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Logo of nihpaAbout Author manuscriptsSubmit a manuscriptNIH Public Access; Author Manuscript; Accepted for publication in peer reviewed journal;
 
Leukemia. Author manuscript; available in PMC May 31, 2013.
Published in final edited form as:
PMCID: PMC3668642
NIHMSID: NIHMS469937
p53 independent epigenetic-differentiation treatment in xenotransplant models of acute myeloid leukemia
Kwok Peng Ng,1* Quteba Ebrahem,1* Soledad Negrotto,1 Reda Z. Mahfouz,1 Kevin A. Link,2 Zhenbo Hu,1 Xiaorong Gu,1 Anjali Advani,3 Matt Kalaycio,3 Ronald Sobecks,3 Mikkael Sekeres,3 Edward Copelan,3 Tomas Radivoyevitch,4 Jaroslaw Maciejewski,1,3 James C. Mulloy,2 and Yogen Saunthararajah1,3
1Department of Translational Hematology & Oncology Research, Taussig Cancer Institute, Cleveland Clinic, Cleveland, USA
2Experimental Hematology and Cancer Biology, Cincinnati Children’s Hospital, Cincinnati, USA
3Department of Hematologic Oncology and Blood Disorders, Taussig Cancer Institute, Cleveland Clinic, Cleveland, USA
4Department of Epidemiology and Biostatistics, Case Western Reserve University, Cleveland, USA
Correspondence: Dr Yogen Saunthararajah, Taussig Cancer Institute, 9500 Euclid Avenue R40, Cleveland, OH 44195, USA. Tel: 216 444 8170. Fax: 216 636 2498. saunthy/at/ccf.org
*These authors contributed equally to the work
Suppression of apoptosis by TP53 mutation contributes to resistance of acute myeloid leukemia (AML) to conventional cytotoxic treatment. Using differentiation to induce irreversible cell cycle exit in AML cells could be a p53-independent treatment alternative, however, this possibility requires evaluation. In vitro and in vivo regimens of the deoxycytidine analogue decitabine that deplete the chromatin modifying enzyme DNA methyl-transferase 1 (DNMT1) without phosphorylating p53 or inducing early apoptosis were determined. These decitabine regimens but not equimolar DNA-damaging cytarabine up regulated the key late differentiation factors CEBPε and p27/CDKN1B, induced cellular differentiation, and terminated AML cell-cycle, even in cytarabine-resistant p53- and p16/CDKN2A-null AML cells. Leukemia initiation by xeno-transplanted AML cells was abrogated but normal hematopoietic stem cell (HSC) engraftment was preserved. In vivo, the low toxicity allowed frequent drug administration to increase exposure, an important consideration for S-phase specific decitabine therapy. In xeno-transplant models of p53-null and relapsed/refractory AML, the non-cytotoxic regimen significantly extended survival compared to conventional cytotoxic cytarabine. Modifying in vivo dose and schedule to emphasize this pathway of decitabine action can bypass a mechanism of resistance to standard therapy.
Although conventional chemotherapeutics for acute myeloid leukemia (AML) can have differing proximal mechanisms of action, such as topoisomerase inhibition or termination of DNA chain synthesis, a final common pathway converges onto p53, a stress and DNA damage sensor, and a master regulator of apoptosis (reviewed in (1)). Therefore, mutation and chromosome deletion at the TP53 locus is associated with treatment resistance both in vitro (2;3) and in vivo: partial or complete remissions in response to intensive chemotherapy were achieved in 81% of AML cases without, and 33% of cases with TP53 mutations (4). Similarly, responses in patients with myelodysplastic syndrome (MDS) treated with intensive chemotherapy or low dose cytarabine were 60% of cases without, and 8% of cases with TP53 mutations (4). Even in cases in which TP53 itself is not directly mutated or deleted, the p53 pathway may be targeted by genetic abnormalities in p53 cofactors: TP53 defects or MDM4 gain was noted in 45.5% of patients with blast transformed myeloproliferative disease, which responds only transiently if at all to conventional cytotoxic therapy (5;6). The rate of TP53 mutation can exceed 70% in MDS and AML cases with complex cytogenetic abnormalities, another group of patients with very poor treatment outcomes (7).
Hence, especially for certain sub-types of MDS and AML, there is a need for treatment that is not mediated through p53 and apoptosis. Interestingly, although p53-null mice are cancer prone, the development of these mice is essentially normal, with normal patterns of differentiation in almost all tissues (reviewed in (8)). This suggests that differentiation-mediated cell cycle exit is usually p53-independent. Using differentiation to terminate cancer cell proliferation was proposed more than 50 years ago (911), and differentiation has been observed in AML and cancer cells treated with drugs that inhibit chromatin modifying enzymes, such as histone deacetylase inhibitors (HDACi), and 5-azacytidine and decitabine that deplete DNA methyl-transferase 1 (DNMT1) (1218). However, the effects of HDACi are not confined to histones; HDACi can alter the acetylation status of structural, signaling and transcription factor proteins, producing wide-spread cellular effects including apoptosis. Similarly, high concentrations of the nucleoside analogues 5-azacytidine and decitabine have anti-metabolite and DNA damaging effects, and can trigger apoptosis. Furthermore, DNA hypomethylation by decitabine can induce expression of apoptosis-mediators such as p73, that can mediate apoptosis independent of p53 (19). Hence, it has not been clear that differentiation-mediated cell cycle exit is the most important therapeutic action of 5-azacytidine or decitabine (reviewed in (20)). There has even been debate about whether inhibition of chromatin-modifying enzymes is the most important effect of these drugs (20). Therefore, demonstration of a p53-independent non-cytotoxic mechanism of action, rationalization of dose and schedule to emphasize this pathway of action, and demonstration of in vivo efficacy, are important translational challenges.
Unlike the cytidine analogues cytarabine or gemcitabine, the sugar moiety of decitabine is unmodified. Therefore, at low concentrations, decitabine can incorporate into the newly synthesized DNA strand during S-phase without terminating chain elongation (21;22). These non-DNA damaging, non-cytotoxic concentrations of decitabine can nonetheless deplete DNMT1, both in vitro and in vivo (12;2125). The first objective was to determine if such concentrations of decitabine, which do not kill normal hematopoietic stem cells (HSC) (low concentrations of decitabine have increased normal hematopoietic stem cell self-renewal in a number of studies (2629)), and which may not induce early apoptosis, can nonetheless induce irreversible cell cycle exit in AML cells. Cell cycle exit is mediated by a family of highly conserved cyclin dependent kinase inhibitors (CDKN): p16/CDKN2A is implicated in apoptotic cell cycle exit, whereas p27/CDKN1B is known to mediate cell cycle exit with differentiation (3033). Therefore, the second objective was to measure changes in CDKN protein expression in response to decitabine and equimolar cytarabine, to differentiate between apoptosis and differentiation-mediated cell cycle exit, and to determine if these changes were dependent on p53. To this end, in vitro experiments were conducted in p53 wild-type and p53-null MLL-AF9 AML cells: treatment effects on p53 upregulation and phosphorylation could be measured in p53 wild-type cells, whereas p53-null cells could be used to confirm p53-independence of observed effects. Finally, the efficacy of a decitabine dose, schedule and route of administration rationalized for a non-cytotoxic mechanism of action in vivo was examined in murine xenotransplantation models of p53-null and relapsed/refractory human AML, to evaluate the translational potential of this alternative, non-cytotoxic treatment approach.
Healthy volunteer and patient samples
Umbilical cord blood was collected during normal full-term deliveries, and bone marrow aspirates were collected from AML patients and healthy volunteers. All collections occurred after written informed consent of the mother, patient or volunteer as per Case Western Reserve University and Cleveland Clinic IRB approved protocols. Anonymized clinical hematopathology data was associated with patient samples.
Isolation of CD34+ cells
CD34+ cells from umbilical cord blood or bone marrow aspirates were purified using a magnetic cell sorting system (CD34 MicroBead Kit #130-046-702, Miltenyl Biotec Inc, Auburn, CA) according to manufacturer instructions. The purity of the CD34+ population (typically from 95 to 99%) was determined by flow cytometry with a FITC-conjugated monoclonal antibodies against CD34 (Clone 581, Beckman Coulter, Miami, FL, USA).
AML cells analyzed
Three types of AML cells were analyzed – (i) p53 wild-type MLL-AF9 cells were generated as described (34). These cells have a gene-expression profile similar to primary human MLL-AF9 leukemia cells (34), and self-renew indefinitely both in vitro and in vivo, initiating invasive AML in transplanted mice (34). (ii) p53-null THP1 cells were purchased from ATCC (Manassas, VA). This morphologically monocytoid AML cell line (M5 morphology) contains an MLL-AF9 fusion and is homozygously mutated at the TP53 and CDKN2A loci. The cells used for xeno-transplantation were transfected to express luciferase. (iii) Primary (fresh) AML cells from a patient with relapsed/refractory AML. These cells had myelomonocytic morphology (M4) and contained t(8;18)(q22:q23) and t(11;13)(q21:q12).
Human hematopoietic cell culture
Normal human hematopoietic cells and p53 wild-type MLL-AF9 cells were cultured in IMDM supplemented with 10% fetal bovine serum and 10ng/ml of the following human cytokines: stem cell factor (SCF), FLT3 ligand (FLT3), thrombopoietin (TPO), interleukin-3 (IL-3) and interleukin-6 (IL-6). THP1 cells were cultured in RPMI 1640 media without cytokine supplementation.
Treatment of cells with decitabine
Decitabine stock solution (5 mM) was generated by reconstituting lyophilized decitabine in 100% methanol. Stock solution was stored at −20 °C for up to 3 weeks. Similar amounts of methanol are added to untreated control cells. For in vitro experiments, cells were treated with decitabine (0.5 µM) on day 1 and 4 unless otherwise specified. For in vitro treatment followed by transplantation of cells into mice by tail-vein injection, cells were treated with decitabine 0.5 µM on day 1, 0.2 µM on day 2, 0.5 µM on day 5, 0.2 µM on day 6, and transplantation on day 7. This alternating schedule was used to increase in vitro decitabine exposure of the normal and leukemia cells without exceeding a decitabine concentration of 0.5 µM (since it was possible that up to 30% of the previous day decitabine could be present in the culture media after 24 hours (35;36)).
Apoptosis detection
Apoptosis was detected by Annexin-V and 7AAD (or PI) co-staining using the APOAF commercial kit (Sigma).
Clonogenic progenitor assays
p53 wild-type and p53 null MLL-AF9 cells in liquid culture were treated with decitabine or cytarabine 0.5 µM on day 1 and 4. On day 5, identical numbers of cells from vehicle and decitabine treated cultures were plated in decitabine free-semisolid media (MethoCult H4434, Stem Cell Technology, 2000 cells/ml). Ten days after plating, colony-forming units (CFU) were identified by morphology and counted under an inverted microscope.
SDS-PAGE and Western Blotting
Approximately 100 µg of cytoplasmic and nuclear protein extracts from cells, together with molecular weight markers, were subjected to SDS-PAGE on 4–12% gradient gels (Invitrogen) followed by transfer to PVDF membranes (Invitrogen). Blots were probed using antibodies for DNMT1 (Abcam ab16632), Phospho-p53 (Cell Signaling #9286), p53 (Sigma P6874), p15 (Cell Signaling #4822), p21 (Cell Signaling #2946), p16 (Santa Cruz Biotech sc-81613 ; Cell Signaling #4824), CEBPα (Santa Cruz Biotech sc-166258), CEPBε (Santa Cruz Biotech sc-25570, PU.1 (Santa Cruz Biotech sc-352), p27 (Cell Signaling #3686) and anti-β-Actin peroxidase (Sigma-Aldrich #A3854).
Murine studies
All experiments were approved by the Cleveland Clinic and Cincinnati Children’s Hospital Medical Center Institutional Animal Care and Use Committees (IACUC). Cultured normal HSC, MLL-AF9 cells, p53-null MLL-AF9 cells (THP1) cells or fresh patient bone marrow AML cells were transplanted by intravenous injection into non-irradiated 6–8 week old NOD/SCID or NSG mice. Mice were anesthetized with isofluorane before transplantation. By extrapolation from previous studies of decitabine pharmacokinetics in mice, a dose of decitabine 0.2 mg/kg was selected, for the objective of decitabine peak plasma concentrations lower than 0.2 µM. Animals were checked daily and were euthanized by an IACUC approved method for signs of distress. Bone marrow was analyzed by flow-cytometry, Giemsa-stain and Western blot. The proportion of human hematopoietic cells in bone marrow was determined by positive staining with PC5-conjugated anti-human CD45 mAb (BD) with isotype-matched immunoglobulin as a control in all experiments. Livers and spleens were weighed and fixed. To anatomically localize THP-1cells in living mice, the substrate D-Luciferin (15 mg/ml D-luciferin in sterile PBS (Promega), was injected IP and mice were imaged after 10 minutes mice using an IVIS-200 CCD camera imaging system (Xenogen, Alameda,CA).
Correlation of KI67 gene expression with GI50
Quality controlled raw data (Affymetrix CEL files, SOFT files) from previously published experiments (GSE5846 (37)) were downloaded from Gene Expression Omnibus (GEO) datasets (www.ncbi.nlm.nih.gov/geo). KI67 gene expression data in 6 leukemia cell lines (CCRF-CEM, HL60, K562, MOLT4, RPMI8226, SR) was correlated with the decitabine concentration that produced 50% growth inhibition (GI50) (data from Developmental Therapeutics Program of the NCI [http://dtp.nci.nih.gov/index.html]). Scatter plots, Spearman and Pearson correlation coefficients were generated using SAS statistical analysis software.
Equimolar decitabine or cytarabine in p53 wild-type MLL-AF9 cells
Identical concentrations of decitabine and cytarabine (cytidine analogues metabolized through the same nucleotide pathways) were added to p53 wild-type MLL-AF9 AML cells (34). Decitabine 0.5 µM depleted DNMT1 (figure 1A) without causing significant apoptosis (figure 1B) (annexin staining quantified by flow-cytometry 24 hours after decitabine or cytarabine treatment). In contrast, an equimolar concentration of cytarabine caused substantial apoptosis (figure 1B). The decrease in DNMT1 protein in response to cytarabine (figure 1A) was likely secondary to apoptosis (DNMT1 levels are increased in actively proliferating cells), since cytarabine, unlike decitabine, does not directly bind and deplete DNMT1. Both decitabine and cytarabine 0.5 µM added on days 1 and 4 decreased AML cell proliferation (figure 1C). Colony formation in methyl-cellulose is an assay for stem and progenitor cell activity. Both decitabine and cytarabine substantially decreased colony formation by p53 wild-type MLL-AF9 cells (figure 1C). However, at day 4, only decitabine treated MLL-AF9 cells displayed morphologic changes of monocyte differentiation (increased cell size, decreased nuclear-cytoplasmic ratio, granulation and vacuolization of the cytoplasm) (figure 1D). Cytarabine treated cells were small and disrupted, suggesting apoptosis and necrosis (figure 1D). Both decitabine and cytarabine treatment increased expression of the monocyte marker CD14 (measured by flow-cytometry on day 4), although the increase produced by decitabine was greater (mean fluorescence intensity DAC 7.85, cytarabine 6.44, vehicle 3.88), quantified by flow-cytometry 96 hours after decitabine or cytarabine treatment) (figure 1E). Neither drug increased expression of the granulocyte marker CD11b.
Figure 1
Figure 1
Non-cytotoxic concentrations of decitabine (DAC) induce differentiation and terminate proliferation of p53 wild-type MLL-AF9 cells
Equimolar decitabine or cytarabine in p53-null MLL-AF9 cells
The effects of equimolar decitabine and cytarabine were then compared in p53-null MLL-AF9 AML cells (the THP1 AML cell line (38)). The concentration of decitabine used depleted DNMT1 without causing significant apoptosis (figure 2A, B). Unlike p53 wild-type MLL-AF9 cells, only decitabine treatment impaired proliferation and decreased colony formation, while cells treated with cytarabine continued to proliferate, after a small initial decrease (figure 2C). Similar to p53 wild-type cells, only decitabine treatment induced morphologic features of myeloid differentiation (decreased nuclear-cytoplasmic ratio, increased cell size, granulation and vacuolization of the cytoplasm). Cytarabine treated cells retained immature morphology (figure 2D). Decitabine treatment markedly increased expression of the granulocyte marker CD11b, with slight effects on CD14 expression. Cytarabine treatment did not affect these differentiation markers (figure 2E).
Figure 2
Figure 2
Decitabine (DAC), but not an identical regimen of cytarabine (AraC), terminated proliferation of p53-null MLL-AF9 cells (THP1 cells (38
Differential regulation of apoptosis and differentiation protein expression by decitabine and cytarabine
Key events associated with apoptosis and cell cycle exit are known; these include p53 serine-15 phosphorylation, upregulation of p53, p16/CDKN2A, and possibly p21/CDKN1A (reviewed in (39)). Myeloid lineage-commitment and differentiation requires lineage-specifying transcription factors such as CEBPα and PU.1 (reviewed in (40)). Late myeloid differentiation and cell cycle exit is associated with upregulation of the key late transcription factor CEBPε (4144) and p27/CDKN1B (p27) (3033), and possibly p21/CDKN1A and p15/CDKN2B (45;46). The regulation of these apoptosis and differentiation events by decitabine and cytarabine was examined in p53 wild-type and p53-null AML cells.
In p53 wild-type MLL-AF9 cells, cytarabine and to a lesser extent decitabine increased p53 serine-15 phosphorylation, p53 and p21/CDKN1A levels (figure 3A). p16/CDKN2A protein was not detected in these cells using two different antibodies (figure 3A), although p16 mRNA was detected (data not shown). With regard to differentiation events, in p53 wild-type cells, CEBPα protein was decreased by both drugs, whereas no change was detected in PU.1 levels. The most striking change was in CEBPε protein, which peaked at 72 hours after decitabine treatment, and p27/CDKN1B protein, which peaked 96 hours after decitabine treatment (figure 3A). Cytarabine had minimal effects on the expression of these key late differentiation proteins (figure 3A). Despite use of two separate antibodies from different manufacturers, we were unable to detect p15/CDKN2B protein. However, decitabine treatment did increase CDKN2B mRNA >2-fold measured by QRT-PCR (data not shown).
Figure 3
Figure 3
Decitabine (DAC) and cytarabine (AraC) differentially regulate apoptosis and differentiation proteins in p53 wild-type and p53-null MLL-AF9 cells
Similar to p53 wild-type cells, the most striking change in p53-null THP1 cells was a decitabine-induced increase in CEBPε and p27/CDKN1B protein levels (figure 3B). Cytarabine did not produce these effects (figure 3B). p21/CDKN1A levels were also increased by decitabine but not by cytarabine. CEBPα levels decreased with both decitabine and cytarabine, whereas PU.1 levels decreased only in decitabine treated cells. Neither p15 nor p16 mRNA nor protein were detected in the THP1 cells (figure 3B, data not shown).
Differential effect of decitabine on AML leukemia initiating cells and normal hematopoietic stem cells
Engraftment in an immuno-compromised murine host is a functional assay for both normal HSC and leukemia initiating cells (47;48). Normal CD34+ hematopoietic cells and p53 wild-type MLL-AF9 cells were treated with the identical regimen of decitabine 0.5 µM (days 1 and day 5) and decitabine 0.2 µM (days 2 and day 6) (the objective was to maximize in vitro exposure to decitabine but without reaching concentrations that produce early apoptosis). On day 7, equal numbers (3 × 105 cells each) of viable normal and MLL-AF9 cells were combined and transplanted into sub-lethally irradiated NOD/SCID recipient mice. The mice receiving the combination of mock treated normal and mock treated MLL-AF9 cells required euthanasia by week 6 and demonstrated extensive bone marrow engraftment with human leukemia cells (figure 4A, B, figure S1). Mice receiving the combination of decitabine-treated normal and decitabine-treated MLL-AF9 cells remained healthy and were sacrificed at week 13 (greater than twice the period of survival of the control group) (figure 4A, figure S1). These mice demonstrated normal human hematopoietic cell engraftment, comparable to that seen in mice receiving 4×106 normal human CD34+ cells without leukemia cells. Analysis of their BM showed no morphologic or flow-cytometric evidence of leukemia cell engraftment (figure 4B, figure S1).
Figure 4
Figure 4
Low concentration decitabine inhibits AML leukemia initiating cells (LIC) but spared normal HSC
Sensitivity of leukemia cell lines to decitabine inversely correlates with the growth fraction
Since decitabine is S-phase specific in its mechanism of action, sensitivity to decitabine treatment may relate to the fraction of the leukemia cell population that is proliferating (growth fraction) during treatment exposure (figure S2). KI67 is expressed only in cycling cells, and is used clinically to estimate growth fraction. Consistent with the importance of growth fraction to decitabine effects, in 6 leukemia cell lines, the concentration of decitabine that produced 50% growth inhibition (GI50) inversely correlated with KI67 expression (figure S3).
Better survival with non-cytotoxic decitabine than with cytotoxic cytarabine in murine xeno-transplant models of p53-null human AML
Since DNMT1 can be depleted at low doses that cause minimal or no measurable cytotoxicity(14;24;25;49;50), it is feasible to increase and distribute windows of drug exposure in order to capture AML cells entering S-phase at different points in time (figure S2). Also, for the objective of DNMT1 depletion with minimal cytotoxicity, sub-cutaneous (SC) administration could have advantages over intravenous (IV) or intra-peritoneal (IP) administration, by producing lower peak levels but longer half-life. Consistent with a non-cytotoxic mechanism of action of decitabine 0.2 mg/kg administered SC 1-2X/week for 8 weeks to non-transplanted NSG mice (n=4), there was no treatment associated cytopenia (figure S4A), and DNMT1 was depleted without an increased phosphatidylserine exposure in bone marrow cells (figure S4B, C), although a small increase in γH2AX (DNA repair marker) occurred (figure S4D).
Weekly SC decitabine and conventional cytotoxic cytarabine were then compared in a xeno-transplant model of p53-null human MLL-AF9 AML. Non-irradiated NSG mice were transplanted with 3×106 THP1 cells by tail vein injection. Starting at day 5 after transplant, mice were treated with vehicle (PBS), cytarabine 75 mg/kg/day IP for five consecutive days (to model conventional chemotherapy (51)), or decitabine 0.2 mg/kg SC 3X/week for 2 weeks then 2X/week for 2 weeks then 1X/week thereafter. Mice treated with decitabine had significantly longer median survival (>20% increase) than cytarabine and vehicle treated mice (median survival 51, 45, and 42 days respectively, Log-Rank p=0.0004) (figure 5A). In vivo luminescence imaging on day 28 of therapy demonstrated disseminated disease in vehicle treated mice and disease concentrated in the region of the liver in decitabine and cytarabine treated mice (figure 5B). This pattern was confirmed at the time of euthanasia: vehicle treated mice demonstrated disseminated tumor masses, but disease was concentrated in the liver in cytarabine and decitabine treated mice (figure 5C) (the liver, and to a lesser extent the spleen, express high levels of cytidine deaminase, the enzyme that rapidly metabolizes cytidine analogues). Similar results were seen when cytarabine was administered at the same low dose, route of administration and schedule as the decitabine (0.2 mg/kg SC 2X/week). Again, mice treated with decitabine had significantly better survival (median survival 48, 39 and 36 days respectively, Log-Rank p=0.0096) (figure S5A), and significantly lower extra-hepatic tumor burden, than cytarabine or vehicle treated mice (figure S5B). However, liver and spleen size and weight were significantly greater in decitabine compared to cytarabine and vehicle treated mice (organs and tumors were harvested at later time points in decitabine treated mice as indicated by the Kaplan-Meier curves) (figure S5C, D).
Figure 5
Figure 5
Better survival with non-cytotoxic decitabine (DAC) than with cytotoxic cytarabine (AraC) in a murine xeno-transplantation model of p53-null human AML
Better survival with non-cytotoxic decitabine than with cytotoxic cytarabine in a murine xeno-transplant model of refractory/relapsed human AML
To complement the above experiments in which AML cell lines were used, a xeno-transplant model was established using fresh AML cells from a patient with relapsed/refractory AML. These AML cells contained multiple chromosome abnormalities including a t(8;18)(q22:q23) and t(11;13)(q21:q12). Non-irradiated NSG mice were transplanted with 1×106 patient cells by tail vein injection. Starting at day 5 after transplant, mice were treated with vehicle (PBS), cytarabine 75 mg/kg/day IP for five consecutive days (51), or decitabine 0.2 mg/kg SC 3X/week for 2 weeks, then 2X/week for 2 weeks, then 1X/week thereafter. Mice treated with decitabine had significantly longer median survival (>100% increase) than cytarabine or vehicle treated mice (median survival 113, 56, and 50 days respectively, Log-Rank p<0.0001) (figure 6A). At euthanasia (at different time-points per the Kaplan-Meier plot), the bone marrow of all mice was replaced by human leukemia cells (figure 6B, figure S6A, B). Despite the later time point of harvest, spleens of decitabine treated mice were significantly decreased in size compared to cytarabine or vehicle treated mice (figure 6C, figure S6C). Unlike the THP1 cells, these primary AML cells did not demonstrate liver tropism (livers were not increased in size or weight at sacrifice).
Figure 6
Figure 6
Better survival with non-cytotoxic decitabine (DAC) than cytotoxic cytarabine (AraC) in a murine xeno-transplantation model of refractory/relapsed human AML
Both in vitro and in vivo, a DNMT1 depleting, but non-cytotoxic, dose and schedule of decitabine was nonetheless able to induce cell cycle exit in AML cells. The absence of early apoptosis or phosphorylation of p53, efficacy in p53- and p16/CDKN2A-null backgrounds, the major increase in CEBPε and p27/CDKN1B, increase in the myeloid membrane differentiation markers CD11b or CD14, and cellular differentiation, were consistent with p53-independent differentiation mediated cell cycle exit. Hence, this approach to treatment could provide a useful alternative or complement to conventional apoptosis-based therapy. The efficacy of this treatment in vivo against cytarabine resistant p53-null cells and primary cells from a patient with refractory/relapsed AML, supports the translational possibilities.
Why does DNMT1 depletion, or histone deacetylase inhibition, induce differentiation of AML cells? One insight comes from experiments with normal HSC. In normal HSC, DNMT1 depletion by shRNA or by decitabine maintains stem cell phenotype even in differentiation promoting conditions, by preventing repression of key stem cell genes by the differentiation stimuli (2629;52). However, after the repression of stem cell genes that occurs with lineage-commitment, decitabine can augment expression of late differentiation genes and accelerate differentiation instead (52). Therefore, baseline differentiation stage is a major determinant of the cell fate response to decitabine treatment. The earliest studies suggested that AML cells with leukemia initiating capacity (measured by xenotransplantation) had a surface phenotype resembling that of normal HSC (CD34+38−) (48;53). This suggested that AML cell populations might recapitulate the hierarchical structure of normal hematopoiesis, with a small sub-set of AML cells with a stem cell phenotype sustaining the bulk cell population (53). Recently, it has been reported that the antibodies used to sort for CD38+ cells can inhibit proliferation and might have technically influenced the earliest studies (54). Accordingly, in a number of other studies, AML initiating cells had a surface phenotype suggesting lineage-commitment (CD34+38+, CLL-1+, CD71+, CD90 -, c-Kit -) (5460). Cross-species barriers also impact leukemia or cancer initiating capacity (61). With use of more immuno-compromised mice, or mice which express human cytokines, AML initiating cells have surface features of lineage-commitment (6163). Differentiation absolutely requires and is driven by lineage-specifying transcription factors such as CEBPA. AML cells, including CD34+ and CD34+38− subsets express high levels of CEBPA, but relatively low levels of the key late differentiation driver CEBPE (submitted manuscript). Similarly, we have noted that the promoter CpG methylation profile of MDS and AML cells is consistent with partial differentiation. It could be the partial differentiation of AML cells at baseline, suggested by surface phenotype, lineage-specifying transcription factor expression and promoter CpG methylation patterns, contributes to the contrasting differentiation responses of normal HSC and AML cells to non-cytotoxic DNMT1 depletion.
Although this treatment can bypass the p53-dependence of conventional cytotoxic treatment, it is still limited by the pharmacologic properties of decitabine. The S-phase specific mechanism of action of decitabine was underlined by the correlation of AML cell line sensitivity with KI67 expression (a measure of growth fraction). Therefore, scheduling and duration of exposure is a critical determinant of treatment efficacy. However, decitabine is rapidly metabolized by ubiquitously expressed cytidine deaminase (rapid metabolism by cytidine deaminase, which is highly expressed in the liver, could explain why the liver was a sanctuary site for liver tropic THP1 cells from the effects of cytarabine and decitabine). Hence, the in vivo half-life of decitabine after IV push is in the order of minutes, compared to many hours in vitro (35;64). An obvious mechanism for treatment failure therefore is that some or many AML cells may complete S-phase while decitabine is absent in vivo. Since decitabine was originally developed to induce apoptosis in malignant cells (68), doses to treat AML were escalated to maximum tolerated levels (up to 80 mg/kg infused over 36–44 hours), requiring many subsequent weeks without treatment to allow for recovery from cytotoxic side-effects (64). A role for differentiation in decitabine-induced cell cycle exit of leukemia cells does not exclude a role for activation of apoptosis genes, anti-metabolite effects, and apoptotic cell cycle exit: these could be the dominant consequences of treatment in some malignant cells, and certainly with higher dose (19;50;6567). However, a decrease in the dose (to 15 mg/m2 infused over 3 hours 3X/day on day 1–3, repeated every 6 weeks) led to United States Food and Drug Administration (FDA) approval of decitabine as a treatment for MDS (69). A further decrease in the daily dose and administration more frequently (20 mg/m2 infused over 1 hour 1X/day on Day 1–5, repeated every 28 days, has further improved MDS treatment clinical results (69;70). The results here provide a biological rationale to continue this towards smaller dose and more frequent administration: very low drug levels are sufficient to deplete DNMT1, and the decrease in toxicity can be used to administer treatment 1-3X/week for months or years, to capture AML cells entering S-phase asynchronously, and decrease treatment-free intervals that allow unimpeded AML cell division (figure S2). Clinical trials in the hemoglobinopathies have shown that decitabine 0.2 mg/kg (~7.5 mg/m2) administered SC has non-cytotoxic DNA hypomethylating and differentiation modifying effects, and can be administered safely from 1–3 X/week (25).
These in vitro and in vivo results provide a rationale for adjusting in vivo dose, schedule and route of administration of decitabine to emphasize a non-cytotoxic, normal HSC sparing, p53-independent mechanism of action. Although pharmacologic barriers to optimal clinical translation remain, these can potentially be addressed through further pre-clinical and clinical investigation.
Supplementary Material
Suppl
ACKNOWLEDGEMENTS
We gratefully acknowledge the following gifts: Mary Laughlin and Nick Greco at the Abraham J and Phyllis Katz Cord Blood Foundation and Cleveland Cord Blood Center for cord blood samples; YS is supported by NIH (1R01CA138858, U54HL090513) and Dept. of Defense (PR081404). KPN and YS are supported by Scott Hamilton CARES Foundation.
Footnotes
Supplementary information accompanies the paper on the Leukemia website (http://www.nature.com/leu).
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