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Synergistic killing effects of homoharringtonine and arsenic trioxide on acute myeloid leukemia stem cells and the underlying mechanisms
Journal of Experimental & Clinical Cancer Research volume 38, Article number: 308 (2019)
The Correction to this article has been published in Journal of Experimental & Clinical Cancer Research 2019 38:407
At present, it is generally believed that leukemia stem cells are the source of AML, so the killing of leukemia stem cells has become important. Previous studies have suggested that HHT combined with ATO can synergistically kill U937 cells, and HHT has also demonstrated the ability to kill leukemia stem cells. We evaluated whether HHT combined with ATO can systematically kill leukemia stem cells (LSCs) and explored the synergistic effect and molecular mechanism.
CCK-8 was used to detect cell viability. The changes of cell cycle (PI staining), apoptosis (Annexin V/PI) and surface markers (CD34, CD38, CD96, CD45) were detected by flow cytometry. The cells of CD34+ primary leukemia and CD38- KG-1, and TF-1 were separated by flow cytometry. High-throughput mRNA sequencing was used to analysis mRNA level changes after the application of the two drugs. Western blot was used to verify the changes of pathway protein expression. NRG mice were used as the receptor of xenograft model. Histological H&E staining assess the invaded ability of leukemia cells, and laser scanning confocal microscopy evaluated the molecule markers change.
HHT and ATO synergistically killed KG-1 (CD34+/CD96+/CD38+/−) and Kasumi-1 (CD34+/CD38−) cells. Their combination had a stronger effect of inducing apoptosis and blocking the cell cycle than HHT or ATO administrator alone, meanwhile significantly reducing the numbers of LSCs. Further, CD34+CD38− cells in KG-1, KG-1a, TF-1, and primary leukemia cells were more sensitive to HHT and ATO. High-throughput mRNA sequencing suggested that HHT alone could significantly upregulate molecules related to the Notch, P53, and NF-κB signaling pathways. When combined with ATO, HHT further upregulated P53, whereas HHT-induced NF-κB pathway activation was significantly suppressed. Western blot analysis verified the change of protein expression in the above pathways and further demonstrated that GSI, could eliminate these effects. In vivo, HHT combined with ATO significantly reduced the LSC burden, and weakened the expression of LSC markers.
This is the first evidence that HHT combined with arsenic can synergistically kill LSCs in vitro and in vivo, along with identification of the underlying mechanism, highlighting a potentially effective treatment strategy.
Acute myeloid leukemia (AML) remains a clinical treatment challenge. Although multi-drug combinational chemotherapy can reduce the remission risk, relapse nevertheless is common. Accumulating evidence points to leukemia stem cells (LSCs) as the root of relapse [1, 2]. Thus, inducing damage to LSCs would be an effective approach to reduce the relapse rate of AML.
LSCs are a specific subgroup of AML cells. The current paradigm states that LSCs of AML are part of the CD34-positive and CD38-negative cell population and thus can be distinguished by various molecular markers . CD96 has recently been applied for the identification of LSCs among CD34+/CD38− AML cells ; however, there are few studies on this marker. Moreover, the multitudinous cell lines KG-1, KG-1a, Kasumi-1, and TF-1 also contain CD34+/CD38− AML cells, with essentially all of these lines being CD34+. Accordingly, these cells are most widely used to study LSCs [5, 6].
Homoharringtonine (HHT) and arsenic trioxide (ATO) have been traditionally used in the treatment of AML in China separately; however, little is known about the effects of their combination. The first report of their combined use was conducted in the multiple myeloma cell line RPMI8226 . Subsequently, these two agents were shown to exhibit a synergistic effect in killing AML cells . However, the synergistic anti-proliferative effects of HHT and ATO on LSCs, and the underlying mechanism, remain to be clarified. Thus, we examined the effects of these two agents on LSCs using the cell lines listed above as well as in a xenograft model in vivo. We further explored the potential effects of these agents alone and in combination on the Notch, p53, and nuclear factor-κB (NF-κB) pathways as a candidate mechanism.
Notch is a cell-surface receptor forming a heterodimer comprising extracellular and transmembrane subunits and is typically expressed in both normal hematopoietic cells and leukemia cells . The main effect of Notch is the induction of stem cell proliferation, although recent studies have identified various roles according to cell and disease types. In lymphopoiesis, Notch1 and Notch2 affect T and B cell differentiation and proliferation, respectively; however, their roles in myeloid lineages, especially in LSCs, are not fully clarified . P53 and p21 are important tumor suppressor proteins, and p53 induces the expression of p21 . HHT has been shown to enhance p53/p21 expression in FLT3-ITD mutant AML , but this effect in LSCs and the consequence for cell proliferation are not well understood. Moreover, p53/p21 expression is induced by Notch ligand in myeloid lineage cells overexpressing Notch/Hes1 . Thus, this effect of HHT on Notch upregulation and subsequent p53/p21 pathway activation might also underlie the killing mechanism of LSCs.
NF-κB is a transcription factor that is constitutively activated in primitive AML cells, and its expression can be reduced by HHT in multiple myeloma cells, while ATO was shown to suppress NF-κB activation in mantle cell lymphoma cells [13,14,15]. Like p53, the NF-κB pathway is also a target of Notch downstream signaling . However, the effects of HHT and ATO on the NF-κB pathway in LSCs are unknown.
Here, we used CD34+/CD38− KG-1 and Kasumi-1 cells along with CD34+ primary-cultured cells from patients with AML to investigate the synergistic effect of HHT and ATO in LSCs in vitro. In addition, NRG mice injected with KG-1 cells were used as an in vivo xenograft model to investigate the effects of treatment with HHT and ATO alone or in combination. Overall, we demonstrate a synergistic effect of HHT and ATO, inducing greater damage to LSCs in vitro and in vivo than these two drugs using alone. and highlight a link between activation of the tumor suppressor P53 pathway and inhibition of the NIK and NF-κB pathways. These findings provide insight into the pathogenesis of AML, while highlighting key molecules to effectively target LSCs and reduce the risk of remission.
Primary patient and cell lines culture
Mononuclear cells were extracted with a Nicoll–plaque (Haoyang, Tianjin, China) gradient centrifugation method from bone marrow blood samples of patients newly diagnosed with AML (n = 7) and samples of benign anemia patients and of allotransplantation patient whose bone marrow showed complete remission (three samples in total), which were preserved when drawing blood for diagnosis after obtaining informed consent. Patients data was listed in Additional file 9: Table S1. Primary cells were cultured in serum-free medium (stemspan™, STEMCELL, Vancouver, Canada) with CC110-cytokine cocktail (Flt3L, IL-6, IL-3, SCF, stemspan™, STEMCELL, Vancouver, Canada). Kasumi-1, TF-1, THP-1 and HEL cells (purchased from ATCC) were cultured in RPMI-1640 medium (Hyclone, Thermo Scientific, Waltham, MA, USA) with 10% fetal bovine serum (Gibco, Life Technologies, Grand Island, NY, USA); 2 ng/ml granulocyte macrophage-colony stimulating factor was added to the medium of TF-1 cells. KG-1 cells and KG-1a were purchased from Kunming Institute of Zoology, Chinese Academy of Science and ATCC respectively, and cultured in IMDM (HyClone) with 20% fetal bovine serum (Gibco). All cells were maintained in a 37 °C incubator with 5% CO2.
Primary CD34+ cells and KG-1, TF-1, CD38−, or CD38+ cells were sorted by staining with CD34-allophycocyanin (CD34–APC; BD Biosciences, Pharmingen, San Diego, CA, USA) and CD38-APC (BD Biosciences), respectively, using flow cytometry on the FACS Aria II system.
Cells (5 × 104 cells/ml for KG-1 and Kasumi-1 cells, and 5 × 105 cells/ml for primary leukemia cells; these same concentrations were used for subsequent Kasumi-1 and primary leukemia cells experiments) were treated with indicated HHT (Minsheng pharma, Hangzhou, China), ATO (As2O3) (Harbin Yida Pharmaceutical Co. Ltd., Harbin, China), or their combination (dissolved in complete culture medium) at 37 °C in a 96-well plate to a final volume of 100 μl culture medium. For the combined treatment, 1 × 105 KG-1 cells/ml were used (the same concentrations were used for subsequent experiments). Subsequently, 10 μl of CCK-8 reagent (Signalway antibody; College Park, MD, USA) was added to each well, and incubated at 37 °C for 4 h. The absorbance was scanned with a BioTek SYNERGY/HTX multi-mode reader at 450 nm, and the half-maximal inhibitory concentration (IC50) of the drugs was calculated to determine the cell viability and cell growth inhibition rate as previously described .
The combination index (CI) was calculated to determine the synergistic cytotoxicity according to the classic isobologram equation: CI = (D)1/(Dx)1 + (D)2/(Dx)2, where Dx is the concentration of one drug that produces the effect, and (D)1 and (D)2 are the concentrations of the two drugs in combination that produce the same effect. CI = 1 indicates an additive effect, CI < 1 indicates synergy, and CI > 1 reflects antagonism between two drugs.
Forty-eight hours after treatment with HHT, ATO, or their combination, the cells were harvested, washed three times with phosphate-buffered saline (PBS), and prepared as a smear. The cells were immobilized with 4% paraformaldehyde (Biosharp, Hefei, Anhui, China) for 30 min, air-dried, washed with PBS, and permeabilized with 0.5% Triton X-100 (Solarbio, Beijing China) for 30 min. After washing with PBS again, the cells were stained with Hoechst 33342 (Cell Signal Technology, Danvers, MA, USA) for 30 min at room temperature to detect apoptosis; the nuclear morphology change was immediately evaluated using a fluorescence microscope (Olympus, Tokyo, Japan) after a final wash with PBS.
Cell cycle, cell apoptosis, and cell surface antigens were detected using flow cytometry. In brief, 48 h after treatment of KG-1, Kasumi-1, KG-1a, TF-1, or primary cells, the cell density was adjusted according to the cell viability assay and prepared for cell cycle analysis as described in our previous report . Cells were stained with Annexin V-fluorescein isothiocyanate (FITC)/propidium iodide (PI) (BD Pharmingen, San Diego, CA, USA) to detect the apoptosis state in accordance with the manufacturer specifications. The CD34+/CD38− population (Kasumi-1 cells) or CD34+/CD38−/CD96+ population (KG-1 cells) was obtained by incubating with CD34–FITC (Biolegend, San Diego, CA USA), CD38–R-phycoerythrin cyanine7 (CD38–PE-Cy™7; Biolegend), and CD96–R-phycoerythrin (CD96-PE; Biolegend) in Cell Staining Buffer (Biolegend); Annexin V–FITC and CD38–PE-Cy™7 were used for KG-1, KG-a, and TF-1 cells, and CD34–APC was also added for primary cells. The procedure was as follows: The cells (1 × 106) were collected and resuspended in 100 μl Cell Staining Buffer, the antibody was added and incubated at 4 °C for 15 min, washed again with cell staining buffer one time, and then subject to the apoptosis assay. To exclude non-viable cells, cells were stained with 7AAD before flow cytometry (BD Versa, San Diego, CA, USA) analysis for antigen detecting.
Real-time fluorescence quantitative polymerase chain reaction (qPCR)
Total RNA was extracted using TRIzol (Invitrogen, MA, USA) and immediately transcribed into cDNA by a Reverse Transcription Kit (Toyobo, Japan). Real-time qPCR was performed with a SYBR Green PCR Kit (Roche, Basel, Switzerland) on an ABI PRISM 7500 PCR instrument (Applied Biosystems). The reaction solution (20 μl) contained 10 μl 2 × QuantiTect SYBR Green PCR Master Mix, 0.5ul of each primers (10 nM), 2 μl of cDNA, and 7 μl of RNase-free water. Amplification was performed in three stages: holding stage (50 °C for 2 min and 95 °C for 10 min), cycling stage (40 cycles of 95 °C for 15 s, 60 °C for 1 min), and melting stage (95 °C for 15 s, 60 °C for 1 min, 95 °C for 30 s, 60 °C for 15 s). Relative gene expression levels were calculated using the 2-ΔΔCt method with β-actin as an internal control. Primer sequence listed in Additional file 10: Table S2.
RNA sequencing analysis
KG-1 cells were dissolved in TRIzol after treatment with HHT, ATO, or their combination for 6 h, and then RNA was isolated. The sequencing reaction was performed using Illumina HiSeq 4000. Differentially expressed genes, cluster analysis, gene ontology (GO) enrichment analysis, pathway enrichment analysis, and other functional annotations were performed at Shanghai Aksomics Company Limited (Shanghai, China).
Western blot analysis
KG-1 cells and primary CD34+ cells were collected and lysed in radioimmunoprecipitation assay lysis buffer (Beyotime, Shanghai, China) with phenylmethanesulfonyl fluoride, protease inhibitor cocktail, and phosphatase inhibitor cocktail (KangCheng Bio-tech, Shanghai, China) after treatment with drugs for 24 h. To ensure uniform sample amounts in each lane (adjusted to the homogeneous internal control from each sample), proteins were separated by 8% sodium dodecyl sulfate-polyacrylamide gel electrophoresis and then transferred to nitrocellulose membranes (Life Science, Germany). After blocking with 5% non-fat milk, the membranes were incubated overnight at 4 °C with the primary antibody (1:1000, all from Cell Signaling Technology, Beverly, MA, USA), followed by secondary horseradish peroxidase-conjugated antibody (1:5000, Cell Signaling Technology) in tris-buffered saline with Tween for 1 h (P53, antibodies for 2 h) at room temperature. Pathway signals were detected using an ECL kit (CWBIO, Beijing, China) and visualized on a ChemiDOC™ imaging system (Bio-Rad, Hercules, CA, USA). GAPDH was used as a loading control.
Animal xenograft leukemia model
NRG mice (Rag1−/−, IL2R γ−/− NOD mice) were purchased from the Nanjing Model Animal Center, and bred in a pathogen-free environment supplied with sterile food and water at the Experimental Animal Center of Fujian Medical University. All animal experimental protocols were approved by Fujian Medical University Animal Care and Use Committee. Adult mice (4–6 weeks old) were sublethally irradiated with 2 Gy of total body irradiation, and then injected with 7 × 106 KG-1 cells 24 h later in 200 μl PBS via the tail vein. The mice were monitored weekly for the percentage of hCD45+ cells in the peripheral blood and were monitored daily for disease symptoms (ruffled coat, hunched back, weakness, and reduced motility) for one month. Along with hCD45+ cells > 1% in peripheral blood of mice, the mice were then assigned randomly to four groups (n = 5 per group) administered daily with: PBS (vehicle), HHT, ATO, or HHT and ATO in combination. The doses were calculated as follows. HHT: 1 mg/60 kg per day × 9.1 = 152 ng/g per day; ATO: 10 mg/60 kg per day × 9.1 = 1.52 μg/g per day. One week after drug administration, the mice were killed and infiltration of leukemia cells was evaluated by hematoxylin and eosin (H&E) staining, FCM and confocal laser-scanning.
The spleens and bone marrow were removed from the mice at the end of the experiment and fixed with 4% paraformaldehyde, embedded in paraffin, and cut into slices. After dewaxing, washing with water, antigen retrieval, and spontaneous fluorescence quenching, the tissues were blocked with 3% bovine serum albumin (for goat antibody) or 10% normal rabbit serum (for other antibodies) for 30 min at room temperature. After incubating with the primary antibody (anti-CD34 and anti-CD45; Goodbio Technology, Wuhan, anti-P53 and anti-NF-κB2, CST) and secondary antibody (Goodbio Technology), the tissue slices were counterstained with DAPI (C1005, Beyotime), and images were taken with a NIKON ECLIPSE CI confocal laser-scanning microscope (Japan).
Group comparisons of parametric data were performed using analysis of variance; for data with a skewed distribution, the Jonckheere-Terpstra test was applied. Two-group comparisons were made with Student’s t-test. Significance was used as p < 0.05 and error bars represent SD. All statistical analyses were carried out with SPSS version 22.0.
HHT and ATO synergistically reduce cell viability in leukemia stem-like cells and CD34+ primary cells.
Based on the results of the CCK-8 assay (data not shown), we selected the cell lines most sensitive to HHT and ATO treatment, Kasumi-1, KG-1, HEL, and THP-1, to evaluate the synergistic effect of the two reagents. Additional file 1: Figure S1 and Additional file 2: Figure S2 demonstrate that HHT and ATO reduced the viability of these four cell lines in time- and dose-dependent manners. Although ATO clearly boosted the cytotoxic effect of HHT on all cell lines (Fig. 1), synergistic effects were only detected for Kasumi-1 and KG-1 cells. These synergistic actions of HHT combined with ATO were also detected in CD34+ primary AML cells (n = 3) (Table 1), demonstrating that these effects are mainly exerted in LSCs. Next, we selected the ATO dose of maxim synergistic effects (bolded number in Table 1) as following experiments.
ATO enhances the ability of HHT to induce cell apoptosis and cell cycle arrest in leukemia stem-like cells
To further identify the mechanism of damage induced to LSCs by HHT and ATO, we detected the apoptosis and cell cycle of Kasumi-1 and KG-1 cells after treatment. Flow cytometry showed that 10 ng/ml of HHT mildly induced the apoptosis of Kasumi-1 cells, and 2 μM ATO had only a slight apoptosis-inducing effect. However, their combination markedly increased the apoptosis rate of Kasumi-1 and KG-1 cells as well, exceeding the total of these two drugs independently (Fig. 2a, b). Moreover, compared with single-agent treatments, HHT + ATO caused increased nucleus fragmentation, as part of the nucleus began to dissolve (Fig. 2c, d).
The cell cycle was arrested in the G0/G1 phase in Kasumi-1 cells after HHT treatment, and this effect was also enhanced by ATO (Additional file 3: Figure S3A). Although the KG-1 cell cycle was also arrested in G0/G1 phase after HHT treatment, there was no further increase in the proportion of G0/G1-phase cells with the addition of ATO; instead, the combined treatment decreased the G2/M-phase cells (Additional file 3: Figure S3B). This suggested that ATO could strengthen the cytotoxic ability of HHT to G0/G1 phase cells, which are resistant to chemotherapy drugs.
ATO enhances the effect of HHT in decreasing the proportion of LSCs
Almost all of the Kasumi-1 cells were CD34+CD38−; however, they did not express the LSC marker CD96 (data not shown). After treatment with 10 ng/ml HHT, the proportion of CD34+CD38− cells was slightly reduced, whereas 20 ng/ml HHT remarkably decreased the proportion of CD34+CD34− cells. Moreover, when combining 10 ng/ml HHT with 1 μM or 2 μM ATO, the proportion of CD34+CD38− cells dramatically declined (Fig. 3a). Similar results were found for KG-1 cells. Moreover, HHT also reduced the proportion of CD34+CD38−CD96+ cells in KG-1 cells, but increasing the concentration of HHT or adding ATO did not cause a further decrease (Fig. 3c). These results were confirmed by qPCR demonstrating downregulation in CD34 expression and upregulation of CD38 expression by HHT, and ATO promoted these effects, in both cell lines. In addition, CD96 expression was also downregulated in KG-1 cells by HHT, and the effect was enhanced by the addition of ATO (Fig. 3b, d).
HHT combined with ATO more effectively killed the CD34+CD38− LSCs than CD34+CD38+ AML cells
To further explore the mechanism for the decreased proportion of CD34+CD38− cells in KG-1 and Kasumi-1 cells, we examined the effect of HHT on cell differentiation of KG-1; however, no differentiation induction was observed (data not shown). To further clarify the mechanism, we used double staining of Annexin V and anti-CD38, which showed that (after excluding dead cells), Annxein V-positive cells mainly assembled in the section of CD38-low KG-1 cells (Fig. 4a). The same result was found in two other two cell lines, KG-1a (Fig. 4b) and TF-1 (Fig. 4c), with similar CD38 expression to KG-1 cells. To further tease apart the effects of apoptosis, which would reduce the contents of all proteins, and low CD38 expression, we analyzed the CD38high and CD38low KG-1 and TF-1 (CD34+) cells separately. Consistently, flow cytometry showed that the combined HHT and ATO treatment more effectively killed the CD34+CD38− LSCs (Additional file 4: Figure S4).
ATO promotes the ability of HHT to damage primary LSCs in serum-free medium with cytokines
To generalize the above findings in LSCs for more complex and universal systems, we treated bone marrow mononuclear cells from AML patients (n = 4) with the two drugs. To simulate the survival condition of primary LSCs, we incubated the primary cells with the drugs in serum-free medium with Flt3L, SCF, IL-3, and IL-6. Similar to the results of the cell lines (KG-1, KG-1a, TF-1), the proportions of CD34+ cells, CD34+/CD38− cells, and CD34+/CD38−/CD96+ cells decreased after treating with HHT, with a more dramatic reduction observed in the combined treatment group (Fig. 5a–d, Additional file 5: Figure S5). However, the proportions of normal CD34+/CD38- cells (n = 3) have no observably decrease (Fig. 5e).
Moreover, HHT more effectively damaged the CD34+/CD38− primary AML cells than CD34+/CD38− cells, and ATO significantly promoted this effect in spite of a lack of an obvious influence on the apoptosis rate of these cells when treated alone (Additional file 6: Figure S6).
HHT upregulates the notch pathway while ATO downregulates the NF-κB pathway
High throughput mRNA-sequencing analysis demonstrated that HHT upregulates the Notch and NF-κB pathway, as well as P53 family members (Additional file 7: Figure S7), suggesting the subsequent inhibition of proliferation in AML cells, at least partly, followed by P53 upregulation and BCL-2 downregulation [9, 12]. In addition, ATO could inhibit the NF-κB pathway in MCL (mantle cell lymphoma) . We also found that ATO downregulated the NF-κB pathway from sequencing analysis data. Thus, we hypothesized that HHT activates the Notch pathway and P53 to kill LSCs, while ATO inhibits the NF-κB pathway to produce the observed synergistic effect.
HHT activates the P53 and NF-κB pathways, and ATO strongly inhibits the NF-κB pathway
To confirm the RNA-sequencing result and test our hypothesis, the effects of the treatments on the relevant protein levels were assessed with western blotting. The HHT (20 ng/ml)-induced upregulation of Notch1 and NF-κB was reversed when combined with ATO (1 μM) in KG-1 cells (Fig. 6a). These effects were further confirmed by the fact that P53 was activated by both HHT and ATO, which was also observed in primary CD34+ cells (Fig. 6b). Further, treatment of gamma secretase inhibitor (GSI)-LY3039478, Notch1 inhibitor to the KG-1 cells incubated with HHT resulted in inhibition of most of the proteins involved in the p53, NIK/IKKα, and NF-κB pathways (Fig. 6c).
HHT and ATO reduce the xenograft burden and proportion of LSCs in the spleen rather than the bone marrow
The burden of human leukemia cells (KG-1 cells) in the spleen of NRG mice was markedly reduced with combined administration of HHT and ATO (P < 0.01). Moreover, ATO enhanced the action of HHT (HHT vs. HHT + ATO, P < 0.05), although there was no significant effect with HHT administration alone (Fig. 7a, d). However, this treatment did not appear to impact the leukemia cells in the bone marrow of mice (Fig. 7a). Further, LSCs were effectively obliterated with the combined drug treatment (P < 0.05), but not with either treatment alone (Fig. 7c), although there was no elimination effect in the bone marrow. Moreover, histological analysis demonstrated that the ability of KG-1 cells to invade the spleen was remarkably impaired in mice treated with HHT and ATO compared with that observed in mice that received vehicle as a control. Again, this effect was not apparent in the bone marrow (Fig. 8a). Confocal laser-scanning microscopy clearly showed that the expression levels of hCD45 (leukemia cell marker) and hCD34 (a LSC marker) were significantly decreased in the combined treatment group compared with those of the other three groups (Fig. 8b). The expression of P53 and NF-κB2 in vivo were also evaluate by confocal laser-scanning. Like the result derived from WB, HHT and ATO could upregulated the expression of P53 and ATO reduce the expression of NF-κB2 which upregulated by HHT in spleens, it is not obvious in BM (Additional file 8: Figure S8).
The main clinical challenge in leukemia treatment remains the effective elimination of LSCs to reduce the chance of remission. Here, we show that HHT and ATO have a synergic effect to inhibit the proliferation of LSCs, which was identified in KG-1, Kasumi-1, primary CD34+ cells from AML patients, and in an in vivo xenograft model. This synergistic effect was found to involve greater induction of cell apoptosis and cell cycle arrest.
Shen et al.  pointed out that HHT may be an effective killing agent of LSCs in vitro, and decreased the ratio of CD34+CD38−CD96 + cells in KG-1 cells. Here, we expand these findings by demonstrating that HHT and ATO synergistically reduced the proportion of LSCs in the Kasumi-1 and KG-1 cells, as well as in primary bone marrow cells. Moreover, we identified the underlying mechanism. However, the reason for the decreasing proportion of LSCs was unknown. At first, despite qPCR results indicating that ATO enhanced the effects of HHT in reducing the expression of levels CD34 and CD96 mRNA and upregulating CD38 expression, cell differentiation was not observed. Thus, we speculated that the mechanism is not underlying in molecule expression regulation. Although a previous study  demonstrated that HHT had a greater potency to kill the CD34+CD38− primary AML cells compared to CD34+CD38+ cells, the sample size was limited. Our results further confirm these findings with a larger sample size along with confirmation in other cell lines. Apoptotic cells (Annexin V+ cells) largely localized in the section of CD38− or CD38low cells in all three cell lines; namely, HHT or HHT combined with ATO more effectively killed CD34+CD38− KG-1, KG-1a, TF-1 cells than CD34+/CD38+ cells. We further validated the decrease of primary CD34+/CD38−/CD96+ cells and a higher apoptosis rate of primary CD34+/CD38− or CD38low cells than CD34+/CD38+ cells in bone marrow cells after treatment with HHT and ATO. These findings were confirmed in CD38+ and CD38− KG-1 and TF-1 cells analyzed separately, demonstrating that HHT does not simply inhibit the expression of all proteins through apoptosis induction . However, it remains unclear why CD34+/CD38− cells are more sensitive to HHT and HHT combined with ATO.
Chen et al.  first uncovered that the synergistic effect of HHT and ATO involved upregulation of the PI3k/Akt pathway by ATO in U937 cells. We found only a slight effect of ATO alone, although it markedly enhanced the actions of HHT on LSCs at the same dose. This suggested further synergic mechanisms, which were identified as regulation of the Notch, NF-kB, and P53 pathways.
Notch is considered to be an oncogene in T-cell acute lymphoblastic leukemia and lymphoma [21, 22]; however, its role in AML has been controversial [12, 23,24,25]. The majority of related studies support that Notch acts as an inhibitor in AML. The Notch pathway also interacts with stemness-related pathways, including the Wnt or Hedgehog signaling pathway . Here, we found that HHT activates the Notch pathway, leading to upregulation of the NF-κB pathway and P53, whereas ATO not only inhibited the NF-κB pathway but also further induced the expression of P53. We believe that this is, at least, part of the mechanism underlying the synergic effect of these two drugs on LSCs. In addition, HHT upregulated Notch1 and downregulated Notch2, confirming a previous study showing that Notch2 knockdown increased the level of Notch1 expression in THP-1 and TMD7 cell lines . However, the mechanism and biological significance of the influence of HHT on Notch1 and Notch2 are unclear and worthy of further study.
Interestingly, in the xenograft model, the leukemia cell burden and LSCs reduction was more remarkable in the spleen with no significant difference in the bone marrow. This may be related to a low sample size or the effect of bone marrow niche. However, the specific mechanism of action of these two drugs in vivo should be further evaluated toward promoting their clinical application and elucidating the mechanism to improve treatment strategies for AML patients.
Overall, our results demonstrate a clear synergistic effect of HHT and ATO on LSCs in vitro and in vivo. We suggest that the chemotherapy regimens including HHT and ATO could decrease the rate of AML relapse.
Availability of data and materials
The datasets used and/or analysed during the current study are available.
from the corresponding author on reasonable request.
leukemia stem cells
nuclear factor-kappa B
phosphate buffered saline
phycoerythrin cyanine 7
Hope KJ, Jin L, Dick JE. Acute myeloid leukemia originates from a hierarchy of leukemic stem cell classes that differ in self-renewal capacity. Nat Immunol. 2004;5:738–43.
Zhang Y, Xia F, Liu X, Yu Z, Xie L, Liu L, et al. JAM3 maintains leukemia-initiating cell self-renewal through LRP5/AKT/beta-catenin/CCND1 signaling. J Clin Invest. 2018;128:1737–51.
Testa U. Leukemia stem cells. Ann Hematol. 2011;90:245–71.
Hosen N, Park CY, Tatsumi N, Oji Y, Sugiyama H, Gramatzki M, et al. CD96 is a leukemic stem cell-specific marker in human acute myeloid leukemia. Proc Natl Acad Sci U S A. 2007;104:11008–13.
Liu Y, Chen F, Wang S, Guo X, Shi P, Wang W, et al. Low-dose triptolide in combination with idarubicin induces apoptosis in AML leukemic stem-like KG1a cell line by modulation of the intrinsic and extrinsic factors. Cell Death Dis. 2013;4:e948.
Alexaki A, Quiterio SJ, Nonnemacher MR, Shah S, Liu Y, Banerjee A, et al. Modeling bone marrow progenitor cell differentiation and susceptibility to HIV-1 infection. MOJ Immunol 2014;1:00009–00009.
Zhou XJ, Zhou YH, Chen XH, Qian WB. [Homoharringtonine combined arsenic trioxide induced apoptosis in human multiple myeloma cell line RPMI 8226: an experimental research]. Zhongguo Zhong Xi Yi Jie He Za Zhi 2013;33:834–839 (in Chinese).
Chen P, Jiang X, You PD, Jin Q, Yuan Q, Huang HF. [Combination of homoharringtonine with arsenic trioxide induces apoptosis of human acute myeloid leukemia cell line U937]. Zhongguo Shi Yan Xue Ye Xue Za Zhi 2016;24:1649–1653 (in Chinese).
Tohda S. NOTCH signaling roles in acute myeloid leukemia cell growth and interaction with other stemness-related signals. Anticancer Res. 2014;34:6259–64.
Kang R, Kroemer G, Tang D. The tumor suppressor protein p53 and the ferroptosis network. Free Rad Biol Medicine. 2018. https://doi.org/10.1016/j.freeradbiomed.2018.05.074.
Li X, Yin X, Wang H, Huang J, Yu M, Ma Z, et al. The combination effect of homoharringtonine and ibrutinib on FLT3-ITD mutant acute myeloid leukemia. Oncotarget. 2017;8:12764–74.
Kannan S, Sutphin RM, Hall MG, Golfman LS, Fang W, Nolo RM, et al. Notch activation inhibits AML growth and survival: a potential therapeutic approach. J Exp Med. 2013;210:321–37.
Guzman ML, Neering SJ, Upchurch D, Grimes B, Howard DS, Rizzieri DA, et al. Nuclear factor-kappaB is constitutively activated in primitive human acute myelogenous leukemia cells. Blood. 2001;98:2301–7.
Chen P, Yuan Q, Yang H, Wen X, You P, Hou D, et al. Homoharringtonine enhances bortezomib antimyeloma activity in myeloma cells adhesion to bone marrow stromal cells and in SCID mouse xenografts. Leukemia Res. 2017;57:119–26.
Jung HJ, Chen Z, McCarty N. Synergistic anticancer effects of arsenic trioxide with bortezomib in mantle cell lymphoma. Am J Hematol. 2012;87:1057–64.
Guo Y, Shan Q, Gong Y, Lin J, Yang X, Zhou R. Oridonin in combination with imatinib exerts synergetic anti-leukemia effect in Ph+ acute lymphoblastic leukemia cells in vitro by inhibiting activation of LYN/mTOR signaling pathway. Cancer Biol Ther. 2012;13:1244–54.
Wu Y, Tan M, Chen ML, Chen YZ. Expression and role of granulocyte macrophage colony-stimulating factor receptor (GM-CSFR) and granulocyte colony-stimulating factor receptor (G-CSFR) on Ph-positive acute B lymphoblastic leukemia. Hematology. 2018;23:439–47.
Shen JP, Yang H, Ni WM, Qian WB. [Cytotoxicity of homoharringtonine on leukemic stem-like cells in AML cell line KG-1]. Zhejiang Da Xue Xue Bao Yi Xue ban. 2012;41:485–490 (in Chinese).
Wang L, You LS, Ni WM, Ma QL, Tong Y, Mao LP, et al. Beta-catenin and AKT are promising targets for combination therapy in acute myeloid leukemia. Leukemia Res. 2013;37:1329–40.
Fresno M, Jimenez A, Vazquez D. Inhibition of translation in eukaryotic systems by harringtonine. Eur J Biochem. 1977;72:323–30.
Ntziachristos P, Lim JS, Sage J, Aifantis I. From fly wings to targeted cancer therapies: a centennial for notch signaling. Cancer Cell. 2014;25:318–34.
Sanchez-Martin M, Ferrando A. The NOTCH1-MYC highway toward T-cell acute lymphoblastic leukemia. Blood. 2017;129:1124–33.
Lobry C, Ntziachristos P, Ndiaye-Lobry D, Oh P, Cimmino L, Zhu N, et al. Notch pathway activation targets AML-initiating cell homeostasis and differentiation. J Exp Med. 2013;210:301–19.
Fu L, Kogoshi H, Nara N, Tohda S. NOTCH1 mutations are rare in acute myeloid leukemia. Leuk Lymph. 2006;47:2400–3.
Tohda S, Murata-Ohsawa M, Sakano S, Nara N. Notch ligands, Delta-1 and Delta-4 suppress the self-renewal capacity and long-term growth of two myeloblastic leukemia cell lines. Int J Oncol. 2003;22:1073–9.
Okuhashi Y, Itoh M, Nara N, Tohda S. NOTCH knockdown affects the proliferation and mTOR signaling of leukemia cells. Anticancer Res. 2013;33:4293–8.
We thank Miss Zhong Na who work as engineer in BD company at Guang Zhou for guiding the FACS sorting technology.
This work was financially supported by Construction project of Fujian medical center of hematology (Min201704),Sponsored by National and Fujian Provincial Key Clinical Specialty Discipline Construction Program, P. R.C.
Ethics approval and consent to participate
This study was approved by review board of the Fujian medical university union hospital. Animal experiments were conducted in accordance with.
the Guide for the Care and Use of Laboratory Animals, which were approved.
by the Fujian medical university Animals center.
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The original version of this article was revised: One of the corresponding emails is changed to firstname.lastname@example.org. Figure 5, Figure 8 and Additional files 5,6,9,10 are corrected.
Figure S1. Homoharringtonine (HHT) reduced the cell viability of acute myeloid leukemia (AML) cell lines. Kasumi-1 cells (A), KG-1 cells (B), THP-1 cells (C), and HEL cells (D) were treated with different concentrations of HHT for 12 h, 24 h, and 48 h, and cell viability was measured by the CCK-8 assay. Error bars represent standard deviations of three independent experiments. (DOCX 301 kb)
Figure S2. Arsenic trioxide (ATO) decreased the cell viability in acute myeloid leukemia (AML) cell lines. Kasumi-1 cells (A), KG-1 cells (B), THP-1 cells (C), and HEL cells (D) were treated with different concentrations of ATO for 1, 2, and 3 days, and cell viability was measured by the CCK-8 assay. Error bars represent the standard deviations of three independent experiments. (DOCX 176 kb)
Figure S3. Arsenic trioxide (ATO) cooperates with homoharringtonine (HHT) to arrest the cell cycle in leukemia stem-like cell lines. Cells were treated with HHT, ATO, or HHT + ATO for 2 days, and DNA contents of Kasumi-1 (A) and KG-1 (B) cells were detected with PI/RNAase and FACS. Error bars represent three independent experiments. (DOCX 154 kb)
Figure S4. Homoharringtonine (HHT) combined with arsenic trioxide (ATO) more effectively killed the CD34+CD38− leukemia stem cells sorted from KG-1 and TF-1 cells. Cells were sorted by FACS Aria II according to the expression of CD38. CD38high or CD38low cells were treated with HHT, ATO, or HHT + ATO for 2 days, and then stained with Annexin V; the apoptosis rate of the cells was detected using FACS. Error bars represent three independent experiments. P < 0.05*, P < 0.01**, P < 0.001***. (DOCX 527 kb)
Figure S5. Homoharringtonine (HHT) combined with arsenic trioxide (ATO) decrease the proportion of primary leukemia stem cells (LSCs) in serum free medium with cytokine cocktail (Flt3L, SCF, IL-3 and IL-6). Quantification of frequencies of CD34+cells (A), CD34+/CD38− cells (B) and CD34+/CD38−/CD96+ cells (C) from patient 4. (D) Display of flow cytometric analysis on bone marrow sample after treatment with HHT and ATO alone or combined. (DOCX 196 kb)
Figure S6. Homoharringtonine (HHT) combined with arsenic trioxide (ATO) more effectively damaged the primary CD34+CD38− cells than CD34+/CD38+ cells in serum-free medium with a cytokines cocktail (Flt3L, SCF, IL-3 and IL-6). (A–C) Quantification of frequencies of Annexin V-positive cells in CD34+CD38− and CD34+CD38+ cells from patient 1 (A), patient 2 (B), patient 3 (C), patient 4 (D). (E) Representative flow cytometric analysis of patient 2 for apoptosis using Annexin V and stem cells markers (CD34, CD38). (DOCX 378 kb)
Figure S7. RNA sequencing and functional enrichment analysis. KG-1 cells were treated with Homoharringtonine (HHT) and arsenic trioxide (ATO) alone or combined for 6 h and then RNA was isolated, after mRNA sequencing performed, cluster analysis and pathway enrichment analysis were applied. (DOCX 224 kb)
Figure S8. Homoharringtonine (HHT) combined with arsenic trioxide (ATO) alter the expression of P53 and NF-κB2. P53 and NF-κB2 levels were detected in the different groups by confocal laser-scanning microscopy in representative 4% paraformaldehyde-fixed spleens and bone marrow samples from NRG mice. Scale bars: 50 μm (DOCX 1214 kb)
Table S1. Patients characteristic (DOCX 21 kb)
Table S2. Primer Sequences for PCR (DOCX 19 kb)
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Tan, M., Zhang, Q., Yuan, X. et al. Synergistic killing effects of homoharringtonine and arsenic trioxide on acute myeloid leukemia stem cells and the underlying mechanisms. J Exp Clin Cancer Res 38, 308 (2019) doi:10.1186/s13046-019-1295-8
- Arsenic trioxide
- Xenograft leukemia model