Background
The tumor microenvironment (TME) is an important factor in successful local treatment and in provoking a systemic immunological response in cancer patients [
1]. Dendritic cells (DCs) that infiltrate the TME are responsible for the uptake of antigens
in situ and maturation in the draining lymph nodes, and the provide the basis for effective anti-tumor T cell immune responses [
2].
In situ DC-based cancer immunotherapy with radiotherapy has been utilized to treat cancer patients, but only a small number of tumor regressions have been observed [
3]. A poor TME can cause DCs to differentiate into immunosuppressive regulatory DCs, which inhibit the effect of cytotoxic T cells activation and promote tumor progression [
4]. The function of DCs is mainly positively affected by a microenvironment that contains fewer immune suppression factors, more immune potentiating factors and an immunogenic hub in the tumor site [
5,
6]. This fact previously motivated us to develop a new strategy to improve the efficacy of
in situ DC vaccination by adding combining heat shock protein (Hsp) [
7] or by electro-gene therapy with cytokine [
8]. How a therapy-induced anti-tumor immunity should be manipulated is not clearly known but immunogenic cancer cell death (ICD) has emerged as the most important sign of a favorable immunogenic TME [
6,
9]. Only a favorable TME can provide the various important functional immunological cells and cytokines that are required for immunotherapy [
10,
11].
Hyperthermia has been used in cancer therapy for decades. A branch of hyperthermia, known as modulated electro-hyperthermia [
12‐
15] (mEHT – trade name: oncothermia) has been developed by the capacitive (impedance-based) coupling of 13.56 MHz amplitude-modulated radiofrequency energy at the tumor site [
15]. The electric field energy may be selected and delivered to the malignant cells by exploiting the larger amount of ionic connective tissue around the tumor area, creating massive apoptosis at mild temperatures (≦42 °C) [
14‐
17]. In Europe, mEHT has been successfully utilized in clinical treatment for over two decades [
18‐
20]. Numerous retrospective studies of cancer patients have revealed that mEHT can treat a very wide range of tumor lesions and various types of tumor, demonstrating that the mEHT is a feasible option for treating cancer [
14]. It is generally applied to treat various forms of malignant tumor, such as lung, liver, pancreas, brain, gastrointestinal, gynecological, and other such tumors. Qin et al. demonstrated that mEHT had an abscopal effect in experiments
in vivo [
21]. However, immature DCs that were used in Qin’s study may have increased the tolerance of antitumor immunity whereas mature DCs induce a strong antitumor immunity when they interact with cancer cells that are undergoing immunogenic cancer cell death (ICD) [
22]. The combination of mEHT and the intra-tumoral injection of DCs may be able to provide a more sustained systemic immunity, enhancing the abscopal effect [
23]. We hypothesize that mEHT is an ideal approach for changing the TME from immune-suppressive to immune-stimulatory. Mature DCs were utilized in this experiment to eliminate interference with the DC maturation process at tumor site and to observe the change in TME-induced mDC activation.
Although hyperthermia, combined with an intratumoral injection of DC, reportedly evokes systemic immunity, two applications of a moderately high temperature (43.7 °C for 1 h) are required to improve the induce an effective acquisition of antigens following three rounds of DCs treatment [
24]. However, the temperature is not easily reached in clinical practice by conventional hyperthermia machine. Mild temperature hyperthermia (>42 °C) cannot generate massive apoptosis or cause a damage-associated molecular pattern (DAMP) in the tumor environment. The lack of release of tumor antigens from apoptotic tumor cells may dampen the effect of combined DCs and hyperthermia [
21,
25‐
27]. mEHT has been demonstrated to induce massive apoptosis and a DAMP-related signal sequence in colorectal cancer xenografts at mild temperatures [
28]. A favorable anti-tumor immune microenvironment at a mild temperature may be more effective in promoting an immunological cell death response [
28]. For the above reasons, this work proposes that combining intratumoral DCs at mild temperature with mEHT may be more effective in generating tumor cell apoptosis and DAMP and in providing a favorable immunological environment eliciting specific immunity. The data obtained herein evidence that mEHT may change TME immune phenotypes, including infiltrated leukocytes and eosinophils, and be feasibly combined with intra-tumoral DCs immunotherapy.
Methods
Cell lines and mice
CT26, a murine colon carcinoma cell line that is derived from a BALB/c mouse, was purchased from the Culture Collection and Research Center (Hsinchu,Taiwan), where fresh batches are thawed every year. CT26 cells were maintained in Dulbecco’s modified Eagle medium (DMEM) was supplemented with 10 % fetal bovine serum (FBS), 100 ng/ml of streptomycin, and 100 U/ml of penicillin (Invitrogen). Female BALB/c mice were obtained from the National Science Council Animal Center, Taipei, Taiwan, and were used at between 6 and 8 weeks of age. This study was approved by the Institutional Animal Care and Use Committee of the Shin Kong Wu Ho-Su Memorial Hospital (Approval No. 0990827008).
Modulated electro-hyperthermia treatment (mEHT)
Electromagnetic heating was conducted using capacitive-coupling with an amplitude-modulated 13.56-MHz radiofrequency (LabEHY, Oncotherm, Germany). The mEHT technical details of the method can be found elsewhere [
29]. An
in vitro heating model was established in an electrode chamber (LabEHY in vitro applicator), which was heated to 42 °C for 30 min at a mean power of 8 ~ 9 W. The cells were placed in a chamber with a culture medium at 42 °C for 30 min. Tumor implants in the right femoral area of BALB/c mice were placed in the parallel electric condenser of the heating circuit, as described elsewhere [
28]. The treatment groups were givena single shot of mEHT for 30 min at a mean power of 1.5 W under 100 mg/kg Ketamine and 10 mg/kg Xylazine anesthesia. Intratumoral temperature was maintained at ~ 42 °C on the treated side of each mice, as measured using optical sensors (Luxtron FOT Lab Kit, LumaSense Technologies, Inc., California, USA). The subcutaneous temperature underneath the electrode was maintained at 38 ~ 40 °C.
Apoptosis assay
Water bath-treated and mEHT-treated CT26 cells were cultured for 24 h, then trypsinized, and washed twice with PBS. Apoptosis was verified using an Annexin V Apoptosis Kit (BD Pharmingen), following the manufacturer’s instructions. Briefly, tumor cells were washed three times with PBS; then, some cells were analyzed immediately for apoptosis using Annexin V/PI staining. Washed cells were supplemented with 1 % BSA and then stained directly with 10 μL of PI and 2.5 μL Annexin V-FITC, following the addition of 222.5 μL of binding buffer. Immediately after 10 min of incubation in the dark on ice, the cells were analyzed by flow cytometry. The percentage of positive cells was determined using a FACSCalibur cytometer and Cell Quest Pro software (Becton Dickinson, Mountain View, CA).
Western blot analysis
For protein analysis, the water bath-treated control and mEHT-treated CT26 cells were lysed for 5 min at room temperature in a buffer of 150 mM NaCl, 50 mM Tris (pH 8.0), 5 mM EDTA, 1 % (v/v) Nonidet p-40, 1 mM phenylmethylsulfonyl fluoride, 20 μg/mL aprotinin, and 25 μg/mL leupeptin (Sigma). The total protein concentration was measured using the Bio-Rad protein assay reagent. Cell lysates (100 μg) were electrophoresed on a 12 % polyacrylamide gel, transferred onto an Immobilon-P PVDF membrane (Millipore, Bedford, MA), and blocked in PBS-Tween 20 and 10 % nonfat milk for 2 h at room temperature. The filter was incubated with specific antibodies to anti-Hsp70 (Santa Cruz Biotechnology, Santa Cruz, CA) and anti-HMGB-1 (Abcam, Cambridge, MA, USA) for 2 h at room temperature in PBS-0.05 % Tween 20 that contained 5 % nonfat milk, followed by 1 h incubation at room temperature with horseradish peroxidase-conjugated secondary antibodies (Jackson ImmunoResearch Laboratories, West Grove, PA) in the same buffer. Blots were developed using a chemiluminescent detection system (ECL; GE Life Science, Buckinghamshire, UK).
Hsp70 release assay
mEHT treated CT26 cells were cultured for 24 h. The culture supernatants were harvested and Hsp70 was measured by using an enzyme-linked immunosorbent assay (ELISA) (Enzo Life Sciences, Farmingdale, USA). A Multiskan Plus (Thermo Scientific, Hudson, NH, USA) was utilized to measure absorbance at 450 nm.
Generation of bone marrow-derived dendritic cells
Bone marrow-derived DCs (BM-DCs) were produced as described elsewhere [
9]. Briefly, BM-DCs were isolated from BALB/c mice by culturing red blood cell-depleted BM cells in a complete medium (RPMI 1640 that was supplemented with 10 % FBS, L-glutamine, and 5 mM 2-mercaptoethanol) that contained 20 ng/ml of recombinant mouse GM-CSF (Peprotech, Rocky Hill, NJ, USA) at 37 °C in a humidified atmosphere with 5 % CO
2 and fed every third day with a medium that contained fresh GM-CSF. On day nine of the culture, the DCs were mixed with 10 μg/ml AH1 (SPSYVYHQF) that had been manufactured at 95 % purity by AnaSpec (Fremont, CA) and 50 μg/ml Hsp70 which was prepared in our laboratory as described elsewhere [
7] for 24 h. On day ten of the culture, non-adherent cells were harvested, washed once in a complete medium, and examined to evaluate the expression of the DC surface markers (MHC class II molecule I-A
d/I-E
d, CD80 (B7-1), CD86 (B7-2), CD11c, and DEC205). The BM-DCs (5–10 × 10
5) were stained with 50 μL of FITC-conjugated antibodies in phosphate-buffered saline (PBS) that contained 1 % bovine serum albumin (BSA) and 0.1 % azide, which was also used as the washing buffer, before being subjected to fluorescence-activated cell sorting (FACS) analysis using a FASCalibur flow cytometer (BD Bioscience, San Diego, California, USA). Cells were stained with the corresponding isotype-matched control IgG (BD Pharmingen, San Diego, CA, USA). Endocytic activity was quantifiedby incubating cells for 2 h with FITC-dextran (100 μg/ml) (Sigma) at 4 °C or 37 °C. Cells were washed extensively with PBS, before being subjected to FACS analysis. Non-specific binding of FITC-dextran to the cell surface was measured by incubating the cells at 4 °C [
30]. The percentage of positive cells was obtained using a FACSCalibur cytometer and Cell Quest Pro software (Becton Dickinson, Mountain View, CA).
Animal study
On day zero, the right femoral areas of BALB/c mice were injected subcutaneously with 5 × 10
5 CT26 tumor cells. On day 14 following injection, the mice received local mEHT treatment (as described above), and then, on the following day, 5 × 10
5 syngeneic DCs or PBS in 25 μL were injected into the right femoral tumor area. Each group comprised ten mice. Sampling was carried out 48 h following treatment, using three mice in each group. Each excised tumor was fixed in 10 % formalin, dehydrated, and embedded in paraffin wax (FFPE). The sizes of the tumors in the other seven mice in each group were measured at least three times weekly: length (L) and width (W) were recorded and the tumor volumes were calculated as L × W
2/2. To evaluate whether specific immunologic memory responses were generated in mice that bore CT26 tumor cells, the mice were re-challenged with 1 × 10
5 tumor cells in the other flank 30 days following the first tumor inoculation [
9]. The mice were examined three times weekly to evaluate tumor development for 30 days after tumor cell transplantation or the first inoculated tumor growth until the tumor was more than 2 cm in diameter.
Cytotoxicity T lymphocyte (CTL) assay
On day 30 following tumor injection, the mice were killed and their spleens harvested. Erythrocyte-depleted splenocytes (1 × 106 cells/ml) were cultured for five days in vitro using mitomycin C-treated CT26 tumor cells (1 × 106 cells/ml) in 24-well plates, during which time 50 IU/ml of recombinant human IL-2 (Proleukin; Novartis Pharmaceuticals, East Hanover, NJ) was added daily. On day five, the cells were collected; dead cells were removed on a density gradient, and the viable cells were tested to evaluate specific cytotoxicity using LDH-release assay (Promega, Madison, WI, USA). The percentage-specific cytotoxicity was calculated as 100 x [(experimental release – spontaneous release)/(maximal release – spontaneous release)].
Enzyme-linked immunosorbent spot (ELISPOT) assay
The ELISPOT assay was conducted using a Mouse IFN-γ Development Module kit (R&D System), following the manufacturer’s instructions. Splenocytes were prepared as described for use in the CTL reactions. The harvested splenocytes (1 × 105 in 100 μL) were then mixed with 100 μL of CT26 tumor lysate (50 μg of protein/ml) in each well of a 96-well filtration plate (MultiscreenTM HTS) that had been previously coated with capture antibodies (1:60 dilution). The negative controls were the medium alone and the splenocytes alone and the positive control was splenocytes plus 20 μg/ml of Con A. After incubation overnight at 37 °C, color was developed using the streptavidin-alkaline peroxidase and BCIP/NBT that was provided in the ELISPOT kits. The spots were counted visually under a dissection microscope; the numbers of spots in the test samples (splenocytes + tumor lysate), spots obtained using splenocytes alone, and spots obtained using medium alone were calculated.
Immunohistochemistry and Luna stain
To conduct immunohistochemical studies, the tumor was resected and fixed in 10 % formalin for 24 h. To stain the sections immunohistochemically, paraffin sections were deparaffinized in xylene and rehydrated in a graded alcohol series, treated with 3 % H
2O
2 for 10 min, and boiled in a citrate buffer (pH 6) for 30 min (anti-F4/80 antibody, Bioss bs-7058R, anti-CD45 antibody, Bioss bs-0522R), before immunoblock (Bio TnA, TAHC03) was applied to prevent non-specific binding for 60 min at room temperature. The sections were incubated with rabbit anti-F4/80 antibody (diluted 1:100) and anti-CD45 antibody (diluted 1:100) for one hour at 37 °C, and analyzed by Mouse/Rabbit Probe HRP labeling (BioTnA, TAHC03) for 30 min at room temperature. Peroxidase activity was developed in a diaminobenzidine- H
2O
2 solution (Bio TnA, TAHC03) for 10 min at room temperature. The sections were then counterstained with hematoxylin. All stained slides were examined by two pathologists who were blind to the treatment group data. The percentage of positively stained cell membranes or cytoplasm was obtained by microscopically examining the entire tissue at high magnification (×400). The numbers of positive cells was calculated in ten fields. The Luna protocol was performed as described elsewhere with slight modifications [
31]. The sections were immersed in working Hematoxylin-Biebrich (Sigma, Cat # H-3136 and Acros, CI 26905, respectively) scarlet solution (for five minutes), and then dipped (∼8x) in 1 % acid alcohol and rinsed in tap water. The sections were then dipped (∼5x) in lithium carbonate solution until they turned blue and washed in running tap water (for two minutes). The numbers of eosinophil on the stained slide were calculated in ten fields (x400).
Statistical analysis
All results were compared using an unpaired t test (two-tailed) or one-way ANOVA. Differences were considered statistically significant at a P value of less than 0.05
Discussion
This study found that the combination of mEHT at a clinical achievable temperature (42 °C) with the intra-tumoral injection of DCs not only elicits a local antitumor response but also induces a systemic anti-tumor immune response. A tumor-specific T cell response was evoked. The ability of mEHT to induce apoptosis in a high percentage of tumor cells and enhance the release of Hsp70 is believed to be a key contributor to the tumor-specific immune response. In our previous study, co-injection of rHsp70 and DCs was found to turn radiation-induced local apoptosis into a systemic anti-tumor immune response. Co-injection of rHsp70 and DCs into the irradiated tumor site caused a more potent anti-tumor immune response than did the injection of DCs alone [
7]. In this study, mEHT caused a heated tumor to release more Hsp70 into extracellular spaces than did other hyperthermic methods. The release of Hsp70 served as a danger signal that made the TME a more immunologically responsive milieu, in which infiltration by eosinophils.
Mukhopadhaya et al. reported that localized hyperthermia, following by heating in a water bath at 43.5 °C, combined with intratumoral DC induced systemic antitumor immunity [
24]. Heat treatment (>43.5 °C) induces both apoptosis and necrosis and the release of Hsp70 from cancer cells and triggers DC activation. However, several points must be addressed. First, heating by a water bath cannot be used in clinical practice. Heating a localized tumor to 43 °C using conventional hyperthermia machines is very difficult. In the experiment in this study, hyperthermia that was generated using a water bath at 42 °C induced only a limited apoptotic or necrotic effect in cancer cells. Another radiofrequency machine, operated at 42 °C for 30 min, also failed to have cause significant apoptosis in cells (unpublished data). Only mEHT induced significant apoptotic cell death at 42 °C for 30 min. Accordingly, the combination of mEHT with intratumoral DC immunotherapy should be clinically feasible. We have previously reported that the intratumoral injection of immature DCs into the irradiated tumor (RT-DC treatment) elicits tumor-specific immunity in hepatocellular carcinoma patients [
3]. The present study recommends a future clinical trial of a combination of mEHT, intra-tumoral injection of DCs and radiotherapy.
The use of mEHT treatment as adjuvant for DC therapy to induce immunogenic apoptotic cell death by has recently been examined [
21,
36]. However, the incubation of stressed, apoptotic tumor cells with syngeneic DCs is generally not strong enough to generate protective immunity, suggesting that the uptake of apoptotic cells by DCs alone may not be sufficiently efficient to activate an immune response, as described by others [
37]. In this study, DC alone was not effective in inducing an immune response. The suppressive monocytes that are formed by a CT26 tumor have an important role in general immunosuppression [
38]. These suppressive monocytes may inhibit the function of therapeutic DC. Therefore, the secondary signals that are required to activate DC function are induced by danger molecular pattern proteins, such as calreticulin, HSPs, and the HMGB1 [
39]. mEHT provides danger molecular pattern proteins and induces inflammatory signals in tumor microenvironments [
28]. Apoptotic cells cannot effectively activate DC activation in the absence of inflammatory signals [
37,
40,
41]. Candido et al. [
42] found that intratumoral administration of DC can partially inhibit the growth of an established tumor, but the co-administration of inflammation cytokine (TNF-α) strengthens the DC-mediated anti-tumor effect, consistent with our observations.
mEHT reversed the immunosuppressive microenvironment to an inflammatory environment and induced a DC-mediated anti-tumor immune response [
21]. The inflammatory environment herein was evidenced by the infiltration of CD45
+ cells and F4/80
+ cells (Fig.
4). Tumor-infiltrating CD45RO
+-cell density has been identified as a prognostic biomarker that is associated with the longer survival of colorectal cancer patients [
43]. mEHT improves the expression of this prognostic biomarker.
Changing the TME into an inflammatory environment is important in ensuring that the DCs function in a manner that triggers systemic immunity and that the effector T cells adequately kill tumors. Although several studies have shown that DC therapy induces immune responses in cancer patients, few reports have demonstrated any clinical benefit of DC treatment perhaps because of the inhibitory effect of the TME. To improve the efficacy of DC therapy, the immunosuppressive status of the TME must be reprogrammed [
44]. Immune checkpoint blockage therapy was recently shown to have a promising therapeutic effect on cancer patients [
45]. The combination of positive immunotherapy with an anti-negative immune checkpoint inhibitor is a synergistic strategy [
46]. The success of immune check point therapy demonstrates that elimination of the inhibitory pathways that block effective antitumor T cell responses is important in cancer therapy. However, the removal of inhibitory pathways from the immune system does not suffice to cure all of a cancer: increasing the number of immunopotentiation tumor-infiltrating cells, including CD45-positive leukocytes [
46] and eosinophils, may be equally important [
35]. However, a tumor tissue that lacks immunological markers may represent a nonimmunologic TME. The TME must be turned into an immunologic TME before DC therapy can activate T cells. Reciprocally, active T cells depend on an immunological TME to have a positive clinical effect. Therefore, combined treatment with mEHT and DCs should help to establish OR an immunogenic TME that has a clinical benefit for patients, independently of whether the preexisting tumor was immunogenic or nonimmunologic. Owing to the clinical feasibility of mEHT, this result suggests future clinical applications.
Acknowledgements
This study was supported by the research fund of the Department of Radiation Oncology, Ditmanson Medical Foundation, Chiayi Christian Hospital, Taiwan and under project SKH-8302-100-DR-20 of the Department of Radiation Therapy and Oncology, Shin Kong Wu Ho-Su Memorial Hospital, Taipei, Taiwan. Ted Knoy is appreciated for his editorial assistance.
Competing interests
The authors disclose no financial interest.
Authors’ contributions
KHC and WTL conceived and designed this study. YWT, CCH, KLY, and MSC contributed to perform the experiments. HCC contributed to analyzed the data. YSW, GA, and AS wrote the manuscript. All authors have read and approved the final manuscript.