Activity of eftozanermin alfa plus venetoclax in preclinical models and patients with acute myeloid leukemia

Apoptosis is a form of regulated cell death involving distinct biochemical and morphologic changes in response to internal and external stimuli.¹ The ability of cancer cells to evade apoptosis is a hallmark of cancer that can lead to tumor progression and drug resistance.¹ The 2 molecular apoptotic signaling pathways are the extrinsic or death receptor (DR) signaling pathway and the intrinsic or mitochondrial pathway. Tumor necrosis factor (TNF)-related apoptosis-inducing ligand (TRAIL), a member of the TNF superfamily of cytokines, preferentially triggers the extrinsic apoptotic pathway by binding as a trimer to 2 closely related cell-surface DRs, TRAIL-R1 (DR4) and TRAIL-R2 (DR5). Cell-surface DR trimerization leads to the formation of a death-inducing signaling complex to recruit and activate caspase-8/10 that, if sufficiently robust, directly activates effector caspase-3 in type I cells to induce apoptosis. In type II cells, in which death-inducing signaling complex–induced caspase-8 activation is insufficient, engagement of the intrinsic/mitochondrial apoptosis-signaling pathway is required to ultimately induce apoptotic cell death.² First-generation TRAIL receptor agonists were well tolerated in patients with cancer but failed to develop compelling objective responses either as monotherapy or combinations with other therapeutic agents.³ This has been ascribed to biologic properties, including short plasma half-life^4,5 and weak higher-order receptor clustering,^6,7 which in some cases requires additional Fc-FcγR–mediated crosslinking.⁸ 

To overcome the lack of clinical outcome with first-generation TRAIL receptor agonists, eftozanermin alfa (formerly ABBV-621; eftoza) was developed as an agonistic fusion protein consisting of a mutant immunoglobulin G1–Fc linked to 2 single-chain trimers of TRAIL receptor–binding domain monomers, resulting in a total of 6 DR-binding sites per molecule, designed to optimize receptor clustering.⁹ Eftoza binds selectively to TRAIL receptors with nanomolar affinity to induce optimal receptor clustering in human solid tumor cancer cells that drives on-target apoptosis. This translates into robust antitumorigenic activity in solid tumor models.⁹ However, the intrinsic apoptosis-signaling pathway that is tightly regulated by the B-cell lymphoma protein-2 (BCL-2) family of proteins is known to play a role in TRAIL receptor agonism resistance. Specifically, overexpression of the BCL-2 family antiapoptotic members can dysregulate the intrinsic apoptotic pathway, promote tumorigenesis, and enable resistance to anticancer therapeutics, including TRAIL.^3,9-11 

BCL-2 plays a critical role in maintaining the survival of acute myeloid leukemia (AML) cell lines and primary patient leukemic blasts, progenitor cells, and stem cells.^12-15 Venetoclax is a first-in-class, orally bioavailable BCL-2 selective inhibitor that binds directly to the BCL-2 homology 3–binding groove of BCL-2 to induce caspase-dependent apoptosis¹⁶ and demonstrates efficacy in the treatment of patients with chronic lymphocytic leukemia,¹⁷ multiple myeloma,¹⁸ and AML.^19,20 AML is the most common acute leukemia in adults (median age, 67 years^21,22) and accounts for the largest number of leukemia-related deaths in the United States (5-year survival rate, 29%^19,23). Results from a phase 2 clinical trial of venetoclax in patients with relapsed/refractory (R/R) AML demonstrated an overall response rate (ORR) of 19%.²⁰ 

Considering that truncated BH3 interacting-domain death agonist, tBID, binds to all antiapoptotic BCL-2 family members because of TRAIL-induced caspase-8 activation,² we sought to evaluate the extrinsic apoptosis-signaling pathway activity of eftoza in AML initially as a monotherapy, subsequently hypothesizing that simultaneously engaging the intrinsic apoptosis-signaling pathway with venetoclax would lead to more durable antitumorigenic activity than either agent alone. To define the mechanisms of eftoza activity as a monotherapy and in combination with venetoclax, we evaluated preclinical models and analyzed a cohort of patients with R/R AML treated with eftoza alone or in combination with venetoclax within the ambit of a larger phase 1 trial.

AML cell lines were purchased from Deutsche Sammlung von Mikroorganismen und Zellkulturen (Braunschweig, Germany), American Type Culture Collection (Manassas, VA), Japanese Collection of Research Bioresources Cell Bank (Osaka, Japan), and Coriell Institute for Medical Research (Camden, NJ) (supplemental Table 1, available on the Blood website). All cell lines were cultured in RPMI 1640 (Gibco, Waltham, MA) supplemented with 10% fetal bovine serum (Invitrogen, Waltham, MA), 1% sodium pyruvate, 25 mM 4-(2-hydroxyethyl)-1-piperazine ethanesulfonic acid, 4.5 g/L glucose, and 1% penicillin/streptomycin (Sigma, Burlington, MA) and maintained in a humidified chamber at 37°C containing 5% CO₂. The authenticity of each cell line was verified by short tandem repeat profiling and tested for mycoplasma at the AbbVie Core Cell Line Facility. Eftoza and venetoclax were synthesized by AbbVie Inc (North Chicago, IL) and Apo2L was obtained from PeproTech (Cranbury, NJ). For in vitro studies, venetoclax was dissolved in anhydrous dimethyl sulfoxide as a 10 mM stock and stored at −20 °C. Eftoza was made up in a buffer containing 200 mM L-arginine, 20 mM tris(hydroxymethyl)aminomethane, and 10 mM succinate, at pH 7.2 and stored at −80 °C. For in vivo studies, venetoclax was formulated in 10% ethanol plus 60% Phosal 50 PG (Sigma, MO) plus 30% polyethylene glycol 400. Eftoza was formulated in phosphate-buffered saline.

Lentiviral transduction of human erythroleukemia (HEL) cells was used to generate cells overexpressing either human DR4 or DR5. CRISPR-Cas9 editing was used to generate BAK1/BAX-deficient OCI-AML5 cells, TP53-deficient MV-4-11 cells, and TP53^R248W-overexpressing MV-4-11 cells. Supplemental Methods include additional details.

Detailed methodology on cell viability assays, determination of caspase-3/7 activation, kinetic live-cell imaging of caspase-3/7 activation, and procedures for quantitative flow cytometry can be found in the supplemental Materials and Methods.

Samples from patients with AML were collected after informed consent had been obtained in accordance with the Princess Margaret Cancer Centre University Health Network review committee (Toronto, ON, Canada). Primary AML cells were isolated using Ficoll and treated in culture media containing Iscove's Modified Dulbecco's Medium (Wisent, St. Bruno, QC, Canada) with 2 mM L-glutamine (Gibco), 10% fetal bovine serum (Wisent), 55 μM β-mercaptoethanol (Gibco), 100 μg/mL Primocin (InvivoGen, San Diego, CA) as well as 100 ng/mL stem cell factor, 50 ng/mL FMS-like tyrosine kinase 3 ligand, 40 ng/mL thrombopoietin, 20 ng/mL interleukin-3, 4 ng/mL granulocyte macrophage colony-stimulating factor, and 30 U/mL interleukin-2 (PeproTech). For viability measurements, cells were treated in triplicate for 24 hours, as part of a broad compound screen, before washing and staining with anti-hCD45–BV421 (1:40; clone 2D1, Thermo Fisher Scientific, Waltham, MA) for 20 minutes. The cells were then washed and resuspended in 100 μL Annexin V Buffer (BD Biosciences, Franklin Lakes, NJ) containing Annexin V-FITC (1:50; BD Biosciences) and 7-AAD (1:650; Invitrogen). Flow cytometry was performed using MACSQuant VYB (Miltenyi Biotec, Bergisch Gladbach, Germany) and FlowJo 10 software (BD Biosciences, Ashland, OR) was used to analyze data.

Subcutaneous tumor cell line xenograft studies were conducted in a specific pathogen-free environment in accordance with the internal Institutional Animal Care and Use Committee and accredited by the American Association of Laboratory Animal Science under conditions that meet or exceed standards set by the US Department of Agriculture Animal Welfare Act, Public Health Service policy on humane care and use of animals, and the National Institutes of Health guide on laboratory animal welfare.

Female CB-17 SCID (SKM-1) mice or female SCID-beige (MV-4-11 and OCI-AML2) mice (Charles River Laboratories, Wilmington, MA) were inoculated with either 2 × 10⁶ SKM-1 cells, 5 × 10⁶ MV-4-11 cells, or 1 × 10⁶ OCI-AML2 cells subcutaneously into the right flank. Mice were injected with a 0.1-mL inoculum of 1:1 cell mixture in culture media and adjuvant Matrigel (BD Biosciences, Bedford, MA). When tumors reached ∼200 to 250 mm³, the mice were size-matched into treatment and control groups and treated as indicated. Tumor volume was measured twice per week with electronic calipers and calculated per the formula (L × W2) ÷ 2. All treatment groups consisted of 8 mice per group.

Disseminated xenograft models derived from patients (PDX) with AML were generated in sublethally irradiated NSG mice and treated with human immunoglobulin G1 (5 mg/kg, every other day for 5 doses, intraperitoneally), eftoza (5 mg/kg, every other day × 5, intraperitoneally), venetoclax (50 mg/kg, daily × 21, by mouth), or eftoza and venetoclax in combination at identical monotherapy doses and schedules. The impact on tumor burden was determined in the bone marrow 1 week after end of treatment (n = 5 mice per treatment).

Leukapheresis studies were performed at Champions Oncology Inc (Rockville, MD). NOG-F mice were sublethally irradiated and inoculated with purified cryopreserved primary patient AML isolates obtained via leukapheresis. After tail vein inoculation (up to 2 × 10⁶ cells per mouse), engraftment was monitored in the blood and bone marrow for up to 12 weeks after inoculation. After engraftment was confirmed in surrogate mice (20-200 huCD33⁺ blasts per μL of peripheral blood), the remaining cohorts were screened and randomized into groups on the basis of blast counts in blood (n = 10) and placed on trial. Mice were treated with eftoza at 3 mg/kg every other day × 5 and venetoclax at 50 mg/kg daily × 21, and the effect on survival (based on animal health observations) was assessed and compared using log-rank statistical analysis.

Linear regression and Spearman correlations were used to determine the correlation between 2 variables, the Mantel-Cox test was used to assess significance between Kaplan-Meier survival curves, and either Mann-Whitney U test, Friedman test, or one-way analysis of variance with Tukey's post hoc test was used to determine statistical significance between data sets. Statistical analyses were performed using GraphPad Prism 9.1.0 (GraphPad Software, La Jolla, CA).

A phase 1, first-in-human, open-label, multicenter study was conducted to evaluate eftoza as single agent and in combination with venetoclax in adult patients (≥18 years old) with previously treated solid tumors or hematologic malignancies (#NCT03082209). The study consisted of 2 parts, dose escalation and dose optimization. The dose range of eftoza (1.25-7.5 mg/kg) used in this clinical study was determined from pharmacokinetic (PK)/pharmacodynamic modeling of the response of mice bearing Colo205 tumors treated with single doses of eftoza.⁹ The results of the dose-escalation portion of the study with eftoza monotherapy in solid tumors have been previously published.²⁴ Patients with an AML diagnosis and with histologically confirmed R/R disease were eligible to enroll in the AML dose-optimization cohort, which we report herein, and received treatment with eftoza as monotherapy or in combination with venetoclax. Key eligibility criteria are in supplemental Table 2. The primary objective of dose optimization was to evaluate the PK profile of eftoza as monotherapy or in combination with venetoclax in patients with R/R AML; secondary objectives were to assess safety and tolerability. Exploratory objectives included evaluation of preliminary antitumor efficacy, and assessment of pharmacodynamic effects and exploratory biomarkers related to drug development.

The study was conducted in accordance with the Declaration of Helsinki and International Conference on Harmonization Good Clinical Practice guidelines. The study protocol was approved by an independent ethics committee/institutional review board. All patients provided written informed consent.

Supplemental Materials and Methods include additional details on treatment, safety, PK, and tumor assessments.

The effect of eftoza on cell viability was determined in a panel of 23 AML cell lines after 24 hours of treatment in vitro (Figure 1A). Eftoza was active in AML cell lines, inducing cell death with EC₅₀ values <10 nM in 16 of 23 (69.6%) AML cell lines with superior potency compared with that of Apo2L (supplemental Table 3). Cell death after eftoza treatment was apoptosis-based, because a loss in cell viability corresponded to a dose- and time-dependent increase in caspase-3/7 activity (Figure 1B; supplemental Figure 1A-B), and the effect of eftoza on cell viability was abrogated by the pan-caspase inhibitor z-VAD-FMK (Figure 1C). The eftoza-sensitive cell line SKM-1 (EC₅₀ = 0.004 nM) was injected subcutaneously into SCID mice to determine single-agent activity of eftoza in vivo (Figure 1D). Eftoza induced robust single-agent antitumor activity with complete regression of SKM-1 tumors.

To explore the molecular mechanism of eftoza-induced apoptosis in AML cell lines, DR4 and DR5 plasma membrane receptor numbers were determined via quantitative flow cytometry (Figure 1E-H). The majority of AML cell lines (18/23) expressed higher DR5 numbers on the plasma membrane than DR4 (Figure 1E,F) and are reflective of data in solid tumor cell lines.⁹ The numbers of both DR4 and DR5 on the plasma membrane correlated well with their corresponding DR4 (TNFRSSF10A) and DR5 (TNFRSF10B) gene expression (supplemental Figure 2). The cellular activity of eftoza highly correlated with DR5 (r = −0.7967; P < .0001) and DR4 plus DR5 (r = −0.8358; P < .0001) receptor number on the cell surface but not DR4 receptor number alone (r = −2646; P = .2225) (Figure 1G,H). TNFRSF10B gene expression (r = −0.7253; P = .004), but not TNFRSF10A gene expression (r = 0.1069; P = .6631), correlated with eftoza activity (supplemental Figure 3). Interestingly, the 7 resistant AML cell lines with EC₅₀ values ≥10 nM also had either lower DR5 or lower DR4 + DR5 numbers on the plasma membrane than the cell lines that responded to eftoza (Figure 1F; supplemental Table 3), suggesting that a minimal number of DR4/DR5 on the plasma membrane is required for eftoza activity. To demonstrate that eftoza activity in AML cells can be mediated by either DR4 or DR5 plasma membrane expression, we ectopically expressed human TNFRSF10A or human TNFRSF10B in HEL cells, which possess low levels of both DR4 and DR5 on the plasma membrane and are inherently resistant to eftoza-induced apoptosis. HEL cells overexpressing human DR4 (+huDR4) or DR5 (+huDR5) on the plasma membrane were more sensitive to eftoza than the parental cells (Figure 1I). HEL +huDR4 cells were less sensitive to eftoza than +huDR5 cells, possibly because of lower overexpression of DR4 on the plasma membrane than DR5.

The expression of DRs is transcriptionally upregulated by p53 via intronic binding sites,^25,26 a tumor suppressor mutated in up to 30% of patients with AML^27-29 and associated with poor responses to therapy.^30,31 All AML cell lines expressing TP53^wt (9/9) were sensitive to eftoza (EC₅₀ < 10 nM) and expressed >1750 total DRs (DR4 plus DR5) on the plasma membrane, an estimated threshold for sensitivity (supplemental Figure 4A-B; supplemental Table 3). Although TP53^mut AML cell lines were collectively less responsive to eftoza treatment compared with their TP53^wt counterparts (supplemental Figure 4A-B), TP53^mut AML cell lines that expressed cell-surface DR levels >1750 (7/14) were equally sensitive (supplemental Figure 4C). These data collectively indicate that TP53-independent regulation of DR4 and DR5 protein expression can enable eftoza sensitivity in patient populations with poor outcomes to existing therapies.

BCL-2 was found to be consistently expressed at higher levels than related antiapoptotic proteins B-cell lymphoma-extra large (BCL-X_L) and myeloid cell leukemia sequence 1 (MCL-1) in AML cell lines (supplemental Table 4). We sought to evaluate the impact of venetoclax treatment on activity of eftoza in the panel of AML cell lines in vitro, using the Bliss independence model³² to determine synergistic cell death. Synergistic cell death (Bliss sum >0) was observed between eftoza and venetoclax in 15 of the 23 AML cell lines tested. (Figure 2A; supplemental Figure 5A-B). The synergy of eftoza with venetoclax was apoptosis-based because caspase-3/7 activation was enhanced in a time- and dose-dependent manner after combined treatment of eftoza with venetoclax, compared with either agent alone (Figure 2B,C), and the synergistic effect of eftoza-venetoclax could be abrogated by deletion of BAK and BAX (Figure 2D,E). The eftoza-venetoclax combination partially overcame some of the resistance imparted by BAX deletion on venetoclax or eftoza single-agent activity in OCI-AML5 cells in vitro (supplemental Figure 5C). In vivo, the combination of eftoza and venetoclax induced robust tumor regression and was superior to either compound treatment alone in the MV-4-11 and OCI-AML2 AML CDX tumor models (Figure 2F,G).

The protein and gene expressions of DR4, DR5, and BC-L2 were characterized to gain further insight into the underlying mechanisms responsible for combinatorial activity between eftoza and venetoclax. Synergistic cell death in AML cells positively correlated with DR5, DR4 + DR5 plasma membrane receptor number, and total BCL-2 protein levels, but not DR4 plasma membrane receptor number alone, as measured via flow cytometry (Figure 2H-J). Synergistic cell death in AML cells also positively correlated with TNFRSF10B and BCL2, but not TNFRSF10A, gene expression levels (supplemental Figure 6). Interestingly, synergistic cell death was observed between eftoza and venetoclax in 14 of the 23 AML cell lines where the total DR number on the plasma membrane (DR4 + DR5) was >1750 copies per cell (supplemental Table 3).

Genomic aberrations, such as FLT3-ITD, ASXL1, and TP53 are frequently detected in patients with AML^33-35 and associated with less durable responses to venetoclax plus hypomethylating agent–based regimens.^20,31,36,37 Synergistic cell death between eftoza and venetoclax was observed in all 4 cell lines harboring ASXL1 mutations (known to confer sensitivity to azacitidine-venetoclax; OCI-AML5, SKM-1, PL-21, and Nomo-1) and all 3 cell lines harboring the FLT3-ITD mutation (MV-4-11, PL-21, and MOLM-13) (supplemental Table 3). Furthermore, in TP53^mut AML cell lines in which total DR number was not limiting (>1750 receptors per cell), eftoza-venetoclax synergy was equivalent to that observed in TP53^wt AML cells (supplemental Figure 4D-E). The impact of TP53 status was further investigated in engineered MV-4-11 cells (TP53^–/– and TP53^R248W) compared with the parental cells (TP53^wt). Despite a decrease in single-agent activity of both venetoclax and eftoza in the TP53^R248W or TP53^–/– cells compared with parental TP53^wt cells (supplemental Figures 5A and 7A-B), the combinatorial activity was equivalent, independent of TP53 status (supplemental Figure 7C,D).

To further investigate the potential consequence of BCL-2 inhibition on the activity of eftoza in AML, we evaluated the effects of eftoza, venetoclax, or eftoza-venetoclax combination treatment on the viability of ex vivo CD45⁺ cells from 45 naive patients and 19 patients with R/R AML. Although DR4/DR5 expression was not determined, the eftoza-venetoclax combination significantly enhanced cell death in ex vivo samples from both naive patients and patients with R/R AML when compared with either treatment alone. The median response to eftoza treatment was superior to venetoclax alone compared with the eftoza-venetoclax combination, although this did not meet statistical significance in the samples of patients who were R/R. Importantly, subgroups of patients with AML, who were either R/R to venetoclax (or samples collected while receiving venetoclax-based therapies) or harbored TP53 mutations, were highly sensitive to combination treatment compared with either agent alone (Figure 3A). Subsequently, 4 xenograft models derived from patients with AML who were positive for DR5 plasma membrane expression were treated with either eftoza or venetoclax alone or the eftoza-venetoclax combination, and the effects on tumor burden in the bone marrow were evaluated (Figure 3B). These patient-derived models captured several different genomic aberrations, including FLT3-ITD (AML-23 and AML-31) or TP53 mutations (AML-55) (supplemental Table 5). In xenograft models AML-23, AML-31, and AML-40 derived from patients with AML, single-agent eftoza or venetoclax treatment each had varying and limited effects on reducing tumor burden compared with combination treatment (Figure 3B). In xenograft model AML-55 derived from patients with AML (TP53^P222L/R248Q mutations), eftoza monotherapy significantly reduced tumor burden (P < .0001) within the bone marrow in the absence of any venetoclax single-agent activity. The addition of venetoclax to eftoza further reduced evidence of disease in AML-55. Similarly, the combination of eftoza and venetoclax extended the loss in the median tumor burden compared with that of either agent alone in 3 additional AML PDX models, with statistical significance observed over venetoclax alone in AML-40 (P < .05) (Figure 3B). Notably, the percentage of DR5⁺ cells was highest in AML-55 compared with the other 3 xenograft models derived from patients with AML (Figure 3B).

Extending these studies to understand the effect of eftoza-venetoclax combination treatment on survival, we leveraged 3 human AML leukapheresis models. In CTG-2229, eftoza treatment alone extended animal survival when compared with vehicle or venetoclax treatment alone, with no added benefit observed from adding venetoclax with eftoza. In the CTG-2226 AML leukapheresis model, venetoclax alone had an overall survival benefit when compared with vehicle treatment, with added benefit observed from addition of eftoza. In the CTG-2238 AML leukapheresis model, in which neither eftoza nor venetoclax monotherapy had an impact on the overall survival, the combination treatment extended the overall survival when compared with vehicle treatment (Figure 3C; supplemental Table 6).

To translate aforementioned preclinical findings into the clinical setting, we initiated a first-in-human clinical trial in patients with R/R AML (#NCT03082209). An eftoza dose range from 1.25 to 7.5 mg/kg was used in this clinical study and determined using PK/pharmacodynamic modeling derived from the response of mice bearing Colo205 tumors treated with a single dose of eftoza.⁹ As of 30 March 2020, a total of 27 patients with R/R AML were enrolled into a dose-optimization cohort and treated with eftoza as monotherapy (n = 4) or in combination with venetoclax (n = 23). Demographics, clinical characteristics, and disposition of patients are summarized in Table 1.

All-grade treatment-related adverse events (TRAEs) reported in monotherapy cohorts (50%; 2/4) were stomatitis and infusion-related reaction (n = 1; 1.25 mg/kg) as well as neutropenia and hypophosphatemia (n = 1; 3.75 mg/kg); grade ≥3 TRAE of neutropenia was reported by 1 patient. The most common all-grade TRAEs for patients in combination cohorts are summarized in Table 2 and include increased alanine aminotransferase and aspartate aminotransferase (AST; n = 8; 35% each); grade ≥3 TRAEs were increased alanine aminotransferase (n = 5; 22%) and increased AST (n = 4; 17%). In the good laboratory practice repeat-dose toxicology study using nonhuman primates treated with weekly intravenous infusions of eftoza up to 100 mg/kg per week for 4 consecutive weeks, no increase in serum liver enzymes or hepatocellular apoptosis were observed.⁹ One patient in the 7.5 mg/kg combination cohort experienced an on-treatment death from pneumonia that was also confounded by the progression of underlying AML. Eftoza demonstrated approximately dose-proportional increase in exposure for the dose range from 1.25 to 7.5 mg/kg administered weekly; findings were similar when administered with and without venetoclax. The harmonic mean terminal elimination half-life of eftoza was ∼29 to 34 hours (Table 3). The maximum plasma concentrations achieved with the 7.5 mg/kg dose of eftoza were ∼103 μg/mL and 134 μg/mL, as a monotherapy and in combination with venetoclax, respectively, corresponding to ∼614 nM and 799 nM. Minimal accumulation was detected after multiple weekly doses. Venetoclax exposures were comparable with those observed historically^38,39 and did not appear to vary with eftoza dose.

Antileukemic activity was not observed in the 4 patients enrolled in monotherapy cohorts. For the 23 patients in combination cohorts, the complete response (CR) or CR with incomplete blood count recovery (CRi) rate was 26% (n = 6), with 4 CR and 2 CRi. In addition, 1 patient achieved a morphologic leukemia-free state (MLFS). The ORR was 30% (7/23) with inclusion of MLFS. Molecular profiles and responses for patients in combination cohorts are presented in Figure 4. Median duration of response (CRi or better) was 7.8 months (95% confidence interval, 1.2 to not reached). The molecular profile in combination cohorts measured by next-generation sequencing showed aberrations, with IDH1/2 and NRAS/KRAS being the most frequently mutated genes. No genetic aberrations were detected in 2 of 6 patients who reported a CR or CRi. Mutations in IDH2 (n = 1) and ASXL1 (n = 1), respectively, were the only aberration noted in the 2 responders. Duration of responses for a patient with IDH2 mutation was >400 days, with treatment ongoing at time of data cut. The remaining 2 responders had genetic abnormalities in ASXL1, TET2, STAG2, NRAS, WT1, WAC, JAK2, DNMT3A, and NPM1. A FLT3-ITD mutation was documented in 1 patient with morphologic relapse; no mutations in TP53 were observed in enrolled patients.

In addition, 13 of the 23 patients from combination cohorts had samples available for quantitation of DR4/DR5 via flow cytometry assay; 6 of these patients’ samples (either peripheral blood or bone marrow aspirate) had myeloblasts positive for DR4/DR5 expression. A 67% (4/6) ORR (CR, CRi, or MLFS) was observed among patients with positive DR4/DR5 myeloblasts. CR is ongoing in 1 patient (>400 days; Figure 4).

Using preclinical models of AML, we demonstrate that the TRAIL receptor agonistic fusion protein eftoza drives caspase-dependent apoptosis in vitro that translates into antitumorigenic activity in vivo that can be enhanced by concurrently inhibiting BCL-2 with venetoclax. Eftoza single-agent or combinatorial activity depends on DR4 and DR5 expression, 2 factors that are independent predictors of poor prognosis in AML.⁴⁰ Importantly, the combinatorial activity between eftoza and venetoclax is observed in AML cell lines, patient samples, and patient-derived xenograft models with TP53 and/or FLT3-ITD mutations; genomic aberrations are associated with less durable responses to venetoclax monotherapy or in combination with hypomethylating agents.^20,31,34-37 Eftoza with or without venetoclax was also active in AML cell lines deficient in BAX, a proapoptotic factor that drives resistance to venetoclax-based therapies,⁴¹ although this was less efficient than in the parental cell line. Given these observations, the development of new venetoclax-based combination regimens with novel therapeutics such as eftoza has the potential to expand treatment options for patients with AML.

In addition to these preclinical data, we demonstrate that treatment with eftoza was tolerated both as monotherapy and in combination with venetoclax in patients with R/R AML (NCT03082209). Although the combination of eftoza plus venetoclax may be associated with an increase in hepatic toxicity, overall, AEs from the combination arm were aligned with those expected from venetoclax monotherapy. Myelosuppression is a predominant toxicity encountered during venetoclax-based therapy^42-44; however, adverse events of anemia, neutropenia, or thrombocytopenia were not prominent in the eftoza-venetoclax combination arm. Notably, there were no cases of tumor lysis syndrome reported for patients treated with eftoza plus venetoclax but larger studies will be needed to address these adverse events.

Eftoza treatment demonstrated approximately dose-proportional increase in exposure in the weekly 1.25- to 7.5 mg/kg dose range that did not vary with or without coadministration of venetoclax. Although limited activity was demonstrated with eftoza monotherapy in preclinical models of AML, no response was observed in the phase 1 monotherapy cohort. Because of low patient numbers (n = 4), conclusions cannot be drawn. Combination therapy with eftoza and venetoclax showed promising antileukemic activity in patients with R/R AML with a CR/CRi rate of 26% (6/23) and ORR of 30% (7/23) with inclusion of MLFS. As a comparison, venetoclax monotherapy in a similar setting reported 19% CR/CRi rate with median duration of response <2 months.²⁰ Conversely, retrospective analysis of outcomes for 86 patients with R/R AML who were treated with venetoclax combinations (hypomethylating agents [azacitidine or decitabine] or low-dose cytarabine) resulted in responses in 31% of patients (CR, 14%; CRi, 10%; MLFS, 7%).⁴³ Notably, an ORR (CR, CRi, or MLFS) of 67% (4/6) was reported in a subgroup of patients positive for DR4/5 receptor expression.

Collectively, these data highlight that simultaneously targeting extrinsic and intrinsic apoptosis-signaling pathways in AML with eftoza and venetoclax, respectively, improves on the activity of either agent alone. This combination is safe and well tolerated in patients with AML and supports further clinical evaluation of eftoza-venetoclax combination in patients with DR4/DR5-positive AML. Effectively activating the extrinsic pathway with the TRAIL receptor agonist eftoza and the intrinsic pathway with venetoclax may lead to more durable antitumor activity in patients with AML.

AbbVie and the authors thank all the trial investigators and the patients who participated in this clinical trial. Medical writing support was provided by Mary L. Smith, Aptitude Health, Atlanta, GA, and funded by AbbVie. The authors also thank Rogier Mous (University Medical Center Utrecht), Lot Devriese (University Medical Center Utrecht), John Reagan (Brown University), Adam Olszewski (Brown University), and Marcel Nijland (University Medical Center Groningen) for their invaluable study contributions; and Mark Minden, Dalia Barsyte-Lovejoy, and Genna Luciani (Princess Margaret Cancer Centre) and Dipica Haribhai (AbbVie Precision Medicine Oncology) for their contribution to the ex vivo viability study design and completion. The authors also thank Jason Huska from AbbVie Oncology Discovery for providing the BAX- and BAK/BAX-deficient OCI-AML5 cells.

Venetoclax is being developed in a collaboration between AbbVie and Genentech. AbbVie funded this study and participated in the study design, research, analysis, data collection, interpretation of data, reviewing, and approval of the manuscript. Genentech participated in the review and approval of the manuscript. No honoraria or payments were made for authorship.

Contribution: Analysis was initially done by S.K.T., C.B., M.S., D.C., M.M., D.S., D.M., F.G.B., S.M.-L., B.A.C., and D.C.P.; and all authors had access to the data and participated in data collection and interpretation and contributed to the drafting, review, revision, and approval of the manuscript.

Conflict-of-interest disclosure: E.C. received honoraria or consultation fees from Astellas, Novartis, Nanobiotix, Pfizer, Janssen-Cilag, GLG Pharma, Psioxus Therapeutics, Merck, Medscape, Bristol-Myers Squibb, Gilead Sciences, Seattle Genetics, Pierre Fabre, Boehringer Ingelheim, Cerulean Pharma, EUSA Pharma, Gehrmann Consulting, AstraZeneca, Roche, Guidepoint, Servier, Celgene, AbbVie, Amcure, OncoDNA, and Alkermes; is on a leadership role as director of clinical research for START Madrid and HM Hospitals Group, Madrid and is the founder and president for nonprofit Foundation INTHEOS; is the codirector of Methods in Clinical Cancer Research (MCCR) Workshop, Zeist, Netherlands (joint ECCO-AACR-EORTC-ESMO Workshop on MCCR); has stocks or ownership in START, Oncoart Associated, and International Cancer Consultants; gets direct research funding as project lead from Novartis, AstraZeneca, BeiGene; received institutional financial support for clinical trials from AbbVie, ACEO, Amcure, Amgen, AstraZeneca, Bristol-Myers Squibb, CytomX Therapeutics, GlaxoSmithKline, Genentech/Roche, H3 Biomedicine, Incyte, Janssen, Kura, Lilly, Loxo, Nektar Therapeutics, MacroGenics, Menarini, Merck, Merus, Nanobiotix, Novartis, Pfizer, PharmaMar, Principia, PUMA, Sanofi, Taiho, Tesaro, BeiGene, Transgene, Takeda, Incyte, Inovio, MSD, Psioxus, Seattle Genetics, Mersana, GSK, Daiichi, Nektar, Astellas, ORCA, Boston Therapeutics, Dynavax, Debiopharm, Boehringer Ingelheim, Regeneron, Millennium, Synthon, Spectrum, and Rigontec; is on the scientific board at Psioxus; has memberships for SEOM, EORTC, ESMO, and ASCO; and has a full/part-time employment in HM Hospitals Group and START, Program of Early Phase Clinical Drug Development in Oncology, as a medical oncologist, director clinical research. B.A.C. received institutional research support from AbbVie, Bayer, AstraZeneca, MedImmune, Astellas, Actuate Therapeutics, Pfizer, Dragonfly Therapeutics; and is on the advisory role for Foundation Medicine, Tempus, G1 therapeutics, Seagen. A.S. received research support from Natera; and is an advisory board member of Taiho Oncology. K.I. received grants from AbbVie, during the conduct of the study; grants from Sanofi, Symbio, Bayer, IQVIA, and Otsuka; grants and personal fees from Novartis; personal fees from Takeda, Celgene, Ono, Chugai, Eisai, SRD, MSD, Micron, and Janssen; and personal fees from Kyowa Kirin, outside the submitted work. D.M. received honoraria from Takeda, AbbVie, and Janssen. M.M. and D.A.M. are former employees of AbbVie and stockholders of AbbVie Inc. T.U., S.K.T., C.B., M.S., D.C., F.G.B., S.M.-L., B.C.M., D.S., and D.C.P. are employees of AbbVie and stockholders of AbbVie Inc. The remaining authors declare no competing financial interests.

Correspondence: Darren C. Phillips, Oncology Discovery, AbbVie Inc, 1 North Waukegan Rd, AP9-2, Rm 02L8B, North Chicago, IL 60064; e-mail: darren.phillips@abbvie.com.