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The CD20 mAb ofatumumab (OFA) induces complement-mediated lysis of B cells. In an investigator-initiated phase II trial of OFA plus chemotherapy for chronic lymphocytic leukemia (CLL), OFA treatment promoted partial CLL B cell depletion which coincided with reduced complement titers. Remaining CLL B cells circulated with bound OFA and covalently bound complement breakdown product C3d, indicative of ongoing complement activation. Presumably neither complement- nor effector cell-based mechanisms were sufficiently robust to clear these remaining B cells. Instead, almost all of the bound OFA as well as CD20 was removed from the cells, in accordance with previous clinical studies which demonstrated comparable loss of CD20 from B cells after treatment of CLL patients with rituximab. In vitro experiments with OFA and rituximab addressing these observations suggest that host effector mechanisms which support mAb-mediated lysis and tumor cell clearance are finite, and they can be saturated or exhausted at high B cell burdens, particularly at high mAb concentrations. Interestingly, only a fraction of available complement was required to kill cells with CD20 mAbs, and killing could be tuned by titrating the mAb concentration. Consequently, maximal B cell killing of an initial and secondary B cell challenge was achieved with intermediate mAb concentrations, whereas high concentrations promoted lower overall killing. Therefore mAb therapies that rely substantially on effector mechanisms subject to exhaustion, including complement, may benefit from lower, more frequent dosing schemes optimized to sustain and maximize killing by cytotoxic immune effector systems.
The B cell-targeting CD20 mAbs, rituximab (RTX) and ofatumumab (OFA), achieve the high levels of cytotoxicity necessary for effective cancer treatment by employing effector mechanisms of the body’s innate immune system (1–11). These mechanisms include complement-dependent cytotoxicity (CDC), antibody-dependent cell-mediated cytotoxicity (ADCC) and phagocytosis. In CDC, mAb-targeted cells activate the classical pathway of complement by which they are covalently tagged with activated complement protein fragments C4b and C3b, and are then lysed due to generation of membrane attack complexes (12–14). However, the increased understanding of immunotherapeutic mAb cytotoxic mechanisms, including that of alemtuzumab (ALM) which also kills targeted cells by CDC (15,16), has not yet led to scientifically formulated fundamental approaches to dosing regimens. Indeed, most modifications of dosing strategies have been empirical, with the unstated presumption that for CD20 mAbs the usual weekly 375 mg/m2 RTX treatment is likely to be close to an optimal dose (17–19). For the CD52 mAb ALM, dosing has been set at 10–30 mg three times weekly.
Because of low CD20 expression on chronic lymphocytic leukemia (CLL) cells together with high tumor burden, the efficiency of OFA-mediated CDC is particularly relevant for CLL treatment (6,8,10,20–22). As part of a phase II trial in CLL (NCT 01145209) combining intravenous OFA infusion with chemotherapy, we investigated the in vivo consequences of OFA treatment on circulating B cells, and evaluated absolute lymphocyte counts (ALC), complement consumption, C3 fragment deposition on cells and levels of B cell-associated CD20 and bound OFA.
At the trial start, patients had high burdens of circulating B cells which were significantly reduced by day 29. In addition, large reductions in complement titers were observed, most notably after the first OFA infusion. Intriguingly, non-depleted cells included B cells with substantial amounts of deposited complement C3 breakdown fragment C3d; these cells could continue circulating for extended time periods. Based on these findings we conducted parallel quantitative in vitro investigations comparing OFA and RTX with respect to their potential to activate and consume complement and to promote CDC upon binding to CD20+ cells.
In vitro studies demonstrated the ability of OFA to induce robust CDC in which only a fraction of available complement components were required to effect cell killing. Using high cell burden conditions, we demonstrated that complement could be severely depleted, leading to inadequate killing of a second target cell challenge. Significantly, we were able to reduce complement consumption and retain killing capability by reducing OFA concentrations. Our studies suggest that standard doses of CD20 mAb, in contrast with current dogma, may be excessive, resulting in wasteful complement consumption which depletes the body’s complement reservoir and cytotoxic capacity. This insight provides a framework for the design of mAb-based immunotherapy regimens that preserve complement as well as other effector functions, thus leading to increased overall tumor cell killing and potentially enhanced efficacy.
Cycle 1: Patients received intravenous OFA (day 1, 300 mg; day 8, 1 g) and either fludarabine (25 mg/m2 days 2–6, FO), or fludarabine 25 mg/m2 and cyclophosphamide 250 mg/m2/d (days 2–4, FCO). Cycle 2: day 29, 1 g of OFA plus chemotherapy. Blood samples from patients N1 to N9 (obtained with informed consent) were drawn immediately before starting OFA infusions and several times after infusions started. Absolute lymphocyte counts (ALC) were determined at the NIH clinical laboratory. Analyses of B cells were based on flow cytometry protocols described in previous studies (23,24). B cells were identified by light scattering and development with PE CD19 and PERCP CD45. CD20 was measured by reacting washed whole blood samples with excess OFA and developed with Alexa (Al) 488 mAb HB43 (specific for human IgG Fc). OFA that bound to cells in vivo was measured by reacting washed blood samples with Al488 mAb HB43. Cells were probed with Al488 mAbs 7C12 (C3b/iC3b specific) or 1H8 (C3b/iC3b/C3d specific) to evaluate C3 fragment deposition. Fluorescence intensities were converted to Molecules of Equivalent Soluble Fluorochome (MESF) for quantitation (25,26). To allow quantitative comparisons for all measurements, all assays were conducted with one reagent set, with constant settings on the flow cytometer (BD FACSCalibur).
CLL cells were obtained from blood samples of de-identified patients at the University of Virginia, in accordance with protocols of the UVA institutional review board. All authors had access to primary clinical data, but only investigators at the NIH knew the identities of the patients (N1–N9) in the trial.
Human Burkitt’s lymphoma cell lines Daudi, Raji (European Collection of Cell Cultures, Porton Down, UK), Z138 mantle cell lymphoma cell line (27) and diffuse large B cell lymphoma cell line SU-DHL-4 (Deutsche Sammlung von Mikroorganismen und Zellkulturen GmbH, Braunschweig, Germany) were cultured in RPMI 1640 containing 10% heat-inactivated calf serum, 100 U/mL penicillin, 100 μg/mL streptomycin, and 4 mM L-glutamine (Invitrogen, Carlsbad, CA) [REF 31]. Wien-133 cells were provided by Dr. George Hale (Oxford University). Blood samples were obtained from CLL patients at the University of Virginia Hospital (not on the trial, numbers V1–V16) and B cells were isolated using Ficoll-Paque (10,28).
Pooled normal human AB serum (NHS) was from Sanquin (The Netherlands), or was prepared from pooled sera (25,29). Complement deficient serum and components were from Quidel (San Diego, CA) and C3-depleted (immunodepleted) sera were from Complement Technology Inc. (Tyler, TX).
Ofatumumab (OFA, 2F2, Arzerra), and 11B8 are human IgG1, CD20 antibodies generated in HuMab mice (6,8,10,20–22). HuMab-KLH (human IgG1), a human antibody against irrelevant antigen (keyhole limpet hemocyanin), is an isotype control. Rituximab (RTX, Mabthera), a chimeric IgG1, was from Roche (Basel, Switzerland) and the UVA pharmacy. Alemtuzumab (ALM, Campath-1H, anti-CD52) was from Genzyme (Cambridge, MA) and the UVA pharmacy. RTX and OFA were labeled with Al 488 (Invitrogen) to the same fluorochrome/protein ratios of 1–2 following the manufacturer’s instructions; CDC activity of labeled mAbs was equal to that of unlabeled starting material (not shown). MAb 5G9, specific for C3b/iC3b, has been described (25,30).
CDC assays were conducted using previously described procedures (10,21,25). Cells were incubated at 37°C with mAbs in NHS for periods of between 15 min and one hr, and after washing, viability was determined by staining with TOPRO-3 or propidium iodide (PI). Under these brief incubation conditions there was no killing of cells reacted with mAbs in the absence of NHS, indicating little, if any apoptosis. In assays described in Supplementary Figures 2–3, cells were opsonized with mAbs for 15 min at room temperature, washed twice, and resuspended in RPMI 1640/10% fetal calf serum and pooled NHS or complement-component deficient sera (20% vol/vol) was added. After incubation for 30–60 min at 37°C, cells were harvested and lysis was detected by flow cytometry (FACSCanto II, BD) based on PI or TOPRO-3 uptake. In CDC experiments described in Figures 2–4 and Supplementary Figure 4, cells (107–108/mL) were combined with media or with pooled NHS (10–50%) and either OFA or RTX added. After incubation for 10–30 min at 37°C, cells were washed and CDC was determined based on staining with TOPRO-3 (FACS-calibur, BD). In two-step experiments (Figure 4) similar procedures were followed, except after the first incubation more PKH26-labeled cells (28,31) were added, with additional mAb, for incubation in step 2.
Deposition of C3b/iC3b fragments on OFA- or RTX-opsonized cells was determined according to published procedures (23,29). To assess cellular C4b deposition, saturating concentrations of mAbs were reacted with B cells for 15 min at room temperature. C5-deficient serum was added (final concentration of 20%) followed by incubation at 37°C for 45 min. After washing, fluorescein isothiocyanate (FITC)-conjugated polyclonal antibodies against C4c (F0169) (DakoCytomation, Glostrup, Denmark) were added (1:100) and samples incubated for 30 min at 4°C and analyzed by flow cytometry, with readouts being mean fluorescent intensities.
To distinguish between C4c deposited on anti-B-cell mAbs, or on B-cell membranes, an acidic wash (RPMI 1640 + 0.3% BSA, pH 2.5) was implemented.(31,32) MAb binding was determined based on staining with FITC-F(ab′)2 fragments of goat anti-human IgG, Fab-specific.
Complement hemolytic assays (CH50) were performed according to standard procedures (33,34). Briefly, washed sheep E (Lampire) were reacted with anti-sheep E stroma (hemolysin, Sigma), washed, and reconstituted to a hematocrit of 2% EA in gelatin veronal buffer supplemented with Ca2+ and Mg2+ (GVB++). Test and standard sera were first diluted 10-fold in GVB++ and then further diluted sequentially by factors of 2 across 6 wells of a conical 96 well plate. The hemolytic reaction was initiated by addition of 25 μl of 2% EA to 25 μl of diluted sera. Assay plates were incubated for 60 min at 37°C. The reaction was stopped by addition of 200 μl ice cold GVB++ to each well. The lysed EA were pelleted by centrifugation at 1800 × g for 3 min, the supernatant removed to a flat bottom plate and the optical densities measured at 405 nm. CH50 titers were reported relative to a NHS pool. Assays were performed in triplicate.
All experiments were conducted independently two or more times, and representative results are presented. Where replicates measurements were performed, means and SD are provided. Unpaired 2-tailed t tests (Sigmastat) were used to compare selected results in Figure 2.
A first group of 9 CLL patients (N1–N9, NCT01145209) was treated with OFA (300 mg for the first dose (day 1) and 1 g for all doses thereafter (days 8 and 29)) in combination with chemotherapy (Table I). Blood samples were collected before, during and after OFA infusions on days 1, 8 and 29. Measurements included absolute lymphocyte counts (ALC), deposition of C3 fragments on target cells, complement titers and binding of OFA to circulating cells.
Significant B cell depletion in peripheral blood was achieved with the first cycle (Figure 1A). However, six of 8 patients had ALC in excess of 2,000 cells/μL on day 29 (one patient withdrew on day 10). The results of our measurements on blood samples taken over the first 29 days reveal several trends. The effect of OFA infusion on ALC was modest within the first 24 hours, achieving a median reduction of 30% (range 15–60%). Cell counts were greatly reduced on day 8 with a median reduction of 90% (range 80–95%) and on day 28 with a median reduction of 95% (range 93–98%). Based on the trial design that reflects current standard of care it is not possible to determine the relative contribution of OFA and chemotherapy to cytotoxicity. OFA infusions promoted substantial decreases in CD20 levels on circulating cells of all patients within 24 hrs (Figure 1B), likely as a result of trogocytosis as described for RTX (27,29,31); however, in many cases CD20 was partially restored on cells before the next infusion (day 8 and day 29). Two hours after starting the first infusion (day 1), substantial levels of OFA were demonstrable on circulating cells, in 6 cases corresponding to saturation of >50% of available CD20 sites (Figure 1C and Table I). This is all the more remarkable as by this timepoint only about 10% of the total dose, i.e. 30 mg of OFA, had been infused. These results indicate that during the first treatment, even when ALC are in the range of 100,000–200,000 cells/μL, relatively low doses of OFA (in the range of 20 mg/m2) (23,24) are adequate to achieve rapid and effective targeting of circulating CLL cells. Binding of OFA to cells decreased by 24 hrs (Figure 1C), likely due to CDC, clearance of OFA-opsonized cells by the mononuclear phagocytic system and trogocytosis of the OFA-CD20 complexes by effector cells expressing FcγR (23,29,31,35,36); indeed CD20 on circulating cells was reduced by 90% ± 5% (mean ± SD), 24 hrs after the start of the first infusion. In cases in which CD20 was partially restored between infusions, modest binding of OFA to circulating cells was demonstrable for subsequent infusions (Figures 1B,C). Notably, in most patients complement levels were reduced considerably due to OFA infusion (Figure 1D), and this was most evident during the first infusion when CD20 levels were initially high (Figure 1B).
OFA promoted deposition of C3d fragments on CLL B cells (Figure 1E). C3d, a degradation product derived from active C3b during complement activation, remains covalently attached to circulating cells that are targeted by complement-fixing antibodies but are not lysed (23,29). In most cases, circulating cells with deposited C3d fragments were demonstrable 24 hrs after OFA infusion. We also found that neither C3b nor iC3b were demonstrable on circulating cells (not shown), indicating these fragments are converted to C3d. A particularly interesting finding centers on the increased levels of C3d deposition on circulating cells of patients 1, 2 and 6 observed between day 9 (24 hrs after the second OFA infusion, when CD20 levels were quite low) and day 29, before the third OFA infusion. The most likely explanation is that after day 9, as CD20 was re-expressed by circulating CLL B cells, the cells were opsonized by circulating OFA, leading to C3b deposition followed by its degradation to C3d. CD20 levels were modestly restored on B cells of patient 6 by day 29 (Figure 1B.). It is also noteworthy that after the start of the OFA infusion on day 29 there was substantial C3d deposition on cells of several of the patients, reflecting binding of OFA and subsequent complement activation, due to partially restored levels of CD20.
To investigate the basis of our in vivo findings, we studied the interplay of complement with OFA-opsonized cells using various in vitro experimental designs. As demonstrated in Supplementary Figures 1–3, cell lines opsonized with OFA demonstrate substantial deposition of C4b directly on the cell surface and are effectively lysed by CDC in the presence of relatively low concentrations of complement components C2 or C3. Indeed maximal OFA-induced CDC required only 10–100 μg/mL C3 which represents less than 10% of the amount present in normal plasma. Nevertheless, killing of high tumor cell loads required high serum concentrations (i.e. 50% NHS) (Supplementary Figure 4). OFA induced substantially more CDC of Daudi and Z138 cells than did RTX.
It has been reported that OFA promotes high levels of CDC and kills CLL B cells more effectively than RTX (6,8,10,20–22). To evaluate this phenomenon quantitatively, we labeled OFA and RTX with fluorophore Al488 (which does not affect CDC potency (10,21)) and evaluated CDC, cell binding and C3b deposition on CLL cells from 10 patients (seen at the University of Virginia (UVA) Hospital) not in the trial (V1–V10, Figure 2). In order to model physiologic conditions, we used 50% NHS and varying cell densities typical for CLL (i.e. 107 and 108 cells/mL). The results, using B cells from two representative CLL patients, reveal the following: saturation of OFA binding to cells in media is achieved at 10 μg/mL OFA (Figures 2B,C) and substantial CDC is observed at this concentration in 50% NHS for both cell burdens. At cell inputs of 108 cells/mL, OFA concentrations of 100 μg/mL and 50% NHS maximize CDC and C3b deposition (Figures 2D–G); less OFA-mediated CDC occurs if less complement (lower %NHS) is available. Finally, even at RTX concentrations of 100 μg/mL, there was little CDC, but complement activation was evident, as demonstrated by C3b deposition; thus RTX would appear to be less efficient in making use of complement to kill cells.
We reported that CD20+ B cell lines opsonized with RTX (100 μg/mL) at high cell burdens (108 cells/mL) activate and deplete complement in vitro (29). The present correlative results for CLL patients treated with OFA demonstrate complement consumption in vivo (Figure 1D). We extended our in vitro measurements to include alemtuzumab (ALM), with Wien cells as targets because these cells can be killed in NHS via CDC induced with either RTX, OFA or ALM. We varied target cell burdens with mAb concentrations held at 100 μg/mL, and measured CDC and complement depletion. In intact 50% NHS, all three mAbs promote CDC, but complement was depleted at high cell burdens (108 cells/mL) (Figure 3A). Similar results for CDC and complement depletion were obtained when OFA and RTX were tested with Daudi cells or Raji cells (not shown).
We next used varying concentrations of CLL cells from six additional UVA CLL patients (V11–V16) and evaluated CDC and complement consumption mediated by OFA, RTX and ALM, in 50% NHS. Representative results from 2 patients are shown in Figures 3B,C. OFA and ALM induced CDC at high cell burdens (108/mL), and complement was consumed. RTX promoted modest CDC of the B cells of patient V11 (Figure 3B), and some complement was consumed. However, RTX-opsonized cells of patient V12 were not killed by CDC, and less complement was consumed for this RTX-treated sample (Figure 3C).
Our findings raise fundamental questions with respect to mAb dosing paradigms in cancer immunotherapy. If a mAb depends on host innate effector systems (CDC, ADCC or ADCP) to mediate cytotoxicity of malignant cells, it would seem important to determine the most effective immunotherapeutic doses, and their optimal timing, rather than to base treatment on maximum tolerated doses. Circulating cell burdens in CLL, readily accessible to infused mAbs, can be quite high (23,24,37,38). The infused mAb may thus promote clearance/destruction of cells at the cost of available effector mechanisms. Therefore, several hours after mAb infusion, as more cells re-equilibrate to the bloodstream from other compartments, effector functions such as complement may be saturated or exhausted for periods of days or weeks. Under these conditions clearance/killing of the next wave of malignant cells may be severely compromised (11,23,39). To examine this potential problem, we established a two-step model to approximate likely scenarios with respect to infusion of mAbs for CLL treatment, based on treatment paradigms currently used for RTX and OFA.
In step 1, varying amounts of OFA were added to multiple identical aliquots of Daudi cells in 50% NHS; after a one hr incubation at 37°C cell death and C3b deposition were determined. In step 2, an equal number of naive PKH26-labeled Daudi cells were added along with additional mAb. These PKH26-labeled cells represent CLL cells re-equilibrating into the bloodstream. The mixtures were incubated for an additional one hour at 37°C and CDC and C3b deposition on the PKH26 cell population was measured. The results for OFA and RTX are shown in Figures 4A–H and 4I–K respectively.
This two-step experiment demonstrates that use of moderate to high concentrations of OFA in step 1 (4 to 100 μg/mL) promotes high levels of CDC of unlabelled Daudi cells (95% CDC) in 50% NHS (Figure 4A, open circles; UNL). However, PKH26-labeled cells added in step 2 (along with an additional 100 μg/mL OFA) are effectively lysed only in samples which contained relatively low concentrations of OFA in step 1 (≤4 μg/mL, Figure 4B, filled circles, PKH). That is, although “excess” additional OFA (100 μg/mL) was added in step 2, only a fraction of PKH26-labeled Daudi cells were killed when added to samples exposed to higher OFA concentrations in step 1 (39% and 23% CDC, for samples reacted with 10 and 100 μg/mL OFA, respectively). The bell shaped curve in Figure 4C represents the sum of CDC achieved for both populations in this two-step experiment (% CDC of unlabeled cells in step 1 plus % CDC of PKH26-labeled cells in step 2). Thus, most effective killing is achieved with an OFA concentration (4 μg/mL) just sufficient to achieve maximal killing in step 1 (Figure 4A). Presumably complement activity is preserved under these conditions and the second wave of B cells is effectively killed in step 2, whereas higher OFA concentrations in step 1 do not markedly increase killing of the first wave of cells but promote exaggerated complement activation and consumption. This interpretation is supported by examining C3b deposition in our two-step paradigm (Figures 4D,E). C3b deposition for unlabeled cells modestly increases as the OFA input increases from 10 to 100 μg/mL in step 1 (Figure 4D), indicating increasing complement activation and deposition even though maximal cell killing is already achieved. In contrast, C3b opsonization of the PKH26-labeled cells (after addition of OFA at 100 μg/mL) decreases continuously for samples in which higher OFA concentrations were used in step 1 (Figure 4E), indicating that complement was consumed in step 1, thus limiting C3b opsonization of the PKH26 cells in step 2.
We next performed a more comprehensive experiment in which OFA doses in step 1 and step 2 were varied (Figures 4F–H), and the findings are consistent with the observations above. Close to the maximum sum of CDC for the two populations was achieved at OFA inputs of only 4 μg/mL in step 1 and 20 μg/mL in step 2 (Figure 4H). Similar patterns were evident based on evaluation of C3b deposition (Figures 4F–G); opsonization with 4 μg/mL OFA in step 1 and 20 μg/mL OFA in step 2 gave more C3b deposition on PKH26-labeled cells than when 100 ug/mL OFA was used in both steps. Finally, we replicated these findings for RTX in similar experiments (Figures 4I–K).
The most important finding in the present study is that the potential of the complement cascade to support mAb-mediated CDC of tumor cells is finite and saturable, and the degree of CDC is strongly influenced by the nature of the opsonizing mAb and its concentration. Our findings in the CLL clinical study demonstrate that at high initial cell burdens, infusion of OFA activates and consumes complement, and this was also made evident by the appearance of C3d-tagged circulating cells (Figures 1D,E). Apparently, after an initial wave of clearance/killing, some complement activation may continue, but complement as well as the mononuclear phagocytic system and NK cell-mediated ADCC are insufficient to deplete the cells (Figure 1A). The increase in net C3d found on cells of three patients by day 29, relative to day 9, suggests that as CD20 is re-expressed by cells, the infused OFA may promote chronic low level complement activation as it targets CD20 on cells.
Our findings of the rapid loss of CD20 due to infusion of OFA are most likely mediated by trogocytosis, but direct internalization of OFA by the CLL B cells may also play a role in loss of CD20 (40,41). However, we have directly compared the relative rates and extent of loss of CD20 for trogocytosis versus internalization, and these experiments demonstrate that trogocytosis reduces CD20 expression more strongly and in a shorter time frame (42).
We compared ALM, OFA and RTX with respect to their potential to utilize and activate individual components of the classical pathway of complement activation. OFA is more effective in promoting C4b deposition on opsonized Wien cells than RTX or ALM (Supplementary Fig. 1). The results are not due to higher densities of cell-bound OFA; binding of RTX and OFA to Wien cells was comparable and OFA binding was lower than ALM binding. Less cell-associated C4b was released from OFA-opsonized cells via acid wash than from RTX- or ALM-opsonized cells, indicating more deposited C4b was covalently bound to the cell membrane; this finding may be because OFA binds close to the cell membrane (6,8,10,20–22). CDC studies in sera depleted of C2 or C3 provide additional support for the concept that cell-bound OFA can use limited amounts of complement to lyse cells and that complete serum therefore initially contains a relatively large excess of complement components required for cell killing (Supplementary Figures 2 and 3).
Indeed, due to downstream amplification in the complement cascade, small amounts of early components are adequate to allow for deposition of large amounts of C3 activation fragments on cells (12–14). However, complement component C2, at lowest concentration in the plasma, is often the limiting factor that is first depleted during classical pathway activation. Based on our previous observations of C2 consumption in CLL patients who received RTX therapy (25,29), it is reasonable to predict that C2 was also first depleted in the present studies. These considerations, taken in context with the work of Ziccardi (43) may also explain the sharp drop in CDC observed for serum concentrations of 25% at the higher cell densities (Supplemental Figure 4). Under these conditions the potential of C1 inhibitor to control C1 activation may be abrogated, thus leading to uncontrolled activation of C1 followed by complete consumption of C2.
In patients with CLL, circulating B cells in excess of 108/mL are commonly observed (23,24,37–39), and we reported that infusion of the usual RTX dose can deplete complement in CLL patients for a week or longer (29). We extended these findings and show that at these physiologically relevant cell burdens complement activity in 50% NHS can be severely depleted (reduced 20-fold) when cells are reacted with mAbs such as ALM or OFA and are killed by CDC (Figure 3). Indeed, under our standard assay conditions, 50% NHS is required to promote effective CDC at 108 cells/mL, and CDC and C3b deposition are substantially reduced if the NHS concentration is reduced only 2-fold to 25% (Figure 2 and Supplementary Figure 4). Moreover, our two-step experiments described in Figure 4 provide dramatic evidence that at moderate to high cell burdens, large amounts of mAb indeed promote effective CDC of CLL cells, but if more mAb is added than essentially required, this leads to exhaustion of complement activity and therefore additional CDC is severely compromised upon challenge with additional cells, even if adequate mAb concentrations are present. The present results, taken along with our previous findings for CLL patients treated with RTX (29), indicate that after the standard (high) mAb doses, patients’ complement levels can be depleted in vivo for periods of several days to more than one week. It would seem reasonable that mAb dosing strategies that take into account patient complement titers as well as other indices of immune function would help provide guidance for more efficacious, individualized therapies.
On the basis of accumulated evidence, high tumor burdens combined with high antibody concentrations may exhaust effector functions of the body’s innate immune system, including mAb-mediated CDC (Figure 5). Our results specifically relate to prominent therapeutic mAbs which are highly dependent on Fc-mediated effector functions for target cell cytotoxicity, such as type I CD20 mAbs. Provocative results in uncontrolled trials with RTX suggest that infusion of fresh frozen plasma to increase or restore complement activity may increase clinical efficacy of single agent treatment in CLL, in support of our findings (29,44–46). Our results support this concept with respect to maximizing the potential CDC that can be achieved by normal complement levels in the bloodstream. It is possible, based on findings in several reports, that other effector functions important in mAb-based immunotherapy of cancer, such as ADCC, are similarly subject to exhaustion, likely as a consequence of down-modulation of CD16 and depletion of NK cell-associated perforin and granzymes (47–51). Moreover, the substantial and protracted loss of CD20 mediated by infusions of large doses of mAb, coupled with the loss of potency of cytotoxic effector systems, would generate a “perfect storm” that can allow malignant cells to continue to proliferate for extended time periods, even after infusion of gram quantities of mAb.
We hypothesize that our results not only apply to OFA or RTX treatment, but impact all therapeutic mAbs which use Fc- or complement-mediated effector functions as part of their cytotoxic mechanisms. Re-formulation of mAb dosing schedules based on more frequent treatments (several times per week) with lower doses may allow for recovery and/or preservation of effector functions between doses (23,24) and should be investigated. Our study emphasizes that the time-honored approach to use drugs at maximum tolerated doses as derived from the chemotherapy field may not necessarily be optimal for mAb-based immunotherapy of cancer.
We thank Marleen Voorhorst for technical assistance and Joost Bakker for graphic design. We thank the patients for their participation in the trial.
1Glaxo Smith Kline funded the correlative studies and provided Ofatumumab for the trial. The clinical trial was funded by NHLBI, NIH. Genmab supported the in vitro studies.
6The online version of this article contains supplemental material.