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Cytokine gene delivery by viral vectors is a promising novel strategy for cancer immunotherapy. Semliki Forest virus (SFV) has many advantages as a delivery vector, including the ability to (i) induce p53-independent killing of tumor cells via apoptosis, (ii) elicit a type-I interferon (IFN) response, and (iii) express high levels of the transgene. SFV vectors encoding cytokines such as interleukin (IL)-12 have shown promising therapeutic responses in experimental tumor models. Here, we developed two new recombinant SFV vectors encoding either murine tumor necrosis factor-α (TNF-α) or murine interferon-γ (IFN-γ), two cytokines with documented immunostimulatory and antitumor activity. The SFV vector showed high infection rate and cytotoxicity in mouse and human lung carcinoma cells in vitro. By contrast, mouse and human macrophages were resistant to infection with SFV. The recombinant SFV vectors directly inhibited mouse lung carcinoma cell growth in vitro, while exploiting the cancer cells for production of SFV vector-encoded cytokines. The functionality of SFV vector-derived TNF-α was confirmed through successful induction of cell death in TNF-α-sensitive fibroblasts in a concentration-dependent manner. SFV vector-derived IFN-γ activated macrophages toward a tumoricidal phenotype leading to suppressed Lewis lung carcinoma cell growth in vitro in a concentration-dependent manner. The ability of SFV to provide functional cytokines and infect tumor cells but not macrophages suggests that SFV may be very useful for cancer immunotherapy employing tumor-infiltrating macrophages.
Viral vectors have been used for cancer immunotherapy to intratumorally deliver and express transgenes and to thereby increase therapeutic protein delivery while simultaneously reducing systemic toxicity (1). Recombinant Semliki Forest virus (rSFV) has been successfully used as a cancer immunotherapy in preclinical tumor models for cytokine gene delivery (2–15) and for immunization with tumor-associated antigens against mastocytoma (2, 16) and human papilloma virus (HPV)-associated cervical cancer (17, 18). Semliki Forest virus (SFV) belongs to the Alphavirus genus of the Togaviridae family and possesses an enveloped nucleocapsid that contains a positive-sense single-stranded (+ss) RNA genome (19). The replication-deficient SFV vector system delivers genes of interest by infecting the cells with viral particles and thereby providing a transiently high level of transgene expression without further virus replication (20). The SFV-based vector is an attractive tool for cancer immunotherapy because of its oncolytic nature and ability to induce p53-independent apoptosis of tumor cells (21), which may facilitate uptake and presentation of tumor antigens from the apoptotic bodies by antigen-presenting cells, thus enhancing cancer immunogenicity (22, 23). In addition, SFV vector elicits endogenous type-I interferon (IFN) responses, which may be required for the therapeutic effect of a vector-encoded cytokine (3).
Cytokines can contribute to antitumor immune responses in the tumor microenvironment (24, 25) and are, therefore, promising tools for cancer immunotherapy. rSFV has been used in preclinical studies to modulate the tumor microenvironment by locally delivering cytokines, such as interleukin (IL)-12 (2–11), IL-18 (12), IFN-α (13), granulocyte-macrophage colony-stimulating factor (14), and endostatin (15). An SFV vector encoding the heterodimeric murine IL-12 (SFV-IL12) was shown to have a strong therapeutic antitumor effect when locally injected in tumor models of melanoma (4), glioma (5), colon adenocarcinoma (3, 6, 7), hepatic colon adenocarcinoma (8), hepatocellular carcinoma (9), mastocytoma (2), fibrosarcoma (7), breast carcinoma (7), and lung carcinoma (3) in mice, orthotopic hepatocellular carcinoma in rats (10), and spontaneous hepatocellular carcinoma in woodchucks (11). The therapeutic activity of SFV-IL12 involved immune responses that were mediated by IL-12 in combination with the virus-induced endogenous type-I IFN (3, 9, 11), which lead to an angiostatic effect (4) and enhanced CD8+ T-cell responses (3, 5–8, 11).
Two well-known cytokines that may be potentially useful for cancer immunotherapy are IFN-γ and tumor necrosis factor-α (TNF-α). The pleiotropic cytokine IFN-γ is a tumor-suppressive factor that protects against carcinogen-induced and spontaneous tumor development (26, 27), inhibits tumor angiogenesis (28–31) and may improve tumor immunogenicity by upregulating major histocompatibility complex class I molecules (32, 33). Furthermore, it has been shown that IFN-γ enhances macrophage activation toward a tumoricidal phenotype in vitro (34–36) and in vivo (31, 37–39). TNF-α was discovered in 1975 as a serum factor inducing haemorrhagic necrosis in tumors (40) and, therefore, this cytokine was proposed as a potential anti-cancer agent. TNF-α has been shown not only to selectively destroy tumor vasculature (41, 42), but also increase tumor vessel permeability, thus, improving drug penetration into tumors (43–45). Moreover, low doses of TNF-α have been shown to promote antitumor immune responses by enhancing T-cell infiltration and by activating macrophages toward a tumor-suppressive phenotype (46). Notably, a synergistic action of IFN-γ and TNF-α was reported in early studies showing tumor growth inhibition in mice (47, 48) and tumor disappearance in patients after local limb perfusions with IFN-γ and TNF-α in combination with a chemotherapeutic agent (49). The antitumor effects were likely due to decreased endothelial cell adhesion and survival in response to TNF-α and IFN-γ leading to destruction of tumor vasculature (50). The synergism may also be explained by the fact that IFN-γ enhances TNF-α receptor expression in malignant cells (51, 52), thus improving TNF-α treatment. Another synergistic action of IFN-γ and TNF-α has been shown on macrophage activation toward a tumoricidal phenotype in vitro (53). However, the clinical usefulness of TNF-α and IFN-γ is limited by their systemic toxicity (54, 55) and short in vivo half-lives (56, 57).
To the best of our knowledge, no previous studies have reported using rSFV vectors that encode the cytokine IFN-γ or TNF-α. To provide new tools for cancer immunotherapy, we developed two rSFV vectors that encoded either murine TNF-α or IFN-γ and tested the functionality of the resulting rSFV-encoded cytokines in vitro. Here, we show that the rSFV vectors were capable of infecting Lewis lung carcinoma (LLC) cells and exploiting them to produce rSFV-encoded TNF-α and IFN-γ. Moreover, in this study, we show that rSFV-encoded IFN-γ effectively enhanced macrophage activation toward a cancer-suppressive phenotype in vitro.
Baby hamster kidney (BHK-21) fibroblasts were obtained from American Type Culture Collection (Cat. No. CCL-10™; ATCC/LGC Prochem, Boras, Sweden) and cultured in Glasgow’s MEM (Cat. No. 11710; Thermo Fisher Scientific, Boston, MA, USA) supplemented with 10% fetal bovine serum (FBS; Cat. No. F7524; Sigma-Aldrich, St. Louis, MO, USA), 10% Tryptose Phosphate Broth solution (Cat. No. T4049; Sigma-Aldrich), 20mM HEPES (Cat. No. H0887; Sigma-Aldrich), 2mM l-Glutamine (Cat. No. 25030; Thermo Fisher Scientific), 100U/mL penicillin, and 100mg/mL streptomycin (Cat. No. P0781, Sigma-Aldrich). The LLC cell line (also called LLC1; Cat. No. CLS 400263) and mouse macrophage cell line J774A.1 (Cat. No. CLS 400220) were obtained from Cell Lines Service (CLS GmbH, Eppelheim, Germany). The LLC cells were grown in RPMI-1640 medium (Cat. No. 61870; Thermo Fisher Scientific) supplemented with 10% FBS (Sigma-Aldrich). The J774A.1 cells were cultured in RPMI-1640 medium supplemented with 10% FBS (Cat. No. S0415; Biochrom GmbH, Berlin, Germany). The human lung carcinoma cell line A549 (Cat. No. CCL-185™) and murine fibrosarcoma cell line L929 (Cat. No. CCL-1™) were obtained from American Type Culture Collection (ATCC/LGC Standards GmbH, Wesel, Germany). The A549 cells were propagated in Advanced Dulbecco’s MEM (Cat. No. 12491; Thermo Fisher Scientific) supplemented with 5% FBS (Sigma-Aldrich) and 2mM L-glutamine. The conditioned medium (CM) of L929 cells was used as a source of macrophage colony-stimulating factor (M-CSF) (58) for the maintenance and differentiation of bone marrow-derived progenitors into macrophages. Briefly, L929-CM was produced by cultivating L929 cells in RPMI-1640 with 10% FBS (Sigma-Aldrich), 100U/mL penicillin and 100mg/mL streptomycin in T75 flasks until confluency. The medium was then removed, 30mL of RPMI-1640 supplemented with 10% FBS (Biochrom) without antibiotics was added, and cells were incubated for 10days. The L929-CM was harvested and spun at 300g for 10min. The collected supernatant was filtered through a 0.22-µm strainer and stored at −20°C until used. All cells were cultured at 37°C in a humidified incubator in an atmosphere containing 5% CO2 and 95% air.
C57BL/6NRj mice (Janvier Labs, Le Genest-Saint-Isle, France) were bred at the Department of Comparative Medicine, Oslo University Hospital, Rikshospitalet (Oslo, Norway). All animal experiments were approved by and performed in accordance with the regulations and guidelines of the Norwegian Food Safety Authority.
Murine BMDMs were differentiated from bone marrow progenitors obtained from C57BL/6NRj mice as previously described (59, 60) with a few modifications. Femur and tibia were aseptically dissected from 8- to 10-week-old C57BL/6NRj mice, and bone marrow cells were collected by flushing the femurs and tibias with RPMI-1640 supplemented with 10% FBS (Biochrom) using a 25G needle. After the cells were centrifuged for 5min at 400g, the erythrocytes were lysed in lysis buffer (150mM NH4Cl, 10mM KHCO3, and 0.1mM EDTA-Na2, pH 7.2–7.4, filtered through a 0.2-µm strainer), and the remaining cells were then filtered through a 70-µm cell strainer (Cat. No. CLS431751; Sigma-Aldrich) and centrifuged. The cells were seeded in 90-mm untreated cell culture dishes (Cat. No. 734-2359; VWR, Radnor, PA, USA) at a concentration of 8×106/dish and then differentiated via cultivation for 7days in medium referred to hereafter as complete BMDM differentiation medium (consisting of RPMI-1640 with 10% FBS and 30% L929-CM containing M-CSF). The adherent cells were considered CD11b+F4/80+ macrophages since flow cytometry revealed that these cells were more than 99% pure (data not shown). After 7days, the cells were detached by incubating them in cold Dulbecco’s phosphate-buffered saline without Mg2+/Ca2+ (referred to as PBS−/−; Cat. No. D8537; Sigma-Aldrich) for 15–20min at 4°C. The harvested cells were centrifuged and frozen in FBS containing 10% DMSO (Cat. No. 0231; VWR). The BMDMs were cultivated in RPMI-1640 supplemented with 10% FBS and 10% L929-CM.
Peripheral blood mononuclear cells (PBMCs) were isolated from human buffy coats via centrifugation in Lymphoprep™ density gradient medium (Cat. No. 1114547; Alere Technologies AS, Oslo, Norway) according to the manufacturer’s protocol. Buffy coats were obtained from the blood bank of St. Olav’s Hospital (Trondheim, Norway). Monocytes were enriched from total PBMCs via plastic adherence in 8-well TC Lab-Tek Chamberslides (Cat. No. 80826; ibidi GmbH, Martinsried, Germany) and maintained in RPMI 1640 medium supplemented with 10% human serum (obtained from the blood bank of St. Olav’s Hospital, Trondheim, Norway). Monocyte-derived macrophages were differentiated from monocytes by incubating the cells in RPMI 1640 containing 10% human serum and 10ng/mL human M-CSF (Cat. No. SRP6165; Sigma-Aldrich) for 7days.
The pSFV1-DsRed vector, which carries a gene for Discosoma sp. red fluorescent protein (DsRed), was generated in our lab as previously described (61) using the pSFV1 vector (20). The pSFV1 and pSFV-Helper1 plasmids (20) were generously provided by Garoff (Karolinska Institute, Stockholm, Sweden).
To generate the pSFV1-Tnfa-Flag plasmid, we used the pSFV1-NruI vector, which is a derivate of pSFV1 that was generated in our lab by deleting a 527bp StuI-HindIII fragment from pSFV1 (bp 7603–8130) and changing a unique SpeI site to a NruI site (62). The murine TNF-α-coding gene (Tnfa) (GenBank No. NM_013693.2) fused to a Flag-tag sequence was inserted into the pSFV1-NruI vector under the control of the SFV 26S subgenomic promoter. The Tnfa-Flag fragment was amplified from the template plasmid pCMV3-mTNF-Flag (Cat. No. MG50349-CF; Sino Biological Inc., Beijing, China) using PCR with the following primers (synthesized by Microsynth AG, Balgach, Switzerland): 5′-GCGGATCCATGAGCACAGAAAGCATGATC-3′ (forward) and 5′-TGCCCGGGTTTACTTATCGTCGTCATCCTTG-3′ (reverse). BamHI and SmaI restriction sites (shown here in bold) were introduced to facilitate the ligation of the PCR fragment into the pSFV1-NruI vector.
The pSFV1/Enh-Luc plasmid was generously provided by A. Merits (Institute of Technology, University of Tartu, Estonia) and has been previously described (63). The pSFV1/Enh-Ifng vector was generated by replacing the XmaI-ApaI fragment (bp 7572-9268), which contained the firefly luciferase gene (Luc) of pSFV1/Enh-Luc, with the murine IFN-γ-coding gene (Ifng) (GenBank No. NM_008337.3). The Ifng gene was amplified from the template plasmid pMD19-mIFNG (Cat. No. MG50709-M; Sino Biological Inc.) using PCR with the following primers (synthesized by Microsynth AG): 5′-TCCGCCCGGGATGAACGCTACACACTGC-3′ (forward) and 5′-TCCGGGCCCTCAGCAGCGACTCCTTTTCC-3′ (reverse). XmaI and ApaI (shown here in bold) restriction sites were incorporated to facilitate cloning into the pSFV1/Enh-Luc vector. The sequences Tnfa-Flag and Enh-2A-Ifng of the constructs were verified by GATC Biotech AG (Constance, Germany) and found to share 100% identity with the reference sequences Tnfa (GenBank No. NM_013693.2), Flag (shown in the product description of pCMV3-mTNF-Flag (Cat. No. MG50349-CF; Sino Biological)), Enh-2A [shown in Ref. (7)] and Ifng (NM_008337.3).
RNAs were synthesized and transfected into BHK-21 cells using electroporation as previously described (63). The plasmids pSFV/Enh-Ifng, pSFV-DsRed, and pSFV-Helper1 were linearized using the restriction enzyme SpeI (Cat. No. ER1251; Thermo Fisher Scientific), and pSFV/Tnfa-Flag was linearized using NruI (Cat. No. ER0111; Thermo Fisher Scientific). The linearized plasmids (1µg of each) were used as templates for the in vitro transcription (SP6 RNA polymerase; Cat. No. AM2071; Thermo Fisher Scientific) of SFV-Helper1 RNA and recombinant RNAs (rRNAs) carrying Ifng, Tnfa, or DsRed. The transcribed rRNAs were capped by adding 1mM 3′-O-Me-m7G(5′)ppp(5′)G cap-structure analog (Cat. No. S1411S; New England Biolabs, Hitchin, UK) during the transcription reaction. To package the rRNAs into viral particles, each of the rRNAs was co-electroporated with the SFV-Helper1 RNA in 1×107 BHK-21 cells by pulsing the mixture twice at 850V, 25mF using a Gene Pulser-II apparatus (Bio-Rad, Hercules, CA, USA). The Helper1 RNA provided in trans the SFV structural proteins (20) for encapsidation of the rRNA. The electroporated BHK-21 cells were resuspended in 15mL of BHK-21 cultivation medium containing 1% FBS (Sigma-Aldrich) and then incubated at 33°C for 48h. The cell growth medium containing the infectious rSFV particles was then harvested, rapidly frozen in liquid nitrogen, and subsequently used as a source of rSFV particles. The titers of the rSFV particles were determined based on the “one virus particle—one infected cell” hypothesis regarding the replication-deficient virus particles. BHK-21 cells were infected with serial dilutions of the rSFV particles. Infected cells expressing DsRed were counted in 10 viewfields using fluorescence microscopy at 24h post-infection. The cells that were infected with either SFV-Tnfa or SFV-Ifng were stained with rabbit polyclonal antibodies that were specific for the nsp1 subunit of SFV replicase (generously provided by A. Merits, Institute of Technology, University of Tartu, Estonia) and with a fluorochrome-conjugated secondary antibody (Cat. No. A11034; Thermo Fisher Scientific). The stained cell monolayers were observed using EVOSfl digital inverted fluorescence microscope (Thermo Fisher Scientific), and infection-positive cells were counted in 10 viewfields using fluorescence microscopy. The rSFV particle titers were expressed as infectious units (IFU)/mL relative to virus infectivity in BHK-21 cells and were used later in this study to calculate multiplicity of infection (MOI), which indicated how many infectious viral particles were added per target cell during infection. Cells infected with the rSFV stocks did not secrete infectious virus particles, as shown in cell reinfection experiments, confirming that the virus stocks contained replication-deficient SFV.
Baby hamster kidney, LLC, A549, and J774A.1 cells and murine BMDMs were seeded in 12-well plates (Cat. No. 150628; Thermo Fisher Scientific) or 24-well plates (Cat. No. 142475; Thermo Fisher Scientific) and cultivated until 50–80% confluency. The cells were washed once with PBS containing Mg2+ and Ca2+ (referred to as PBS+/+; Cat. No. 14040; Thermo Fisher Scientific), and 140—600µL of an infectious suspension containing SFV-DsRed at a MOI=10 or MOI=15 (defined as 10 or 15IFU in BHK-21 cells) in PBS+/+ was added to duplicate sets of wells. PBS+/+ was used as a negative control. After the cells were incubated at 37°C for 80min, the infectious suspension was replaced with cell-specific growth medium, and the expression of DsRed in the infected cells was observed 24–48h later using an EVOSfl digital inverted fluorescence microscope (AMG). The LLC and J774A.1 cells were detached via scraping, the BHK-21 cells were detached using a 0.25% trypsin-EDTA solution (Cat. No. T4049; Sigma-Aldrich), and the BMDMs and A549 cells were detached by treatment with accutase (Cat. No. A6964; Sigma-Aldrich). The cells were then centrifuged and DsRed-positive cells were quantified 24h post-infection using BD FACSCalibur flow cytometer (BD Biosciences, San Jose, CA, USA). To evaluate cell viability BHK-21 and LLC cells were labeled 48h post-infection with 1µg/mL of fluorescein isothiocyanate (FITC)-conjugated annexin V (annexin V-FITC from Apoptosis Detection Kit; Cat. No. 556547; BD Biosciences) for 15min followed by staining with 3µM of DAPI (Cat. No. 422801; BioLegend, San Diego, CA, USA) for 5min. Cells were immediately quantified using BD LSRFortessa flow cytometer (BD Biosciences). The data were analyzed using FlowJo V10 software (FlowJo LLC., Ashland, OR, USA).
After differentiation in 8-well TC Lab-Tek Chamberslides (Cat. No. 80826; ibidi GmbH), HMDMs were washed once with PBS+/+ and incubated for 1h with 200µL of an infectious suspension containing SFV-DsRed at a MOI=15 (defined as 15IFU in BHK-21 cells) diluted in PBS+/+. A recombinant paramyxoviral vector Sendai virus (SeV)-GFP that was based on a wild-type infectious SeV clone that carried a supplemental GFP transgene (64) was generously provided by D. Kolakofsky (Department of Microbiology and Molecular Medicine, University of Geneva School of Medicine, Geneva, Switzerland) and used at a MOI=15 as a positive control for HMDM infection. The infectious suspension was replaced with normal cell growth medium, and the cells were observed at 24h post-infection using phase-contrast and confocal fluorescence microscopy with a Zeiss Axiovert 100-M inverted microscope equipped with a LSM 510 laser-scanning unit and a 1.4 NA×63 Plan-Apochromat oil-immersion objective. To calculate the percentage of fluorescent protein-expressing cells, the total number of cells was manually counted in at least 10 viewfields using phase-contrast microscopy. Fluorescent protein-expressing cells were simultaneously counted within the same viewfields using fluorescence microscopy.
Baby hamster kidney cells (1.97×104 cells/well) and LLC cells (7.03×104 cells/well) were plated in 96-well plates (Cat. No. 3595; Corning, Corning, NY, USA) and incubated for 22h. The cells were then washed once with PBS+/+ and incubated at 37°C for 80min with 50µL of an infectious suspension containing rSFV particles at MOI=15 (defined as 15 infectous units in BHK-21 cells) diluted in PBS+/+. The infectious suspension was then replaced with normal BHK-21 or LLC growth medium. Cells incubated in PBS+/+ without viral particles were used as a negative control. Cell morphology was observed 47h after infection using bright-field microscopy, and 1μCi of [methyl-3H]-thymidine (3H-TdR; Cat. No. MT6032; Hartmann Analytic GmbH, Braunschweig, Germany) per 1mL of cell growth medium was then added. After a further 24h of incubation, the cells were subjected to two freeze/thaw cycles and harvested using a Tomtec-96 cell harvester (Tomtec, Hamden, CT, USA) onto fiberglass filters (Cat. No. 1450-421; PerkinElmer Inc., Waltham, MA, USA). Cell growth was determined by measuring the incorporation of 3H-TdR into proliferating cells as counts per minute (cpm) using a microplate scintillation counter (MicroBeta Trilux 1450, PerkinElmer Inc.).
To produce rSFV-encoded TNF-α and IFN-γ, BHK-21 cells were cultivated in 75cm2 cell culture flasks (Cat. No. CLS430641; Sigma-Aldrich) until 80% confluency, washed once with PBS+/+ and then incubated at 37°C for 80min with 5mL of a suspension containing 1.92×108 IFU of SFV-Tnfa or 1.21×108 IFU of SFV-Ifng in PBS+/+. The virus-containing suspensions were then replaced with BHK-21 cultivation medium containing 1% FBS. After 36h, the cell growth medium was harvested and centrifuged at 300g for 5min to remove the cells before the supernatants were transferred to a new tube, which was then centrifuged at 11,000g for 8min. The remaining supernatants were stored at −80°C and used as a source of vector-derived (vd) TNF-α or vdIFN-γ. The concentrations within the supernatants of the cytokines vdTNF-α or vdIFN-γ were 332.28 and 795.92ng/mL, respectively. The levels of cytokines within the supernatants were quantified using Luminex bead-based assay with Bio-Plex Mouse Cytokine Group I IFN-γ or TNF-α sets (Cat. No. 171G5017M and 171G5023M; Bio-Rad, Hercules, CA, USA) according to the manufacturer’s instructions.
Baby hamster kidney and LLC cells were plated in 24-well plates (Cat. No. 142475; Thermo Fisher Scientific) and cultivated until the next day when the cells had reached 100 and 50% confluency, respectively. The cells were washed once with PBS+/+, and 600µL of infectious suspension containing either SFV-Tnfa or SFV-Ifng particles at a MOI=1, MOI=10 or MOI=40 (calculated according to the titration in BHK-21 cells) in PBS+/+ was added per well. After cells were incubated with the infectious suspension for 80min at 37°C, the infectious suspension was discarded, and 500µL of fresh cell growth medium was added per well. The cells were cultured for 24h before the growth medium was collected and centrifuged for 6min at 300g. The supernatant was then transferred to a new tube, which was centrifuged at 11,000g for 10min. The supernatants were stored at −80°C, and the levels of secreted vdTNF-α and vdIFN-γ were determined using Luminex bead-based assay with Bio-Plex Mouse Cytokine Group I IFN-γ and TNF-α sets (Cat. No. 171G5017M and 171G5023M; Bio-Rad) according to manufacturer’s recommended protocols.
L929 fibroblasts or LLC cells were plated in 24-well plates (Cat. No. 142475; Thermo Fisher Scientific) and cultivated in RPMI 1640 containing 10% FBS (Sigma-Aldrich) for approximately 24h until the cells reached 50–90% confluency. To verify the functional activity of vdTNF-α, it was added to L929 cells in parallel with recombinant (r)TNF-α (Cat. No. 315-01A; PeproTech, Rocky Hill, NJ, USA) to reach a final concentration of 6.6, 20, or 60ng/mL, and the cells were then cultivated for 24h. L929 cells that were treated with 1µM staurosporine (Cat. No. S4400; Sigma-Aldrich) for 24h were used as the positive control for apoptosis induction (65), and untreated cells were used as the negative control. LLC cells were treated with either 50ng/mL rTNF-α or 100ng/mL rIFN-γ for 48h to test cytotoxicity of cytokines to LLC cancer cells. LLC cells were also treated with 50ng/mL rTNF-α in combination with 100ng/mL rIFN-γ for 24h or 48h. LLC cells were pretreated with 100ng/mL rIFN-γ for 24h followed by 24h treatment with 50ng/mL rTNF-α. Untreated cells were used as the negative control, whereas L929 cells that were treated with 50ng/mL of rTNF-α were used as the positive control for apoptosis induction. After treatments L929 or LLC cells were detached using 0.25% trypsin-EDTA and centrifuged before they were labeled with annexin V-FITC and PI using an Apoptosis Detection Kit (Cat. No. 556547; BD Biosciences) according to the manufacturer’s protocol. Briefly, the cell pellet was resuspended in 100µL 1 x annexin V binding buffer and stained using 1µg/mL annexin V-FITC and 5µg/mL PI by incubating the cells at RT for 15–20min. Then, 400µL of additional annexin V binding buffer was added. The cell suspension was immediately analyzed using flow cytometry in a BD LSRFortessa instrument (BD Biosciences). The data were analyzed using FlowJo V10 software.
Murine BMDMs (4×106 cells/dish) were seeded in 90-mm nontreated cell culture dishes (Cat. No. 734-2359; VWR) and cultivated in complete BMDM growth medium (RPMI-1640 with 10% FBS (Biochrom) and 10% L929-CM) for 2–3days. The BMDMs were detached by incubating the cells in cold PBS−/− at +4°C for 15–20min and then harvested via centrifugation for 6min at 300g. To block cell proliferation, the BMDMs were incubated with 10µg/mL mitomycin C (Cat. No. M4287; Sigma-Aldrich) at 37°C for 2h. The cells were then washed twice with PBS−/− and plated in triplicate at one of three different densities (i.e., 6×104, 3×104, and 3×103 cells/well) in 96-well plates in 200µL of macrophage growth medium. The cells were then cultivated for 24h. To stimulate the macrophages, we treated them with 100ng/mL of the toll-like receptor (TLR) 2/1 heterodimer agonist Pam3CSK4 (referred to as Pam3; Cat. No. tlrl-pms; InvivoGen, San Diego, CA, USA), 100ng/mL of recombinant (r)IFN-γ (Cat. No. 315-05; PeproTech) or 100ng/mL of vdIFN-γ for 24h. Untreated BMDMs served as the negative control, and BMDMs that were treated with 100ng/mL of Pam3 in combination with 100ng/mL of rIFN-γ were used as the positive control. Some BMDMs were treated for 24h at 37°C with 100ng/mL of Pam3 in combination with fourfold dilutions of rIFN-γ at concentrations ranging from 0.0015 to 100ng/mL. Alternatively, other BMDMs were treated with 100ng/mL of Pam3 in combination with 16-fold dilutions of vdIFN-γ at concentrations ranging from 0.0015 to 100ng/mL. After 24h of treatment, 100µL of the cell culturing medium was replaced with 100µL of a LLC cell suspension containing 3×104 cells/mL to form co-cultures of macrophages and cancer target cells. The resulting macrophage:cancer cell ratios were 20:1, 10:1, and 1:1. BMDMs that were incubated alone served as the negative control for macrophage growth, and LLC cells that were incubated alone served as the positive control for normal LLC cell growth. After 20h, 3H-TdR was added to all the wells at a concentration of 1μCi per 1mL of growth medium, and the cultures were incubated for an additional 24h. Next, the plates were submitted to two freeze/thaw cycles and then harvested using a Tomtec-96 cell harvester onto fiberglass filters. Cell growth was analyzed by measuring the incorporation of 3H-TdR into proliferating cells as cpm using a microplate scintillation counter (MicroBeta Trilux 1450).
Nitrite () levels were measured using the Griess test in cultivation medium harvested from BMDMs at 24h post-treatment. Cultivation medium (100µL) was obtained from the wells with the highest densities of BMDMs and transferred to new 96-well round-bottom plates (Cat. No. 3799; Sigma-Aldrich). These were centrifuged for 6min at 400g. Then, 50µL of the supernatant was pipetted into new 96-well flat-bottom plates (Cat. No. 3595; Corning), and an equal volume of a solution containing 1% sulfanilamide (Cat. No. S9251; Sigma-Aldrich) and 5% phosphoric acid (Cat. No. 345245; Sigma-Aldrich) in H2O was added. The plates were incubated in the dark for 10min at RT to allow the sulfanilic acid to convert to diazonium salt. After the incubation period, 50µL of 0.1% N-(1-naphthyl)ethylenediamine (NED; Cat. No. N9125; Sigma-Aldrich) in H2O was added to the samples, standards, and blank to induce the immediate formation of azo dye. Solutions of sodium nitrite (NaNO2) in twofold dilutions at concentrations ranging from 3.13 to 100µM were used as the standard and set up in triplicate. Water was used as the blank. Absorbance was measured at 540nm using a microplate spectrophotometer (Epoch; BioTek Instruments, Winooski, VT, USA).
We constructed two new replication-deficient SFV-based vectors that encoded either mTNF-α or mIFN-γ (Figure (Figure1A).1A). To express mTNF-α in the SFV vector, a sequence containing the Tnfa gene followed by a Flag-tag-encoding sequence at the 3-prime end was subcloned into the pSFV1-NruI vector (Figure (Figure1A).1A). The pSFV-Ifng vector was made by inserting the mIFN-γ gene (Ifng) into the pSFV1/Enh vector downstream and in-frame with the SFV capsid translation enhancer sequence (Enh) that was fused to the 2A auto-protease sequence of foot and mouth disease virus (FMDV) (Figure (Figure1A).1A). The 2A-encoding sequence was included to induce the cleavage of the vdIFN-γ protein from the 34 amino acid-long peptide that was translated from the Enh sequence. It has been shown that by incorporating an enhancer element within SFV vector, the expression of the heterologous protein can be increased by up to 10-fold due to enhanced translation (7, 66). In contrast to the SFV-Ifng construct, we did not incorporate the enhancer element into the SFV-Tnfa vector aiming to retain low levels of translated TNF-α if necessary since lower levels of TNF-α might be important for normalization of tumor vasculature (46). The previously constructed vector pSFV-DsRed, which encode a fluorescent protein (Figure (Figure1B),1B), was used as a control to detect cell infection. All vectors comprised the prokaryotic SP6 RNA polymerase promoter for in vitro transcription of recombinant SFV replicons, as well as the vectors encoded SFV replicase complex, which consists of non-structural proteins (nsP) 1–4 (Figures (Figures1A–C).1A–C). The SFV structural proteins C, p62, 6K, and E1, which are necessary for the formation of infectious virus particles, were encoded by the SFV-Helper1 vector (Figures (Figures1C,D).1C,D). The heterologous genes (HGs) and the genes encoding the structural SFV proteins were inserted downstream of the SFV 26S promoter (Figures (Figures1A–C).1A–C). In this study, replication-deficient rSFV particles were produced by BHK-21 cells that were co-transfected with RNA transcribed from the SFV-Helper1 vector and RNA transcribed from a vector encoding a HG (Tnfa, Ifng, or DsRed) (Figure (Figure1D).1D). The rSFV viral particles were quantified in BHK-21 cells and revealed titers ranging from 107 to 108IFU/mL. More specifically, the mean viral titers were 1.15×108IFU/mL of SFV-Tnfa, 7.23×107IFU/mL of SFV-Ifng, and 1.46×108IFU/mL of SFV-DsRed. The SE of the mean viral titers between decuplicates did not exceed 10%.
We wanted to use rSFV to deliver cytokine genes into cancer cells for subsequent production of the tumor-suppressive factors. Cell susceptibility to viral infection is a prerequisite for successful gene delivery into cells using a viral vector. We investigated the ability of rSFV particles to infect both cancer cells and macrophages using the reporter vector SFV-DsRed. We infected cells with SFV-DsRed at a concentration 15 virus particles per cell (i.e., MOI=15). We observed the expression of the DsRed fluorescent protein using fluorescence microscopy and quantified the DsRed-expressing cells using flow cytometry at 24-h post-infection (Figures (Figures2A–E).2A–E). In all the tested cell types, non-infected cells were used as the negative control for DsRed expression. The BHK-21 cell line was used as a positive control due to being highly susceptible to SFV infection, as demonstrated by flow cytometry analysis that showed that 88.2% of the BKH-21 cells were infected under the experimental conditions used in this study (Figure (Figure2A).2A). We verified that both the murine (LLC) and the human (A549) lung carcinoma cell lines were infected by the rSFV particles because 41% of both cell types were DsRed-positive (Figures (Figures2B,C).2B,C). However, we also found that neither the mouse BMDMs nor the murine macrophage cell line J774A.1 was susceptible to SFV because less than 1.5% of the cells were DsRed-positive (Figures (Figures2D,E).2D,E). Macrophages remained resistant to SFV infection also when we increased the concentration of SFV particles during infection (data not shown).
To confirm these findings in human macrophages, we differentiated macrophages from blood-derived monocytes and infected the cells with SFV-DsRed virus particles at a MOI=15 (calculated according to the titer that was determined in BHK-21 cells). The SeV is known to infect human macrophages (67), and we therefore included a SeV that encoded GFP (SeV-Gfp) at a MOI=15 as a positive control. In parallel, we infected the human lung carcinoma cell line A549 with both types of recombinant viruses at a MOI=15, and used the infected A549 cells as a positive control for SFV infection. To calculate the percentages of infected cells, we counted the total number of cells as well as the number of fluorescent protein-expressing cells within the same viewfields (multiple viewfields per sample) using phase-contrast and fluorescence microscopy at 24h post-infection. In these experiments, 30% of the positive control sample (the human cancer cell line A549) was infected with SFV-DsRed, whereas the HMDMs remained uninfected (Figure (Figure3,3, middle panel). Contrary to our findings for SFV, SeV-Gfp infected both HMDMs and A549 very efficiently, with 82 and 95% of the HMDMs and A549 cells, respectively, being positive for GFP (Figure (Figure3,3, lower panel). Taken together, these data show that lung carcinoma cells are efficiently infected by rSFV, whereas primary mouse and human macrophages are resistant to SFV infection, suggesting that rSFV may be used to deliver genes for cancer therapy without killing tumor-associated macrophages.
We wanted to test macrophage viability after challenge with rSFV particles. Both J774A.1 macrophages and LLC cancer cells were subjected to rSFV-DsRed particles at MOI=10 during 80-min infection protocol. Cell infection rate was determined 48h post-infection by quantifying DsRed-expressing cells using flow cytometry. Cells were also stained with annexin V-FITC and DAPI followed by flow cytometry analysis to determine cell viability.
As expected, we observed that 98% of non-infected macrophages stayed viable after 48h as determined using flow cytometry and retained round morphology, which is characteristic to J774A.1 cells in normal culture conditions (Figure (Figure4A).4A). Also 48h after challenge with rSFV-DsRed particles 90% of macrophages remained viable, whereas 6% of macrophages were single-positive for Annexin V (Figure (Figure4B).4B). Interestingly, light microscopy revealed that macrophages changed morphology 48h after challenge with rSFV by gaining spindle-like or polygonal shape (Figure (Figure4B).4B). LLC cells were used in parallel as a positive control for cell infection. As expected, the non-infected LLC cells showed 92% viability and were characterized by mixed population of adherent and floating cells with round or spindle-like morphology (Figure (Figure4C).4C). However, the infected LLC cells underwent cell death 48h after infection with rSFV, and only 35% of LLC cells were viable (Figure (Figure4D).4D). We observed that 33% of rSFV-challenged LLC cells were double-positive for Annexin V-FITC and DAPI suggesting apoptotic/necrotic cell death. A LLC population of 30% was single-positive for DAPI 48h after infection suggesting affected cell membrane permeability (Figure (Figure4D).4D). Light microscopy revealed that LLC cells possess apoptotic morphology characterized by round swollen cells with translucent cytoplasm after infection with rSFV (Figure (Figure4D).4D). We observed microscopically that both DsRed-positive (infected) and DsRed-negative (non-infected) cells undergo apoptosis after challenge with rSFV particles (Figure (Figure4D,4D, red and white arrows), whereas part of infected DsRed-expressing cells remain viable 48h post-infection (Figure (Figure4D,4D, yellow arrows). Flow cytometry analysis revealed that 69% of all DsRed-expressing cells undergo cell death characterized mostly by being double-positive for Annexin V-FITC and DAPI (Figure (Figure4E).4E). Our data show that macrophages are not only resistant to SFV infection but also remain viable after challenge with rSFV particles.
It has been shown that SFV infection induces cellular death via p53-independent apoptosis (21). To determine whether rSFV has a direct effect on cancer cell growth, we used in vitro assay to evaluate proliferation of infected LLC cells. The cells were cultivated until approximately 70–80% confluency, and they were then infected with SFV-Ifng or SFV-Tnfa viral particles at MOI=15. To determine cell growth, a radioactive thymidine, which incorporates into new DNA strands during cell division, was added to the cell cultures at 47h post-infection. The experimental setup is illustrated in Figure Figure55A.
BHK-21 cells were used in parallel as a positive control for efficient cell infection by SFV and showed nearly complete growth inhibition (Figure (Figure5B).5B). Growth inhibition was similar independent on whether SFV carried a gene encoding TNF-α or IFN-γ (Figure (Figure5B).5B). It was observed using light microscopy that BHK-21 cells lost confluency and gained apoptotic cell morphology characterized by translucent cytoplasm, granularity, or round shape 47h post-infection (Figure (Figure5C).5C). LLC cell growth was inhibited by half 47h after infection with SFV-Ifng and by 80% after infection with SFV-Tnfa (Figure (Figure5D).5D). Light microscopy revealed that LLC cells acquired apoptotic cell morphology characterized by round shape, granularity, and translucent cytoplasm 47h after infection with either SFV-Ifng or SFV-Tnfa viral particles (Figure (Figure5E).5E). The data show that rSFV particles encoding murine IFN-γ or TNF-α efficiently inhibited LLC cell growth at 47h post-infection.
In the next set of experiments, we sought to determine whether LLC cells secrete cytokines after infection with SFV-Tnfa and SFV-Ifng virus particles. In this experiment, BHK-21 cells were used as a positive control. The LLC and BHK-21 cells were cultivated until 50 and 100% confluency, respectively, before they were infected with SFV-Tnfa or SFV-Ifng at a MOI=1, MOI=10, or MOI=40 (calculated according to the titration in BHK-21 cells). After 24h, the levels of secreted vdIFN-γ and vdTNF-α in the cell cultivation medium were analyzed using Luminex bead-based assay. LLC cells infected with SFV-Tnfa secreted vdTNF-α (range, 103–104pg/mL for all tested MOIs) (Figure (Figure6A).6A). There was no clear correlation between the MOI of the virus particles and the level of vdTNF-α (Figure (Figure6A).6A). The vdTNF-α was not detected in the medium of non-infected cells or in the medium of cells infected with SFV-Ifng, confirming that the secreted vdTNF-α was derived from the Tnfa gene that was delivered using SFV (Figure (Figure66A).
In LLC cells, infection with SFV-Ifng resulted in the secretion of vdIFN-γ into the growth medium at a concentration ranging from 2.9 to 9.9×102 ng/mL at 24h after infection (Figure (Figure6B).6B). The concentration of vdIFN-γ appeared to correlate with the concentration of viral particles, and the highest tested MOI resulted in the highest level of vdIFN-γ (Figure (Figure6B).6B). The vdIFN-γ was not detected in media obtained from non-infected cells or from cells infected with SFV-Tnfa, indicating that the vdIFN-γ originated from the SFV-delivered cytokine gene (Figure (Figure6B).6B). In conclusion, these results show that both BHK-21 and LLC cells produce and secrete vdTNF-α and vdIFN-γ when infected with the rSFV vectors described in this study.
To determine whether the vdTNF-α is biologically active, we utilized a known property of TNF-α which is to induce necrotic cell death in the murine fibrosarcoma cell line L929 by binding to TNF receptor-1 (68). In these experiments, L929 cells were cultivated until 90% confluency; we then added rTNF-α or vdTNF-α at concentrations varying from 2.2 to 60ng/mL to the cells. The culture medium of BHK-21 cells infected with SFV-Tnfa particles was used as the source of vdTNF-α. At 24h after treatment, the morphology of the L929 cells was evaluated using bright-field microscopy. Then cells were stained with annexin V-FITC to determine phosphatidylserine exposure, whereas staining with PI was used to determine loss of membrane integrity in order to quantify the numbers of viable (Annexin V−PI−), apoptotic (Annexin V+PI−), and necrotic (Annexin V+PI+) cells using flow cytometry (Figures (Figures7A–J).7A–J). Untreated L929 cells were used as a control, and viable cells were defined as those that were annexin V-negative/PI-negative (Figure (Figure7A).7A). Treatment with staurosporine was used as the control for apoptotic cell death (65), where annexin V-positive/PI-negative cells were regarded as early apoptotic, whereas annexin V-positive/PI-positive cells were regarded as late apoptotic undergoing secondary necrosis (Figure (Figure77B).
In the absence of any treatment, the L929 cells reached 100% confluency after 24h and had a normal fibroblast-like, slightly polygonal cell morphology (Figure (Figure7A).7A). The untreated L929 cells were also analyzed using flow cytometry and used to set the gates for the viable (Annexin V−PI−) cell population, which accounted for 99% of all events (Figure (Figure7A).7A). After cells were treated with 1µM staurosporine, cell confluency was lost, and an apoptotic cell morphology characterized by cell shrinkage, a round shape and granularity was observed (Figure (Figure7B).7B). Only 11% of the staurosporine-treated cells were viable. The remaining cells were undergoing apoptosis and secondary necrosis (Figure (Figure7B).7B). In cells that were incubate with increasing concentrations of rTNF-α or vdTNF-α (2.2, 6.7, 20, or 60ng/mL), we observed a concentration-dependent increase in the proportion of apoptotic (Annexin V+PI−) and necrotic (Annexin V+PI+) cells (Figures (Figures7C–J)7C–J) in a similar manner between rTNF-α and vdTNF-α. Treatment with vdTNF-α and rTNF-α at the lowest concentration (2.2ng/mL) induced apoptosis in 9–13% and necrosis in 19–20% of the cells (Figures (Figures7C,D),7C,D), whereas the highest concentrations of rTNF-α and vdTNF-α (60ng/mL) induced apoptosis in 18–23% and necrosis in 46–62% of the cells (Figures (Figures7I,J).7I,J). Moreover, after treatment with rTNF-α or vdTNF-α, we observed necrotic cell morphology characterized by round, swollen cells with translucent cytoplasm. These data verify the functionality of the vdTNF-α protein because it was able to induce apoptosis and necrosis in L929 cells in a concentration-dependent manner that was similar to that observed for rTNF-α.
It has been previously shown that LLC cells are resistant to cell death induced by TNF-α (69). Based on previous studies, where IFN-γ was shown to enhance TNF-α receptor expression in cancer cells (51, 52), we wanted to test whether IFN-γ may sensitize LLC cancer cells to TNF-α treatment. Therefore, we tested induction of cell death in LLC cells after combined treatment of recombinant cytokines TNF-α and IFN-γ. LLC cells were single-treated with either TNF-α or IFN-γ for 48h. LLC cells were treated with TNF-α in combination with IFN-γ for 24h or 48h. LLC cells were also pretreated with IFN-γ for 24h followed by 24h treatment with TNF-α. L929 fibroblasts, which were treated with TNF-α, were used as a positive control. Untreated cells were used as a negative control. Cell morphology after treatments was evaluated using bright-field microscopy. Cells were stained with annexin V-FITC to determine phosphatidylserine exposure, whereas staining with PI was used to determine loss of membrane integrity in order to quantify the numbers of viable (Annexin V−PI−), apoptotic (Annexin V+PI−), and necrotic (Annexin V+PI+) cells using flow cytometry (Figures (Figures88A–H).
In the absence of any treatment for 48h, 99% of L929 control cells and 94% of LLC cancer cells remained viable and showed normal cell morphology (Figures (Figures8A,B).8A,B). The positive control of L929 cells, which were treated with TNF-α for 48h, lost their confluency and showed apoptotic morphology characterized by round swollen cells with translucent cytoplasm (Figure (Figure8C).8C). Only 26% of the TNF-α-treated L929 cells were viable (Figure (Figure8C).8C). By contrast, LLC cells were resistant to treatment with TNF-α for 48h, showed 86% viability and retained normal cell morphology (Figure (Figure8D).8D). Treatment with IFN-γ for 48h was not cytotoxic to LLC cells, and 90% of the treated LLC cells remained viable (Figure (Figure8E).8E). Interestingly, combined treatment of LLC cells with both cytokines for 24h also did not induce cytotoxicity in LLC cells (Figure (Figure8F).8F). However, a prolonged incubation of LLC cells with both cytokines for 48h induced cytotoxicity in LLC cells resulting in 38% cells being double-positive for Annexin and PI (Figure (Figure8G).8G). Also pretreatment of LLC cells with IFN-γ for 24h followed by treatment with TNF-α for 24h was cytotoxic to LLC cells and induced apoptosis in 10% and necrosis in 41% of the cells (Figure (Figure8H).8H). Cell morphology of LLC cells changed after the combined treatments of LLC with both cytokines simultaneously for 48h or with IFN-γ pretreatment followed by TNF-α (Figures (Figures8G,H).8G,H). After combined treatments with both cytokines, we observed cells with apoptotic cell morphology as well as live cells that had spread in an elongated shapes possibly due to access of free space resulting from cells dying in proximity (Figures (Figures8G,H).8G,H). All in all, combined treatment with IFN-γ and TNF-α was effective in inducing cell death in LLC cancer cells, which were resistant to single-treatments with these cytokines.
To verify that vdIFN-γ is a functional protein, we used an in vitro assay based on cancer cell growth inhibition mediated by activated macrophages. The macrophages were treated with mitomycin C to block their proliferation, and they were activated by applying either vdIFN-γ or rIFN-γ in combination with a second stimulus. Based on previous experiments performed in our lab, we chose to stimulate the BMDMs with IFN-γ and TLR2/1 agonist Pam3 because this combination leads to efficient inhibition of cancer cell growth (70). After the BMDMs were stimulated for 24h, LLC cells were added, and the co-cultures were cultivated for an additional 20h. Finally, to enable the detection of proliferating cancer cells, we added radiolabeled thymidine to the cultures at 24h before they were harvested (Figure (Figure99A).
In the first experiment, we treated cells with different concentrations of rIFN-γ in combination with 100ng/mL Pam3 to identify the lowest effective dose of IFN-γ that is necessary to activate BMDMs toward a cancer-suppressive phenotype (Figure (Figure9B).9B). The results revealed that adding rIFN-γ within the range 100–1.56ng/mL effectively inhibited cancer cell growth (cpm below 750 when the ratio of BMDMs:LLC cells was 20:1) in a concentration-dependent manner. Some growth inhibition was also observed at 0.098–0.39ng/mL rIFN-γ, but minor or no effect was observed at concentrations ≤0.024ng/mL (Figure (Figure99B).
All controls included in this assay produced the expected results (Figures (Figures9B,C).9B,C). Treating the BMDMs with mitomycin C resulted in counts lower than 650cpm, confirming that the treatment hindered proliferation (Figures (Figures9B,C;9B,C; first group of bars from the left). Unstimulated macrophages did not inhibit growth in LLC cells since more than 15,000cpm were measured in the wells (Figures (Figures9B,C;9B,C; second group of bars from the left). These results were comparable to the average cpm in LLC cells that were cultivated alone (Figures (Figures9B,C;9B,C; orange line). Treating cells with either Pam3, rIFN-γ, or vdIFN-γ alone resulted in growth rates similar to those observed in LLC cells cultivated alone (Figures (Figures99B,C).
To analyze the functionality of vdIFN-γ, we treated BMDMs with the same concentrations that were used to test rIFN-γ. The vdIFN-γ was produced by infecting BHK-21 cells with SFV-Ifng viral particles and harvesting the cell culture medium to use as a source of vdIFN-γ. The results were similar to what was observed for rIFN-γ in that incubating macrophages with vdIFN-γ in combination with Pam3 resulted in efficient cancer cell growth inhibition in a concentration-dependent manner. The lowest effective concentration of vdIFN-γ was 6.25ng/mL, which produced less than 1,050cpm (Figure (Figure9C).9C). In all the experiments, the most efficient inhibition of cancer cell growth was observed when the ratio of BMDMs to LLC cells was 20:1 or 10:1 (Figures (Figures9B,C).9B,C). Finally, the pattern of effective IFN-γ doses and the extent of growth inhibition they produced was similar between rIFN-γ and vdIFN-γ (Figures (Figures9B,C).9B,C). Based on these data, we conclude that vdIFN-γ has biological activity and can substitute for rIFN-γ.
Using TLR ligands in combination with IFN-γ provides a classical set of stimuli that activates macrophages toward an M1-phenotype, which can produce NO through inducible NO synthase (70). We, therefore, determined NO production as a readout to verify that vdIFN-γ triggers macrophage activation potentially toward an M1-phenotype. We measured , which is the end product of the rapid oxidation of NO, in cell culture media using the Griess test. First, we verified that the BMDMs produced NO in a concentration-dependant manner at 24h after stimulation with both rIFN-γ and Pam3 (Figure (Figure10A).10A). We then stimulated BMDMs with both vdIFN-γ and Pam3, and the results were similar to those observed for rIFN-γ in that the levels of varied according to the concentration of vdIFN-γ (Figure (Figure10B).10B). The highest levels of were observed when rIFN-γ and vdIFN-γ were used in a range from 0.39 to 100ng/mL. At IFN-γ concentrations ≤0.098ng/mL, the levels of were lower (Figures (Figures10A,B).10A,B). Stimulation with rIFN-γ alone resulted in the production of only small amounts of in the cell culture medium (Figure (Figure10A).10A). The levels of were also low in cultures stimulated with vdIFN-γ alone (Figure (Figure10B)10B) or Pam3 alone (Figures (Figures10A,B).10A,B). Thus, IFN-γ and Pam3 had a synergistic effect on the ability of macrophages to produce NO. The higher levels of that were observed following stimulation with higher doses of IFN-γ (Figures (Figures10A,B)10A,B) were well-correlated with the enhanced cancer cell growth inhibition that was observed in the growth inhibition experiments (Figures (Figures9B,C).9B,C). Taken together, data from the growth inhibition assay demonstrated that vdIFN-γ is a potent agent at very low concentrations that when combined with Pam3 induces an antitumor phenotype in macrophages that suppresses growth in LLC cells.
In this study, we developed two new rSFV vectors encoding either murine TNF-α or IFN-γ and showed by in vitro studies that the two rSFV-encoded cytokines are functional. The rSFV efficiently infected mouse and human lung carcinoma cells in vitro, whereas murine and human macrophages were resistant to SFV infection. The rSFV inhibited LLC cell growth, induced cancer cell death and simultaneously exploited cancer cells for production of SFV-encoded TNF-α and IFN-γ at levels that are functional in vitro. The functionality of SFV-encoded TNF-α was shown via cell death induction in L929 cells. The rSFV-encoded IFN-γ activated macrophages toward a tumoricidal phenotype in vitro.
Recombinant SFV has been used to express various cytokine genes in experimental tumor models resulting in therapeutic effects (2–15). For example, the same replication-deficient SFV/enh vector used in this study was previously applied for IL-12 expression in mouse breast and colon cancer models, resulting in inhibition of tumor growth upon intratumoral vector inoculation (7). Because of the antitumor potential of TNF-α (40–46) and IFN-γ (28–39) or both in combination (47–50, 53), we subcloned these cytokines in a safe replication-deficient SFV vector, which provides high and transient expression of the transgene without further virus replication (20). In order to form viral particles, we used SFV-Helper1 system (20), which encodes SFV structural proteins. We produced infectious SFV-Tnfa and SFV-Ifng recombinant virus particles in BHK-21 cells at titers 107–108 IFU/mL.
Various mouse and human cancer cell lines are susceptible to SFV infection although the transduction rates may differ between cell types (71–73). The hamster kidney fibroblast cell line BHK-21, which is commonly used for production of SFV particles, is efficiently infected by SFV (71). In the current study, the high susceptibility of BHK-21 cells to SFV infection was confirmed. Two cell lines of particular interest for development of lung cancer immunotherapy are mouse and human lung carcinoma cell lines, LLC and A549, respectively, which proved to be susceptible to SFV infection with a comparable transduction level of 41% 24h post-infection for both cell lines when SFV was used at MOI=15. This is in agreement with a previous study showing that A549 cells are susceptible to SFV infection (72). Our results encouraged us using LLC cells as target murine cancer cells further because they were successfully infected by rSFV particles and were able to express rSFV-encoded proteins.
In contrast to the tested cancer cell lines, macrophages were found to be resistant to SFV infection. Similar data were obtained with primary mouse and human macrophages, as well as with the mouse macrophage cell line J774A.1. Moreover, macrophages retained their viability after challenge with rSFV particles. The fact that macrophages are not killed by SFV but instead serve as effector cells responding to SFV-encoded factors may be an advantage for immunotherapy based on the activation of tumor-associated macrophages. Cancer cells, due to their susceptibility to SFV infection, may be exploited to produce such SFV-encoded factors. The mechanism by which macrophages remained resistant to SFV infection is unclear. The life cycle of replication-deficient rSFV particles is a several-step process comprising viral entry via endocytosis, a pH-dependent release of virus nucleocapsid from the endosome, capsid disassembly, viral RNA replication in the cytoplasm, and subsequent translation of the transgene (74). The suppression in either of the abovementioned steps may have resulted in lack of SFV-encoded transgene expression in macrophages as we observed. Furthermore, fresh isolated peritoneal mouse macrophages were also resistant to infection with the replication-deficient SFV-DsRed virus as was confirmed by absence of fluorescent signal in the infected cells (data not shown). In contrast to our results, a study from 1976 described that a replication-competent SFV was able to infect and multiply at very low yields within peritoneal mouse macrophage cultures in vitro (75). The authors tested the presence of SFV within cell growth medium of peritoneal macrophages post-infection by titrating plaque forming units in chick embryo cell cultures. Similarly, another study from 1988 reported low susceptibility of mouse spleen-derived Mac-1-positive cells to infection with replication-competent or first-generation avirulent SFV (76). The differences between the protocols and SFVs used in our study and studies by van der Groen et al. or Wu et al. make it difficult to compare the results. However, a possible explanation for the macrophage low susceptibility toward SFV in the studies mentioned (75, 76) could be that the ex vivo isolated peritoneal or spleen cells, which the authors used as a source of macrophages, also contained other cell types that served as host cells for SFV multiplication. The main difference though is that the authors used replication-competent SFVs, including a wt SFV, which was isolated from mosquitos and was produced by replication in chick embryo cell cultures, or first-generation avirulent SFV. Our data based on use of pure macrophage cultures clearly show that mouse and human macrophages are resistant to infection with SFV particles that are based on the replication-deficient rSFV1 vector and that have been produced in BHK-21 cells.
Infection with SFV inhibited proliferation of BHK-21 and LLC cells in vitro independent on whether SFV-encoded TNF-α or IFN-γ. The inhibition of cancer cell growth is likely caused by the ability of SFV particles to induce p53-independent apoptosis in infected cells, which is linked to viral RNA replication and appearance of double-stranded RNA intermediates in cell cytoplasm (21). This property is of particular interest for lung cancer therapy since a mutated p53 is one of the key molecular markers in many solid cancers, including human lung cancers (77). In fact, the target LLC cancer cells used in this study were shown to undergo cell death after infection with replication-deficient rSFV particles. The infected cancer cells were shown to express rSFV-encoding transgene while undergoing cell death. Thus, rSFV has therapeutic potential not only as a transgene delivery vehicle but may also elicit a direct oncolytic effect on cancer cells. Moreover, intratumoral injection of rSFV particles has been shown to inhibit tumor growth in preclinical mice models by induction of apoptosis (78).
Early after infection with rSFV particles the host cells shut down the translation of endogenous cellular proteins (79), whereas the heterologous protein encoded by rSFV is produced at high levels (80). In the present study, we embraced this property in order to produce tumor-suppressive cytokines within cancer cells. We showed that LLC cells can produce and release rSFV-encoded TNF-α and IFN-γ in the cell culture medium at levels that are functional in vitro. Whereas vdIFN-γ was present at 100ng levels in the supernatant, the amount of vdTNF-α was in several nanograms. The relatively low levels of vdTNF-α that we detected might be explained by the lack of translational enhancer in a vector, as well as by the fact that TNF-α is primarily produced as a transmembrane protein (81), and cleavage of the transmembrane form is needed before soluble TNF-α can be released into the cell culture medium (82).
Nevertheless, the levels of vdTNF-α detected were sufficient to elicit a functional response in vitro as shown by induction of cell death in mouse fibroblast cell line L929. TNF-α is known to induce either caspase-dependent apoptotic cell death or caspase-independent programmed necrotic cell death (necroptosis) downstream of TNFR1 signalling depending on microenvironment and cell type (83, 84). We induced mainly necrotic cell death in L929 cells in a dose-dependent manner after treatment with either vdTNF-α or rTNF-α, which is in agreement with previous reports showing that L929 cells undergo caspase-independent necroptosis in response to TNF-α treatment (68, 85). In accordance with a previous study (65) we also observed an annexin V-positive/PI-negative cell population after treatment with vdTNF-α, which may represent not only apoptotic but also primary necrotic cells according to studies showing phosphatidylserine exposure during early necrosis (oncosis) before the integrity of the membrane is lost (86, 87). By inducing fibroblast cell death in vitro, we verified that SFV-encoded TNF-α is biologically active. However, in vivo effects of TNF-α differ and comprise increased vessel permeability used to improve drug penetration (43–45) and destruction of tumor vasculature (41, 42) leading to hemorrhagic tumor necrosis (40, 88). By using recombinant cytokines, we also showed that TNF-α is a cytokine that may induce cytotoxicity in mouse lung carcinoma cells but only when combined with IFN-γ. Such observations can be explained by a previously reported IFN-γ property to enhance TNF-α receptor expression (51, 52), thus sensitizing cancer cells to TNF-α-induced cell death. Furthermore, in the context of cancer immunotherapy TNF-α may serve as an adjuvant in order to enhance T-cell infiltration (46, 89).
In this study, we showed that rSFV-encoded IFN-γ was functional in activating macrophages in vitro toward a tumoricidal phenotype, which is consistent with previous studies showing that IFN-γ renders macrophages tumoricidal in vitro (34–36). We observed that in order to activate macrophages, presence of both vdIFN-γ and the TLR2/1 agonist Pam3 was required. Also previous studies showed that two signals, IFN-γ in combination with a second signal are required to render macrophages tumoricidal (39) and able to induce NO production (90). It is known that classically activated or M1 macrophages increase the expression of inducible NO synthase and, thus, produce NO (91). We showed that vdIFN-γ synergized with TLR2/1 agonist Pam3 to induce NO production in macrophages in a concentration-dependent manner, similarly as observed by combining rIFN-γ with another TLR agonist, CpG-containing DNA, respectively, in a previous study (90). Our observation that high level of NO, which was produced by activated macrophages, correlated with increased cancer cell growth inhibition is in agreement with the early studies reporting that tumoricidial abilities of macrophages in vitro are based on NO being cytotoxic to cancer cells (92, 93).
Macrophages are common immune cells in many tumors and often are considered to inhere a pro-tumoral phenotype associated with angiogenesis, metastasis, and suppression of T cell activation (94). By contrast, M1 macrophages suppress tumor growth and angiogenesis (95) and might be positively associated with patient survival (95–97). Several in vivo studies have shown the therapeutic benefit of redirecting tumor-associated macrophages to M1 phenotype by agents such as TLR9 ligand CpG in combination with antibody to IL-10R (88), TLR7/8 agonist 3M-052 (98), or liposomal nanoparticle-encapsulated hydrazinocurcumin (99). Previous studies suggest IFN-γ as a good candidate for tumor-associated macrophage re-education due to the ability of IFN-γ to re-polarize tumor-associated macrophages toward an M1 phenotype in vitro (100) and its ability to render macrophages tumor-suppressive in mouse tumor models in vivo (31, 37–39). The results from this study suggest that SFV-delivered vdIFN-γ is as efficient as rIFN-γ in rendering macrophages tumoricidal in vitro, which along with our finding that macrophages but not cancer cells are resistant to SFV infection encourages a possible application of SFV-Ifng vector for activation of tumor-associated macrophages toward tumor-suppressive M1 phenotype in further studies in vivo. Moreover, either IFN-γ or TNF-α delivery by rSFV vector may comprise not only a direct effect of the rSFV-delivered cytokines but may also benefit from the inherent ability of SFV vector to induce p53-independent apoptosis (21) and elicit endogenous type-I IFN responses, which may be required for the therapeutic effect of a vector-encoded cytokine (3).
In summary, the present study shows that rSFV can efficiently infect lung carcinoma cells in vitro and exploit them for production of functional rSFV-encoded TNF-α and IFN-γ. The rSFV-encoded IFN-γ was able to activate macrophages toward an antitumor phenotype in vitro. Our results set the basis for application of SFV-Tnfa and SFV-Ifng vectors to modulate the cytokine milieu in the tumor microenvironment in further studies using mouse models for lung cancer.
This study was carried out in accordance with the recommendations of The Norwegian Regulation on Animal Experimentation, Norwegian Food and Safety Authority.
AZ and AC conceived the study. All authors contributed to the design of experiments, data analysis, and interpretation of data. BK, EM, PC, IJ, BS, and IØ performed experiments. BK wrote the manuscript; and IØ, AC, and AZ contributed in writing the manuscript. All authors critically revised the manuscript and approved the final version. AC and AZ contributed equally to this work.
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest. The reviewer CS and handling Editor declared their shared affiliation.
We would like to thank Kahsai Beraki for technical help.
Funding. This study was supported by EEA and Norway Grants (project contract NFI/R/2014/051), South-Eastern Norway Regional Health Authority, The Research Council of Norway, Latvian National Research Programme Biomedicine for Public Health (Biomedicine) 2014–2017, and ERA Net Rus Plus Alphachit project.
3H-TdR, [methyl-3H]-thymidine; BHK-21, baby hamster kidney fibroblasts; BMDM, bone marrow-derived macrophage; CM, conditioned medium; cpm, counts per minute; DsRed, Discosoma sp. red fluorescent protein; FBS, fetal bovine serum; FITC, fluorescein isothiocyanate; GFP, green fluorescent protein; HMDM, human monocyte-derived macrophage; IFU, infectious units; LLC, Lewis lung carcinoma; MOI, multiplicity of infection; NO, nitric oxide; NO2-, nitrite; Pam3, Pam3CSK4; PBS−/−, phosphate-buffered saline without magnesium and calcium; PBS+/+, phosphate-buffered saline with magnesium and calcium; PI, propidium iodide; rIFN-γ, recombinant interferon-γ; rSFV, recombinant Semliki Forest virus; rTNF-α, recombinant tumor necrosis factor-α; SeV, Sendai virus; SFV, Semliki Forest virus; TLR, toll-like receptor; vdIFN-γ, vector-derived interferon-γ; vdTNF-α, vector-derived tumor necrosis factor-α.