Background
Acute myeloid leukemia (AML) remains a disease with a poor clinical prognosis. Although most of patients achieve remission by induction chemotherapy, nearly all of them relapse and need consolidation chemotherapy or hematopoietic stem cell transplantation (HSCT). The majority of patients will ultimately die of their disease, and the 5-year survival rate is only 40–50% [
1]. The FMS-like tyrosine kinase-3 (FLT3), a tyrosine kinase receptor, was one of the most frequently mutated genes in AML and accounted for approximately 30% of AML cases [
2]. Internal tandem duplication (ITD) mutations of the FLT3 gene occurred in nearly 24% of adult AML patients [
3]; the other common mutant type of FLT3 which occurred in the activation loop of the tyrosine kinase domain (TKD), mainly at aspartic acid 835, was found in approximately 7% of AML patients [
4]. FLT3-ITD mutations, as well as TKD mutations, led to constitutive activation of FLT3 kinase and triggered several downstream signaling pathways, including the Raf/MEK/ERK pathway, JAK/STAT5 pathway, and PI3K/Akt pathway, which promoted the progression of AML [
5]. In general, AML patients with FLT3 mutation represented poor outcomes [
6]. Although the development of FLT3 inhibitors might improve the clinical outcome, the only effective treatment for FLT3 mutant AML patients remained allogeneic HSCT currently [
7]. Therefore, it is necessary to investigate a new treatment strategy for AML patients with FLT3 mutation.
Chimeric antigen receptor (CAR) T-cell therapy is breaking an innovative new age in treating refractory and recurrent lymphocytic leukemia patients. In particular, CD19-targeted CAR-T cell therapy has achieved dramatic clinical success in treating acute lymphoblastic leukemia (ALL) patients [
8]. Up to 90% patients achieved complete remission treating with CD19 CAR-T cells [
9]. One major challenge in achieving the amazing clinical success of CAR-T cells in ALL to other types of cancer, including AML, is choosing a proper tumor-associated antigen (TAA) as target. Up to now, several TAAs have been reported as AML antigens against by CAR-T cells such as CD33 and CD123 [
10], but previous CAR-T cell therapy trials in AML did not result in long-term responses and exhibited toxicity toward normal hematopoietic progenitor stem cells (HPSCs). Recent study has reported CAR-T cells targeting FLT3 using the single-chain variable fragment (scFv) as recognizing domain of CAR [
11], but FLT3 scFv-based CAR-T cells failed to identify wild-type FLT3 from mutated FLT3.
In this study, we tried the ligand-based CAR-T cells to target FLT3. The ligands of FLT3, FLT3L as the recognizing domain and 4-1BB and CD3ζ as the intracellular signal domain, were used to generate a novel FLT3L CAR. T cells were modified to express the FLT3L CAR through a lentivirus system. Then, the functions of CAR-T cells were examined. It showed that FLT3L CAR-T cells were able to robustly kill FLT3+ leukemia cells in vitro and showed more potent cytotoxicity toward FLT3-ITD cells than FLT3 wild-type (WT) cells. The downstream signaling pathway of FLT3-WT cells was activated by FLT3L CAR-T, rather than FLT3-ITD cells. The in vivo treatment revealed that FLT3L CAR-T cells could prolong the survival of xenograft AML mice. Moreover, FLT3L CAR-T cells showed a limited toxicity against normal CD34+ umbilical cord blood stem cells in vitro. To our knowledge, there was no previous report that ever described such an approach of using ligand-based CAR-transduced effector cells to target the FLT3 molecule in AML treatment.
Methods
Cell culture
293T cells were maintained in Dulbecco’s modified Eagle’s medium supplemented with 10% FBS and glutamine. REH, THP-1, MOLM13, and U937 cells were grown in RPMI-1640 with 10% FBS. MV4-11 cells were maintained in Iscove’s modified Dulbecco’s medium supplemented with 15% FBS.
Identification of FLT3-ITD mutations
The multiple mutation domains of FLT3 gene in exons 14 and 15 were amplified from genomic DNA of cells using the following primers: forward 5′-GCAATTTAGGTAT GAAAGCCAGC-3′ and reverse 5′-CTTTCAGCATTTTGACGGCAACC-3′. A total volume of 50 μl containing 900 ng of genomic DNA was used under the following conditions: denatured at 95 °C for 5 min; annealed at 95 °C for 30 s, 60°C for 30 s, and 72°C for 30 s; and extended at 72 °C for 10 min. The products of PCR were electrophoresed in 3% agarose gels, stained with ethidium bromide, and observed under UV light.
Construction of FLT3L CAR lentiviral vectors
The FLT3 binding domain of FLT3L [
12] (FLT3L-BD) was cloned from the cDNA of a patient’s peripheral blood mononuclear cells (PBMC) by PCR via the following primers: forward 5′-CGCGGATCCACCCAGGACTGCTCCTTCCA-3′ and reverse 5’-CCGGAATTCCTGACACTGCAGCTCCAGGC-3′. The FLT3L-BD was subsequently cloned into pCDH-4-1BB-CD3ζ plasmid which was constructed before [
13]. The empty plasmid pCDH was used as control vector.
Lentivirus production
Recombinant lentivirus was packaged as we previously described [
13].
T cell isolation and infection
The detailed protocol of CD3
+ T cell isolation has been described previously [
13]. Briefly, T cells maintained in X-VIVO15 (LONZA, USA) with 5% FBS, Dynabeads® Human T-Activator CD3/CD28 (Stem Cell, USA), and 50 IU/ml rhIL-2 (R&D, USA) were inoculated in 24-well plates with a cell density of 1 × 10
6/ml. After 24 h, cells were transduced with FLT3L-CAR lentivirus. Cells transduced with empty plasmid pCDH lentivirus as control (VEC-T). The transduced cells were centrifuged and incubated for another 24 h. The culture medium was changed every other day, and cells were kept in flasks at a density of 3–5 × 10
5/ml with 50 IU/ml rhIL-2.
CAR expression and CAR-T cell phenotype analysis
Four days after infection, T cells were harvested and washed once with PBS, stained with rabbit anti-FLT3L antibody (Abcam, USA) for 1 h at 4 °C, and washed twice. Then PE donkey anti-rabbit IgG antibody (Biolegend, USA) was added, incubated at 4 °C for 30 min, and analyzed by flow cytometry using CantoII flow cytometer (BD Biosciences, San Jose, CA, USA) [
14]. For T cell phenotype analysis, T cells were harvested 7 days after infection and washed once with PBS, stained with anti-CD4-PE/Cy7 (Biolegend, USA), anti-CD8-PerCP-Cy5.5 (Biolegend, USA), anti-CCR7-PE (Biolegend, USA), and anti-CD45RA-Pacific Blue (Biolegend USA) 30 min at 4 °C, then washed and resuspended in PBS for flow cytometry analysis [
15].
CAR-T specific killing assay
CART-T specific killing assay for cell lines
FLT3L CAR-T (or VEC-T) cells and target cells were co-cultured in a 24-well plate with an E:T ratio of 1:8, 1:4, 1:2, and 1:1 in 1 ml medium (X-VIVO15 with 5% FBS) for 48 h. Cells were harvested and washed once, stained with anti-CD3-APC/Cy7 (Biolegend, USA) and anti-CD19-APC (REH cells) or anti-CD33-APC (THP-1, MOLM13, MV4-11 and U937 cells) for 30 min at 4 °C, then washed and resuspended in PBS for flow cytometry analysis. The percentage of CD19+ cells (REH) or CD33+ cells (THP-1, MOLM13, MV4-11 and U937) represented the residual level of target cells.
CART-T specific killing assay for primary AML cells
Bone marrow mononuclear cells (BMMCs) containing 44~ 98% AML blasts were isolated from bone marrow aspirates of AML patients through Ficoll-Paque density centrifugation and frozen in liquid nitrogen until use. All the samples obtained from the patients enrolled in the Institute of Hematology and Blood Diseases Hospital were collected under informed consent.
FLT3L CAR-T (or VEC-T) cells and primary AML cells were co-cultured in a 24-well plate with an E:T ratio of 1:4 in 1 ml medium (X-VIVO15 with 5% FBS) for 48 h. The followed staining steps were performed as mentioned above. AML cells were detected using anti-CD33-APC antibody. The percentage of CD33+ cells represented the residual level of target cells.
Degranulation assay
FLT3L CAR-T (or VEC-T) cells and target cells were co-cultured in a 96-well plate with an E:T ratio of 1:1 in triplicate in 200 μl medium with anti-CD107a-PE antibody and monensin (Sigma, USA). After 4 h, cells were labeled with anti-CD3-APC/Cy7 antibody and analyzed by flow cytometry.
Cytokine release assay
FLT3L CAR-T (or VEC-T) cells and target cells were co-cultured in a 24-well plate with an E:T ratio of 1:1 in triplicate in 1 ml medium for 24 h. Supernatants were harvested and assayed for the production of IFN-γ, TNF-α, and IL-2 by ELISA (R&D, USA), and the absorbance at 450 nm was measured using Synergy H4 Hybrid Microplate Reader (Biotek, Winooski, VT, USA).
CD34+ cells from cord blood were sorted after labeling with CD34 magnetic beads (Miltenyi Biotec, Germany) according to manufacturer’s instructions. Viability and purity of the sorted CD34+ cells were determined by flow cytometry. CD34+ cells were co-cultured with CAR-T or VEC-T cells for 24 h, and then, 500 CD34+ cells from each group were seeded in a methylcellulose medium (H4434, Stem Cell, Canada) and incubated at 37 °C, 5% CO2. After being cultured for 14 days, colonies (determined as 100 cell/colony) were scored and recorded by Nikon Eclipse Ti-U fluorescent microscopy under a × 10 objective (Nikon, Japan).
Intracellular phosphorylated protein staining assay
FLT3L CAR-T (or VEC-T) cells and target cells were co-cultured in a 24-well plate with an E:T ratio of 1:8 in triplicate in 1 ml medium for 4 h. Cells were fixed by adding an equal volume of IC Fixation Buffer (eBioscience, USA) and vortexed to mix. Cells were incubated for 1 h at room temperature (RT), protected from light, and then, cells were washed and fixed by using 1 ml ice-cold methanol. Cells were vortexed to mix and incubated for 30 min at 4 °C. Cells were washed twice in PBS then resuspended in 300 μl PBS within 1 μl intracellular phospho-epitope antibody (anti-p-STAT5-PE, anti-p-ERK-PE, or anti-p-AKT-PE, eBioscience, USA) and 1 μl anti-CD33-APC for 30 min at RT. Washed cells were resuspended in PBS and analyzed by flow cytometry.
In vivo NOD/SCID murine studies
Female NOD/SCID mice about 6 to 8 weeks old were obtained from Institute of Laboratory Animal Sciences (CAMS&PUMC, China). After sublethal irradiation, 14 mice were inoculated with 5 × 106 MV4-11 cells intravenously. Seven days after inoculation, mice were randomized into two treatment groups. Group CAR-T and group VEC-T were respectively injected intravenously with 1 × 107 CAR-T cells or VEC-T cells at day 7 and day 14. Body weight and the overall survival of mice were recorded. Dead mice were dissected for pathological and flow cytometry analysis to confirm the diagnosis of leukemia. All animal experiments were approved by the Institutional Animal Care and Use Committee of Peking Union Medical College.
Statistical analysis
Values were expressed as mean ± SD. Significance were determined by Student’s t test using GraphPad Prism (version 5.0). The survival of mice was analyzed by Kaplan-Meier methods and a log-rank test. p values < 0.05 were considered statistically significant. *p < 0.05, **p < 0.01, and ***p < 0.001 in comparison.
Discussion
AML patients with favorable prognostic factors responded well to conventional chemotherapy which combined with cytarabine and anthracycline compounds. However, patients with adverse prognostic factors inevitably relapse and have poor prognosis after chemotherapy. To achieve better or even optimal treatment response and reduce treatment-related mortality, strategies such as immunotherapy have been applied to the treatment of hematologic malignancies [
23].
Over the past decade, the novel immunotherapy strategy CAR-T cells have revolutionized leukemia treatment, especially CD19 CAR-T. Chimeric antigen receptor (CAR) is an artificial structure including antigen-binding domain which could recognize TAA, transmembrane region, and signal transduction region which could activate T cell to kill tumor cells. A large amount of studies have shown that CD19 CAR-T had striking clinical responses in relapsed ALL and CLL [
24]. Meanwhile, researchers are trying to treat AML patients with CAR-T therapy and several AML CAR-T cell therapies targeting relatively specific AML-associated surface markers are under clinical investigation [
24,
25]. Up to now, potential target antigens for AML treatment by CAR-T cells were under investigation, including CD33 [
26], CD123 [
22], CD38 [
27], CD44v6 [
28], FRβ [
29], PR1/HLA-A2 [
30], CLL-1 [
31], and LeY [
32]. CD33 and CD123 are highly expressed on primary AML cells and are the most commonly used antigens for AML treatment by CAR-T therapy [
22,
33]. However, these antigens did not only restrictively express on AML cells, they also expressed in various degrees on normal HSPCs, immune cells, and normal healthy tissues. Therefore, looking for AML-associated surface antigens which are specifically expressed on leukemia cells (or even leukemia stem cells), but are low or not expressed on normal cells and tissues, is an ideal strategy to develop CAR-T clinical application [
25]. Besides, hematopoietic malignancies always arise with cytogenetic alterations, so the choice of AML-related target antigens involved in leukemogenesis may be a feasible approach for AML CAR-T therapy.
Due to the high expression of FLT3 in 70 to 100% of AML patients and in a high percentage of ALL cases [
3], and approximately 30% of AML patients carried the FLT3 mutation which confers proliferative and survival advantages for leukemia cells, FLT3 may become the potential and ideal target for generating CAR-T cells and possess even more effective cytotoxicity on FLT3-ITD AML. The scFv-based FLT3 CAR-T therapy had been developed and demonstrated its potential on the treatment of FLT3 AML. Although it had been reported that FLT3 CAR-T cells did not deplete CD34
+ HSPCs and preserved HSPC differentiation [
11], the scFv-based FLT3 CAR-T cells had similar cytotoxic effect on the cells with FLT3-WT and mutant FLT3 phenotypes.
In our study, a novel type of CAR to target FLT3 using its ligand as recognizing domain, the FLT3L CAR, was constructed. FLT3L CAR-T could interact and eradicate both FLT3
+ leukemia cell lines and primary AML cells at the E:T ratio as low as 1:8. Nevertheless, the effect of specific cytolysis seemed independent of FLT3 expression level on leukemia cells but relied on whether they carried FLT3-ITD mutation, and the FLT3-ITD-positive leukemia cells were more sensitive to FLT3L-based CAR-T cells than the FLT3 wild-type leukemia cells. Since FLT3 ligand promotes the dimerization and phosphorylation of FLT3 within 5–15 min and subsequently activates several pathways involved in cell survival and proliferation, such as RAS/RAF/Erk, PI3K/Akt/mTOR, and JAK/STAT [
34], it was supposed that FLT3L expressed by CAR-T cells might promote dimerization and activation of FLT3 in FLT3-WT cells, and activation of the signal transduction cascades in FLT3 wild-type leukemia cells may promote their survival and relieve damage. To address this question, we measured the phosphorylation level of STAT5, AKT, and ERK in FLT3
+ leukemia cells after being co-cultured with CAR-T or VEC-T cells and found the increased activation of pERK in FLT3-WT and heterozygous FLT3-ITD leukemia cells, which indicated that the expression of FLT3L on CAR-T cells is involved in activating downstream proliferative Ras-Raf-Mek-Erk pathways. As a result, proliferation and survival of FLT3-WT leukemia cells were promoted. In other words, this may be the reason why the FLT3 wild-type leukemia cells were insensitive to FLT3L-based CAR-T cells. Besides that, FLT3L CAR-T may show comparative stronger cytotoxic capability on leukemia cells harboring FLT3-ITD mutation which is reflecting a very poor prognosis.
TAAs which are restricted to express on tumor cells are ideal target candidates for CAR-T therapy. Unfortunately, antigens used in previous CAR-T studies are also expressed on normal cells and tissues. In clinical application, the on-target/off-tumor toxicities may arise during CAR-T therapy. Rosenberg et al. reported that T cells transduced with a CAR-recognizing ERBB2 could also recognize low levels of ERBB2 on lung epithelial cells, which caused patient’s serious respiratory distress and cytokine storm, eventually leading to the death of the patient [
35]. Maude et al. also reported that some CD19 CAR-T treated patients suffered from clinically tolerable B-lymphocyte aplasia for months to years [
36]. However, AML CAR-T therapy may induce severe on-target/off-tumor myeloablation and may even threaten life [
37]. Kenderian et al. [
38], Gill et al. [
39], and Wang et al. [
40] have reported that CD33 CAR-T treatment could impair normal hematopoiesis. As early myeloid and lymphoid progenitor cells also express FLT3, we detected the FLT3 expression on CD34
+ HSPCs, which showed no significant difference compared with five leukemia cell lines and leukemia cells of ten AML patients using SFI as an index (Additional file
1: Figure S2). Therefore, CAR-T cell that recognizes FLT3 may induce on-target/off-tumor toxicities. scFv-based FLT3 CAR-T [
11] showed no cytotoxicity to PBMCs of healthy donors, and CD34
+ HSCs isolated from cord blood in vitro and in vivo. To test whether FLT3L CAR-T could be more safe, colony formation assay of pre-treated CD34
+ HSCs derived from umbilical cord blood with CAR-T cells was performed in our study. It showed that FLT3L CAR-T cells did not inhibit colony formation of normal CD34
+ cells. It was reported that FLT3 and FLT3L combination and activation of the downstream pathway had a pivotal role in the regulation of hematopoietic cells, including phospholipid metabolism, transcription, proliferation, and apoptosis [
34]. Based on our results described above, FLT3L CAR-T has the potential to activate survival-associated signaling pathways of CD34
+ HSPCs expressing FLT3-WT and reduce cytotoxicity to some extent, which is also indicating the possible safe use of FLT3L CAR-T. However, clinical application of FLT3L CAR-T requires more evidences to verify its on-target/off-tumor toxicity.
Proliferation and activation of CAR-T cells in vitro or in vivo occurred with a sharp increase of inflammatory cytokines, leading to cytokine release syndrome (CRS) which was the most common and lethiferous side effect in CAR-T therapy. CAR-T cells co-cultured with target AML cells enhanced secretion of inflammatory cytokine such as IFN-γ, IL-2, and TNF-α. Recent research found that scFv-based FLT3 CAR-T cells released significantly increased IL-2 and IFN-γ when co-cultured with target cells [
11], while in our study, IL-2 was slightly increased when co-cultured with FLT3-ITD leukemia cells and nearly not changed when co-cultured with FLT3-WT leukemia cells. Similar to the cell line results, IL-2 was nearly not detectable in the system of CAR-T cells co-cultured with primary FLT3
+ AML cells. We suppose that this may relate with different recognizing domains of CAR, FLT3L, and scFv and result in different interaction patterns and different types of cytokine profiles released by CAR-T.
CRS and on-target/off-tumor effect are the prominent toxicities of CAR-T therapy. Over the years, improvements in CAR-T cells have been performed to make AML CAR-T therapy more safe and effective. Effective means such as suicide gene, inhibitory CAR, dual-antigen receptor, on-switch CAR, and combination with checkpoint blockade therapy have been studied to control CAR-T cells effectively in vivo [
41]. Researchers were also trying to find specific or even unique antigens for CAR-T therapy and avoid irreversible on-target/off-tumor cytotoxicity on normal cells. However, unique antigen expressed only on leukemia cells was scarcely to be found, and on-target/off-tumor toxicity may happen at various degrees. The toxicity is mainly due to the inability of CAR-T cell to distinguish between normal cells and tumor cells. To find one type of recognizing domain which can distinguish between normal cell and tumor cell will have a significant impact on CAR-T therapy. For this goal, we described a new type of CAR-T cell directed to FLT3 using its ligand as recognizing domain, the FLT3L CAR-T cell, and demonstrated that it had potent but diverse antitumor activity to FLT3-WT and FLT3-ITD leukemia cells. FLT3 ligand-based CAR-T might induce activation of proliferation-related signaling of FLT3-WT cells, indicating that FLT3L CAR-T was able to distinguish between FLT3 wild-type cells and FLT3 mutant cells. Besides that, as distinct from scfv-based FLT3 CAR-T, our study showed diverse release of inflammatory cytokine. More importantly, the FLT3L CAR-T had little off-target cytotoxicity on normal HSPCs. In vivo FLT3
+ leukemia model showed that FLT3L CAR-T could significantly prolong the survival of leukemia beard mice. In conclusion, FLT3 ligand-based CAR-T cells exhibited specific cytotoxicity against FLT3+ leukemia cell and had the ability to distinguish between FLT3 wild-type cells and FLT3-ITD mutant cells, which may be an ideal candidate that specifically target AML with FLT3 mutation.