Ibrutinib is a bruton’s tyrosine kinase (BTK) inhibitor approved for the treatment of multiple B-cell malignancies, including chronic lymphocytic leukemia (CLL). In addition to blocking B-cell receptor signaling and chemokine receptor-mediated pathways in CLL cells, that are known drivers of disease, ibrutinib also affects the microenvironment in CLL via targeting BTK in myeloid cells and IL-2–inducible T-cell kinase (ITK) in T-cells. These non-BTK effects were suggested to contribute to the success of ibrutinib in CLL. By using the Eµ-TCL1 adoptive transfer mouse model of CLL, we observed that ibrutinib effectively controls leukemia development, but also results in significantly lower numbers of CD8+ effector T-cells, with lower expression of activation markers, as well as impaired proliferation and effector function. Using CD8+ T-cells from a T-cell receptor (TCR) reporter mouse, we verified that this is due to a direct effect of ibrutinib on TCR activity, and demonstrate that co-stimulation via CD28 overcomes these effects. Most interestingly, combination of ibrutinib with blocking antibodies targeting PD-1/PD-L1 axis in vivo improved CD8+ T-cell effector function and control of CLL. In sum, these data emphasize the strong immunomodulatory effects of ibrutinib and the therapeutic potential of its combination with immune checkpoint blockade in CLL.
Within the last decade, a new era of therapeutic opportunities for patients with chronic lymphocytic leukemia (CLL) has begun.1 Treatment responses, also in patients with relapsed and refractory disease or unfavorable genetic profile, have dramatically improved with the development and approval of kinase inhibitors that target B-cell receptor (BCR) signaling, a well-known driver of disease.2,3 Ibrutinib is an orally bioavailable, irreversible inhibitor of Bruton’s tyrosine kinase (BTK). Both in vitro and in patients, ibrutinib has been shown to potently inhibit BCR signaling, prevent lymphocyte adhesion and homing, and inhibit protective effects of the microenvironment, which yields high response rates and durable remissions in patients with CLL if applied continuously.4,5
In addition to pro-survival pathways in malignant cells, like BCR signaling, T cells represent an attractive therapeutic target in CLL. In patients and mouse models of CLL, T cells expand along with the disease course.6,7 Our recent work has demonstrated a non-redundant role of CD8+ T cells in suppressing CLL progression in an IFN-dependent manner.8 Yet chronic exposure to tumor-derived antigens in secondary lymphoid organs leads to their continuous activation, upregulation of inhibitory receptors, such as PD-1, and ultimately exhaustion.8 Therefore, targeting inhibitory receptors, such as PD-1 and Lag3, offered novel opportunities of therapeutic reactivation of adaptive anti-tumor immunity by immune checkpoint blockade.9,10 Notably, immune checkpoint blockade showed promising activity in a subgroup of CLL patients with Richter’s transformation, suggesting that unleashing inhibited T cells results in better control of leukemia progression.11 Besides its direct cytotoxic activity against malignant B cells, ibrutinib also exerts immunomodulatory effects (reviewed by Maharaj et al.).12 Ibrutinib-mediated inhibition of STAT3 results in decreased expression of immunosuppressive molecules, such as PD-L1 and IL-10, by CLL cells.13 Gunderson et al. have demonstrated that BTK inhibition in tumor-associated myeloid cells reprograms them towards M1-like immunostimulatory phenotypes resulting in enhanced anti-tumoral T-cell activity.14 In addition to modulating BTK-expressing cells in the microenvironment, ibrutinib has been shown to impact natural killer (NK)- and T-cell activity due to its non-BTK effects on IL- 2-inducible T-cell kinase (ITK).15,16 In a preclinical study, ITK inhibition by ibrutinib was shown to impair Fc receptor- mediated NK-cell functions and to antagonize cytotoxicity of rituximab.16 However, NK-cell-mediated cellular cytotoxicity was significantly recovered 12 hours (h) after ibrutinib has been removed, which may be attributed to turnover of ITK.17 Inhibition of ITK by ibrutinib was further shown to modulate TCR signaling in CD4+ T cells and enhance Th1 response in vitro.15 In addition, a reduced number or percentage of regulatory T cells in peripheral blood of ibrutinib-treated patients was reported.18,19 Interestingly, ibrutinib was recently approved for the treatment of refractory chronic graft-versus-host-disease (cGvHD) after allogeneic hematopoietic stem cell transplantation, indicating its potent immunomodulatory effect in vivo.20
The strong immunomodulatory activity of ibrutinib encouraged several pre-clinical and clinical studies assessing its potential combination with other immunotherapeutic drugs, primarily immune checkpoint blockade.21 The success of these immunotherapeutic approaches relies on enhancing the functional capacities and proliferation of anti-tumoral CD8+ T cells. Despite a large body of evidence highlighting the immunomodulatory activity of ibrutinib, its exact impact on CD8+ T cells in CLL remains less defined. While Long et al. observed an increase in CD4+ and CD8+ T-cell numbers in ibrutinib-treated patients,19 a drop in T-cell numbers, activation, and proliferation was reported in another patient cohort.22 Moreover, it was suggested that ibrutinib can enhance anti-tumoral CD8+ T-cell function in CLL patients by fostering a switch of T-helpercell polarization towards anti-tumoral Th1 cells.15 However, this change in Th1 polarization could not be confirmed in a cohort of ibrutinib-treated patients.19 Thus, in this study, we utilized the E-TCL1 adoptive transfer (TCL1 AT) model of CLL to monitor CD8+ T-cell differentiation and function under ibrutinib treatment. Through this, we observed that this drug reduces the functionality of CD8+ T cells which could be overcome by combining ibrutinib with immune checkpoint blockade in the TCL1 AT model. The relevance of these findings for therapeutic applications has to be proven in ongoing clinical trials combining ibrutinib with anti()PD-L1 antibody durvalumab for treatment of B-cell lymphoma and CLL patients. (Trial registered at clinicaltrials.gov identifiers: NCT02401048 and NCT02733042).
E-TCL1 (TCL1) mice on C57BL/6 background were kindly provided by Dr. Carlo Croce (Ohio State University, OH, USA).23 C57BL/6 wild-type (WT) mice were purchased from Charles River Laboratories (Sulzfeld, Germany), and Nr4a1GFP mice24 were kindly provided by Dr. Markus Feuerer (DKFZ, Heidelberg, Germany).
TCL1 tumor cells of C57BL/6N background were propagated once by adoptive transfer in C57BL/6N mice to ensure having enough tumor cells from the same donor for all treatment arms. Adoptive transfer of TCL1 tumors was performed as previously described.9,25 Briefly, 1-2x107 leukemic TCL1 splenocytes (CD5+CD19+ content of purified cells was typically above 90%) were transplanted by intraperitoneal (i.p.) injection into 2-3- month-old C57BL/6N WT females. All animal experiments were carried out according to governmental and institutional guidelines and approved by the local authorities (Regierungspräsidium Karlsruhe, permit numbers: G-36/14, G-123/14, G-16/15, and G- 53/15).
In vivo treatment
Two to three weeks after tumor cell transplantation, tumor load in blood (defined as the number of CD5+CD19+ CLL cells/L) was measured, and mice were assigned to different treatment arms to achieve comparable tumor load in all groups at baseline prior to treatment. Ibrutinib (provided by Pharmacyclics LLC, an AbbVie Company) was administered in drinking water containing sterile control vehicle (1% HP--CD) at a concentration of 0.16 mg/mL, as previously described.26 For PD-1/PD-L1 blockade, mice were injected i.p. with 0.2 mg of PD-1 (clone: RMP1-14), PD-L1 (clone: 10F.9G2), or rat IgG2a isotype control antibody (clone: 2A3; all from BioXcell, West Lebanon, NH, USA) every 3 days for 4 weeks.
Flow cytometry and functional assays
Single cell suspensions from peripheral blood (PB) or lymphoid tissues were prepared and flow cytometric analyses of cell surface proteins and transcription factors were performed as detailed in the Online Supplementary Appendix and described before.8,27 Gating strategies are depicted in the Online Supplementary Appendix and antibodies are listed in Online Supplementary Table S1.
Cytokine release, granzyme B production and degranulation capacity of CD8+ T cells were assayed as previously described with minor modifications, as outlined in the Online Supplementary Appendix.9
Human PB mononuclear cells (PBMC) or mouse splenocytes were pre-treated for 30 minutes (min) with ibrutinib, CC-292 or ACP-196 (Selleckchem, Munich, Germany), then stimulated with 1 g/mL CD3 antibodies (clone HIT3a or 145-2C11, respectively) in 96-well round-bottom microtiter plates at a density of 2x106/mL and incubated at 37°C and 5% CO2 until analyzed by flow cytometry. For assessment of proliferation, cells were stained with 5 M carboxyfluoresceinsuccinimidyl ester (CFSE; eBioscience) prior to drug treatment and stimulation as previously described.28
Sample size was determined based on expected variance of read-out. No samples or animals were excluded from the analyses. No randomization or blinding was used in animal studies. Data were analyzed using Prism 5.04 GraphPad software. Statistical tests of data were one-way ANOVA followed by multiple comparison test or unpaired Student t-test with Welch approximation to account for unequal variances. When appropriate, paired Student t-test was used. P<0.05 was considered to be statistically significant. All graphs show means±standard error of mean, unless otherwise indicated.
Ibrutinib modulates effector CD8+ T-cell differentiation and proliferation in the TCL1 adoptive transfer model
To investigate effects of ibrutinib on CD8+ T cells in vivo, we utilized the TCL1 AT model of CLL.9,25 We transplanted C57BL/6 WT mice with TCL1 splenocytes, and after 2 weeks mice were assigned to treatment with ibrutinib or vehicle according to tumor load in PB. In line with published data,29 ibrutinib treatment resulted in a significant decrease in CLL development in comparison to vehicle-treated mice, as evident by a decrease in CD5+CD19+ cell counts in PB and decreased splenomegaly and hepatomegaly (Figure 1A and B). Moreover, CLL cell proliferation was significantly reduced, as measured by Ki-67 staining (Figure 1C), confirming efficient cytotoxic activity of the drug.
We then evaluated the effect of ibrutinib on antitumoral CD8+ T cells. We have recently shown that CLL development in TCL1 mice induces the differentiation of an anti-tumoral, oligoclonal effector CD8+ T-cell population that controls tumor development in an IFN-dependent manner.8 Accordingly, we analyzed the splenic CD8+ T-cell composition using CD44 and CD127, which divide CD8+ T cells into CD127hiCD44low naïve, CD127hiCD44hi memory, and CD127lowCD44int-hi effector subsets (Figure 1D). As expected, CLL development induced a sizable expansion of CD127lowCD44+ effector T cells in vehicletreated mice in comparison to untransplanted WT controls (Figure 1D and E). Interestingly, the percentage and absolute numbers of the effector population were lower in ibrutinib-treated mice (Figure 1D and E). This was accompanied by decreased expression of activation markers like CD69 and CD137 on CD8+ T cells (Figure 1F), and decreased expression of transcription factors that regulate effector T-cell differentiation, such as T-box transcription factor T-bet and Eomesodermin (Eomes) (Figure 1G).30 Furthermore, CD8+ T-cell proliferation was significantly lower in ibrutinib- compared to vehicle-treated TCL1 mice, reaching levels similar to non-tumor control mice (Figure 1H). The drop in the effector population, activation markers and proliferation of CD8+ T cells was also observed when treatment started at later stages of disease when all mice had more than 5,000 CLL cells/L of blood, the leukemic threshold in CLL patients (Online Supplementary Figure S1A).
We next examined whether the observed changes in CD8+ T cells are caused by a direct impact of ibrutinib on these cells or rather reflect a secondary normalization of the T-cell compartment due to the decrease in tumor load. Thus, we analyzed CD8+ T cells in vehicle- and ibrutinibtreated mice having a similar disease load, as measured by CLL-cell infiltration in spleen and liver. While the vehicletreated mice showed signs of overt leukemia with severe hepato-splenomegaly after 3 weeks of starting the treatment, ibrutinib successfully suppressed CLL development during that time. Nonetheless, mice continuously receiving ibrutinib succumbed to full-blown leukemia at week 4 post treatment exhibiting similar disease load to vehicle group at week 3 (Online Supplementary Figure S1B). Analysis of the spleen CD8+ T-cell compartment of endstage vehicle or ibrutinib-treated mice with comparable tumor load revealed a decrease in effector T-cell percentage and numbers, accompanied by a significant drop in activation marker expression and proliferation in the latter group (Online Supplementary Figure S1C-E). This suggests that the observed differences in CD8+ T cells in ibrutinibversus vehicle-treated mice were not secondary to changes in tumor load.
Ibrutinib modulates CD8+ T-cell function in the TCL1 adoptive transfer model
We next examined the impact of ibrutinib treatment on the expression of inhibitory receptors like PD-1, CD244 and Lag3 on CD8+ T cells. We observed a substantial drop in the expression of these markers in the ibrutinib cohort Figure 2A). As T-cell inhibitory receptors are mainly induced upon activation of tumor-reactive T cells,31 we evaluated whether the drop in their expression reflects an improvement in T-cell function or is rather a consequence of the drop in T-cell activation in ibrutinib-treated mice (Figure 1F). Thus, we analyzed the functional capacities of CD8+ T cells using intracellular flow cytometric staining following mitogen PMA/ionomycin stimulation. CD8+ T cells from ibrutinib-treated mice exhibited lower degranulation potential, as measured by CD107a presentation on the cell surface (Figure 2B). Furthermore, granzyme A (GzmA) and GzmB expression in CD8+ T cells significantly dropped in these mice (Figure 2C). Moreover, production of IFNwas significantly lower in CD8+ T cells from ibrutinib-treated mice (Figure 2D), collectively indicating poor cytotoxic and effector function of these cells. The changes in cytokine production and cytolytic abilities were primarily attributed to the decrease in the effector CD8+ fraction after ibrutinib treatment. Nonetheless, degranulation capacity, GzmA and GzmB levels were also decreased when focusing the analysis on the minor effector or PD-1+ population in ibrutinibtreated mice (Online Supplementary Figure S2A-F). In summary, these data indicate that in vivo ibrutinib treatment alters activation, effector differentiation and function of CD8+ T cells in the TCL1 AT model.
Ibrutinib modulates T-cell receptor signaling in CD8+ T cells in vitro
We then investigated the mechanisms that control the above-mentioned changes in T-cell function. While ibrutinib can indirectly impact T cells through BTK inhibition in CLL cells or other antigen-presenting cells in the microenvironment, the drug can potentially affect T-cell function in a direct manner through its off-target effects on ITK. To examine these possibilities, we tested the effect of different BTK inhibitors on TCR signaling using a reporter mouse line for Nr4a1, an immediate target of TCR activation. 24 Splenocytes from Nr4a1-GFP mice were pre-treated with ibrutinib or dimethyl sulfoxide (DMSO) as control and then stimulated with CD3 for 6 hours (h). We primarily used ibrutinib in a dose range of 100-1,000 nM, which results in ITK occupancy of up to 50% corresponding to the level observed in vivo in ibrutinib-treated CLL patients.15 CD3 stimulation resulted in a rapid increase of the Nr4a1-GFP signal in CD8+ T cells in DMSO controls (Figure 3A). Interestingly, ibrutinib treatment resulted in a 15% decrease in the Nr4a1-GFP MFI at 100 nM and abrogation of Nr4a1-GFP induction in most of the cells at a concentration of 1 M (Figure 3A). Similarly, the induction of early activation marker CD69 was significantly reduced at a concentration of 100 nM or higher (Figure 3A). We compared these effects to the more specific BTK inhibitors, CC-292 and ACP-196, which have ITK IC50 values of 24 and 1,000 nM, respectively, compared to that of 4.9 nM of ibrutinib.32 Interestingly, we observed that the decrease in Nr4a1-GFP and CD69 signals was less pronounced in CC-292 and was entirely absent upon ACP- 196 treatment (Figure 3A), indicating that these effects are BTK-independent. In line with these results, ibrutinib, but not ACP-196 treatment of mouse splenocytes, inhibited the expression of other activation markers like CD25, CD44 and CD137 on CD8+ T cells in response to CD3 stimulation (Figure 3B and Online Supplementary Figure S3A-C). In addition, CFSE dilution assays showed that ibrutinib, but not ACP-196, inhibited CD8+ T-cell proliferation (Online Supplementary Figure S3D). Similar to murine splenocytes, treatment of human PMBC with ibrutinib resulted in a dose-dependent decrease in proliferation of CD8+ T cells in response to CD3 stimulation (Figure 3C). Collectively, these data suggest that ibrutinib can modulate CD8+ T-cell response to TCR stimulation in a BTKindependent manner.
Strong co-stimulatory signals can rescue CD8+ T cells from inhibitory effects of ibrutinib in vitro
We next evaluated potential approaches to unleash CD8+ T cells from ibrutinib’s inhibitory effects. Previous work has shown that CD28 signaling is intact in the absence of ITK.33 Thus, we hypothesized that strong CD28 co-stimulation can hijack ibrutinib inhibitory effects on CD8+ T cells. Therefore, we evaluated the effect of the drug on murine CD8+ T cells stimulated with CD3 alone or CD3 plus CD28. The addition of CD28 antibody had no impact on the drop of Nr4a1-GFP signal after ibrutinib treatment (Figure 4A), which is in line with previous work demonstrating that Nr4a1 induction by TCR stimulation is independent of CD28 co-stimulation and remains intact in cd28-/- mice.24 Interestingly, CD28 costimulation completely abolished the inhibition of activation marker expression that is caused by ibrutinib (Figure 4A). Moreover, CD8+ T-cell proliferation was rescued to normal levels when co-stimulated by CD28 (Figure 4B). Similar results were observed by addition of CD28 antibody to human CD8+ T cells (Figure 4C), confirming that strong co-stimulatory signals can circumvent the TCR inhibitory effects of ibrutinib.
Blocking the PD-1/PD-L1 axis enhances the antileukemic activity of ibrutinib
In the subsequent experiments, we investigated possible immunomodulatory drugs that can recapitulate the in vitro effects of CD28 antibodies and thereby reverse the block of CD8+ T-cell differentiation in the TCL1 AT model. In light of recent results showing CD28 signaling as the primary target of PD-1 blockade,34,35 we reasoned that blocking the PD-1/PD-L1 axis can enhance anti-tumoral T-cell activity and improve therapeutic efficacy of ibrutinib. Thus, we treated CLL-bearing mice with ibrutinib alone or in combination with PD-1 or PD-L1 antibodies. As shown in Online Supplementary Figure S4, all treatment groups had comparable tumor load at the start of the treatment. Consistent with our previous work, blocking the PD-1/PD-L1 axis by PD-L1 resulted in delayed CLL development in PB, spleen and bone marrow (BM) (Figure 5A-C). The effects were more pronounced for PD-L1 compared to PD-1 treatment, which is likely due to the additional effects of PD-L1 antibodies on tumor-associated myeloid cells, as shown by us and others.9,36 Interestingly, combination of ibrutinib with PD-1 or PDL1 blocking antibodies resulted in enhanced disease control in PB, spleen and BM, which was most pronounced in the PD-L1/ibrutinib combination (Figure 5A-C), confirming a therapeutic efficacy of this combination.
Blocking the PD-1/PD-L1 axis expands the effector population and enhances the functional capacity of CD8+ T cells
We then examined the effect of PD-1/PD-L1 combination with ibrutinib on CD8+ T-cell activity. We restricted our analysis to PD-1 plus ibrutinib treatment as these mice had more comparable tumor load to the ibrutinib single arm (Figure 5A-C), and thereby we could exclude changes in T cells that are caused by differences in disease load. In line with our previous data, ibrutinib reduced the percentage of effector population, and decreased activation, proliferation and functional capacities of CD8+ T cells (Figure 6A-D). Interestingly, combination of ibrutinib with PD-1 resulted in a significant increase in effector CD8+ T-cell percentages (Figure 6A), which was accompanied by an increase in activation marker expression on CD8+ T cells (Figure 6B). Moreover, CD8+ T-cell functional capacity was improved by the combination treatment, as shown by a significant increase in degranulation capacity and IFNproduction (Figure 6C and D). The increase in degranulation capacity and IFNproduction was also observed when focusing the analysis on the CD8+ effector T-cell population (Online Supplementary Figure S5A and B). Collectively, these data show that blocking the PD-1/PDL1 pathway can improve CD8+ T-cell function and enhance CLL control after ibrutinib treatment.
Ibrutinib has been approved as a successful inhibitor of BTK for treatment of CLL and other B-cell lymphomas. In addition, it was also the first clinically available inhibitor of ITK.15 ITK is expressed in T cells in which, as a major player in TCR signaling, it is responsible for calcium mobilization, cytoskeleton reorganization, synapse formation and adhesion.37 Deletion or inhibition of ITK in CD8+ T cells results in their decreased expansion, delayed expression of cytolytic effector molecules, and defective degranulation upon TCR activation.38 This leads to a global defect in the cytolysis of pathogens, and as a consequence, to reduced viral clearance. In line with this, dramatic in vivo immunomodulation by ibrutinib has led to its approval for the treatment of refractory cGvHD,20 but the mechanisms underlying this clinical efficacy are poorly understood.
So far, modulating effects of ibrutinib on the differentiation of CD4+ T cells, like Th1, Th2, Th17 and Treg cells, have been described.15,19,22 In the current study, we observed a negative impact of ibrutinib on CD8+ T-cell proliferation and function in the TCL1 AT model, which reduces their phenotype to a level of tumor naïve control mice. As our in vitro data confirmed CD8+ T-cell inhibition by ibrutinib, but not the specific BTK inhibitor ACP-196, this effect is BTK-independent and most likely mediated by inhibition of ITK downstream of the TCR. Along this line, CC-292, an inhibitor with a higher selectivity for BTK, had a lower impact on T-cell activity in vitro, and has been previously shown not to impair T-cell function in the TCL1 AT model.39 But as these drugs might have different efficacies in patients, caution must be exercised when extrapolating clinical effects from these pre-clinical observations. Our observations in the TCL1 AT model seem to be in contrast to published data describing an increase of CD8+ T-cell numbers and their reduced expression of inhibitory receptors, like PD-1, in CLL patients after 8-20 weeks of treatment with ibrutinib.19 The results of this study suggest that this may be due to diminished activation- induced cell death of T cells through ITK inhibition. As our data demonstrate that inhibition of ITK by ibrutinib decreases TCR signaling and thereby activation of T cells, a consequence of that is not only reduced functional properties, as we show, but also diminished activationinduced cell death, confirming the observations of Long et al. in CLL patients.19 A further study documented that ibrutinib decreases CD8 T-cell proliferation and activation in patients 8 weeks after treatment start.22 However, these results have been largely viewed as a sign of favorable immune normalization under ibrutinib treatment, rather than a direct side effect of the drug. In light of our in vitro and in vivo results, it is more likely that these findings in CLL patients are due to the off-target effects of ibrutinib on ITK. In a further study that investigated T cells in CLL patients before and after 1 year of treatment with ibrutinib, disease-associated, elevated T-cell numbers and T-cell-related cytokine levels in PB had normalized, and T-cell repertoire diversity had increased significantly in treated patients.40 Considering the broad effects of BTK blockade on functional properties of many immune cell types, these changes in the T-cell compartment might be due to ibrutinib’s ability to rewire the carefully constructed, supportive microenvironmental network in CLL, which presumably contributes to the therapeutic success of this drug.41 But as ibrutinib, first-of-all, considerably redistributes malignant B cells from lymph nodes to blood, which ultimately results in a reduction of tumor burden, this suggests that normalization of the T-cell compartment under ibrutinib treatment is secondary to the effect of the drug on CLL-cell numbers and their localization. This is supported by our previous results as well as published data of others showing that T-cell expansion and exhaustion positively correlates with tumor load and predominantly occurs in secondary lymphoid organs.7-9 Along this line, enhanced engraftment and efficacy of CLL patientderived chimeric antigen receptor (CAR) T cells after more than 1 year of treatment with ibrutinib can be also explained by a normalization of T cells associated with a reduction of exhaustion phenotype, secondary to the effective control of CLL by the drug.42 In this study, the authors further show that ex vivo treatment of CLL CAR T cells with ibrutinib does not impact on their proliferation or function. Our data here clearly show that this observation is due to a commonly used stimulation protocol for T cells in vitro in which CD3 and CD28 antibodies are combined as stimuli. Co-stimulation of CD8+ T cells with CD28 was also used by Dubovsky et al. who describe that ibrutinib does not affect TCR signaling and function of these cells.15 This observation was in contrast to results obtained in ITK-deficient mice which show impaired TCR-dependent signaling and CD8+ T-cell effector function in response to viral infections.43 We now show that inhibition of T-cell activity by ibrutinib can be overcome by co-stimulatory signaling mediated by CD28, which is known to be independent of ITK.33 In line with our findings, stimulation of ITK-deficient CD8+ T cells with CD3 only leads to impaired expansion and activity.43
Considering our observations that ibrutinib negatively impacts on the activity of CD8+ T cells, one needs to investigate whether patients under long-term ibrutinib treatment have reduced adaptive immunity. In early clinical studies and applications of ibrutinib, this was hard to assess, as treated patients were relapsed and refractory, as well as high-risk CLL who have a profound immune suppression and perturbation of both innate and adaptive immunity, and therefore an increased susceptibility to infections is likely to be caused by the disease.44 Only more recently, with the approval of ibrutinib as first-line therapy for CLL, have high rates of infectious complications in patients on ibrutinib monotherapy and in combination with other drugs been observed.45 However, in comparison to the severe effects chemotherapy has on the immune system of patients, ibrutinib is reasonably welltolerated, and by monitoring the impact of ibrutinib on patients’ immune status, or by preventing immunosuppressive adverse effects by rational combination treatment approaches with drugs that improve T-cell effector function, outcome for patients can be even further improved. Recent data of clinical trials with the highly selective BTK inhibitor acalabrutinib showed overall response rates of 85% in treatment-naïve CLL patients and 94% in relapsed/refractory cases.46,47 Most adverse events (AE) observed in these trials were mild or moderate (grade 1-2) and were most commonly diarrhea and headache. It was hypothesized that due to its greater selectivity for BTK, acalabrutinib has favorable pharmacokinetic properties and an improved toxicity profile than ibrutinib. Considering, however, the short history of acalabrutinib treatment compared to ibrutinib, and the lack of a headto- head comparison of the two drugs in CLL patients, it remains unclear whether the long-term immune side effects of the drugs are comparable.
Interestingly, the immunomodulatory effect of ibrutinib can be even of therapeutic advantage, as shown in patients with relapsed CLL after allogeneic hematopoietic stem cell transplantation, in which ibrutinib was tolerable and effective.48
Our data in the TCL1 AT model show that combining ibrutinib with immune checkpoint blockade leads to enhanced CD8+ T-cell function and reduced CLL progression. Both PD-1 and PD-L1 treatment improved the therapeutic effect of ibrutinib, with better results observed with PD-1. As PD-L1 is expressed by CLL and myeloid cells in this model,25 this antibody has a broader activity compared to PD-1. Besides blocking the interaction with PD-1, PD-L1 but not PD-1 antibodies were shown to modulate myeloid cell subsets within the tumor microenvironment via activating Fcreceptors.36 Furthermore, blocking PD-L1 directly on tumor cells dampens their glycolysis, leaving more available glucose in the extracellular tumor milieu for T cells, which enhances their activity.49
Testing the combination of ibrutinib with immune checkpoint blockade in the mouse model allowed us to monitor tumor load in all organs affected by disease. In line with observations in CLL patients, ibrutinib as singleagent was not able to reduce malignant cells in the BM, which explains why patients and mice relapse if therapy is discontinued. Interestingly, if combined with PD-1 or PD-L1, tumor control in the BM was as efficient as in spleen and blood, suggesting that the combination of ibrutinib with checkpoint blockade might be able to eradicate CLL cells more efficiently, eventually leading to a cure.
- Received September 11, 2019
- Accepted March 3, 2020
No conflicts of interest to disclose.
Contributions BSH designed the study, performed experiments, analyzed and interpreted data, prepared figures, and wrote the manuscript; HY, YD, PMR and RS performed experiments, analyzed and interpreted data. SS and PL critically advised the study and reviewed the manuscript; MS designed and supervised the study, interpreted data, and wrote the manuscript.
This study was supported by the German José Carreras Foundation (13R/2018), the German Cancer Aid (grant number 112069), the BMBF-Network “PRECiSe” (031L0076A), the ERA-NET TRANSCAN-2 program JTC 2014–project FIRECLL, and the Cooperation Program in Cancer Research of the DKFZ and Israel’s Ministry of Science, Technology and Space. SS was supported by the DFG (SFB1074 subproject B1).
- Burger JA, O’Brien S.. Evolution of CLL treatment - from chemoimmunotherapy to targeted and individualized therapy. Nat Rev Clin Oncol. 2018; 15(8):510-527. https://doi.org/10.1038/s41571-018-0037-8PubMedGoogle Scholar
- Wiestner A. The role of B-cell receptor inhibitors in the treatment of patients with chronic lymphocytic leukemia. Haematologica. 2015; 100(12):1495-1507. https://doi.org/10.3324/haematol.2014.119123PubMedPubMed CentralGoogle Scholar
- Farooqui MZH, Valdez J, Martyr S. Ibrutinib for previously untreated and relapsed or refractory chronic lymphocytic leukaemia with TP53 aberrations: a phase 2, single-arm trial. Lancet Oncol. 2015; 16(2):169-176. https://doi.org/10.1016/S1470-2045(14)71182-9PubMedPubMed CentralGoogle Scholar
- Badar T, Burger JA, Wierda WG, O’Brien S.. Ibrutinib: a paradigm shift in management of CLL. Exp Rev Hematol. 2014; 7(6):705-717. https://doi.org/10.1586/17474086.2014.977862PubMedPubMed CentralGoogle Scholar
- Davids MS, Brown JR. Ibrutinib: a first in class covalent inhibitor of Bruton’s tyrosine kinase. Future Oncol. 2014; 10(6):957-967. https://doi.org/10.2217/fon.14.51PubMedPubMed CentralGoogle Scholar
- Hofbauer JP, Heyder C, Denk U. Development of CLL in the TCL1 transgenic mouse model is associated with severe skewing of the T-cell compartment homologous to human CLL. Leukemia. 2011; 25(9):1452-1458. https://doi.org/10.1038/leu.2011.111PubMedGoogle Scholar
- Riches JC, Davies JK, McClanahan F. T cells from CLL patients exhibit features of T-cell exhaustion but retain capacity for cytokine production. Blood. 2013; 121(9):1612-1621. https://doi.org/10.1182/blood-2012-09-457531PubMedPubMed CentralGoogle Scholar
- Hanna BS, Roessner PM, Yazdanparast H. Control of chronic lymphocytic leukemia development by clonally-expanded CD8+ T cells that undergo functional exhaustion in secondary lymphoid tissues. Leukemia. 2019; 33(3):625-637. https://doi.org/10.1038/s41375-018-0250-6PubMedGoogle Scholar
- McClanahan F, Hanna B, Miller S. PDL1 checkpoint blockade prevents immune dysfunction and leukemia development in a mouse model of chronic lymphocytic leukemia. Blood. 2015; 126(2):203-211. https://doi.org/10.1182/blood-2015-01-622936PubMedPubMed CentralGoogle Scholar
- Wierz M, Pierson S, Guyonnet L. Dual PD1/LAG3 immune checkpoint blockade limits tumor development in a murine model of chronic lymphocytic leukemia. Blood. 2018; 131(14):1617-1621. https://doi.org/10.1182/blood-2017-06-792267PubMedPubMed CentralGoogle Scholar
- Ding W, LaPlant BR, Call TG. Pembrolizumab in patients with CLL and Richter transformation or with relapsed CLL. Blood. 2017; 129(26):3419-3427. https://doi.org/10.1182/blood-2017-02-765685PubMedPubMed CentralGoogle Scholar
- Maharaj K, Sahakian E, Pinilla-Ibarz J.. Emerging role of BCR signaling inhibitors in immunomodulation of chronic lymphocytic leukemia. Blood Adv. 2017; 1(21):1867-1875. https://doi.org/10.1182/bloodadvances.2017006809PubMedPubMed CentralGoogle Scholar
- Kondo K, Shaim H, Thompson PA. Ibrutinib modulates the immunosuppressive CLL microenvironment through STAT3-mediated suppression of regulatory B-cell function and inhibition of the PD- 1/PD-L1 pathway. Leukemia. 2018; 32(4):960-970. https://doi.org/10.1038/leu.2017.304PubMedPubMed CentralGoogle Scholar
- Gunderson AJ, Kaneda MM, Tsujikawa T. Bruton tyrosine kinase-dependent immune cell cross-talk drives pancreas cancer. Cancer Discov. 2016; 6(3):270-285. https://doi.org/10.1158/2159-8290.CD-15-0827PubMedPubMed CentralGoogle Scholar
- Dubovsky JA, Beckwith KA, Natarajan G. Ibrutinib is an irreversible molecular inhibitor of ITK driving a Th1-selective pressure in T lymphocytes. Blood. 2013; 122(15):2539-2549. https://doi.org/10.1182/blood-2013-06-507947PubMedPubMed CentralGoogle Scholar
- Kohrt HE, Sagiv-Barfi I, Rafiq S. Ibrutinib antagonizes rituximab-dependent NK cell-mediated cytotoxicity. Blood. 2014; 123(12):1957-1960. https://doi.org/10.1182/blood-2014-01-547869PubMedPubMed CentralGoogle Scholar
- Ng PP, Lu DK, Sukbuntherng J. Ibrutinib enhances the activity of anti- CD20 antibodies in an MCL mouse model: effect of drug at clinically relevant concentrations on ADCC and ADCP. Blood. 2015; 126(23):3998-3998. https://doi.org/10.1182/blood.V126.23.3998.3998PubMedGoogle Scholar
- Podhorecka M, Goracy A, Szymczyk A. Changes in T-cell subpopulations and cytokine network during early period of ibrutinib therapy in chronic lymphocytic leukemia patients: the significant decrease in T regulatory cells number. Oncotarget. 2017; 8(21):34661-34669. https://doi.org/10.18632/oncotarget.16148PubMedPubMed CentralGoogle Scholar
- Long M, Beckwith K, Do P. Ibrutinib treatment improves T cell number and function in CLL patients. J Clin Invest. 2017; 127(8):3052-3064. https://doi.org/10.1172/JCI89756PubMedPubMed CentralGoogle Scholar
- Miklos D, Cutler CS, Arora M. Ibrutinib for chronic graft-versus-host disease after failure of prior therapy. Blood. 2017; 130(21):2243-2250. https://doi.org/10.1182/blood-2017-07-793786PubMedPubMed CentralGoogle Scholar
- Sagiv-Barfi I, Kohrt HE, Czerwinski DK. Therapeutic antitumor immunity by checkpoint blockade is enhanced by ibrutinib, an inhibitor of both BTK and ITK. Proc Natl Acad Sci U S A. 2015; 112(9):E966-972. https://doi.org/10.1073/pnas.1500712112PubMedPubMed CentralGoogle Scholar
- Niemann CU, Herman SEM, Maric I. Disruption of in vivo chronic lymphocytic leukemia tumor–microenvironment interactions by ibrutinib - findings from an investigator-initiated Phase II study. Clin Cancer Res. 2016; 22(7):1572-1582. https://doi.org/10.1158/1078-0432.CCR-15-1965PubMedPubMed CentralGoogle Scholar
- Bichi R, Shinton SA, Martin ES. Human chronic lymphocytic leukemia modeled in mouse by targeted TCL1 expression. Proc Natl Acad Sci U S A. 2002; 99(10):6955-6960. https://doi.org/10.1073/pnas.102181599PubMedPubMed CentralGoogle Scholar
- Moran AE, Holzapfel KL, Xing Y. T cell receptor signal strength in Treg and iNKT cell development demonstrated by a novel fluorescent reporter mouse. J Exp Med. 2011; 208(6):1279-1289. https://doi.org/10.1084/jem.20110308PubMedPubMed CentralGoogle Scholar
- Hanna BS, McClanahan F, Yazdanparast H. Depletion of CLL-associated patrolling monocytes and macrophages controls disease development and repairs immune dysfunction in vivo. Leukemia. 2016; 30(3):570-579. https://doi.org/10.1038/leu.2015.305PubMedGoogle Scholar
- Chang BY, Huang MM, Francesco M. The Bruton tyrosine kinase inhibitor PCI- 32765 ameliorates autoimmune arthritis by inhibition of multiple effector cells. Arthritis Res Ther. 2011; 13(4):R115. https://doi.org/10.1186/ar3400PubMedPubMed CentralGoogle Scholar
- Haderk F, Schulz R, Iskar M. Tumorderived exosomes modulate PD-L1 expression in monocytes. Sci Immunol. 2017; 2(13):eaah5509. https://doi.org/10.1126/sciimmunol.aah5509PubMedGoogle Scholar
- Quah BJ, Warren HS, Parish CR. Monitoring lymphocyte proliferation in vitro and in vivo with the intracellular fluorescent dye carboxyfluorescein diacetate succinimidyl ester. Nat Protoc. 2007; 2(9):2049-2056. https://doi.org/10.1038/nprot.2007.296PubMedGoogle Scholar
- Ponader S, Chen SS, Buggy JJ. The Bruton tyrosine kinase inhibitor PCI-32765 thwarts chronic lymphocytic leukemia cell survival and tissue homing in vitro and in vivo. Blood. 2012; 119(5):1182-1189. https://doi.org/10.1182/blood-2011-10-386417PubMedPubMed CentralGoogle Scholar
- Kaech SM, Cui W.. Transcriptional control of effector and memory CD8+ T cell differentiation. Nat Rev Immunol. 2012; 12(11):749-761. https://doi.org/10.1038/nri3307PubMedPubMed CentralGoogle Scholar
- Fuertes Marraco SA, Neubert NJ, Verdeil G, Speiser DE. Inhibitory receptors beyond T cell exhaustion. Front Immunol. 2015; 6:310. https://doi.org/10.3389/fimmu.2015.00310PubMedPubMed CentralGoogle Scholar
- Barf T, Covey T, Izumi R. Acalabrutinib (ACP-196): a covalent Bruton tyrosine kinase inhibitor with a differentiated selectivity and in vivo potency profile. J Pharmacol Exp Ther. 2017; 363(2):240-252. https://doi.org/10.1124/jpet.117.242909PubMedGoogle Scholar
- Li C-R, Berg LJ. Cutting Edge: Itk is not essential for CD28 signaling in naive T cells. J Immunol. 2005; 174(8):4475-4479. https://doi.org/10.4049/jimmunol.174.8.4475PubMedGoogle Scholar
- Kamphorst AO, Wieland A, Nasti T. Rescue of exhausted CD8 T cells by PD-1- targeted therapies is CD28-dependent. Science. 2017; 355(6332):1423-1427. https://doi.org/10.1126/science.aaf0683PubMedPubMed CentralGoogle Scholar
- Hui E, Cheung J, Zhu J. T cell costimulatory receptor CD28 is a primary target for PD-1-mediated inhibition. Science. 2017; 355(6332):1428-1433. https://doi.org/10.1126/science.aaf1292PubMedPubMed CentralGoogle Scholar
- Dahan R, Sega E, Engelhardt J. FcRs modulate the anti-tumor activity of antibodies targeting the PD-1/PD-L1 axis. Cancer Cell. 2015; 28(3):285-295. https://doi.org/10.1016/j.ccell.2015.08.004PubMedGoogle Scholar
- Bunnell SC, Diehn M, Yaffe MB. Biochemical interactions integrating Itk with the T cell receptor-initiated signaling cascade. J Biol Chem. 2000; 275(3):2219-2230. https://doi.org/10.1074/jbc.275.3.2219PubMedGoogle Scholar
- Kapnick SM, Stinchcombe JC, Griffiths GM, Schwartzberg PL. Inducible T cell kinase regulates the acquisition of cytolytic capacity and degranulation in CD8+ CTLs. J Immunol. 2017; 198(7):2699-2711. https://doi.org/10.4049/jimmunol.1601202PubMedPubMed CentralGoogle Scholar
- Lee-Vergés E, Hanna BS, Yazdanparast H. Selective BTK inhibition improves bendamustine therapy response and normalizes immune effector functions in chronic lymphocytic leukemia. Int J Cancer. 2019; 144(11):2762-2773. https://doi.org/10.1002/ijc.32010PubMedGoogle Scholar
- Yin Q, Sivina M, Robins H. Ibrutinib therapy increases T cell repertoire diversity in patients with chronic lymphocytic leukemia. J Immunol. 2017; 198(4):1740-1747. https://doi.org/10.4049/jimmunol.1601190PubMedPubMed CentralGoogle Scholar
- Bachireddy P, Wu CJ. Arresting the inflammatory drive of chronic lymphocytic leukemia with ibrutinib. Clin Cancer Res. 2016; 22(7):1547-1549. https://doi.org/10.1158/1078-0432.CCR-15-3106PubMedPubMed CentralGoogle Scholar
- Fraietta JA, Beckwith KA, Patel PR. Ibrutinib enhances chimeric antigen receptor T-cell engraftment and efficacy in leukemia. Blood. 2016; 127(9):1117-1127. https://doi.org/10.1182/blood-2015-11-679134PubMedPubMed CentralGoogle Scholar
- Atherly LO, Brehm MA, Welsh RM, Berg LJ. Tec kinases Itk and Rlk are required for CD8+ T cell responses to virus infection independent of their role in CD4+ T cell help. J Immunol. 2006; 176(3):1571-1581. https://doi.org/10.4049/jimmunol.176.3.1571PubMedGoogle Scholar
- Kipps TJ, Stevenson FK, Wu CJ. Chronic lymphocytic leukaemia. Nat Rev Dis Primers. 2017; 3:16096. https://doi.org/10.1038/nrdp.2016.96PubMedPubMed CentralGoogle Scholar
- Tillman BF, Pauff JM, Satyanarayana G, Talbott M, Warner JL. Systematic review of infectious events with the Bruton tyrosine kinase inhibitor ibrutinib in the treatment of hematologic malignancies. Eur J Haematol. 2018; 100(4):325-334. https://doi.org/10.1111/ejh.13020PubMedGoogle Scholar
- Sharman JP, Banerji V, Fogliatto LM. ELEVATE TN: Phase 3 study of acalabrutinib combined with obinutuzumab (O) or alone vs O plus chlorambucil (Clb) in patients (Pts) with treatment-naive chronic lymphocytic leukemia (CLL). Blood. 2019; 134(Suppl 1):31. https://doi.org/10.1182/blood-2019-128404PubMedGoogle Scholar
- Byrd JC, Wierda WG, Schuh A. Acalabrutinib monotherapy in patients with relapsed/refractory chronic lymphocytic leukemia: updated phase 2 results. Blood. 2020; 135(15):1204-1213. https://doi.org/10.1182/blood.2018884940PubMedPubMed CentralGoogle Scholar
- Ryan CE, Sahaf B, Logan AC. Ibrutinib efficacy and tolerability in patients with relapsed chronic lymphocytic leukemia following allogeneic HCT. Blood. 2016; 128(25):2899-2908. https://doi.org/10.1182/blood-2016-06-715284PubMedPubMed CentralGoogle Scholar
- Chang C-H, Qiu J, O’Sullivan D. Metabolic competition in the tumor microenvironment is a driver of cancer progression. Cell. 2015; 162(6):1229-1241. https://doi.org/10.1016/j.cell.2015.08.016PubMedPubMed CentralGoogle Scholar
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