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Optimally effective antitumor therapies would not only activate immune effector cells, but engage them at the tumor. Folate-conjugated to immunoglobulin (F-IgG) could direct innate immune cells with Fc receptors to folate receptor–expressing cancer cells. F-IgG bound to human KB and HeLa cells, as well as murine L1210JF, a folate receptor (FR) overexpressing cancer cell line, as determined by flow cytometry. Recognition of F-IgG by NK cell Fc receptors led to phosphorylation of the ERK transcription factor and increased NK cell expression of CD69. Lysis of KB tumor cells by NK cells increased about 5-fold after treatment with F-IgG, an effect synergistically enhanced by treatment with IL2, IL12, IL15, or IL21 (P < 0.001). F-IgG also enhanced the lysis of chronic lymphocytic leukemia cells by autologous NK cells. NK cells significantly increased production of IFNγ, MIP-1α, and RANTES in response to F-IgG–coated KB target cells in the presence of the NK cell–activating cytokine IL12, and these coculture supernatants induced significant T cell chemotaxis P < 0.001). F-IgG–coated targets also stimulated FcR-mediated monocyte effector functions. Studies in a murine leukemia model confirmed the intratumoral localization and antitumor activity of F-IgG, as well as enhancement of its effects by IL12 (P = 0.05). The antitumor effect of this combination was dependent on NK cells and led to decreased tumor cell proliferation in vivo. Thus, F-IgG can induce an immune response against FR-positive tumor cells that is mediated by NK cells and can be augmented by cytokine therapy.
Folate is a water soluble B vitamin that functions as a cofactor in various cellular metabolic processes, such as nucleic acid synthesis and protein biosynthesis. Green vegetables, fresh fruits, and fortified foods are sources of folate (1). Cellular uptake of folate is mediated by at least three distinct transporters, which include the proton-coupled high affinity folate transporter, the reduced folate carrier (RFC), and the folate receptor (FR) (2). The proton-coupled high affinity transporter is a major folate transporter in low pH environments, such as the intestines, and appears to be the principal transporter in the gastric absorption of folate (3). The RFC, a bidirectional low-affinity transmembrane anion carrier, is ubiquitously expressed in normal tissues and is the predominant folate transporter in normal cells, but it will not transport folic acid (oxidized form) or folate conjugates (4). In contrast, the FR is a membrane bound high affinity unidirectional folate transporter protein that binds folic acid, chemical conjugates of folic acid, as well as folate‐linked immunological agents. The FR has three well-established isoforms: α and β (both linked to glycosylphosphatidylinositol; GPI), and γ (5).
FR expression is normally low and limited to specific tissues, such as the choroid plexus, epididymis and kidney. In normal polar epithelial cells, the FR is predominantly located on the luminal (nonvascular) side of the cell. Thus, the FR expressed on normal cells is largely inaccessible to circulating folate or folate conjugates (5). The oncogenic potential of the FR was first observed by Sidney Farber in 1948, where an accelerated leukemic process was observed in children treated with derivatives of folate (6). The FR is overexpressed on the surface of malignant cells, such as cancers of the cervix, breast, testes, and ependymal brain tumors (2, 7-9). This accessibility, relative to that of normal cells, makes the FR an attractive therapeutic target. Once a folate conjugate is bound, it may be taken up via endocytosis while a fraction remains engaged with the FR on the cell surface (5). These parameters are thought to create a favorable toxicity profile for folate‐conjugated antitumor compounds (2).
NK cells are bone marrow–derived lymphocytes that can lyse malignant cells with altered expression of major histocompatibility antigens. NK cells express killer cell immunoglobulin receptors (KIRs), cellular adhesion molecules, and multiple cytokine receptors (e.g., receptors for IL12, IL15, and IL18). NK cells also produce several cytokines with antitumor effects (i.e., IFNγ, TNFα, and MIP‐1α) and possess the ability to lyse malignant cells using cytolytic granules that contain perforin and granzymes. NK cells also express the FcγRIIIa (CD16) receptor, a low-affinity activating receptor that recognizes the constant (Fc) region of IgG. This receptor is critical in mediating antibody‐dependent cellular cytotoxicity (ADCC) against antibody (Ab)-coated targets (10).
A folate-conjugated immunoglobulin (F-IgG) that is able to bind specifically to FR-bearing tumor cell lines was tested for its ability to mediate ADCC and cytokine production by NK cells. We also characterized the antitumor and immune effects of the F-IgG conjugate when used in combination with NK-activating cytokines that activate Fc receptor (FcR)‐bearing NK cells.
F-IgG (derived from all classes of IgG) and F-IgG-fluorescein isothiocyanate (FITC) were synthesized as described (11). Three folates per IgG were utilized for these studies. Unmodified human or murine IgG1 molecules were used as controls (C‐IgG). The molecular weight of the F-IgG construct is approximately 151 kDa.
The FR+ human cell lines KB (gift from Dr. Philip S. Low, Purdue University in 2006), HeLa, and F01 (human cervical and melanoma; ATCC obtained in 2002); OSU-NB and OSU-CLL (normal B and CLL cell lines, derived by J. Byrd from a CLL patient in 2012); and L1210JF (murine leukemia, gift from Robert J. Lee, Ohio State University in 2007); as well as the FR-negative cell line A549 (human alveolar adenocarcinoma; ATCC obtained in 2006) were propagated in folate-free RPMI 1640 (Invitrogen, Grand Island, NY) supplemented with 10% heat‐inactivated fetal bovine serum (FBS) and 1% antibiotic‐antimycotic. The identity of these cell lines was not authenticated by testing genomic DNA and cells were kept under passage number ten for all experiments.
NK cells, monocytes, and B cells were isolated from fresh peripheral blood leukopacks (American Red Cross, Columbus, OH) or whole patient blood using RossetteSep cell specific cocktails (Stem Cell Technologies, Vancouver, BC) (12). Cells were cultured in folate-free RPMI 1640 (Cleveland Clinic Media Preparation Service, Cleveland, OH) supplemented with 10% heat‐inactivated pooled human AB serum (HAB; C‐Six Diagnostics, Germantown, WI) and 1% antibiotic‐antimycotic. Normal donor NK cell Fc receptors (FcγRIIIa or CD16) were genotyped as described (13).
Total RNA from KB, HeLa, and A549 cells was extracted in TRIZOL® Reagent using the RNeasy Mini Kit (Qiagen, Valencia, CA) following the manufacturer’s protocol. RNA was converted to complementary DNA by reverse transcription and used as a template for RT-PCR using folate receptor alpha primers with the internal control 36B4 (14, 15).
KB tumor cells were treated with C-IgG– or F-IgG–FITC for 30 min at 37°C and collected at the designated time points. Cells were washed with flow buffer (5% FBS in PBS), fixed in 1% formalin in PBS, mounted on 25 × 75 × 1 mm slides (Erie Scientific, Portsmouth, NH) and stained with DAPI for nuclear identification (Vector Labs, Burlingame, CA) prior to analysis by immunofluorescence (IF) microscopy. Intracellular analysis of NK cell ERK phosphorylation was also assessed following coculture with KB tumor cells. NK cell activation was assessed 48 hours post coculture via FACS analysis with CD56‐phycoerythrin (PE), CD158-allophycocyanin (APC), CD57‐FITC, NKG2A-PE (Beckman Coulter, Brea, CA), CD56‐APC, CD3‐V450, CD16‐FITC, NKG2D-APC, CD69–phycoerythrin-cyanin 7 (Pe-Cy7) and KIR/NKAT2‐FITC, CD94‐APC, NKp46/CD335-APC antibodies (BD Biosciences, San Jose, CA). In murine studies, IF microscopy of tumor sections was performed (16). Sections were analyzed on an Olympus Fluoview 1000 laser scanning confocal microscope. In murine studies with C‐IgG– and F‐IgG–FITC, tissues were harvested in the dark at indicated times. Tumors were dissociated (17) and stained with FR‐α–APC (R&D Systems, Minneapolis, MN). FR+/FITC+ populations were assessed using a Becton Dickinson FACS Calibur flow cytometer (Becton‐Dickinson, San Jose, CA) (16).
Plates were coated with 50 μg/mL control IgG (C-IgG) or F‐IgG overnight at 4°C then plated with NK cells. After 15 min at 37°C, cells were lysed in TN1 or 0.5% Brij‐98 lysis buffer and probed with anti‐phospho‐ERK or ERK primary antibodies (Cell Signaling Technology, Beverly, MA), FR (FL‐257, Santa Cruz Biotechnology, Santa Cruz, CA) or β‐actin antibodies (Sigma, St. Louis, MO) (18).
For ADCC assays, purified NK cells or monocytes were plated with medium supplemented with IL2 (10 ng/mL), IL12 (0.5 ng/mL or 10 ng/mL), IL15 (10 ng/mL), or IL21 (10 ng/mL). F‐IgG or C‐IgG-treated (100 μg/mL) 51Cr‐labeled target cells were added at various effector:target (E:T) ratios for 4 h (NK cells) or 18 h (monocytes). Supernatants were harvested and 51Cr was quantified (19).
KB and A549 cell lines were coated with F-IgG or C-IgG (100 µg/mL) and cocultured with NK cells or monocytes with medium containing IL2, IL12, IL15, IL18, or IL21 (10 ng/ml) (12). After 48 h, supernatants were analyzed for IFNγ, MIP-1α, TNFα, and RANTES content by ELISA and utilized in T cell chemotaxis experiments (20). For MDSC coculture experiments, MDSC were generated (21) and added to NK cell cocultures at a ratio of 0.5:1 MDSC:NK cell.
Mice were placed on a folate‐deficient diet (AIN-90G, Dyets, Bethlehem, PA) one week prior to tumor cell injection (11). Age‐matched, female DBA/2NCrl mice (Strain code 026; Charles River, Wilmington, MA) were injected with 10 × 106 L1210JF cells subcutaneously (s.c.). For intra‐tumoral localization studies, age‐matched, female athymic mice Crl:NU(NCR)‐Foxn1nu (Strain code 490; Charles River, Wilmington, MA) were inoculated with 4 × 106 human KB cells. Once tumors were palpable, mice were treated twice a week intraperitoneally (i.p.) with C-IgG or F‐IgG (100 mg/kg), 2.5 ng mIL12 (Wyeth Pharmaceuticals, Madison, NJ), or the combination. Tumor volumes were assessed thrice weekly (16). To deplete monocytes/macrophages, 1 mg/kg of clodronate liposomes was administered on the day of tumor implantation and 0.5 mg/kg every four days thereafter (22). NK cells were depleted via anti‐asialo GM1 (16).
Murine tissues were harvested and processed immediately. Tumors were then sectioned and stained and quantified using the ScanScope XT and Positive Pixel Count Algorithm ImageScope software (Aperio Technologies) as described (16, 23).
The synergistic effects of F‐IgG and cytokines on NK cell mediated ADCC, IFNγ, or MIP‐1α production were tested using linear mixed models to account for the correlated responses from the same cell types and the same donor cells. Treatment groups (C-IgG, F-IgG or the combination of C-IgG or F-IgG plus cytokines), E:T ratios were considered as a fixed effect. Ratios and treatment interactions were also included in the model. To control for type 1 error gate keeping strategies were used in each experiment at a significance level of 0.05, we first tested the difference between the combination treatments to the C-IgG treatment group (control) across different E:T ratios. If the difference was significant (P < 0.05), then the differences across different E:T ratios was further tested for the combination treatments versus F-IgG or C-IgG, and F-IgG versus C-IgG. The P values for each hypothesis was based on the corresponding interaction contrasts of the fixed effects parameters estimated from the linear mixed models using the Estimate or Lsmeans statement in the Proc Mixed procedure. T cell migration studies were analyzed using a two-way ANOVA with Turkey methods to correct for multiple comparisons. Changes in tumor volume over time were assessed via a linear mixed model for longitudinal data. Tumor values were log‐transformed in the model, and the differences in tumor volume were calculated at baseline and at the end of each study time points based on a linear mixed model. All data analyses were performed using the SAS V9.4 statistical software.
Both the human KB and HeLa tumor cell lines expressed the FR-α transcript, as indicated by RT‐PCR (Fig. 1A), but not the A549 cell line. FR protein content was confirmed by immunoblot analysis in the HeLa, KB, and murine L1210JF cell lines (Fig. 1B). Surface expression of the FR was detected on the KB and L1210JF cell lines as determined by flow cytometry using a F‐IgG‐FITC labeled conjugate. The specificity of the interaction between F-IgG and the FR is supported by F-IgG binding inhibition in KB cells pretreated with folate (200 nM) (Fig. 1C). In addition, F‐IgG–FITC binding was maintained for greater than 24 hours, as assessed by confocal microscopy, whereas C-IgG-FITC did not exhibit this binding (Fig. 1D). No FR was detected on NK cells (data not shown). Based on these experiments, the KB and L1210JF cell lines were utilized for in vitro and murine studies.
NK cells can interact with antibody-coated target cells via an activating, low-affinity Fc receptor (CD16), which can activate the MAPK/ERK signaling pathway (12, 19, 20). Stimulation of this pathway is critical for FcR-mediated NK cell lytic function and cytokine production. We hypothesized that binding of human NK cells to immobilized F-IgG would activate this pathway and result in the phosphorylation of ERK. As predicted, NK cells stimulated with F‐IgG (or C-IgG) exhibited striking ERK activation at 15 minutes, as compared to the PBS‐stimulated cells (Fig. 2A). NK cell ERK phosphorylation was also determined following exposure to F‐IgG-coated tumor cells. An increase in the phosphorylation of ERK was observed in NK cells that were cocultured with F-IgG coated KB tumor cells after 45 minutes of treatment (Fig. 2B). CD69 upregulation on NK cells is associated with a productive antitumor response (24). CD69 expression on NK cells increased in response to F‐IgG–coated tumor cells in both the CD56 bright and CD56 dim subsets (Fig. 2C). Activated NK cells also decreased CD16 expression when incubated with F-IgG, compared to C-IgG, an indication of Fc receptor occupation (data not shown) (25). No difference in the surface expression of NKG2D, CD57, NKp46/CD335 (activating receptors), CD158, NKG2A, CD94, or KIR/NKAT2 (inhibitory receptors) was observed (data not shown).
The effect of F-IgG on NK cell ADCC of FR+ tumor targets was examined using KB tumor cells as targets in a standard 4 h ADCC assay with healthy donor human NK cells as effectors (19). NK cell‐mediated ADCC with F-IgG coating of targets was significantly enhanced at all effector:target (E:T) ratios and in every donor tested, as compared to C-IgG (P < 0.0001) (Fig. 2D). F-IgG treatment did not enhance the lysis of the FR-negative cell line A549 (Fig. 2E). The difference in the average percent lysis between F-IgG and C-IgG was significantly greater in the KB cell line as E:T ratios increased (P < 0.001) (Fig. 2D). This trend was not observed in A549 cells (Fig. 2E).
Next, several NK cell–activating cytokines were evaluated for their ability to augment NK cell ADCC against F‐IgG–treated KB tumor cells. NK cells were pretreated with cytokines (IL2, IL12, IL15, or IL21) and cocultured with F‐IgG–coated tumor cells at various E:T ratios in a 51Cr release assay (19). With every cytokine tested, F‐IgG or cytokine‐mediated lysis was significantly higher than that of C-IgG treatment alone (all P < 0.01). The combination of F-IgG and IL2 (Fig 3A), IL12 (Fig. 3B), IL15 (Fig. 3C), or IL21 (Fig. 3D) resulted in significantly higher tumor cell lysis than either F-IgG or cytokine treatment alone across all E:T ratios (all P < 0.001). A significant synergistic lysis effect was observed following treatment with every cytokine evaluated across different E:T ratios (IL2 P = 0.001, IL12 P < 0.0001, IL15 P = 0.0017, IL21 P < 0.0003). Next, FR blocking experiments were conducted in which the KB tumor cells were treated with varying amounts of folate to create high, medium, and low FR availability, and validated by flow cytometry (data not shown). NK cell ADCC was then assessed. As predicted, NK cell killing directly correlated with the level of available FR (Supplementary Fig S1A). In addition, NK cells from 8 normal donors were genotyped for CD16 variants and ADCC assays were conducted. The data for one representative F/F (lower affinity-Donor 3) and F/V donor (intermediate-Donor 7) are shown in (Supplementary Fig. S1B) (no high affinity V/V donors were identified). The expression of the intermediate affinity FcR by NK cells did not appear to confer an increased ability to conduct ADCC as compared to NK cells with the low affinity FcR (present in approximately 36% of the population) (26).
Our group is also interested in immune-based approaches for the treatment of chronic lymphocytic leukemia (CLL). We therefore examined the effects of F-IgG in this context. The expression of the FR in CLL has been described (27) and was validated in CLL patients by our group (Fig. 3E). The ability of CLL patient NK cells (TIL) to kill F-IgG–coated KB (Fig. 3F, left) or autologous CLL target cells (Fig. 3F, right) was determined in a standard ADCC assay, in which care was taken to remove FR-bound folate from target cells (28). Here, freshly isolated NK TILs from CLL patients mediated significant lysis against both targets and the cytolytic activity of these NK cells was markedly enhanced following stimulation with IL12 (P < 0.0005) (Fig. 3F).
Costimulation of NK cells via the IL12R and CD16 leads to enhanced production of IFNγ due to colocalization of these receptors at cell membrane lipid rafts and subsequent enhancement of signal transduction (18). We hypothesized that NK cell–activating cytokines would enhance NK cell production of IFNγ following exposure to F‐IgG–coated KB tumor cells. An in vitro assay was performed in which purified NK cells were cocultured with F-IgG-coated FR‐positive tumor cells (12). KB (FR+) and A549 (FR-) cells were treated with F-IgG or C‐IgG and plated with purified NK cells in the presence or absence of IL2, IL12, IL15, IL18, or IL21. Supernatants were harvested 48 h later and assayed for IFNγ content. As was observed in the ADCC experiments, F‐IgG treatment not only resulted in a significant increase in NK cell IFNγ secretion (all P < 0.0001), but also demonstrated a significant interaction with IL2, IL12, IL15, IL18, and IL21 (P < 0.01) (Fig. 4A). As the coactivation of the IL12R and CD16 can stimulate the secretion of other cytokines, the concentrations of MIP-1α and RANTES were also measured. NK cell production of MIP1-α (Fig. 4B) and RANTES (Fig 4C) was enhanced following treatment with F‐IgG coated tumor cells and IL12, compared to C-IgG (P < 0.0001). Treatment of the FR– cell line A549 with F‐IgG did not enhance NK cell IFNγ production in response to any cytokine (data not shown).
NK cell–derived factors produced in response to immobilized IgG can serve as a powerful stimulus to T cell chemotaxis (20). As predicted, T cell chemotaxis was significantly enhanced upon exposure of T cells to coculture supernatants that were obtained following treatment of NK cells with F‐IgG–coated tumor cells and IL12, compared to C-IgG (P < 0.01) (Fig. 4D). These results provide evidence that coadministration of cytokines with F-IgG can significantly enhance NK cell production of chemokines, which have the ability to recruit T cells to sites of inflammation. Human NK cells stimulated with F-IgG–coated tumor cells plus IL12 increased CD69 expression, a finding that is consistent with dual activation of the IL12R and FcR (Fig. 4E).
Experiments were conducted to determine if F-IgG could enhance the effector functions of monocytes, another immune cell population that is critical to antibody‐mediated immune responses (29). Lysis of FR+ KB tumor cells by normal monocytes was significantly enhanced by pretreatment of the target cells with F‐IgG (P < 0.0001), an effect that was further enhanced by activation of monocytes for 18 hours with IL12 (Fig. 5A). In addition, peripheral blood monocytes (PBM) secreted significantly large quantities of TNFα when exposed to plate- (Fig. 5B) and tumor-bound F-IgG (Fig. 5C), as compared to controls (P < 0.001). Monocytes also secreted IL12 in response to F-IgG–coated KB tumor cells (Fig. 5D) (P < 0.04). The role of monocytes in mediating the effects of F-IgG plus IL12 therapy were examined via the use of monocyte-depleting clodronate liposomes (22). Mice treated with clodronate liposomes bearing s.c. L1210JF tumors were treated twice a week via i.p. injections of 100 mg/kg murine C-IgG or F-IgG plus 2.5 ng murine IL12 and tumor volume was assessed. Depletion of monocytes/macrophage was confirmed by flow cytometric analysis, but this manipulation did not impact the efficacy of combination therapy (Fig. 5E). The difference between mock and clodronate depleted mice treated with F-IgG plus IL-12 was not significantly different. As other groups have indicated that exhausted or inhibited NK cells may have a negative impact on tumor growth control and survival (30, 31), we examined the potential role of myeloid‐derived suppressor cells (MDSC) in modulating the NK cell response to F-IgG–coated tumor cells. Notably, overnight coculture of MDSC with human NK at a ratio of 0.5:1 significantly inhibited NK cell lysis of F‐IgG–coated KB cells and also reduced the NK cell IFNγ secretion in response to this stimulus (Supp. Fig. 2). These results indicate that immune suppressor cells within the tumor microenvironment can impact the NK cell response to F-IgG–coated tumor cells.
We evaluated the cytotoxic potential of purified murine NK cells against F‐IgG–coated L1210JF tumor cells in a 51Cr-release assay (20). Folate was conjugated to a murine IgG molecule to create a murine F-IgG construct. Freshly isolated murine NK cells were cultured with low dose recombinant murine (rm) IL15 (0.5 ng/ml) (32), treated with medium alone or medium containing rmIL12 (10 ng/mL) and plated with L1210JF target cells. C‐IgG or F‐IgG–coated target cells were only minimally lysed by NK cells in the absence of cytokine treatment. In contrast, pretreatment of NK cells with IL12 significantly increased lysis of F‐IgG–coated tumor cells at the 50:1 E:T ratio (13.05 ± 0.84% vs. 1.37 ± 0.77% lysis; P < 0.05).
Based on our in vitro findings, prior preclinical work from our laboratory, and the results of phase I clinical trials, we chose IL12 for further study (16, 33). The ability of the F‐IgG conjugate to penetrate into the tumor microenvironment and specifically bind to tumor cells was evaluated. A F‐IgG‐FITC construct was utilized to assess its intratumoral penetration in a KB xenograft model. A strong fluorescence signal was detected 72 h later only in F‐IgG–FITC treated mouse tumors (Fig. 6A, upper panel). Flow cytometric analysis confirmed that specific fluorescence was detectable only in FR+ tumors (Fig. 6A, bottom panel). Even at this early time point, approximately 40% of the FR+ tumor cells were targeted by F-IgG-FITC. A FR+ murine leukemia tumor model was employed to determine whether IL12 could enhance the effect of an antitumor F‐IgG construct in an immune competent model. Mice bearing s.c. L1210JF tumors were treated twice a week via i.p. injections of murine C‐IgG or F‐IgG (at 100 mg/kg), with or without murine IL12 (2.5 ng). No significant tumor volume differences were observed at baseline. However, by day 18 of treatment, the average tumor volumes of mice receiving either IL12 (453 ± 83 mm3) or F-IgG alone (223 ± 68 mm3) were significantly smaller than those of the C‐IgG-treated mice (615 ± 152 mm3) (P < 0.05). Mice that received the combination of IL12 and F-IgG had significantly smaller tumors (84 ± 43 mm3) than those of mice receiving control treatments (P = 0.05) (Fig. 5B). Normal tissues from mice treated with F‐IgG exhibited no histological damage (Supp. Fig. 3). These data demonstrate that the F-IgG conjugate specifically targets tumor cells, while sparing normal tissues in vivo and that IL12 can enhance the effects of F‐IgG in a murine leukemia tumor model.
Based on our previous work, we hypothesized that NK cells were the key mediators of the tumor response mediated by IL12 plus F‐IgG (16). Mice bearing s.c. L1210JF tumors were depleted of NK cells via anti-asialo GM1 antibodies, which resulted in > 97% NK cell depletion (data not shown). Mock‐depleted mice received injections of an isotype-matched control antibody. Mice were then treated with IL12 plus F‐IgG. Tumor growth was significantly inhibited in mock‐depleted mice receiving IL12 and F-IgG (P < 0.0001). In contrast, treatment with F-IgG and IL12 had a minimal effect on tumor growth in the absence of NK cells (Fig. 7A). Activated intra-tumoral NK cells were observed only in the non‐depleted treatment group (Fig. 7B). There was a marked inhibition of Ki67 in mice receiving IL12 plus F-IgG, but not in NK cell depleted mice, as indicated by immunohistochemical staining (Fig. 7C). These data suggest that the antitumor effect of IL12 and F‐IgG is dependent on NK cells.
We have demonstrated that a F‐IgG construct could bind to the FR of tumor cells. Tumor‐bound F‐IgG triggered the MAPK pathway in NK cells and coating FR‐bearing tumor cells with F‐IgG led to enhanced NK cell–mediated ADCC and CD69 expression. Pretreatment of NK cells with IL2, IL12, IL15, or IL21 enhanced ADCC beyond that observed with F‐IgG alone. The addition of IL12 to the F‐IgG stimulus resulted in robust production of IFNγ, MIP‐1α, and RANTES by NK cells, significantly exceeding concentrations observed with either stimulus alone. Cytokines produced from the coculture of NK cells and FIgG coated tumor cells treated with IL-12 mediated significant T cell chemotaxis. The conjugate bound to FR+ tumor cells in vivo, but normal tissues showed no obvious adverse effects. Administration of IL12 in combination with F‐IgG elicited an antitumor response in a murine tumor model when compared to mice receiving IL12, F‐IgG, or C‐IgG alone. The antitumor effects of the combination therapy were dependent on NK cells and associated with reduced tumor cell proliferation. These results support the utility of administering cytokines with the F-IgG conjugate as a possible cancer therapeutic.
In murine models, the administration of high doses of folate is linked with tumor progression (34). Although it is not known whether FR‐expression is needed by malignant cells, folic acid supplementation increases tumor cell growth and decreases patient survival in the context of FR+ tumors (35). Conversely, a blockade of folate uptake decreases tumor cell proliferation, migration, invasion, and tumor burden, implicating folate in the survival, growth, and injury repair of malignant cells (34, 36-38). The reason for FR overexpression in tumor versus normal tissues remains elusive. It is possible that the FR might somehow confer a growth advantage by modulating folate uptake from serum, but direct evidence is lacking (39).
The present folate-IgG construct had binding and intracellular distribution characteristics in FR+ cells that were similar to those of earlier radiolabeled folate‐conjugated immunoglobulin constructs (40). Binding assays from studies conducted by Henriksen et al. estimated the binding affinity of a folate-conjugated immunoglobulin to be within the KD range of 10−9 to 10−10 M, which is comparable to the reported high affinity binding of FRα for folic acid (KD~ 10−9 M) (34). Biodistribution experiments using 125I- and 211At-labelled folate‐immunoglobulin conjugates in Balb/C mice indicate that folate-conjugation to the antibody has a minor effect on the distribution of the conjugated antibody (40). Therefore, it is reasonable to conclude that the pharmacokinetic parameters of the present F-IgG would be similar to that of other therapeutic IgG-type monoclonal antibodies, including a relatively long half-life (days), low clearance (~0.5 L/d), and a small volume of distribution (approximate to the plasma volume) (41, 42). The present studies indicate that FR binding of F‐IgG was evident as early as 30 minutes after treatment and retained on the cell surface for up to 24 hours in vitro. Moreover, in vivo, F-IgG was present in the tumor up to 72 hours after injection.
The FR has been previously utilized for the investigational delivery of cytotoxic drugs, radiopharmaceuticals, nanoparticles, liposomes, and immunotherapy (2, 13). Lu et al. showed that folic acid can carry a conjugated hapten to the tumor cell surface (the hapten forming a bridge between the cell surface FR and antibodies to it) and elicit primarily a T cell– and NK cell–based immune response to the tumor. This led to the generation and accumulation of autologous antibodies to haptens on the tumor surface, stimulating Fc receptor–bearing immune cells to mount an antitumor response against the opsonized tumor cells (43). The results of the present study suggest that the F-IgG construct is able to promote a direct interaction of FcR-bearing cells with FR-expressing cancer cells rather than relying on the induction of an Ab response.
Thompson et al. devised a method to specifically target T cells to FR overexpressing tumors utilizing a light‐activated folate–anti-CD3 construct. Here, the folate portion of the construct binds to FR+ cancer cells while the anti-CD3 portion binds T cells. Specific tumor targeting and T-cell binding was observed in a murine model (44). In contrast, the F-IgG construct described here can localize NK cells to tumor cells while simultaneously stimulating FcR‐mediated effector functions. These studies support the development of FR-directed therapeutic immunoconjugates and suggest that co-administering cytokines would augment the activity of these reagents. The ability of F-IgG to mediate lysis of target cells derived from both leukemias and solid tumors speaks to the broad applicability of this therapeutic approach.
F-IgG–mediated ADCC was investigated in this study due to the importance of ADCC in the antitumor mechanisms of monoclonal antibody therapy (13, 45, 46). A study in patients receiving trastuzumab for HER2/neu+ metastatic breast cancers demonstrated that ADCC plays a significant role in the antitumor response (46). Park et al. also demonstrated in vivo that the therapeutic effects of anti‐HER2/neu antibody occur primarily through ADCC, lending further support to the theory that ADCC is an important mechanism by which antitumor monoclonal antibodies function (10, 45). We have previously shown that the dual engagement of NK cell CD16 and cytokine receptors by cytokines such as IL2, IL12, or IL21 results in synergistic ADCC and IFNγ production (12, 16, 19, 20, 33). We observed robust and synergistic increases in ADCC and the levels of IFNγ, MIP-1α, and RANTES produced by NK cells when they were exposed to the combination of IL12 and F‐IgG–coated tumor cells, as compared to either stimulus alone. Supernatants from cultures of F-IgG and IL12-activated NK cells induced T-cell chemotaxis, highlighting the antitumor microenvironment provided by NK cell costimulation. Administration of IL12 in combination with F‐IgG elicited a significant antitumor response that was NK cell‐dependent in a murine tumor model. Thus, the coadministration of IL12 and the F‐IgG construct could be expected to promote an NK‐dependent antitumor response in the clinical setting.
Dual stimulation with IL12 and F-IgG stimulates NK cells to secrete MIP-1α and RANTES, factors that exert a strong chemotactic effect upon monocytes (47). Therefore, NK cell infiltration of F‐IgG–treated tumor deposits might be followed by a wave of monocyte migration, especially in the presence of IL12, which further augments NK cell chemokine production. Conversely, monocyte-derived TNFα is a well known activator of NK cell cytolytic activity (48) and could potentially sensitize tumor targets to NK cell cytolytic activity and apoptotic stimuli. The concurrent activation of NK cell and monocyte effector functions by IL12 and F-IgG has the potential to induce a synergistic antitumor immune response that relies upon the pre‐programmed interdependence of these two innate immune cell populations.
Therapeutically, F‐IgG may confer several advantages over other constructs. Studies of F-IgG localization in vivo demonstrate that the conjugate penetrates into the tumor microenvironment and specifically target tumor cells. About 40% of tumor cells are targeted by F-IgG after 72 h of treatment. This persistence may contribute to the ability of this agent to mediate tumor shrinkage. It is also possible that greater tumor targeting might be observed at later time points, with higher doses of F-IgG or that lower F-IgG binding was not detectable by flow cytometry. Specific engagement of tumor cell surface receptors, while sparing normal tissue, also results in a favorable toxicity profile, as demonstrated in this study. Being fully humanized, hypersensitivity reactions to F‐IgG are unlikely to occur (49).
We have shown that F-IgG complexes can be utilized to specifically enhance immune responses by NK cells and monocytes against FR+ malignancies. Treatment of NK cells and monocytes with immune stimulatory cytokines synergistically augmented their ability to lyse FR targeted tumor cells, in vitro. In vivo, the coadministration of IL12 and F-IgG resulted in significant tumor reduction, an effect that was dependent on the NK cell compartment. Thus, F-IgG and IL12 can selectively target NK cells to cancer cells by means of the FR.
Grant support: This work was supported by NIH Grants P01 CA95426, K24 CA93670, P30 CA16058 (W.E. Carson III, S. Tridandapani, J.C. Byrd, M.A. Caligiuri), T32 GM068412/F32 CA186542-01A1/Pelotonia Post Doctoral Fellowship (A.C. Jaime-Ramirez), T32 CA90338-27 (A. Mani), C.C. Skiner was a Pelotonia Fellow.
The authors have no conflicts of interest to disclose.