Abstract
Tafasitamab is an Fc-modified monoclonal antibody that binds to CD19, a cell-surface antigen that is broadly expressed on various types of B-cell non-Hodgkin’s lymphoma (NHL). Antibody-dependent cellular cytotoxicity (ADCC), a key mode of action of tafasitamab, is mediated through the binding of tafasitamab’s Fc region to FcγRIIIa receptors on immune effector cells and results in antitumor activity. Despite the proven clinical activity of tafasitamab in combination with lenalidomide in the treatment of diffuse large B-cell lymphoma (DLBCL), a higher number of immune cells in cancer patients may improve the activity of tafasitamab. Here, we characterized two ex vivo-expanded FcγRIIIa receptor—expressing cell types—γδ T and MG4101 natural killer (NK) cells—as effector cells for tafasitamab in vitro, and found that in the presence of these cells tafasitamab was able to induce ADCC against a range of NHL cell lines and patient-derived cells. We also explored the concept of effector cell supplementation during tafasitamab treatment in vivo by coadministering MG4101 NK cells in Raji and Ramos xenograft models of NHL. Combination treatment of tafasitamab and allogeneic MG4101 NK cells in these models demonstrated a survival benefit compared with tafasitamab or MG4101 monotherapy (Raji: 1.7- to 1.9-fold increase in lifespan; Ramos: 2.0- to 4.1-fold increase in lifespan). In conclusion, adoptive cell transfer of ex vivo-expanded allogeneic NK or autologous γδ T cells in combination with tafasitamab treatment may potentially be a promising novel approach to increase the number of immune effector cells and enhance the antitumor effect of tafasitamab.
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Introduction
Tafasitamab (MOR208) is an Fc-modified, humanized monoclonal antibody that binds to the human B-cell surface antigen CD19 [1, 2]. CD19 is broadly and homogeneously expressed across B-cell malignancies, including diffuse large B-cell lymphoma (DLBCL), chronic lymphocytic leukemia (CLL), Burkitt’s lymphoma (BL), and mantle cell lymphoma (MCL) [3]. Tafasitamab’s modes of action include antibody-dependent cellular cytotoxicity (ADCC), antibody-dependent cellular phagocytosis, and direct cytotoxicity (apoptosis) [1, 2]. In vitro, tafasitamab has shown cytotoxicity against a range of B-cell lymphoma and leukemia cell lines [1, 2]. In a Phase II clinical study with relapsed or refractory (R/R) DLBCL patients, tafasitamab in combination with the immunomodulatory drug lenalidomide was well tolerated and resulted in 60% of patients achieving an objective response, with a median duration of 21.7 months [4]. Based on this study, tafasitamab in combination with lenalidomide received accelerated approval by the Food and Drug Administration in 2020 for the treatment of transplant-ineligible adult patients with R/R DLBCL.
Tafasitamab has two amino acid substitutions in the Fc region (S239D/I332E) that increase its affinity for Fcγ receptors, including FcγRIIIa (CD16) [2]. FcγRIIIa plays a key role in mediating ADCC and is expressed on the surface of natural killer (NK) cells and most γδ T cells [5]. The ADCC potency of tafasitamab in vitro is 100- to 1000-fold higher relative to an unmodified anti-CD19 IgG1 analogue [2], suggesting an important role for CD16-positive immune effector cells in ADCC-mediated antitumor activity.
Several clinical trials have reported that low numbers of NK cells in peripheral blood adversely affect the treatment outcomes of patients with lymphomas undergoing immunotherapy [6, 7]. Furthermore, γδ T cells in cancer patients have been found in reduced numbers and with a diminished proliferative capacity relative to healthy donors [8,9,10]. A Phase I clinical study of patients with malignant lymphoma or advanced solid tumors who were treated with healthy human donor–derived, ex vivo-expanded allogeneic NK cells (MG4101) reported stable disease in 8 of 17 evaluable patients (47.1%) and a promising safety profile [11]. Similarly, adoptive immune cell therapy with autologous γδ T cells demonstrated a low toxicity profile with modest therapeutic efficacy as monotherapy in several clinical trials [10]. Therefore, combination of tafasitamab with adoptive NK or γδ T cell therapy may potentially be a promising novel approach to increase the number of immune effector cells in the tumor microenvironment and enhance the antitumor effects of tafasitamab. Prior studies have shown enhanced cytotoxicity of γδ T cells or allogeneic NK cells against a variety of tumor types upon combination with therapeutic antibodies, including rituximab and trastuzumab [12,13,14,15].
To explore this concept for tafasitamab, we confirmed the ability of ex vivo-expanded γδ T or allogeneic NK cells (MG4101) to mediate tafasitamab-induced ADCC against lymphoma cells in vitro. In addition, we investigated the potential of adoptive cell therapy in combination with tafasitamab by supplementing tafasitamab treatment with MG4101 ex vivo-expanded NK cells in disseminated tumor mouse models of NHL.
Materials and methods
Antibodies
Tafasitamab and XmAb5603, an anti-CD19 analogue of tafasitamab with a wild-type IgG1 Fc region, were provided by MorphoSys AG. As controls, either a polyclonal IgG1 isotype control (Sigma I5154) or an IgG control (Sigma I4506) were used.
Cell isolation and culture
γδ T cells
γδ T cells were generated by zoledronate and interleukin-2 stimulation and culture of peripheral blood mononuclear cells (PBMCs) from different healthy donors for 9–12 days as described previously [16].
MG4101 NK cells
PBMCs were isolated from healthy donors by leukapheresis. NK cells were enriched, expanded, and cryopreserved as described previously [17].
Primary human leukemia and lymphoma cells
Primary human leukemia and lymphoma cells were isolated from heparinized peripheral blood or bone marrow biopsies of patients recruited at the Nuremberg University Hospital, Germany.
Cell lines
Jeko-1, Mino, Daudi, U-2932, Raji, and Ramos cell lines were obtained from the German Collection of Microorganisms and Cell Cultures or the American Type Culture Collection and cultured in standard medium.
Cytotoxicity assays
γδ T cells as effector cells
ADCC with γδ T cells was determined by flow cytometry as described previously [16]. After incubation of carboxyfluorescein succinimidyl ester (CFSE)-labeled target cells (T) with antibody and effector cells (E) for 4 h at 37 °C and E/T ratios ranging from 0.7:1 to 20:1, cells were harvested, stained with TO-PRO-3, and evaluated by flow cytometry. Cell lysis at each E/T ratio was calculated using the following formula: \({\text{Cell lysis}}\,\left( \% \right) = \frac{{\left( {\% {\text{TO-PRO-3-positive cells}} - \% {\text{TO-PRO-3-positive cells in target cell-only culture}}} \right)}}{{\left( {{100} - \% {\text{TO-PRO-3-positive cells in target cell-only culture}}} \right)}} \times {100}.\)
Allogeneic NK cells as effector cells
For quantification of ADCC, target cells were labeled with calcein-AM. Monoclonal antibodies (tafasitamab or control IgG) were added to the target cells and incubated with MG4101 NK effector cells at an E/T ratio of 3:1. After incubation for 2 h, plates were centrifuged and calcein release was quantified using a fluorescence microplate reader. As a control, maximal lysis (release) was induced with 1% Triton X-100. The percentage of ADCC-mediated cell lysis was measured by calcein release from target cells and calculated using the following formula: \({\text{Cell lysis}}\; \left( \% \right) = \frac{{\left( {{\text{sample release}} - {\text{spontaneous release}}} \right)}}{{\left( {{\text{maximal release}} - {\text{spontaneous release}}} \right)}} \times {100}. \)
In vivo lymphoma xenograft models
For the disseminated Raji model, 1 × 105 Raji cells/mouse were intravenously (i.v.) injected into the tail vein of CB17/Icr-Prkdcscid/CrlCrlj (CB-17 SCID) mice on Day 0 and cryopreserved MG4101 NK cells (2 × 107 cells/mouse) or freezing medium (vehicle control) were administered i.v. on Days 1, 3, 6, 8, and 10. Tafasitamab was administered subcutaneously (s.c.) once on Day 1 at a dose of 2.5 μg/kg. In the disseminated Ramos model, 1 × 106 Ramos cells/mouse were injected i.v. on Day 0 and MG4101 NK cells were administered i.v. on Days 4, 7, 11, 14, 18, and 21. Tafasitamab was administered i.v. on Days 3, 6, 10, 13, 17, and 20 at a dose of 10 mg/kg. Mice were monitored daily for tumor-associated morbidity, mortality, and hind limb paraplegia.
All animal experiments were approved by the Institutional Animal Care and Use Committee of the Korea Research Institute of Bioscience & Biotechnology.
Data and statistical analysis
Statistical significance in ADCC experiments was calculated using a two-tailed paired t test. Increased life span (%) in mouse models of survival was calculated using the following formula: \({\text{Increased life span}}\;\left( \% \right) = \frac{{\left( {{\text{median survival treatment}} - {\text{median survival control}}} \right)}}{{\text{median survival control }}}{ } \times {100}. \)The log-rank test was used to compare survival of control and test groups. A P value < 0.05 was considered statistically significant for all experiments.
Results
Tafasitamab induced killing of NHL cell lines and primary CLL and MCL cells by γδ T cells
ADCC assays using γδ T cells expanded from PBMCs of three healthy human donors demonstrated that tafasitamab induced cytotoxicity against Mino and Jeko (MCL) cell lines in an E/T ratio-dependent manner (Fig. 1a, b). Furthermore, part of this activity was related to tafasitamab’s Fc-enhancement because an unmodified IgG1 analogue (XmAb5603) induced a lower ADCC. Although similar levels of tafasitamab-induced cytotoxicity were observed against U-2932 (DLBCL) cells, no meaningful conclusion could be drawn for Daudi (BL) cells because of high background levels of cell death (Fig. 1c, d).
Next, we analyzed the ADCC of γδ T cells in combination with tafasitamab against primary CLL and MCL cells derived from two individual patients per indication. Whereas tafasitamab induced tumor cell death in an E/T ratio–dependent manner, XmAb5603 showed no substantial increase in cell death compared with background levels (Fig. 2). Altogether, these findings demonstrate that γδ T cells could serve as effector cells for tafasitamab by mediating ADCC against NHL cell lines and primary tumor cells.
Combination of tafasitamab and allogeneic NK cells led to increased antitumor activity in disseminated BL mouse xenograft tumor models
Prior to in vivo studies, the ability of ex vivo-expanded, cryopreserved MG4101 NK cells (isolated from three healthy donors) to mediate tafasitamab-induced ADCC was evaluated in vitro using Raji and Ramos cell lines. Compared with the IgG isotype control, tafasitamab induced increased ADCC against both Raji and Ramos cell lines (Fig. 3).
Next, tafasitamab in combination with MG4101 immune cell supplementation was evaluated in two disseminated BL survival models in severe combined immunodeficiency (SCID) mice. First, in a preventive Raji model, a single subcutaneous low dose of 2.5 μg/kg tafasitamab was given on Day 1 after tumor inoculation, and MG4101 cells were administered i.v. on Days 1, 3, 6, 8, and 10. Combination treatment resulted in a greater increase in lifespan (ILS) than tafasitamab and MG4101 monotherapies (ILS 100% vs. 57% and 51%, respectively; increase in lifespan 1.7- to 1.9-fold; Fig. 4a).
Second, in a Ramos BL tumor model, SCID mice were treated i.v. with 6 doses of 10 mg/kg tafasitamab on Days 3, 6, 10, 13, 17, and 20 after tumor inoculation. In this model, increased survival was observed for the tafasitamab-treated mice compared with the IgG isotype control group (ILS 49.2%; Fig. 4b). MG4101 cell therapy was given on Days 4, 7, 11, 14, 18, and 21, leading to an ILS of 24.6%. In contrast, combination therapy (tafasitamab plus MG4101 cells) resulted in an ILS of 103.3%, which was more than additive of the ILS of each monotherapy (increase in lifespan 2.0- to 4.1-fold; Fig. 4b).
Discussion
This study examined the suitability of ex vivo-expanded NK and γδ T cells as effector cells for tafasitamab-induced cytotoxicity against various NHL subtypes, including MCL, CLL, and BL, in vitro and in vivo. In clinical trials of immunochemotherapy-treated NHL patients, low numbers of NK cells in peripheral blood or tumor tissue prior to treatment have been linked with poor outcomes [4, 6, 7]. Therefore, we hypothesized that supplementing effector cells could potentially enhance tafasitamab’s antitumor activity.
The feasibility of such an approach has been reported recently in a Phase I clinical study of R/R B-cell NHL patients who were treated with the CD20-targeted antibody rituximab and MG4101 allogeneic NK cells [18]. Here, we explored the feasibility of using tafasitamab, a therapeutic antibody that targets a different antigen: CD19. In SCID mice carrying disseminated Ramos tumors, MG4101 plus tafasitamab combination treatment significantly increased survival compared with the respective monotherapies. A similar survival benefit was also observed when using a single low dose of tafasitamab in a preventive Raji model to simulate minimum residual disease and potentially low antibody concentrations in the tumor. These data are in line with an earlier study using a Raji tumor model where mice treated with rituximab plus NK cells showed a significant increase in survival [19].
As an alternative to adoptive NK cell therapy, we focused on γδ T cells, which are able to infiltrate different cancerous tissues and inhibit tumor growth and metastases [16]. Hoeres et al. previously demonstrated that combination of γδ T cells with the CD20-targeted antibodies rituximab and obinutuzumab resulted in elimination of MCL and CLL lymphoma cells in vitro [16]. However, as CD16 expression on γδ T cells is weaker than on NK cells, and CD19 is often expressed at lower levels on target lymphoma cells than CD20 [5, 20], it was important to confirm that these immune cells can indeed serve as effector cells for tafasitamab, especially against primary lymphoma cells. The activity of tafasitamab observed in our study was similar to the activity previously reported with CD20-targeted antibodies [16].
In vitro analyses of ex vivo-expanded NK and γδ T cells by Niu et al. showed that γδ T cells had a higher proliferative capacity than NK cells, whereas NK cells had a stronger ability to secrete cytokines and a higher overall cytotoxicity [21]. These data provide rationale that the clinical administration of either cell type in combination with tafasitamab treatment could potentially be beneficial for patients. Overall, allogeneic immune cell–antibody combination therapies may have advantages over autologous cell transfer strategies because the former have fewer manufacturing challenges and cryopreserved batches are readily available for treatment. Moreover, whereas allogeneic NK cell therapy and tafasitamab treatment have both been reported to be well tolerated as monotherapies in clinical trials [4, 22], other cellular therapies such as CAR-T cells are often associated with toxicities such as cytokine release syndrome and neurotoxicity [23].
In conclusion, we have provided preclinical evidence showing that combinations of tafasitamab with γδ T or allogeneic NK cells could be promising strategies for leveraging the full therapeutic potential of tafasitamab against CD19-positive B-cell tumors.
About tafasitamab
Tafasitamab is a humanized Fc-modified cytolytic CD19-targeting monoclonal antibody. In 2010, MorphoSys licensed exclusive worldwide rights to develop and commercialize tafasitamab from Xencor, Inc.
Tafasitamab incorporates an XmAb® engineered Fc domain, which mediates B-cell lysis through apoptosis and immune effector mechanism including antibody-dependent cell-mediated cytotoxicity (ADCC) and antibody-dependent cellular phagocytosis (ADCP).
In January 2020, MorphoSys and Incyte entered into a collaboration and licensing agreement to further develop and commercialize tafasitamab globally. Following accelerated approval by the U.S. Food and Drug Administration in July 2020, tafasitamab is being co-commercialized by MorphoSys and Incyte in the United States. Incyte has exclusive commercialization rights outside the United States.
XmAb® is a trademark of Xencor, Inc.
Availability of data and materials
Data may be provided for reasonable academic studies upon request by the corresponding author.
Code availability
Not applicable.
References
Awan FT, Lapalombella R, Trotta R et al (2010) CD19 targeting of chronic lymphocytic leukemia with a novel Fc-domain-engineered monoclonal antibody. Blood 115:1204–1213. https://doi.org/10.1182/blood-2009-06-229039
Horton HM, Bernett MJ, Pong E et al (2008) Potent in vitro and in vivo activity of an Fc-engineered anti-CD19 monoclonal antibody against lymphoma and leukemia. Cancer Res 68:8049–8057. https://doi.org/10.1158/0008-5472.CAN-08-2268
Olejniczak SH, Stewart CC, Donohue K, Czuczman MS (2006) A quantitative exploration of surface antigen expression in common B-cell malignancies using flow cytometry. Immunol Invest 35:93–114. https://doi.org/10.1080/08820130500496878
Salles G, Duell J, González Barca E et al (2020) Tafasitamab plus lenalidomide in relapsed or refractory diffuse large B-cell lymphoma (L-MIND): a multicentre, prospective, single-arm, phase 2 study. Lancet Oncol 21:978–988. https://doi.org/10.1016/S1470-2045(20)30225-4
Braakman E, van de Winkel JGJ, van Krimpen BA et al (1992) CD16 on human γδ T lymphocytes: expression, function, and specificity for mouse IgG isotypes. Cell Immunol 143:97–107. https://doi.org/10.1016/0008-8749(92)90008-D
He L, Zhu HY, Qin SC et al (2016) Low natural killer (Nk) cell counts in peripheral blood adversely affect clinical outcome of patients with follicular lymphoma. Blood Cancer J 6:e457. https://doi.org/10.1038/bcj.2016.67
Klanova M, Oestergaard MZ, Trneny M et al (2019) Prognostic impact of natural killer cell count in follicular lymphoma and diffuse large b-cell lymphoma patients treated with immunochemotherapy. Clin Cancer Res 25:4632–4643. https://doi.org/10.1158/1078-0432.CCR-18-3270
Wistuba-Hamprecht K, Martens A, Haehnel K et al (2016) Proportions of blood-borne Vδ1+ and Vδ2+ T-cells are associated with overall survival of melanoma patients treated with ipilimumab. Eur J Cancer 64:116–126. https://doi.org/10.1016/j.ejca.2016.06.001
Wilhelm M, Kunzmann V, Eckstein S et al (2003) γδ T cells for immune therapy of patients with lymphoid malignancies. Blood 102:200–206. https://doi.org/10.1182/blood-2002-12-3665
Hoeres T, Smetak M, Pretscher D, Wilhelm M (2018) Improving the efficiency of Vγ9Vδ2 T-cell immunotherapy in cancer. Front Immunol 9:800. https://doi.org/10.3389/fimmu.2018.00800
Yang Y, Lim O, Kim TM et al (2016) Phase I study of random healthy donor-derived allogeneic natural killer cell therapy in patients with malignant lymphoma or advanced solid tumors. Cancer Immunol Res 4:215–224. https://doi.org/10.1158/2326-6066.CIR-15-0118
Tokuyama H, Hagi T, Mattarollo SR et al (2008) Vγ9Vδ2 T cell cytotoxicity against tumor cells is enhanced by monoclonal antibody drugs-Rituximab and trastuzumab. Int J Cancer 122:2526–2534. https://doi.org/10.1002/ijc.23365
Braza MS, Klein B, Fiol G, Rossi JF (2011) γδT-cell killing of primary follicular lymphoma cells is dramatically potentiated by GA101, a type II glycoengineered anti-CD20 monoclonal antibody. Haematologica 96:400–407. https://doi.org/10.3324/haematol.2010.029520
Capietto A-H, Martinet L, Fournié J-J (2011) Stimulated γδ T cells increase the in vivo efficacy of trastuzumab in her-2 + breast cancer. J Immunol 187:1031–1038. https://doi.org/10.4049/jimmunol.1100681
Sanchez-Martinez D, Allende-Vega N, Orecchioni S et al (2018) Expansion of allogeneic NK cells with efficient antibody-dependent cell cytotoxicity against multiple tumors. Theranostics 8:3856–3869. https://doi.org/10.7150/thno.25149
Hoeres T, Pretscher D, Holzmann E et al (2019) Improving immunotherapy against b-cell malignancies using γδ T-cell-specific stimulation and therapeutic monoclonal antibodies. J Immunother 42:331–344. https://doi.org/10.1097/CJI.0000000000000289
Min B, Choi H, Her JH et al (2018) Optimization of large-scale expansion and cryopreservation of human natural killer cells for anti-tumor therapy. Immune Netw 18:e31. https://doi.org/10.4110/in.2018.18.e31
Yoon DH, Koh Y, Jung M, et al (2020) Feasibility of allogeneic natural killer cells, MG4101 in combination with rituximab in patients with relapsed or refractory non-Hodgkin lymphomas; a Phase 1, open-label, multicenter study. In: EHA Library, p 293988
Lim O, Lee Y, Chung H et al (2013) GMP-compliant, large-scale expanded allogeneic natural killer cells have potent cytolytic activity against cancer cells in vitro and in vivo. PLoS ONE 8:e53611. https://doi.org/10.1371/journal.pone.0053611
Boltežar L, Prevodnik VK, Perme MP et al (2018) Comparison of the algorithms classifying the ABC and GCB subtypes in diffuse large B-cell lymphoma. Oncol Lett 15:6903–6912. https://doi.org/10.3892/ol.2018.8243
Niu C, Jin H, Li M et al (2015) In vitro analysis of the proliferative capacity and cytotoxic effects of ex vivo induced natural killer cells, cytokine-induced killer cells, and gamma-delta T cells. BMC Immunol 16:61. https://doi.org/10.1186/s12865-015-0124-x
Veluchamy JP, Kok N, van der Vliet HJ et al (2017) The rise of allogeneic natural killer cells as a platform for cancer immunotherapy: recent innovations and future developments. Front Immunol 8:631. https://doi.org/10.3389/fimmu.2017.00631
Yáñez L, Sánchez-Escamilla M, Perales MA (2019) CAR T cell toxicity: current management and future directions. HemaSphere 3:e186. https://doi.org/10.1097/HS9.0000000000000186
Acknowledgements
Medical writing and editorial support were provided by Tony Ferrar of Porterhouse Medical Group. This support was funded by MorphoSys AG, Planegg, Germany, in accordance with Good Publication Practice (GPP3) guidelines.
Funding
These studies were funded by GC LabCell Corporation, MorphoSys AG, and grants from the ‘Verein Hilfe für Krebskranke e.V.’ and the W. Lutz Stiftung. gc labcell corporation, morphosys ag, w. lutz stiftung, verein hilfe für krebskranke e.v
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Conception and design of the work were performed by Jung Hyun Her, Dominik Pretscher, Sung Yoo Cho, Yu Kyeong Hwang, Timm Hoeres, Rainer Boxhammer, Martin Wilhelm, Stefan Steidl, Jan Endell. All authors were responsible for acquisition, analysis, or interpretation of the data; preparation or revision of the initial and/or subsequent manuscript drafts and revision and approval of the submitted manuscript.
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MP, JS, RB, CH, SS, and JE are employees of MorphoSys AG, Planegg, Germany. SS owns shares of MorphoSys AG. GC LabCell and MorphoSys AG report a joint patent application.
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All animal experiments were approved by the Institutional Animal Care and Use Committee of the Korea Research Institute of Bioscience and Biotechnology. Written informed consent was obtained from patients and healthy donors prior to the studies, in accordance with the Declaration of Helsinki.
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Her, J.H., Pretscher, D., Patra-Kneuer, M. et al. Tafasitamab mediates killing of B-cell non-Hodgkin’s lymphoma in combination with γδ T cell or allogeneic NK cell therapy. Cancer Immunol Immunother 71, 2829–2836 (2022). https://doi.org/10.1007/s00262-022-03165-w
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DOI: https://doi.org/10.1007/s00262-022-03165-w