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Human leukemic stem cells, like other cancer stem cells, are hypothesized to be rare, capable of incomplete differentiation, and restricted to a phenotype associated with early hematopoietic progenitors or stem cells. However, recent work in other types of tumors has challenged the cancer stem cell model. Using a robust model of xenotransplantation based on NOD/SCID/IL2Rγc-deficient mice, we confirmed that human leukemic stem cells, functionally defined by us as SCID leukemia-initiating cells (SL-ICs), are rare in acute myelogenous leukemia (AML). In contrast to previous results, SL-ICs were found among cells expressing lineage markers (i.e., among Lin+ cells), CD38, or CD45RA, all markers associated with normal committed progenitors. Remarkably, each engrafting fraction consistently recapitulated the original phenotypic diversity of the primary AML specimen and contained self-renewing leukemic stem cells, as demonstrated by secondary transplants. While SL-ICs were enriched in the Lin–CD38– fraction compared with the other fractions analyzed, SL-ICs in this fraction represented only one-third of all SL-ICs present in the unfractionated specimen. These results indicate that human AML stem cells are rare and enriched but not restricted to the phenotype associated with normal primitive hematopoietic cells. These results suggest a plasticity of the cancer stem cell phenotype that we believe has not been previously described.
Leukemic stem cells (LSCs) were the first cancer stem cells described, and studies of LSCs have been instrumental in developing the definition of cancer stem cells (1). In 1997, Bonnet and Dick observed that only CD34+CD38– cells were able to reconstitute human acute myelogenous leukemia (AML) in nonobese diabetic mice with severe combined immunodeficiency (NOD/SCID mice) (2, 3). Based on these data, they suggested that LSCs are rare, capable of partial differentiation, and restricted to the immature phenotype associated with hematopoietic stem cells in normal blood differentiation. Subsequent work in other malignancies, also using the NOD/SCID mouse as a model, suggested similar conclusions for breast and colon cancers (4, 5). However, Quintana and colleagues recently reevaluated these results using NOD/SCID/IL2Rγcnull mice (6). In contrast to earlier results, they demonstrate that single melanoma cells, regardless of phenotype, can reconstitute the disease in this more immunocompromised mouse strain. This result has challenged the original concept(s) of cancer stem cell.
Over the last 15 years, immunocompromised mice, such as NOD/SCID mice, have been the model of choice to study morphological and biological characteristics of human AML and other cancers in vivo (3, 7, 8). For AML, however, the engraftment levels in NOD/SCID mice are frequently low, with typical levels ranging from 0.1% to 10% of the mouse BM (7). In addition, prolonged engraftment of leukemic cells in this breed of mice was limited by the development of spontaneous thymic lymphomas and a reduced life span (9, 10). Newer strains of mice engineered with targeted deletion of the β2-microglobulin gene within a NOD/SCID background have resulted in models with decreased NK cell function better suited for studying the progression of diseases such as human AML (11). More recently, reports have demonstrated that a targeted deletion in the γ-common chain in NOD/SCID mice (NSG mice) results in the elimination of residual NK cell activity and provides an improved environment for growth and development of human cells (12, 13). NSG mice are not prone to development of thymomas and have an increased lifespan (12). Engraftment of normal human blood cells is enhanced in these mice, and we and others have demonstrated that AML engraftment is enhanced in this model (14, 15). These observations suggest that the characteristics of the immunodeficient recipient may play an important role in our ability to reveal the functional potential of human LSCs.
The phenotypic characterization of normal and malignant human blood cells has evolved over many years. It was originally observed that selection for CD34+ cells enriched for normal HSCs (16). Subsequent observations showed this population could be further enriched by selecting for lineage-depleted (Lin–) and CD38– cells (17, 18). As noted, the original work on AML stem cells focused on the CD34+CD38– fractions of cells (19). AML cells frequently express markers of granulocytic or monocytic differentiation, although expression of these markers is variable within and between samples (20). The role of lineage depletion in enrichment of AML stem cells has not been previously described. Recent studies have suggested the need to reevaluate the phenotypic definition for LSCs. A recent report demonstrates that treatment of AML mononuclear cells with anti-CD38 antibodies prior to transplantation inhibits engraftment in NS mice, suggesting that CD38+ subsets may contain LSCs (21). Also, several groups have shown that treatment of mice with anti-CD44, anti-CD47, or anti-CD123 can inhibit growth of LSCs or their engraftment in NS mice (22–24). It is not clear whether these antibodies interfere with BM homing or stimulation of intracellular signaling or through Fc-mediated clearance of antibody-labeled cells (22). Furthermore, Taussig et al. have observed that both CD34– and CD34+ fractions from the majority of primary NPM1-mutated AML contained LSCs (25). Taken together, these results challenge the original phenotypic description of LSCs.
In this study, we demonstrate that human AML stem cells are rare (in contrast to melanoma stem cells) and phenotypically heterogeneous. Our characterization of a diverse set of AML specimens reveals that only a minority of the specimens are strongly positive for CD34 expression, while the majority show low CD34 expression. We have sorted AML cells based on lineage marker, CD34, CD38, and CD45RA expression and tested the capacity of these fractions to recapitulate the disease in NSG mice. All cell fractions demonstrated some ability to engraft, although results are variable from sample to sample. Quantitative analysis using limiting dilution analysis demonstrated that, although LSCs are found at the highest frequency in the Lin–CD38– fraction, they are not restricted to that fraction. This enriched but rare fraction contains only a minority of the total number of LSCs present in AML cells. The majority of LSCs are found in cell fractions with a more mature phenotype, i.e., expressing CD38 and lineage markers. Remarkably, CD38- and lineage-expressing LSCs can also reconstitute NSG mice with the phenotypic diversity of AML cells found in primary samples, suggesting that LSCs can either dedifferentiate or display lineage infidelity. These data suggest that LSCs are rare, heterogeneous, and may not necessarily arise from primitive hematopoietic cells.
We initially performed engraftment analysis on primary specimens from 11 different AML patients, representing multiple different French-American-British (FAB) subtypes (except M3), various karyotypes, and molecular features in terms of the mutational status of 8 genes known to be associated with AML (FLT3, NPM1, WT1, CEBPA, K-RAS, NRAS, IDH1, and IDH2) (Table (Table1).1). All specimens were capable of recapitulating the disease in NSG mice at 12–18 weeks after transplantation, as described previously (14). To determine the frequency of LSCs (functionally defined as SCID leukemia-initiating cells [SL-ICs]) in these specimens, we performed a limiting dilution analysis on unfractionated AML cells from 7 of these samples (Table (Table2).2). We injected 50,000 to 10,000,000 AML cells by tail vein injection into adult NSG mice and analyzed the engraftment level after 12–18 weeks after transplantation. The SL-IC frequency in unfractionated samples ranged from 1 SL-IC in 150,000 to 4,500,000 mononuclear cells, confirming that SL-ICs are rare and that the frequency varies broadly between patients (Table (Table2). 2).
To evaluate the diversity of AML cell phenotypes, we analyzed primary AML specimens for expression of cell surface markers used to enrich for normal BM stem cells and progenitors. We included lineage markers (as a cocktail of CD3, CD14, CD16, CD19, CD20, and CD56 to identify mature lymphocytes and myeloid cells), CD34, CD38, CD123, and CD45RA. These markers are used in normal BM to distinguish stem cells and primitive progenitors (Lin–CD34+CD38–) from more mature progenitors (CD34+CD38+), including common myeloid progenitors (CMPs) (CD34+CD38+CD45RA+CD123–) and granulocyte-monocyte progenitors (GMPs) (CD34+CD38+CD45RA+CD123+) (26). An example of such phenotyping using CD34+-enriched samples from normal BM is shown in Figure Figure11 (bottom row). We then studied the phenotype of 19 primary AML specimens, and we consistently found 3 distinct populations based on the expression of lineage markers: a lineage bright (Lin+) population composed of mature lymphocytes (mostly CD3+ and CD19+ cells), a population with low expression of lineage markers (Lindim), and a lineage-negative (Lin–) population (Figure (Figure1,1, first column). We further focused on the lineage dim and lineage-negative fractions to determine the pattern of CD34 expression. We observed that CD34 expression is highly variable between specimens (Figure (Figure1,1, second column). These AMLs were subdivided into 3 groups based on CD34 expression: (a) samples with a high level of CD34 expression, such as specimen 348, were the least frequent (21%, 4 out of 19 specimens); (b) those with dim CD34 expression, such as specimen 53, were the most common (47%, 9 out of 19); and (c) AMLs with no CD34 expression, representing 32% (6 out of 19) of the specimens evaluated. For each sample, the CD34 expression pattern was the same in the Lin– and Lindim fractions (Figure (Figure1,1, compare second and fourth columns). These results demonstrate that CD34 expression is highly variable among AML samples. Furthermore, since all the samples were capable of engrafting in NSG mice, our results indicate that, in 32% of the samples, SL-ICs did not express CD34. In contrast to CD34 expression, all the AML samples had a similar pattern of CD38 expression, with a majority of CD38+ cells in both Lin– and Lindim fractions (Figure (Figure1).1). Finally, we also characterized the expression of CD45RA and CD123 in the Lin–CD38+ fractions to evaluate the presence of cells with myeloid progenitor-like phenotypes (Figure (Figure1,1, third column). Regardless of their CD34 expression status, we observed a CD123+CD45RA+ population in all samples. Overall, these results illustrate the heterogeneity of phenotypes in AML samples. The absence of CD34 expression in some samples capable of engrafting in NSG mice led us to reevaluate and ask whether SL-ICs are completely restricted to the immature cell phenotype.
To determine whether SL-ICs were restricted to a population of cells that do not express lineage markers (Lin–), we first sorted Lin– and Lindim cells from 6 different primary AML samples and injected 0.1 × 106 to 4.3 × 106 cells per mouse (Figure (Figure2).2). To ensure that these and other sorted cells did not have contamination, postsorting cell purity was checked for all samples and averaged at least 95% pure (Supplemental Table 1; supplemental material available online with this article; doi: 10.1172/JCI41495DS1). Surprisingly, for each sample, both Lin– and Lindim fractions were capable of recapitulating the disease, demonstrating that SL-ICs are not only found in the rare Lin– fraction but also in the more abundant Lindim population. Interestingly, Lindim cells from samples 325 and 348 provided a higher level of leukemia engraftment than Lin– cells when injected at similar doses in NSG mice. This suggests that in these samples SL-ICs could be as frequent in the Lindim fraction as in the Lin– fraction. Overall, these data demonstrate that both Lin– and Lindim fractions contain SL-ICs, suggesting that expression of lineage markers associated with commitment and differentiation is not necessarily associated with a loss of LSC function.
Next, we examined whether SL-ICs were restricted to CD34+ cells in AML samples with high CD34 expression. In normal human hematopoiesis, SCID-repopulating cells (SRCs) are most abundant in the Lin–CD34+CD38– fraction, although rare SRCs have been reported in Lin–CD34– cells (18). As noted, only a minority of samples demonstrated robust CD34 positivity. These samples had few CD34– cells, making analysis of CD34– engraftment challenging. Nonetheless, 3 primary AML CD34+ specimens were sorted based on their CD34 expression. To isolate CD34 as a variable, we compared CD34–38– cells with CD34+CD38– cells as shown in Figure Figure1.1. Only 2 mice of 6 injected with CD34– cells showed a significant engraftment (higher than 0.1% of human cells in murine BM), consistent with the idea that, in the subset of AML samples with clear CD34+ staining, SL-ICs are depleted in the CD34– fraction (Figure (Figure3A).3A). As expected, 36 out of 37 mice injected with their CD34+ counterpart engrafted in mice (Figure (Figure3A).3A). To next determine whether CD34 staining is necessary for the LSC phenotype, we characterized the engraftment of CD34negative samples. In these samples, insufficient CD34+ cells are present to allow for separate analysis of engraftment of rare CD34+ cells from these patients. All mice injected with CD34negative specimens engrafted in NSG mice after 12 weeks after transplantation (Figure (Figure3B).3B). Taken together, these data suggest that, in a subset of AML samples with a clear CD34positive fraction of cells, CD34 staining enriches for SL-ICs. However, expression of CD34 is not necessary for engraftment potential. Rather, these data demonstrate the phenotypic heterogeneity of AML samples.
Although the phenotype of SL-ICs was originally described as CD38–, recent data showing that preincubation of AML cells with an anti-CD38 antibody can suppress engraftment led us to reevaluate whether SL-ICs are indeed restricted to CD38– cells (21). AML samples from 9 patients were sorted into CD38– and CD38+ fractions, and cells from each fraction were injected into NSG mice. As demonstrated in Figure Figure4A,4A, SL-ICs were not restricted to CD38– cells, as the CD38+ fraction tested was capable of recapitulating the disease in NSG mice. Remarkably, CD38+ cells provided levels of engraftment equal or superior to the levels observed with CD38– cells in 5 out of the 9 patients. These results may under-represent the engraftment potential of CD38+ cells to engraft, since Taussig et al. demonstrated that incubation of human AML cells with anti-CD38 antibodies, but not control antibodies, decreased engraftment (21). We confirmed this observation by incubating AML samples overnight with the anti-CD38 antibody (HIT2 clone). As shown by Taussig and colleagues, this incubation abrogates engraftment of both AML samples tested (Figure (Figure4B4B and ref. 21). Overall, these results demonstrate that SL-ICs are present in the CD38+ fraction of AML cells.
These results made us question whether there is a specific cytotoxic effect of the HIT2 anti-CD38 antibody or whether antibody labeling of AML cells generally decreases engraftment. We analyzed the impact of incubation of AML cells with an antibody cocktail (lineage, CD34, CD38, CD123, and CD45RA) used for sorting on engraftment levels in NSG mice (Figure (Figure4C).4C). In 4 patient samples, we observed that a 1-hour incubation with these antibodies significantly decreased the level of engraftment 12 weeks after transplantation. We next performed a limiting dilution analysis of 2 specimens (specimens 53 and 325) after incubation with these antibodies and observed that the frequency of SL-ICs was not affected (Supplemental Table 2). Taken together, these results suggest that incubation of AML cells with antibodies can qualitatively affect the level of engraftment (as evaluated 12 weeks after injection) but does not quantitatively affect SL-IC levels.
These results show that the use of antibodies impairs our ability to reveal the full potential of CD38-expressing SL-ICs, suggesting caution in interpreting quantitative studies aimed at determining the frequency of SL-ICs in such fraction. To explore this further, we studied whether CD38 expression is reversible and dependent on cell cycle status, as previously demonstrated in normal CD34+ cells by McKenzie et al. (27). While the expression of CD38 is highest in cells in G2/M in most samples, we did not observe a consistent difference in expression of CD38 between cells in G0 and G1 from 6 samples (Supplemental Figure 1). Overall, there does not appear to be a robust correlation of CD38 expression with cell cycling in AML cells.
Studies in murine models of leukemia have demonstrated that SL-ICs can be found in cell fractions with phenotypes associated with CMPs or GMPs. In humans, CMPs and GMPs express CD34, CD38, and CD123 and vary in expression of CD45RA. In AML samples with a clear CD34+CD38+ population, we further sorted cells based on CD45RA expression and analyzed their engraftment potential in NSG mice. As shown in Figure Figure5,5, in 4 patients, SL-ICs could be detected in both CD45RA+ and CD45RA– fractions, indicating that, within the CD34+CD38+ fraction, SL-ICs are found in both CMP-like and GMP-like cells. Furthermore, SL-ICs were also found in both CD45RA+ and CD45RA– fractions from 1 AML specimen, which is CD34negative sample 325. Thus, similar to murine models of leukemia, SL-ICs can be found in phenotypic CMPs and GMPs in human AML.
To determine whether each engrafting fraction could reconstitute the phenotypic heterogeneity of the original AML sample, we compared the phenotypes of the AML cells before and 12 weeks after transplantation. We observed that each sorted fraction was capable of reconstituting the mice with AML cells with the same phenotypic diversity seen in the unsorted primary AML samples (see a representative example with sample 325 in Figure Figure6).6). For example, Lin–CD38– cells (Figure (Figure6,6, A and B) injected into mice gave rise to Lin–CD38– (Figure (Figure6,6, C and D), Lin–CD38+ (Figure (Figure6,6, C and D), and Lin+ cells (Figure (Figure6,6, C–E) at 12 weeks after transplantation. Interestingly, LindimCD38+ cells (Figure (Figure6,6, A–F) gave rise to both LindimCD38+ cells (Figure (Figure6,6, G–I) and Lin–CD38– cells (Figure (Figure6,6, G and H) after 12–16 weeks. Moreover, these 2 populations arising from LindimCD38+ cells represent approximately the same percentages of total AML cells in the primary sample and at 12 weeks after transplant. These results demonstrate that each cell fraction tested for engraftment in NSG mice could closely recapitulate the phenotypic diversity of AML cells observed in primary samples, fulfilling one of the criteria of a LSC.
Next, we used transplantation into secondary NSG recipients to assess the self-renewal capacity of SL-ICs in different sorted fractions from 5 samples. All engrafting subsets from primary recipients were capable of engraftment in secondary recipients (Table (Table3),3), showing that the sorted fractions contained SL-ICs capable of both recapitulating the phenotypic heterogeneity of the primary AML and self-renewal. For 3 cases (sample 53 [with the mutations FLT3-ITD, NPM1c, WT1 exon 7], sample 325 [with the mutations FLT3-TKD, NPM1c, IDH1 R132S], and sample 973 [with the mutations FLT3-ITD, NPM1c, WT1 exon 7]), we were able to check the presence of mutations in sorted cell fractions from primary and secondary NSG recipients (Supplemental Table 3). For samples 53 and 973, the 3 mutations were present in every sorted fraction tested. For sample 325, only the IDH1 R132S and NPM1c mutations were still present in all sorted fractions of patient sample and engrafted mice recipients. In contrast, the FLT3-TKD mutation in this case was uniquely present in sorted fractions coming from the primary recipient but was absent in all fractions of the secondary recipient, suggesting that in this 1 sample, expression of mutant Flt3 is not necessary for a stem cell phenotype. The ability to reconstitute animals long term after secondary transplantation, along with the ability to develop a diverse phenotype that recapitulates the original disease phenotype, ensures that the cell fractions studied in these experiments represent bona fide SL-ICs and not transient populations.
To determine whether SL-ICs are preferentially enriched in specific fractions, we used cells from sample 53 to perform a limiting dilution analysis on 4 fractions based on lineage and CD38 expression followed by injection in NSG mice (Table (Table4).4). The frequency of SL-ICs in each fraction was calculated using regression analysis (L-Calc). We observed that Lin–CD38– cells contained the highest frequency of SL-ICs (1 in 38,030 cells) compared with that of LindimCD38– cells (1 in 372,259 cells) and Lin–CD38+ cells (1 in 345,807 cells). The fraction with the lowest frequency of SL-ICs was LindimCD38+ (1 in 1,023,815 cells). In comparison, the frequency of SL-ICs in unfractionated cells was 1 in 430,240 (Table (Table2).2). This demonstrates that SL-ICs are indeed enriched in the Lin–CD38– fraction in this sample. Considering that the incubation of AML cells with an anti-CD38 antibody can decrease engraftment in NSG mice, the frequency of SL-ICs in both CD38+ subsets may be underestimated. We used the SL-IC frequency and the percentage of the total cells found in each phenotype to calculate the absolute numbers of SL-ICs associated with each fraction for specimen 53. For instance, Lin–CD38– cells contain the highest frequency of SL-ICs (1 in 38,030 cells), with 11-fold enrichment compared with that of the unfractionated sample (Supplemental Table 5). However, Lin–CD38– cells represent only 3% of all mononuclear cells in patient 53 (Figure (Figure7,7, top bar). Normalizing to 100 SL-ICs, we determined that, in spite of having the highest frequency of SL-ICs, the Lin–CD38– fraction contains only 34% of all SL-ICs (Figure (Figure7,7, bottom bar). In comparison, the LindimCD38+ fraction contains the lowest frequency of SL-ICs, but it is the most represented fraction in patient 53 (61% of cells; Figure Figure7,7, top bar) and contains 25% of all SL-ICs (Figure (Figure7,7, bottom bar). Overall, the CD38+ and Lindim fractions contain 29% and 62% of all SL-ICs, respectively. Assuming that we sort each fraction from 100 × 106 cells (containing 332 SL-ICs at the frequency of 1:430,240), Lin–CD38– fraction will contain 61 × 106 total AML cells and 79 SL-ICs at the frequency of 1:38,030 (Supplemental Table 4). Thus, the total number of SL-ICs summed from all sorted fractions is 236 SL-ICs (e.g., 71% of the total number of SL-ICs presorting; Supplemental Table 4). These data demonstrate that SL-ICs are widely distributed throughout different phenotypes and that the absolute distribution of LSCs does not correlate with immunophenotypic distribution (Figure (Figure7).7). Importantly, at least one-third of SL-ICs detected in the NSG model are found in CD38+ fractions previously described as devoid of LSC activity.
Of note, we had several cell doses for Lin–CD38– and Lin–CD38+ subsets from 4 additional specimens, although we were not able to do a complete LDA on these samples (Supplemental Table 5). This data allowed us to approximate the SL-IC frequency in several fractions of these samples. We observed the highest frequency of SL-ICs in Lin–CD38– in 1 sample (sample 973), similar frequency in both fractions in 1 sample (sample 348), and the lowest frequency in Lin–CD38– from a 3rd sample (sample 258). Although not conclusive, this data suggests that the degree of enrichment of SL-ICs in the immature, Lin–CD38– fraction, as assayed in the NSG mouse, may be highly variable. Overall, our results indicate that in AML, LSCs are rare, heterogeneous in phenotype, and may be distributed through multiple compartments of AML cells.
In this study, we have reexamined the characteristics of LSCs in human AML using the NSG xenotransplantation model. Recent results from our laboratory have demonstrated enhanced engraftment of primary AML specimens in NSG mice compared with that in NOD/SCID mice, suggesting that the functional assay used to measure LSCs may be more sensitive in the NSG model than in the NOD/SCID model (14). In spite of this enhanced sensitivity, our quantitative analysis of SL-IC frequency in a diverse group of 7 AML patients shows that LSCs are rare cells within AML samples (range, 1 in 0.15 × 106 to 4.1 × 106 LSCs). The rarity of SL-ICs in AML has been a consistent finding regardless of the strain of immune-deficient mice used over the past 15 years. Lapidot et al. used SCID mice to estimate the frequency of SL-ICs at 1 in 2.5 × 105 (19). When NOD/SCID mice were used, SL-IC frequencies ranged from 1 SL-IC in 104 cells to 1 in 1.4 × 107 cells (3, 7). Overall, these results indicate that the use of increasingly immunodeficient and permissive mouse strains to assay AML-initiating cells is not associated with an increase in the frequency of SL-ICs. This is in contrast with a recent report on human melanoma, showing that the use of NSG mice instead of NOD/SCID mice increased the frequency of tumorigenic cells by several orders of magnitude (6). These contrasting results between AML and melanoma in NSG mice could reflect the fact that the microenvironment in this strain is particularly favorable to melanoma cell growth. Human AML stem cells remain a rare population of cells.
We demonstrate that the phenotype of LSCs is heterogeneous and not restricted to the immature phenotype CD34+CD38– as originally described by Bonnet and Dick (3). We report here that for each sample evaluated SL-ICs are consistently found in both Lin– and Lindim fractions, indicating that the transition to lineage marker expression is not necessarily associated with a loss of capacity to initiate AML. Remarkably, we found that none of the cell surface markers (Lin, CD34, CD38, CD45RA, and CD123) used to identify hematopoietic stem cells and myeloid progenitors in normal BM could be used to consistently segregate AML-initiating and self-renewing cells. The heterogeneity in CD34 and CD38 expression within and between AML specimens has been previously reported (28). Interestingly, the 3 specimens (specimens 245, 325, and 878) devoid of CD34+ cells engrafted well in NSG mice, indicating that AML-initiating cells do not necessarily express CD34. We found that, in specimens containing both CD34+ and CD34– cells, SL-ICs could be found in both fractions, as reported by Terstappen et al. (17) and Blair et al. (28). At this time, we can not directly address whether the difference between our results and the original model proposed by Bonnet and Dick is a consequence of the switch to the NSG mouse model for xenotransplantation or the heterogeneity of the disease, since we have not tested the AML fractions studies here for engraftment in NOD/SCID animals.
Taussig et al. recently reported that CD34+CD38+ cells can recapitulate AML in NSG mice, but they did not evaluate the self-renewal capacity of these cells (21). We demonstrate that both CD38– and CD38+ fractions contain SL-ICs for all 9 samples evaluated. In addition, we report that CD38+ cells are capable of self-renewal as revealed by long-term AML engraftment in secondary recipients and, importantly, that CD38+ cells will reconstitute CD38– cell populations. Thus, we have demonstrated that CD38+ cells meet the formal criteria for SL-ICs. Interestingly, in 5 out of 9 AML samples, the CD38+ fractions provided equal or superior engraftment levels compared with those obtained with CD38– fractions (using comparable injected cell numbers). This is particularly remarkable, considering that we, and others, have shown that anti-CD38 antibodies can decrease or even inhibit AML engraftment (21). Given this, our studies may underestimate the frequency of SL-ICs in CD38+ AML cell fractions.
In this report, we provide the first quantitative evaluation of the SL-ICs distribution as a function of cell surface phenotype. Our data and others indicate that SL-ICs may be most enriched in the Lin–CD34+/dimCD38– fraction. However, this fraction represents a small percentage of all AML cells in individual samples. We isolated 4 fractions based on Lin and CD38 expression and used limiting dilution analysis to determine the frequency and absolute numbers of SL-ICs found in each fraction. We found that, in one sample, 71% of all SL-ICs do not express CD38 and 29% of all AML-initiating cells reside in the CD38+ fraction. These results show that self-renewing SL-ICs with previously unrecognized phenotypes can represent a substantial portion of all SL-ICs in a patient. This has important implications for the development of curative therapies.
This study does not address the important question relating to the nature of the cell responsible for initiating AML. The phenotypic heterogeneity of SL-ICs and, in particular, our characterization of SL-ICs with myeloid progenitor-like phenotypes strengthen the concept that AML-initiating cells are not necessarily derived from hematopoietic stem cells as initially hypothesized (3). It remains unclear whether SL-ICs can originate directly from the transformation of committed myeloid progenitors, as shown in mouse models. Alternatively, SL-ICs could originate first from normal hematopoietic stem cells and then, as a secondary event, from preleukemic progenitors acquiring self-renewal capacity (29).
The data described here present a fundamental challenge to the LSC model as it was originally proposed. The original model described a binary model of tumor heterogeneity in which there were cells capable of tumor reconstitution in a NOD/SCID mouse (stem cells) and cells that had no capacity for tumor reconstitution (Figure (Figure8,8, top). Furthermore, LSCs were proposed to reside only in the immature compartment of hematopoietic cells, suggesting that limited differentiation within tumor cells recapitulated normal hematopoietic differentiation. In contrast, our results demonstrate that cells with features resembling a more mature hematopoietic cell can reconstitute a leukemia within the more sensitive NSG mouse model. There are 3 possible explanations. It is possible that the original model is correct in that there are cells with tumor reconstitution potential and cells with no tumor reconstitution potential. However, the tumor-reconstituting cells are not phenotypically the same as normal HSCs but are marked by an as yet undescribed cell marker (Figure (Figure8,8, missing marker model). Alternatively, in many models, as assays have improved, it has become clear that leukemic cells with phenotypic features of transit amplifying cells have some level of self-renewal capacity. Thus, it is possible that AML cells do have limited differentiation that recapitulates normal myelopoiesis in some aspects, but the loss of stem cell potential that normally accompanies acquisition of lineage-specific markers is attenuated (Figure (Figure8,8, modified differentiation model). Thus, as described in a murine model system, leukemic cells may simultaneously have features of differentiated progenitor cells and stem cells. The third alternative is that the stem cell model is fundamentally incorrect and that, in fact, all tumor cells retain the potential for tumor regeneration (Figure (Figure8,8, tumor plasticity model). Proof of the first hypothesis would rest on discovery of an improved LSC marker and quantitative proof that selection for such a marker enhances for LSCs. Discrimination of the latter theory will require further quantitative analysis of engraftment potential in defined cell populations, which do or do not express differentiation markers. If the pattern is consistent that engraftment potential decreases with acquisition of lineage-specific markers, this would favor the hypothesis that leukemic maturation mirrors normal myelopoiesis but with a delayed loss of stem cell potential. On the other hand, if other AML samples actually demonstrate increased stem cell potential in populations expressing differentiation markers, this would suggest that leukemic cells do not recapitulate normal differentiation but are in a neomorphic state characterized by aberrant regulation of expression of differentiation markers. This type of plasticity is similar to that recently described for chemotherapy resistant cancer cells. Sharma et al. recently demonstrated that in cancer cell lines, chemotherapy resistance can track as a reversible trait secondary to epigenetic changes in cells over time (30). The discrimination between the 2 latter models may be dependent on the disease progression and treatment. At diagnosis, the stem cell model will fit with the modified differentiation model, while after chemotherapies, the stem cell theory will follow the tumor plasticity model. Further work should clarify these 2 latter models, but both models are in contrast to the original stem cell hypothesis, which completely restricted leukemic reconstitution potential to the immature cell fraction.
AML samples were obtained from the Stem Cell and Xenograft Core Facility at the University of Pennsylvania School of Medicine. Samples were obtained from patients presenting with acute myeloid leukemia at the Hospital of the University of Pennsylvania. Informed consent was obtained under a protocol reviewed and approved by the Institutional Review Board at the University of Pennsylvania. Leukopheresis samples were frozen in fetal calf serum with 10% DMSO and stored in liquid nitrogen. Samples that had previously shown high engraftment capability were chosen for this study (14). FAB or WHO classification and cytogenetics in AML samples were determined at time of diagnosis by the Laboratory of Pathology and Medicine at the Hospital of the University of Pennsylvania. Each collection was immunophenotyped using the following antibody panel: FITC-conjugated lineage cocktail 1 (CD3, CD14, CD16, CD19, CD20, and CD56), APC-conjugated anti-CD38, APC-Cy7-conjugated anti-CD45, PE-conjugated anti-CD44, PE–Texas Red–conjugated anti-CD33, PE-Cy5-conjugated anti-CD123, PE-Cy5.5-conjugated anti-CD34, and PE-Cy7-conjugated anti-CD45RA. All antibodies were purchased from BD Biosciences or Invitrogen. Analyses were performed on a BD Life Science Research II (LSR II) flow cytometer after cells were resuspended in a DAPI solution.
The mutational status of 8 genes (FLT3, NPM1, WT1, CEBPA, KRAS, N-RAS, IDH1, IDH2) was analyzed by high-resolution melting (HRM) methods (Table (Table1).1). DNA mutation screening of FLT3-TKD exon 20, IDH1 and IDH2 exon 4, N-RAS and KRAS exons 2 and 3, and WT1 exons 7 and 9 was performed by HRM PCR with the use of LightCycler 480 in High Melting Resolution Master Mix 1X (Roche Applied Science), with 10 ng genomic DNA, 0.1 μmol/l of each primer (see below), and 25 mmol/l MgCl2. HRM PCR cycling conditions were initial denaturation at 95°C for 10 minutes, followed by 50 cycles at 95°C for 10 seconds, 50 cycles at 63°C for 15 seconds, and 50 cycles at 72°C for 25 seconds. Melting curve was measured from 72°C to 95°C, with 25 acquisitions per degree centigrade. Primer sequences are as follows: FLT3_X20_F2, TCACAGAGACCTGGCCGC; FLT3_X20_R1, TGCCCCTGACAACATAGTTGG; IDH1_X4_F1, GGCTTGTGAGTGGATGGGTAA; IDH1_X4_R2, GCATTTCTCAATTTCATACCTTGCTTA; IDH2_X4_F1, GAAAGATGGCGGCTGCAGT; IDH2_X4_R3, TGTTTTTGCAGATGATGGGC; NRAS_X2_F2, CTGATTACTGGTTTCCAACAGGTTCT; NRAS_X2_R2, TGGGTAAAGATGATCCGACAAGT; NRAS_X3_F1, TTGTTGGACATACTGGATACAGCTG; NRAS_X3_R1, CATTTCCCCATAAAGATTCAGAACAC; KRAS_X2_F4, GGCCTGCTGAAAATGACTGAA; KRAS_X2_R4, AATTAGCTGTATCGTCAAGGCACTC; KRAS_X3_F2, TCCCTTCTCAGGATTCCTACAGG; KRAS_X3_R2, ACAGGGATATTACCTACCTCATAAACATT; WT1_X7_F2, CCCTCAAGACCTACGTGAATGTT; WT1_X7_R2, GGAGCTCTTGAACCATGTTTGC; WT1_X9_F1, TAGGGCCGAGGCTAGACCTT; and WT1_X9_R1, TCTCATCACAATTTCATTCCACAATA. FLT3 exon 13 ITD and NPM1c mutation screening were performed using a multiplex PCR using Gold Taq DNA polymerase (Applied Biosystems) and the following primers: HsNPM1_X12_F1, 5′-GAAGTGTTGTGGTTCCTTAAC; HsNPM1_X12_R1FAM, 5′(FAM) TGGACAACACATTCTTGGCA; FLT3_NEM_E, 5′ TGGTGTTTGTCTCCTCTTCATTGT 3′; and FLT3_NEM_Qned, 5′(NED) GTTGCGTTCATCACTTTTCCAA 3′. PCR products were analyzed on a sequencer using sizing fragment analysis. CEBPA screening was performed according to Pabst et al. (31).
Animals were used in accordance to a protocol reviewed and approved by the Institutional Animal Care and Use Committee of the University of Pennsylvania. NOD/LtSz-scid IL-2Rγchainnull mice were produced at the University of Pennsylvania using breeders obtained from The Jackson Laboratory. Mice were housed and human primary AML cells were transplanted as reported previously (14). BM (mixed from tibias and femurs) and spleen were dissected in a sterile environment, flushed in PBS, and made into single cell suspensions for analysis by flow cytometry (FACS Calibur, BD) using FITC-conjugated anti-CD2, PE-conjugated anti-CD33, PerCP-Cy5.5-conjugated anti-CD19, and APC-conjugated anti-CD45 (all antibodies from BD) as well as using the LSR panel outlined above.
Specific cell doses of 7 primary AML samples, ranging from 5 × 104 to 10 × 106 cells, were injected into at least 3 NSG mice per dose. Twelve to eighteen weeks after transplantation, the BM and the spleen were assessed for the engraftment. An engraftment criterion of more than 0.1% of human CD45+CD33+ in murine BM mononuclear cells assessed by flow cytometry was used as the biologically significant cutoff. The frequency of SL-ICs was calculated using Poisson statistics with the L-Calc Software for limiting dilution analysis (version 1.1; StemCell Technologies).
Eight primary AML patient samples were stained with FITC-conjugated lineage cocktail 1 (CD3, CD14, CD16, CD19, CD20, and CD56), APC-conjugated anti-CD38, PE-conjugated anti-CD123, PE-Cy5.5-conjugated anti-CD34, and PE-Cy7-conjugated anti-CD45RA, before resuspension in a DAPI solution of PBS containing 2% FBS. Sorting was performed on a BD FACS Vantage SE/DiVA cell sorter, equipped with 3 lasers and 8 fluorescence detectors. High-speed cell sorting was performed within a BSL3 laboratory. Live gates were set up to exclude nonviable cells and debris with DAPI, and the forward scatter lineage-negative gate was defined as 5% of the live cell population expressing lineage markers at the lowest level. Purity checks were performed to ensure sort quality. The purities of the Lin–, Lindim, CD38–, CD38+, Lin–CD38–, Lin–CD38+, LindimCD38–, and LindimCD38+ fractions were 96.7% ± 2.1%, 96.2% ± 0.5%, 97.8% ± 1.9%, 95.9% ± 2.2%, 97.8% ± 1.2%, 95.9% ± 1.8%, 96.1% ± 2.0%, and 96.8% ± 1.5%, respectively (Supplemental Table 1). Highly purified subpopulations of 0.1 to 4 million cells were then injected into NSG mice. For 1 primary AML sample (sample 53), a LDA was performed on the 4 purified subpopulations of cells as well as the unprocessed cells. 1 × 104 to 5 × 106 cells were injected into 2–5 NSG mice. Nine to eighteen weeks after transplantation, the BM and the spleen were assessed for the engraftment. The frequency of SL-ICs was determined as described above.
Mononuclear cells from 1 AML patient sample (sample 53) were incubated overnight in fully supplemented endothelial growth medium (EGM-2; Lonza) at 37°C with anti-CD38 antibody (clone HIT2; BD) and isotype control (IgG1, clone MOPC-21; Sigma-Aldrich). After incubation, a 50-μl aliquot of each cohort was used to analyze the cell viability and the immunophenotypical frequency by LSR II flow cytometer using DAPI, FITC-conjugated lineage cocktail 1 (CD3, CD14, CD16, CD19, CD20, and CD56), APC-conjugated anti-CD38, APC-Cy7-conjugated anti-CD45, PE-conjugated anti-CD44, PE–Texas Red–conjugated anti-CD33, PE-Cy5-conjugated anti-CD123, PE-Cy5.5-conjugated anti-CD34, and PE-Cy7-conjugated anti-CD45RA. The cell suspensions were centrifuged, resuspended in PBS containing 2% FBS, and injected into 5 irradiated NSG mice. Twelve weeks after transplantation, the BM and the spleen were assessed for engraftment by FACS analysis.
Adult mice (8–10 weeks old) were sublethally irradiated with 250 cGy total body irradiation 24 hours prior to secondary transplantation. Engrafted BM samples were lysed with 0.8% ammonium chloride solution (StemCell Technologies), washed twice in PBS containing 2% FBS, and suspended in 200 μl PBS containing 2% FBS at a final concentration of 1 to 10 million human CD45+CD33+ viable cells from BM of primary recipients per mouse for intravenous injection. Twelve to eighteen weeks after transplantation, the BM and the spleen were assessed for the engraftment.
Previously described methods were used with minor modifications (27, 32). Cryopreserved cells were thawed and 1 million of viable cells were incubated at 37°C (27) for 60 minutes in 1 ml Hanks buffered solution with 2% FBS and Hoechst 33342 at 5 μg/ml in presence of 100 μM verapamil. Pyronin Y was then added to a final concentration of 1 μg/ml, and incubation continued for another 30 minutes. Cells were washed in Hanks buffered solution with 2% FBS; then stained with 7AAD, FITC-conjugated lineage cocktail 1 (CD3, CD14, CD16, CD19, CD20, and CD56), APC-conjugated anti-CD34, APC-Cy5.5-conjugated anti-CD38, PE-Cy7-conjugated anti-CD45; and analyzed by LSR II flow cytometer (Becton Dickinson).
We assessed the statistical analysis of the difference between 2 sets of data using nonparametric Mann-Whitney U test. P values of less than 0.05 were considered to be significant.
We would like to thank Charles (Hank) Pletcher and Paul Hallberg from the University of Pennsylvania Flow Core for invaluable help. Thanks to the many colleagues who have assisted with the development of this project. M. Carroll is supported in part by the United States Veterans Administration. This work was supported in part by Sanofi-Aventis. P.V. Sanchez is supported by NIH grant KO1-CA-129151-01; R. Perry is a fellow of the St. Baldric’s Foundation and is supported in part by NIH grant K12CA07693 and an ASCO Young Investigator Award.
Conflict of interest: Martin Carroll has received research support from Sanofi-Aventis. G. Danet-Desnoyers receives research support from Centocor Research and Development Inc. Christian Recher has received consultation fees from Celgene Corporation and Genzyme Corporation.
Citation for this article: J Clin Invest. 2011;121(1):384–395. doi:10.1172/JCI41495.