To the Editor:
Clonal diversity plays a key role in poor therapeutic outcomes in acute myeloid leukemia (AML) and myeloproliferative neoplasm (MPN) patients [1, 2]. Therefore, targeting all clones is required to eradicate these diseases. To achieve this goal, we integrated genetic clonal landscape of individual patient samples with the response to DNA double-strand break repair (DSBR) inhibitors to track individual clones’ sensitivity to these drugs. We decided to target DSBR pathways because AML and MPN accumulate high numbers of DSBs, the most lethal of all DNA lesions resulting from altered metabolism [3, 4]. Thus, survival and proliferation of AML and MPN cells depend on DSBR mechanisms which represent a promising targetable vulnerability (Supplementary Fig. S1) [5].
We reported that AML/MPN - associated somatic mutations, e.g., FLT3(ITD) and JAK2(V617F) accompanied by TET2mut and/or DNMT3Amut can be applied to track clonal sensitivity to PARP and Polθ inhibitors [4, 6]. Thus, AML and MPN clones may respond differently to DSBR inhibitors depending on their mutational profile, and the treatment should be tailored to the mutation sets carried by malignant clones.
To integrate clonal composition with response to DSBR inhibitors we developed a single-cell targeted DNA sequencing (sctDNA-seq) myeloid panel which illustrated clone-by-clone response to DSBR inhibitors and unraveled the clonal landscape of AML and MPN at a single-cell resolution before and after the treatment (Supplementary Fig. S2). We used AML and MPN somatic mutations as trackable clonal biomarkers to design a patient-tailored therapeutic regimen (“clonal attack”) utilizing DSBR inhibitors simultaneously targeting all malignant clones.
Incubation of Lin-CD34 + cells from AML-MD2 patient with six DNA damage response (DDR) inhibitors were overall sensitive to PARPi, ATMi, ATRi and RAD52i, but resistant to Polθi and DNA-PKi (Fig. 1A). sctDNA-seq followed by phylogenetic tree analysis revealed branched multi-clonal architecture with eight clones carrying specific sets of mutations (Fig. 1B-left). Fish plot analysis demonstrated staggering differences between the sensitivity of various clones to ATRi and to PARPi, ATMi and RAD52i (Fig. 1B-right, C). For example, three clones carrying EZH2(V679M), EZH2(V679M) + TET2(L1721W) and EZH2(V679M) + TET2(L1721W) + FLT3(D835Y) were resistant to ATRi ( ~ 8%, 61% and 26% survivors, respectively) but more sensitive to PARPi ( ~ 4%, 33% and 12% survivors, respectively) and ATMi (~3%, 39% and 15% survivors, respectively). Conversely, three other clones carrying EZH2(V679M) + TET2(L1721W) + RUNX1(D160Y), EZH2(V679M) + TET2(L1721W) + RUNX1(D160Y) + EZH2(E54*), and EZH2(V679M) + TET2(L1721W) + RUNX1(D160Y) + EZH2(E54*) + BCOR1(R1334Tfs*32) + NRAS(G13R) were sensitive to ATRi (~1%, 2% and 0.5% survivors, respectively) while less responsive to PARPi (~4%, 44% and 1% survivors, respectively) and ATMi (~2%, 38% and 1% survivors, respectively).
Based on this observation, we hypothesized that simultaneous treatment with ATRi + PARPi or ATRi + ATMi should result in elimination of numerous, if not all AML-MD2 clones. In agreement with this hypothesis, these drug combinations were 20–30× more effective in eliminating clonogenic growth of AML-MD2 cells when compared to individual inhibitors (Fig. 1D). Remarkably, combinations of these inhibitors (ATRi + PARPi and ATRi + ATMi) were only modestly toxic to normal hematopoietic cells (Fig. 1D) bolstering their therapeutic potential. Moreover, combination of the inhibitors displaying similar clonal targeting specificity such as PARPi + RAD52i was only 2× better than individual inhibitors against clonogenic activity of AML-MD2 cells. The effect might result from the induction of intracellular dual synthetic lethality [7].
As expected, AML cells accumulated approximately 3× more spontaneous DSBs detected by γH2AX immunofluorescence when compared to normal counterparts (Fig. 1E, Vehicle). Only the DSBR inhibitors which reduced survival of AML-MD2 cells (PARPi, ATRi, ATMi, RAD52i) increased the percentage of γH2AX-positive leukemia cells. Moreover, the magnitude of sensitivity of leukemia cells to the combinations of PARPi + ATRi and PARPi + RAD52i was proportional to detection of cells with DSBs (γH2AX+). A low number of γH2AX + cells was detected in normal hematopoietic cell populations treated with these DSBR inhibitors.
PARPi and ATRi - mediated accumulation of γH2AX+ AML-MD2 cells and reduction of cell survival was accompanied by induction of differentiation (increased of CD14+/CD11b+, CD11c+, and HLA-DR+ living cells) (Supplementary Fig. S3) which might contribute to strong anti-leukemia activity of the combination [8].
To determine if the “clonal attack” with DSBR inhibitors eradicates AML in vivo, we treated mice bearing AML-MD2 primary leukemia xenografts with PARPi and/or ATRi (Fig. 2A). Individual drugs reduced the number of hCD45+ AML-MD2 cells in bone marrow and spleen by approximately 2× and 3×, respectively (Fig. 2B, C). Remarkably, the combination of PARPi +ATRi eliminated > 99% of leukemia cells in bone marrow and in spleen of 7/10 and 10/10 mice, respectively. No obvious toxicity in mice was attributed to treatment with PARPi + ATRi in concordance with other studies showing high efficacy and tolerable toxicity of low doses of ATRi + PARP1i [9].
Altogether, these results highlight the remarkable efficiency of a “clonal attack” with the DSBR inhibitors tailored to attack all AML clones in a patient thus reducing the probability of development of time-dependent acquired resistance (Fig. 2D). In comparison, standard treatment (Fig. 2E) often employs chemotherapeutics with or without tyrosine kinase inhibitor (TKi). Chemotherapy dosages are limited by side effects and TKi requires prolonged treatment to effectively eliminate malignant clones. Thus, clones that are inherently resistant to the treatment, not detected by next generation sequencing, and/or those emerging during the prolonged treatment cause the disease relapse. The potential combinatorial effects of DSBR inhibitors and FDA approved drugs (e.g., tyrosine kinase inhibitors, and hypomethylating, genotoxic and pro-apoptotic agents) need to be tested.
To test if clonal targeting by DSBR inhibitors may have broader applicability, additional patient samples were tested. Lin-CD34+ cells from MPN P349 patient were sensitive to PARPi, ATMi, ATRi, RAD52i and DNA-PKi (Supplementary Fig. S4A). sctDNA-seq followed by fish plot analysis revealed similarities and differences between the sensitivity of the clones to these inhibitors (Supplementary Fig. S4B, C). For example, the clone carrying KMT2A(L2373H) + SETBP1(H1100R) was more sensitive to ATRi (24% survivors) than RAD52i (59% survivors), conversely clones with KMT2A(L2373H) and KMT2A(L2373H) + SETBP1(H1100R) + FLT3(R834L) were more sensitive to RAD52i (~40% and 1% survivors, respectively) than ATRi (72% and 4% survivors, respectively). Remarkably, the combination of RAD52i + ATRi was >100× more effective than individual inhibitors against clonogenic growth of P349 cells (Supplementary Fig. S4D). On the other hand, combination of RAD52i + ATMi, the two DSBR inhibitors displaying similar pattern of clonal targeting was only 2x better than individual inhibitors.
Lin-CD34+ cells from MPN P350 patient were sensitive to ATMi, ATRi, and RAD52i, and modestly sensitive to PARPi (Supplementary Fig. S4E). Again, sctDNA-seq followed by fish plot analysis revealed clonal similarities and differences in response to DSBR inhibitors (Supplementary Fig. S4F, G). Clone carrying TET2(P363L) + NRAS(G12D) was more sensitive to ATRi (~51% survivors) than PARPi (~ 79% survivors), whereas clones with TET2(P363L) + NRAS(G12D) + DNMT3A(W330C) and TET2(P363L) + NRAS(G12D) + DNMT3A(W330C) + IDH1(R132C) responded better to PARPi (~0.1% and 0% survivors, respectively) than ATRi (~22% and 3% survivors, respectively). The combination of PARPi + ATRi was >9x more effective in inhibiting clonogenic growth of P349 cells, whereas RAD52i + ATMi displaying similar pattern of clonal targeting were only 2× better than individual inhibitors (Supplementary Fig. S4H).
Clonal targeting by DSBR inhibitors may not be applicable to all AML and MPN samples. For example, Lin-CD34+ cells from AML V18 patient were sensitive to ATMi, ATRi and DNA-PKi (Supplementary Fig. S5A) but no significant differences in major clones’ response were detected (Supplementary Fig. S5B, C). As expected in this context, combinations of ATMi + ATRi and ATMi + DNA-PKi did not exert more potent anti-leukemia effect than individual inhibitors (Supplementary Fig. S5D).
Moreover, Lin-CD34+ cells from AML V20 patient sample were overall resistant to all tested DSBR inhibitors (Supplementary Fig. S5E) and combinations of the inhibitors did not exert significant anti-leukemia effect when compared to individual inhibitors (Supplementary Fig. S5F–H). AML V20 cells accumulated spontaneous DSBs (Supplementary Fig. S5I) therefore resistance to DSBR inhibitors was likely associated with a DSB repair mechanism(s) not targeted by these inhibitors.
The mechanistic aspects of clonal response to DSBR inhibitors are scarcely available. For example, the presence of DNMT3A(R882S) in AML V20 was associated with resistance to DSBR inhibitors of almost all clones (Supplementary Fig. S5E–H). DNMT3A mutations (e.g., at the R882) are frequently detected in AML and were associated with resistance to anthracyclines [10]. Remarkably, acquisition of TET2(P562Qfs*6) reversed the resistant phenotype and rendered the clone to be sensitive to multiple DSBR inhibitors. This observation is supported by our report that while DNMT3Amut promoted resistance to PARPi in FLT3(ITD)-positive cells, DNMT3Amut;TET2mut;FLT3(ITD)-positive counterparts were HR-deficient and highly sensitive to PARPi [6]. In conclusion, we postulate that acquisition of a mutation known to modulate DSBR may be a biomarker of the clonal response to DSBR inhibitor(s).
Altogether, “clonal attack” by the combinations of DSBR inhibitors revealed remarkable efficiency in simultaneous eradication of malignant clones from a cohort of AML and MPN patients. This novel approach which, instead of using genotoxic agents to induce DNA damage, takes advantage of metabolic/replication stress-induced DSBs and targets clone-specific vulnerabilities in DSBR pathways. While PARP inhibitors are widely used to treat patients with homologous recombination-deficient tumors including AML [11], ATR, Polθ, ATM, DNA-PKcs kinase inhibitors have been evaluated in cancer clinical trials (NCT04991480) [12,13,14] and RAD52 inhibitor still awaits clinical development. Moreover, newly developed inhibitors should broaden the spectrum of AML and MPN clones sensitive to DSBR inhibitors [15].
References
Morita K, Wang F, Jahn K, Hu T, Tanaka T, Sasaki Y, et al. Clonal evolution of acute myeloid leukemia revealed by high-throughput single-cell genomics. Nat Commun. 2020;11:5327.
Campbell PJ, Green AR. The myeloproliferative disorders. N Engl J Med. 2006;355:2452–66.
Nieborowska-Skorska M, Maifrede S, Dasgupta Y, Sullivan K, Flis S, Le BV, et al. Ruxolitinib-induced defects in DNA repair cause sensitivity to PARP inhibitors in myeloproliferative neoplasms. Blood. 2017;130:2848–59.
Vekariya U, Toma M, Nieborowska-Skorska M, Le BV, Caron MC, Kukuyan AM, et al. DNA polymerase theta protects leukemia cells from metabolically induced DNA damage. Blood. 2023;141:2372–89.
Trenner A, Sartori AA. Harnessing DNA double-strand break repair for cancer treatment. Front Oncol. 2019;9:1388.
Maifrede S, Le BV, Nieborowska-Skorska M, Golovine K, Sullivan-Reed K, Dunuwille WMB, et al. TET2 and DNMT3A mutations exert divergent effects on DNA repair and sensitivity of leukemia cells to PARP inhibitors. Cancer Res. 2021;81:5089–101.
Sullivan-Reed K, Bolton-Gillespie E, Dasgupta Y, Langer S, Siciliano M, Nieborowska-Skorska M, et al. Simultaneous targeting of PARP1 and RAD52 triggers dual synthetic lethality in BRCA-deficient tumor cells. Cell Rep. 2018;23:3127–36.
Stubbins RJ, Karsan A. Differentiation therapy for myeloid malignancies: beyond cytotoxicity. Blood Cancer J. 2021;11:193.
Zimmermann M, Bernier C, Kaiser B, Fournier S, Li L, Desjardins J, et al. Guiding ATR and PARP inhibitor combinationswith chemogenomic screens. Cell Rep. 2022;40:111081.
Guryanova OA, Shank K, Spitzer B, Luciani L, Koche RP, Garrett-Bakelman FE, et al. DNMT3A mutations promote anthracycline resistance in acute myeloid leukemia via impaired nucleosome remodeling. Nat Med. 2016;22:1488–95.
Le BV, Podszywałow-Bartnicka P, Piwocka K, Skorski T. Pre-existing and acquired resistance to PARP inhibitor-induced synthetic lethality. Cancers. 2022;14:5795.
Barnieh FM, Loadman PM, Falconer RA. Progress towards a clinically-successful ATR inhibitor for cancer therapy. Curr Res Pharmacol Drug Discov. 2021;2:100017.
Lavin MF, Yeo AJ. Clinical potential of ATM inhibitors. Mutat Res. 2020;821:111695.
Hu S, Hui Z, Lirussi F, Garrido C, Ye XY, Xie T. Small molecule DNA-PK inhibitors as potential cancer therapy: a patent review (2010-present). Expert Opin Ther Pat. 2021;31:435–52.
Groelly FJ, Fawkes M, Dagg RA, Blackford AN, Tarsounas M. Targeting DNA damage response pathways in cancer. Nat Rev Cancer. 2023;23:78–94.
Acknowledgements
The authors thank Mission Bio for providing assistance with data generation, data analysis, and data interpretation. This work was supported by R01s CA237286, CA244044, 244179, 247707 and LLS TRP 6628-21 to T.Skorski. The Division of Hematology Biorepository at University of Utah is supported by the National Cancer Institute of the National Institutes of Health under Award Number P30CA042014. The content is solely the responsibility of the authors and does not necessarily represent the official views of the NIH. Additional funding came from the Huntsman Center of Excellence in Hematologic Malignancies and Hematology as well as the Hematologic Malignancies and Hematology Disease Center, both at Huntsman Cancer Institute, University of Utah. We thank Dr. Sara H. Small (Robert H. Lurie Comprehensive Cancer Center, Northwestern University, Chicago, IL, USA) for critical reading of the manuscript.
Author information
Authors and Affiliations
Contributions
MMT, MN-S and MP performed experiments, AK and KNC provided bioinformatic analysis, PV, EH and T. Stoklosa provided patient samples, T. Skorski conceived the idea, supervised the project, and wrote the manuscript.
Corresponding author
Ethics declarations
Competing interests
The authors declare no competing interests.
Additional information
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Supplementary information
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Toma, M.M., Karami, A., Nieborowska-Skorska, M. et al. Clonal medicine targeting DNA damage response eradicates leukemia. Leukemia 38, 671–675 (2024). https://doi.org/10.1038/s41375-024-02138-5
Received:
Revised:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1038/s41375-024-02138-5