregulated in cancer stem cells. b GSEA demonstrated enrichment in genes regulated by EWS/FLI1 oncogene. Corresponding heat-maps are shown

GLI1 can be activated in a SMO-independent manner and GLI1 inhibition diminishes the proliferation and clonogenic potential of human AML and MDS cell lines

To determine the role of GLI1 in human MDS and AML, we examined the expression of pathway components in several AML and MDS cell lines. We observed that GLI1 activation may occur in both: SMO-dependent and SMO-independent fashion. In TF1 leukemia cell line for instance, GLI1 expression was coupled with the Hh pathway signaling components SMO and PTCH1 (Figure S6a) suggesting canonical Hh signal transduction. In contrast, GLI1 expression was observed in the absence of SMO in the secondary AML cell line arising from MDS (MDS-L) suggesting SMO-independent GLI1 activation (Figure S6a). These findings suggest the key role of GLI1 that may be activated in a SMO-independent manner. To further delineate the role of SMO and GLI1 in oncogenic process we focused on TFI1 (SMO and GLI1 expresser) and MDS-L (GLI1 expresser). To investigate the role of SMO we carried out short hairpin (shRNA) gene silencing and protein inhibition using PF04449913 in TF1 (Figure S6b). SMO knockdown and protein inhibition negatively impacted TF1 cell growth (Figure S6c) but had no effect on clonogenic potential (Figure S6d). However, both GLI1 knockdown and treatment with GANT61 resulted in both diminished cell growth and clonogenic potential (Figure S6c, d). To examine the role of SMO-independent GLI1 activation we carried out GLI1 loss-of-function experiment in MDS-L secondary leukemia cell lines. GLI1 knockdown and inhibition with GANT61 resulted in decreased cell proliferation (Fig. 6a) and colony formation (Fig. 6b). As expected, the SMO inhibition with PF04449931 had no effect on cell proliferation (Fig. 6a) or colony formation (Fig. 6b). We next sought to elucidate the mechanism of impaired cell growth and clonogenic potential. The treatment with GANT61 but not with PF04449931 induced apoptosis in MDS-L cells. While increased apoptosis may explain impaired cell growth, it may not affect clonogenic potential. Differentiation, however, is nearly uniformly associated with decreased self-renewal. The treatment of MDS-L blasts with GANT61 resulted in acquisition of myeloid differentiation marker CD11b as well as morphological changes indicative of increased differentiation. As expected, PF04449931 showed no differentiation potential (Fig. 6c–e). We further sought to determine the relationship between GLI1 expression level and response to GLI1 and SMO inhibition using primary human secondary AML and healthy, age-matched CD34+ cells. We identified two patients: AML1 with complex cytogenetics and high GLI1, and AML2 with normal cytogenetics and low GLI1 mRNA level (Figure S6e). SMO inhibition with PF04449931 had no impact on colony formation of either AML1 or AML2 compared to normal CD34+ cells. However, GLI1 inhibition significantly decreased clonogenic potential of AML1 (GLI1 high), but not AML2 (GLI1 low) human leukemia (Fig. 6f). Our data imply that GLI1 can be transcriptionally activated in a SMO-independent fashion and inhibition of the pathway at the level of GLI1, rather than upstream SMO may result in a superior anti-leukemic effect.

Fig. 6
figure6

GLI1 inhibition at the mRNA and protein level impedes MDS and leukemic cell growth and clonogenic potential in vitro. a MDS-L cell proliferation with GLI1 knockdown and inhibition with GANT61 as well as SMO inhibition with PF04449913 is shown along with shLuc- and DMSO-treated controls, respectively. Mean and standard deviation from three replicates are shown. b MDS-L colony formation in GLI1 knockdown cells relative to shLuc control as well as PF04449931 and GANT61-treated cells relatively to DMSO-treated controls. Box plot represents mean and standard deviation from three replicates. c Flow cytometric apoptosis assay utilizing Annexin V antibody and 7AAD. Representative flow cytometry plots are shown. Bar graphs represent percentage of Annexin V-positive cells, mean and standard deviation calculated from experimental replicates (n = 3). d Flow cytometric analysis of CD11b acquisition by MDS-L blasts in response to SMO and GLI1 inhibition as well as DMSO-treated controls. e Morphology of MDS-L cells after cytospin and modified Wright-Giemsa. Black arrowheads represent immature cells (blasts) with scant cytoplasm, open chromatin, and prominent nucleoli. Blue arrowheads represent differentiating myeloid cells with increased chromatin condensation, prominent cytoplams, and the absence of nucleoli. f Clonogenic potential of bone marrow cells obtained from sAML patients: AML1 (GLI1 high) and AML2 (GLI1 low) treated with PF004449931 and GANT61. Presented values are relative to CD34+ cells obtained from age-matched healthy donors. Mean and standard deviation calculated from experimental replicates (n = 3)

Discussion

We report that Hh pathway activation marks disease progression in a subset of patients with MDS. GLI1, a pure transcriptional activator, is not present in healthy HSPC but becomes aberrantly activated in a subset of patients with MDS upon leukemic transformation. Using a murine model, we demonstrate that GLI1 activation via canonical Hh signaling accelerates the leukemic transformation of NHD13 mice through pathologic activation of a self-renewal program in differentiated progenitors. Moreover, in human disease, GLI1 can be activated in a SMO-independent fashion and the inhibition of GLI1 at the mRNA or protein level reduces proliferation and clonogenic potential of human AML and MDS cells. Therefore, Hh inhibition appears to be an attractive therapeutic approach in patients with MDS and AML.

We have previously demonstrated the cooperative role of Hh signaling with FLT3-ITD in leukemic transformation of myeloproliferative neoplasm and the advantage of combination therapy with Hh and FLT3 inhibitors [18]. While Hh signaling has already emerged as an important pathway in certain myeloid and lymphoid malignancies, its role in MDS has not been extensively studied. Several groups have shown the role of Hh ligands and Hh interacting protein in the maintenance of MDS clones [33, 34]. Hh activation and GLI1 expression was recently found to be associated with high-risk disease and GLI1 inhibitors enhanced the effects of HMA agents [35]. Based on these findings, SMO inhibitors were tested as a single agent in phase 1 and in combination with low-dose chemotherapy in randomized phase 2 clinical trials and showed promising activity with improved complete remission rate and overall survival [23, 24, 36].

In our current studies, we used a constitutively active Smo mutant to activate GLI1 via canonical Hh signaling. Even though we found the evidence of transcriptional activation of GLI1 in cell lines and primary MDS samples, the genetic mutations and abnormal expression of upstream pathway components like SMO and PTCH are infrequent in human MDS and AML (The Cancer Genome Atlas (TCGA) http://cancergenome.nih.gov). In addition to canonical Hh signaling, the activity of GLI TFs can be modulated by other pathways frequently involved in human tumorigenesis like Wnt, Notch, TGF-β, MAPK, and PI3K/AKT [14,15,16,17, 37, 38]. Our data suggest that GLI1 expression is not always coupled with the presence of upstream pathway components, indicating that its activation may be modulated in a SMO-independent manner (Fig. 7). Similar findings were recently published in AML [39]. Thus, GLI1 TFs seem to be a convergence point of multiple cancer-associated pathways and may confer an attractive target with broader therapeutic effects than currently used SMO inhibitors.

Fig. 7
figure7

Schematic of GLI activation in human leukemia. a Posttranslational modifications of GLI to activator forms mediated by SMO-dependent Hh signaling and SMO-independent mechanisms. Green arrows depict activation and red lines depict inhibition of GLI activation. Stars mark genes with loss-of-function mutations and/or haploinsufficiency described in human MDS or AML. b Direct translational activation of GLI1

We previously found that Hh pathway drives aberrant self-renewal within putative cancer stem cells in multiple myeloma, pancreatic carcinoma, and glioblastoma [40,41,42]. The precise role of Hh signaling in myeloid disorders is unclear as mouse models have revealed that it is required for the maintenance of chronic myeloid leukemia stem cells but not for the development of mixed-lineage leukemia (MLL)-driven AML [28, 43]. Our data suggest that pathologic activation of Hh signaling accelerates progression of MDS via aberrant activation of self-renewal in a normally non-self-renewing compartment. Acquisition of abnormal self-renewal in GMP compartment via activation of Wnt signaling was also observed in HoxA9-Meis1 and MLL-AF9 mouse models of AML [44]. Similar activation of self-renewal in myeloid progenitors was found during leukemic transformation of chronic myeloid leukemia [45]. Consistent with the aforementioned findings, the gene expression analysis of GMPs from NHD13/SmoM2 and NHD13 controls revealed relative enrichment in transcriptional targets of not only Hh but also other developmental pathways like Wnt and TGF-β. Interestingly, transcriptome of NHD13/SmoM2 GMPs resembled the profile of EWS/FLI1-driven leukemia. Notably, EWS/FLI1 was shown to exert its effect via abnormal activation of self-renewal and expansion of hematopoietic progenitors [29]. We have previously shown that GLI1 is a direct target of EWS/FLI1 oncoprotein suggesting GLI1 as a key mediator of oncogenic transformation [30].

Initial reports revealed that Hh signaling is dispensable in normal definitive hematopoiesis [27, 28]. Subsequent data showed only minor impact of Hh perturbations on hematopoietic stem cell frequencies and function [46]. These findings indicate that Hh inhibition may selectively target malignant cells while sparing healthy counterparts. This is further supported by the lack of hematologic toxicities with the use of SMO inhibitors in clinical trials [47]. Our data using MDS and AML cell lines showed that inhibition of GLI1 either with shRNA or GANT61 reduced cell proliferation and clonogenic potential more effectively than SMO inhibition. The lack of SMO expression in MDS-L cells suggests that GLI1 activation may also occur in a SMO-independent fashion. Consistently with our data, GLI1 knockdown was shown to inhibit cell proliferation and induce cell cycle arrest and apoptosis in MDS bone marrow cells [48]. The use of GANT61 resulted in growth arrest, apoptosis, and cell differentiation in AML cells [49, 50]. In a recent study, T-cell acute lymphoblastic leukemia cells with high GLI1 expression were sensitive to GANT61 in ex vivo cultures and in vivo xenograft models [19]. In summary, our data suggest that both SMO-dependent and -independent activation of GLI1 is frequent in MDS/sAML and therapeutic strategies targeting Gli TFs may be more effective than currently used SMO inhibitors.

Materials and methods

Clinical specimens, cell lines, and drug treatment

The study was approved by the Institutional Review Board at the Johns Hopkins School of Medicine. Bone marrow specimens were obtained from patients with MDS at the time of diagnosis and upon progression to AML. CD34+ cells were selected using MicroBeads (Miltenyi Biotec, SanDiego, CA) and the expression of effectors of Hh signaling was determined by quantitative PCR. Human whole bone marrow with >80% AML blasts were cultured in stem cell media H4435 (Stem Cell Technologies) supplemented with FLT3-ligand, stem cell factor, and interleukin (IL)-6. Human cell lines TF1 (American Type Culture Collection) and MDS-L (kindly provided by Dr. Daniel Starczynowski) were cultured in RPMI medium supplemented with 10% fetal bovine serum, 1% l-glutamine, 1% penicillin/streptomycin, and granulocyte macrophage colony-stimulating factor (2 ng/ml) or recombinant IL-3 (10 ng/ml), respectively. Drug treatments were done with PF04449913 (Sigma-Aldrich), GANT61 (Stem Cell Technologies), or dimethyl sulfoxide vehicle control for 72–96 h. Cell proliferation was assayed by Trypan blue dye exclusion or MTT assay (Abcam). Apoptosis was determined by flow cytometry after Annexin V-PE (BD PharmingenTM) staining. Cell differentiation was determined by increase in CD11b expression and histologically after cytospin and modified Wright-Giemsa staining. Colony formation assay was performed by growing cells (100–500 cells/ml) in methylcellulose for 11 days, and counting colonies using an inverted Nikon microscope.


Mice

All animal procedures were approved by the Institutional Animal Care and Use Committee. SmoM2 and Mx1Cre C57Bl6 mice were obtained from Jackson Laboratories and crossed with NHD13 C57Bl6 mice. Genotyping was determined by PCR. NHD13 mice and mice carrying the Mx1Cre allele alone (WT) were used as littermate controls. All mice were treated with five doses of poly(I:C) (300 μg, Sigma) intraperitoneally every other day. Successful transgene excision in NHD13/SmoM2 and SmoM2 animals was confirmed by PCR and YFP expression by flow cytometry (FACSCalibur, BD Biosciences) of peripheral blood cells (Figure S1a). Development of AML was assessed by the presence of Mac1+Gr1dim cells in the peripheral blood and/or bone marrow. Complete blood counts were quantified using a Procyte Dx Hematology analyzer (Idexx). Formalin-fixed tissues were stained with hematoxylin and eosin, and blood smears with Wright-Giemsa stain. At least three mice per experimental or control group were used for each experiment as a sample size estimate limited by the number of mice per litter for littermate controls. Animals who were found dead for >24 h were excluded from obtaining tissue and therefore not analyzed. The criteria were pre-established. No randomization or blinding was used for these studies on observations based on individual mouse genotype.


Antibodies and fluorescence-activated cell sorting

Monoclonal antibodies against Mac1, Gr1, and B220 (eBioscience) were used for peripheral blood analysis using FACSCalibur flow cytometers (BD Biosciences). Biotinylated antibodies against Gr1, Ter119, B220, and CD3 (eBioscience) were used for lineage staining of whole bone marrow cells. Bone marrow cells were also stained with antibodies against cKit, Sca1, CD16/32, CD34, FLT3, and IL7R (eBioscience), and analyzed on a LSRII cytometer (BD Biosciences) (Table S1). Cells were sorted using a MoFlo Instrument (Beckman Coulter). Flow cytometry data were analyzed with FlowJo v.8.7 software, with gating strategy shown in Supplemental Fig. 4


Quantitative real-time PCR analysis

Total RNA was extracted using RNeasy Plus Mini kit (Qiagen) and reverse transcribed with Superscript III reverse transcriptase (Invitrogen) according to the manufacturers’ protocol. Quantitative real-time PCR (qRT-PCR) was carried out with Taqman and/or SYBR Green assays (Applied Biosystems) and analyzed using StepOne Plus instrument (Applied Biosystems). Primer and probe sequences are listed in Table S2.


Microarray and GSEA analysis

A published dataset available from TCGA and the NCBI Gene Expression Omnibus database (GSE 58831) [51] were analyzed for expression levels of the Hh signaling pathway and correlated with risk stratification and overall survival. The results published here are in whole or part based upon data generated by the TCGA Research Network: http://cancergenome.nih.gov/. RNA was extracted as described above from GMPs obtained from bone marrow of age-matched NHD13 and NHD13/SmoM2 mice, and gene expression profiling was carried out using Mouse Gene Expression Microarray Kit v2 (Agilent). Microarray data were analyzed using R and GSEA software (see supplementary methods).


Short hairpin RNA

TF1 and MDS-L cell lines were transfected with pLKO Tet-On lentiviral shRNA vectors targeting GLI1, SMO, and luciferase (Table S3). Successful knockdown of genes was determined by qRT-PCR 72 h after doxycycline treatment.


Statistics

The data were normally distributed. p Values were determined using an unpaired two-tailed Student’s t test. p Values < 0.05 were considered statistically significant. Survival was assessed using Kaplan-Meier analysis. GraphPad Prism v.6 was used for statistical analysis. Estimate of variance was determined for each group and were similar between groups. The detailed description of gene expression data analysis is described in Supplementary Methods.

References

  1. 1.

    Tefferi A, Vardiman JW. Myelodysplastic syndromes. N Engl J Med. 2009;361:1872–85.

  2. 2.

    Garcia-Manero G. Myelodysplastic syndromes: 2015 Update on diagnosis, risk-stratification and management. Am J Hematol. 2015;90:831–41.

  3. 3.

    Greenberg P, Cox C, LeBeau MM, Fenaux P, Morel P, Sanz G, et al. International scoring system for evaluating prognosis in myelodysplastic syndromes. Blood. 1997;89:2079–88.

  4. 4.

    Malcovati L, Germing U, Kuendgen A, Della Porta MG, Pascutto C, Invernizzi R, et al. Time-dependent prognostic scoring system for predicting survival and leukemic evolution in myelodysplastic syndromes. J Clin Oncol. 2007;25:3503–10.

  5. 5.

    Meggendorfer M, de Albuquerque A, Nadarajah N, Alpermann T, Kern W, Steuer K, et al. Karyotype evolution and acquisition of FLT3 or RAS pathway alterations drive progression of myelodysplastic syndrome to acute myeloid leukemia. Haematologica. 2015;100:e487–90.

  6. 6.

    Makishima H, Yoshizato T, Yoshida K, Sekeres MA, Radivoyevitch T, Suzuki H, et al. Dynamics of clonal evolution in myelodysplastic syndromes. Nat Genet. 2017;49:204–12.

  7. 7.

    Jiang Y, Dunbar A, Gondek LP, Mohan S, Rataul M, O’Keefe C, et al. Aberrant DNA methylation is a dominant mechanism in MDS progression to AML. Blood. 2009;113:1315–25.

  8. 8.

    Fenaux P, Giagounidis A, Selleslag D, Beyne-Rauzy O, Mufti G, Mittelman M, et al. A randomized phase 3 study of lenalidomide versus placebo in RBC transfusion-dependent patients with low-/intermediate-1-risk myelodysplastic syndromes with del5q. Blood. 2011;118:3765–76.

  9. 9.

    Krug U, Rollig C, Koschmieder A, Heinecke A, Sauerland MC, Schaich M, et al. Complete remission and early death after intensive chemotherapy in patients aged 60 years or older with acute myeloid leukaemia: a web-based application for prediction of outcomes. Lancet. 2010;376:2000–8.

  10. 10.

    Walter RB, Othus M, Borthakur G, Ravandi F, Cortes JE, Pierce SA, et al. Prediction of early death after induction therapy for newly diagnosed acute myeloid leukemia with pretreatment risk scores: a novel paradigm for treatment assignment. J Clin Oncol. 2011;29:4417–23.

  11. 11.

    McMillan R, Matsui W. Molecular pathways: the Hedgehog signaling pathway in cancer. Clin Cancer Res. 2012;18:4883–8.

  12. 12.

    Denef N, Neubuser D, Perez L, Cohen SM. Hedgehog induces opposite changes in turnover and subcellular localization of patched and smoothened. Cell. 2000;102:521–31.

  13. 13.

    Ruiz i, Altaba A. Catching a Gli-mpse of Hedgehog. Cell. 1997;90:193–6.

  14. 14.

    Borycki A, Brown AM, Emerson CP Jr. Shh and Wnt signaling pathways converge to control Gli gene activation in avian somites. Development. 2000;127:2075–87.

  15. 15.

    Ringuette R, Atkins M, Lagali PS, Bassett EA, Campbell C, Mazerolle C, et al. A Notch-Gli2 axis sustains Hedgehog responsiveness of neural progenitors and Muller glia. Dev Biol. 2016;411:85–100.

  16. 16.

    Liu Z, Li T, Reinhold MI, Naski MC. MEK1-RSK2 contributes to Hedgehog signaling by stabilizing GLI2 transcription factor and inhibiting ubiquitination. Oncogene. 2014;33:65–73.

  17. 17.

    Johnson RW, Nguyen MP, Padalecki SS, Grubbs BG, Merkel AR, Oyajobi BO, et al. TGF-beta promotion of Gli2-induced expression of parathyroid hormone-related protein, an important osteolytic factor in bone metastasis, is independent of canonical Hedgehog signaling. Cancer Res. 2011;71:822–31.

  18. 18.

    Lim Y, Gondek L, Li L, Wang Q, Ma H, Chang E, et al. Integration of Hedgehog and mutant FLT3 signaling in myeloid leukemia. Sci Transl Med. 2015;7:291ra296.

  19. 19.

    Dagklis A, Demeyer S, De Bie J, Radaelli E, Pauwels D, Degryse S, et al. Hedgehog pathway activation in T-cell acute lymphoblastic leukemia predicts response to SMO and GLI1 inhibitors. Blood. 2016;128:2642–54.

  20. 20.

    Hahn H, Wicking C, Zaphiropoulous PG, Gailani MR, Shanley S, Chidambaram A, et al. Mutations of the human homolog of Drosophila patched in the nevoid basal cell carcinoma syndrome. Cell. 1996;85:841–51.

  21. 21.

    Johnson RL, Rothman AL, Xie J, Goodrich LV, Bare JW, Bonifas JM, et al. Human homolog of patched, a candidate gene for the basal cell nevus syndrome. Science. 1996;272:1668–71.

  22. 22.

    Xavier-Ferrucio JM, Pericole FV, Lopes MR, Latuf-Filho P, Barcellos KS, Dias AI, et al. Abnormal Hedgehog pathway in myelodysplastic syndrome and its impact on patients’ outcome. Haematologica. 2015;100:e491–3.

  23. 23.

    Martinelli G, Oehler VG, Papayannidis C, Courtney R, Shaik MN, Zhang X, et al. Treatment with PF-04449913, an oral smoothened antagonist, in patients with myeloid malignancies: a phase 1 safety and pharmacokinetics study. Lancet Haematol. 2015;2:e339–46.

  24. 24.

    Lancet JE, Komrokji RS, Sweet KL, Duong VH, McGraw KL, Zhang L, et al. Phase 2 trial of smoothened (SMO) inhibitor PF-04449913 (PF-04) in refractory myelodysplastic syndromes (MDS). Blood. 2016;128:3174.

  25. 25.

    Lin YW, Slape C, Zhang Z, Aplan PD. NUP98-HOXD13 transgenic mice develop a highly penetrant, severe myelodysplastic syndrome that progresses to acute leukemia. Blood. 2005;106:287–95.

  26. 26.

    Mao J, Ligon KL, Rakhlin EY, Thayer SP, Bronson RT, Rowitch D, et al. A novel somatic mouse model to survey tumorigenic potential applied to the Hedgehog pathway. Cancer Res. 2006;66:10171–8.

  27. 27.

    Gao J, Graves S, Koch U, Liu S, Jankovic V, Buonamici S, et al. Hedgehog signaling is dispensable for adult hematopoietic stem cell function. Cell Stem Cell. 2009;4:548–58.

  28. 28.

    Hofmann I, Stover EH, Cullen DE, Mao J, Morgan KJ, Lee BH, et al. Hedgehog signaling is dispensable for adult murine hematopoietic stem cell function and hematopoiesis. Cell Stem Cell. 2009;4:559–67.

  29. 29.

    Torchia EC, Boyd K, Rehg JE, Qu C, Baker SJ. EWS/FLI-1 induces rapid onset of myeloid/erythroid leukemia in mice. Mol Cell Biol. 2007;27:7918–34.

  30. 30.

    Beauchamp E, Bulut G, Abaan O, Chen K, Merchant A, Matsui W, et al. GLI1 is a direct transcriptional target of EWS-FLI1 oncoprotein. J Biol Chem. 2009;284:9074–82.

  31. 31.

    Zwerner JP, Joo J, Warner KL, Christensen L, Hu-Lieskovan S, Triche TJ, et al. The EWS/FLI1 oncogenic transcription factor deregulates GLI1. Oncogene. 2008;27:3282–91.

  32. 32.

    Joo J, Christensen L, Warner K, States L, Kang HG, Vo K. et al. GLI1 is a central mediator of EWS/FLI1 signaling in Ewing tumors. PLoS ONE. 2009;4:e7608

  33. 33.

    Kobune M, Iyama S, Kikuchi S, Horiguchi H, Sato T, Murase K, et al. Stromal cells expressing hedgehog-interacting protein regulate the proliferation of myeloid neoplasms. Blood Cancer J. 2012;2:e87.

  34. 34.

    Zou J, Hong Y, Tong Y, Wei J, Qin Y, Shao S, et al. Sonic hedgehog produced by bone marrow-derived mesenchymal stromal cells supports cell survival in myelodysplastic syndrome. Stem Cells Int. 2015;2015:957502.

  35. 35.

    Kang HJ, Kim YI, Kim HC, Jae HJ, Hur S, Chung JW. Does establishing a safety margin reduce local recurrence in subsegmental transarterial chemoembolization for small nodular hepatocellular carcinomas? Korean J Radiol. 2015;16:1068–78.

  36. 36.

    Cortes JE, Heidel FH, Heuser M, Fiedler W, Smith BD, Robak T, et al. A phase 2 randomized study of low dose Ara-C with or without glasdegib (PF-04449913) in untreated patients with acute myeloid leukemia or high-risk myelodysplastic syndrome. Blood. 2016;128:99.

  37. 37.

    Seto M, Ohta M, Asaoka Y, Ikenoue T, Tada M, Miyabayashi K, et al. Regulation of the hedgehog signaling by the mitogen-activated protein kinase cascade in gastric cancer. Mol Carcinog. 2009;48:703–12.

  38. 38.

    Brechbiel J, Miller-Moslin K, Adjei AA. Crosstalk between hedgehog and other signaling pathways as a basis for combination therapies in cancer. Cancer Treat Rev. 2014;40:750–9.

  39. 39.

    Chaudhry P, Singh M, Triche TJ, Guzman M, Merchant AA. GLI3 repressor determines Hedgehog pathway activation and is required for response to SMO antagonist glasdegib in AML. Blood. 2017;129:3465–75.

  40. 40.

    Peacock CD, Wang Q, Gesell GS, Corcoran-Schwartz IM, Jones E, Kim J, et al. Hedgehog signaling maintains a tumor stem cell compartment in multiple myeloma. Proc Natl Acad Sci USA. 2007;104:4048–53.

  41. 41.

    Feldmann G, Dhara S, Fendrich V, Bedja D, Beaty R, Mullendore M, et al. Blockade of hedgehog signaling inhibits pancreatic cancer invasion and metastases: a new paradigm for combination therapy in solid cancers. Cancer Res. 2007;67:2187–96.

  42. 42.

    Bar EE, Chaudhry A, Lin A, Fan X, Schreck K, Matsui W, et al. Cyclopamine-mediated hedgehog pathway inhibition depletes stem-like cancer cells in glioblastoma. Stem Cells. 2007;25:2524–33.

  43. 43.

    Zhao C, Chen A, Jamieson CH, Fereshteh M, Abrahamsson A, Blum J, et al. Hedgehog signalling is essential for maintenance of cancer stem cells in myeloid leukaemia. Nature. 2009;458:776–9.

  44. 44.

    Wang Y, Krivtsov AV, Sinha AU, North TE, Goessling W, Feng Z, et al. The Wnt/beta-catenin pathway is required for the development of leukemia stem cells in AML. Science. 2010;327:1650–3.

  45. 45.

    Jamieson CH, Ailles LE, Dylla SJ, Muijtjens M, Jones C, Zehnder JL, et al. Granulocyte-macrophage progenitors as candidate leukemic stem cells in blast-crisis CML. N Engl J Med. 2004;351:657–67.

  46. 46.

    Merchant A, Joseph G, Wang Q, Brennan S, Matsui W. Gli1 regulates the proliferation and differentiation of HSCs and myeloid progenitors. Blood. 2010;115:2391–6.

  47. 47.

    Sekulic A, Migden MR, Oro AE, Dirix L, Lewis KD, Hainsworth JD, et al. Efficacy and safety of vismodegib in advanced basal-cell carcinoma. N Engl J Med. 2012;366:2171–9.

  48. 48.

    Zou J, Zhou Z, Wan L, Tong Y, Qin Y, Wang C. et al. Targeting the sonic Hedgehog-Gli1 pathway as a potential new therapeutic strategy for myelodysplastic syndromes. PLoS ONE. 2015;10:e0136843

  49. 49.

    Wellbrock J, Latuske E, Kohler J, Wagner K, Stamm H, Vettorazzi E, et al. Expression of Hedgehog pathway mediator GLI represents a negative prognostic marker in human acute myeloid leukemia and its inhibition exerts antileukemic effects. Clin Cancer Res. 2015;21:2388–98.

  50. 50.

    Long B, Wang LX, Zheng FM, Lai SP, Xu DR, Hu Y, et al. Targeting GLI1 suppresses cell growth and enhances chemosensitivity in CD34+ enriched acute myeloid leukemia progenitor cells. Cell Physiol Biochem. 2016;38:1288–1302.

  51. 51.

    Gerstung M, Pellagatti A, Malcovati L, Giagounidis A, Porta MG, Jadersten M, et al. Combining gene mutation with gene expression data improves outcome prediction in myelodysplastic syndromes. Nat Commun. 2015;6:5901.

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Acknowledgements

We would like to acknowledge Dr. David Huso, previously an Associate Professor in the Department of Molecular and Comparative Pathobiology at Johns Hopkins, for preparing the histology slides; and Dr. Hao Zhang, Research Associate in the Department of Molecular Microbiology and Immunology at Johns Hopkins, for helping to sort the murine bone marrow for cell subpopulations. This work was supported by grants from the National Institute of Health (K08 HL136894) (LPG) and Edward P. Evans Foundation (LPG). Flow cytometry and microarray analysis was performed with the support of the Sidney Kimmel Comprehensive Cancer Center Core Facilities (P30 CA006973).

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The authors declare that they have no conflict of interest.

Correspondence to William Matsui or Lukasz P. Gondek.

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