Abstract
Neurofibromatosis type 1 (NF1) is caused by germline mutations in the NF1 gene and is characterized by café au lait spots and benign tumours known as neurofibromas. NF1 encodes the tumour suppressor protein neurofibromin, which negatively regulates the small GTPase Ras, with the constitutive activation of Ras signalling resulting from NF1 mutations being thought to underlie neurofibroma development. We previously showed that knockdown of neurofibromin triggers epithelial-mesenchymal transition (EMT) signalling and that such signalling is activated in NF1-associated neurofibromas. With the use of a cell-based drug screening assay, we have now identified the antiallergy drug tranilast (N-(3,4-dimethoxycinnamoyl) anthranilic acid) as an inhibitor of EMT and found that it attenuated the expression of mesenchymal markers and angiogenesis-related genes in NF1-mutated sNF96.2 cells and in neurofibroma cells from NF1 patients. Tranilast also suppressed the proliferation of neurofibromin-deficient cells in vitro more effectively than it did that of intact cells. In addition, tranilast inhibited sNF96.2 cell migration and proliferation in vivo. Knockdown of type III collagen (COL3A1) also suppressed the proliferation of neurofibroma cells, whereas expression of COL3A1 and SOX2 was increased in tranilast-resistant cells, suggesting that COL3A1 and the transcription factor SOX2 might contribute to the development of tranilast resistance.
Similar content being viewed by others
Introduction
The NF1 tumour suppressor gene is located at human chromosomal region 17q11.2 and encodes a 2818–amino acid protein termed neurofibromin1. Neurofibromin, which is localized to the cytoplasm of numerous cell types, contains a mammalian Ras GTPase-activating protein (RasGAP) domain that negatively regulates the Ras signalling pathway by promoting the conversion of GTP-bound (active) Ras to the GDP-bound (inactive) state. Loss or mutation of neurofibromin thus results in hyperactivation of Ras and engagement of its downstream effectors2,3.
Mutations of the NF1 gene give rise to neurofibromatosis type 1 (NF1), also known as von Recklinghausen disease4. NF1 is an autosomal dominant inherited disease that affects one in ~3000 live births, with 30% to 50% of NF1 mutations arising de novo. Individuals with NF1 manifest a variety of clinical symptoms including peripheral and central nervous system tumours, pigmentary changes such as multiple café au lait spots, bone defects, cardiovascular abnormalities, and learning disabilities. The most common symptom of NF1 is the development of benign peripheral nerve sheath tumours known as neurofibromas. In addition, patients with NF1 are at an increased risk for the development of leukaemia, rhabdomyosarcoma, pheochromocytoma, gastrointestinal stromal tumours, early-onset breast cancer, and high-grade malignant glioblastoma5,6. Various clinical trials of molecularly targeted drugs are under way for NF1, with the results of phase II trials of several agents including imatinib, tipifarnib, pirfenidone, and sirolimus for the treatment of plexiform neurofibromas of NF1 patients having been presented7,8,9,10,11. At the present time, however, there are no effective therapeutic agents for benign neurofibromas.
The epithelial-mesenchymal transition (EMT) is defined by the loss of epithelial characteristics and the acquisition of mesenchymal phenotypes and is mediated by activation of EMT transcription factors (EMT-TFs) such as Snail, Slug, Twist, ZEB1, and ZEB2 (ref.12). A key molecular feature of EMT is down-regulation of E-cadherin, a cell adhesion molecule present in the plasma membrane of most normal epithelial cells. However, recent studies have shown that EMT signalling is also activated in nonepithelial tumours, including gliomas, hematopoietic malignancies, and sarcomas, and that it plays an important role in disease progression and prognosis13. We have previously shown that EMT-TFs are activated in neurofibromin-depleted cells and in NF1-associated neurofibroma specimens14. EMT is also associated with increased production of extracellular matrix (ECM) components by cells as well as with an enhanced migratory capacity and resistance to apoptosis, suggesting that EMT signals might serve as therapeutic targets for the treatment of NF1-associated neurofibromas.
To identify inhibitors of EMT, we performed a drug screening assay based on focus formation. We thereby identified tranilast (N-(3,4-dimethoxycinnamoyl) anthranilic acid) as an inhibitor of EMT. Tranilast is an antiallergy drug that is also administered for the treatment of keloids and hypertrophic scars. In the present study, we examined the effects of tranilast on neurofibromin-deficient cell lines as well as on neurofibroma cells derived from NF1 patients.
Results
Tranilast inhibits TNF-α– and TGF-β2–induced aggregation of ARPE-19 cells
We developed a cell-based screening assay to identify inhibitors of EMT. We previously showed that the combination of tumour necrosis factor–α (TNF-α) and transforming growth factor–β2 (TGF-β2) activates EMT signalling and induces cell aggregation in the human retinal pigment epithelial cell line ARPE-19 (ref.15). This cell aggregation, or focus formation, involves production of ECM components including collagen and hyaluronic acid (HA) and is a characteristic feature of EMT activation16,17,18,19,20. We thus examined focus formation by ARPE-19 cells as an indicator of EMT. Focus formation induced by TNF-α and TGF-β2 was inhibited by exposure of the cells to the TGF receptor inhibitor SB431542, which was tested as a positive control (Fig. 1a). Compounds that inhibited focus formation by ≥20% with minimal cytotoxicity at a concentration of 20 μM were considered positive. Screening of >1500 compounds approved by the U.S. Food and Drug Administration identified eight drugs that were able to inhibit TNF-α/TGF-β2–induced focus formation. One of these putative EMT inhibitors was tranilast, an antiallergy drug that is also used for the treatment of inflammatory conditions and keloids21,22. Tranilast thus inhibited focus formation at a concentration of 20 µM (Fig. 1a), with the median inhibitory concentration being 35.86 ± 17.78 µM (Fig. 1b). We also examined the effect of tranilast on HA production, which is induced by EMT signals23,24,25,26. Fluorescence microscopic analysis of cells stained with biotinylated HA binding protein (HABP) revealed that tranilast inhibited the production of HA induced by TNF-α/TGF-β2 (Fig. 1c). These data thus suggested that tranilast inhibits EMT induced by TNF-α and TGF-β2 in ARPE-19 cells.
Tranilast suppresses EMT characteristics in neurofibromin-deficient cells
Depletion of neurofibromin in HeLa human epithelial carcinoma cells by transfection with a specific small interfering RNA (siRNA) induced a change in cell morphology from cuboidal to spindle-shaped, with reverse transcription (RT) and real-time polymerase chain reaction (PCR) analysis also revealing that depletion of neurofibromin increased the expression of mesenchymal marker genes including those encoding fibronectin (FN1) and N-cadherin (CDH2) as well as that of those for the EMT-TFs Slug (SNAI2) and Twist (TWIST1) (Supplementary Fig. S1). These results confirmed our previous observations that deficiency of neurofibromin is associated with EMT signalling14.
We next examined the effects of tranilast on the NF1-mutated human Schwann-like cell line sNF96.2. Immunoblot analysis revealed that expression of mesenchymal markers—including fibronectin, collagen type I, and N-cadherin—was decreased by treatment of these cells with tranilast (Fig. 2a). Quantitative RT-PCR analysis also showed that expression of the genes for various EMT-TFs, collagens, hyaluronan synthases, and integrins in these cells was inhibited by tranilast (Supplementary Fig. S2). Furthermore, tranilast attenuated in particular the expression of collagen type III in sNF96.2 cells as revealed by both immunofluorescence analysis (Fig. 2b) and an enzyme-linked immunosorbent assay (ELISA) (Fig. 2c). These results suggested that tranilast suppresses the mesenchymal phenotypes of sNF96.2 cells including the expression of various ECM components.
We subjected tumours formed by sNF96.2 cells in the brain of NOD/SCID recipient mice to histological analysis by Masson’s trichrome staining for collagen fibres including collagen type I, Gitter staining for reticular fibres including collagen type III, Elastica van Gieson staining for elastic fibres, and Alcian blue staining for acid mucosubstances and acidic mucins (Fig. 2d). Small collagen fibres rendered dark blue by Masson’s trichrome stain were detected between the tumour cells, and abundant thick reticular fibres rendered black by Gitter staining were also apparent surrounding the tumour cells. Elastic fibres (black staining) were not detected by Elastica van Gieson staining, whereas Alcian blue–positive material was observed in regions of low cell density.
We previously showed that EMT-TFs including ZEB1 are activated in neurofibromin-depleted cells and in NF1-associated neurofibroma specimens14. We further examined whether the mesenchymal marker vimentin and EMT-related collagens are also expressed in NF1-associated neurofibroma specimens. Immunohistochemical analysis of formalin-fixed tissue samples from two patients revealed the expression of ZEB1, vimentin, collagen type I, collagen type III, and SOX2 (Supplementary Fig. S3). These results thus supported the notion that EMT signals might be therapeutic targets for the treatment of NF1-associated neurofibromas.
Tranilast suppresses the proliferation of NF1-mutated cells in vitro
We examined the effect of tranilast on the proliferation of sNF96.2 cells in vitro. Exposure of the cells to tranilast for 48 h resulted in a concentration-dependent reduction in the number of viable cells compared with that for control cultures incubated in the absence of the drug (Fig. 3). Given that tranilast did not appear to induce cell death, these data indicated that tranilast inhibits the proliferation of sNF96.2 cells. The median inhibitory concentration of tranilast for this effect was >200 µM, a concentration that appears to be achievable clinically given that the administration of tranilast at 200 mg three times a day for 7 days in humans was previously estimated to result in a maximum plasma concentration of 73.0 μg/ml, which corresponds to 223 μM27.
To clarify the relation between neurofibromin deficiency and tranilast sensitivity, we examined the effects of the drug on HeLa cells transfected with control or neurofibromin siRNAs. Tranilast inhibited the proliferation of HeLa cells depleted of neurofibromin to a much greater extent than it did that of the control cells (Fig. 4a,b). We also found that tranilast suppressed the growth of NIH3T3 mouse embryonic fibroblasts expressing either of two short hairpin RNAs (shRNAs) specific for NF1 mRNA to a greater extent than it did that of those expressing a control shRNA (Fig. 4c). These data suggested that loss of NF1 expression is directly related to tranilast sensitivity.
Tranilast attenuates the expression of angiogenesis-related genes
Like normal organs, tumours require a blood supply to satisfy their demands for oxygen and nutrients as well as to accomplish other metabolic functions. Angiogenesis, the process by which new blood vessels develop from a pre-existing vascular network, is regulated by cancer cells and by components of the tumour microenvironment including tumour-associated stromal cells, cytokines, growth factors, ECM, and secreted microvesicles28. We found that tranilast down-regulated the abundance of mRNAs for TGF-β, interleukin (IL)–8, vascular endothelial growth factor (VEGF), and matrix metalloproteinase 2 (MMP2) in sNF96.2 cells (Fig. 5). All of these factors are thought to promote angiogenesis and have been found to be associated with tumour angiogenesis29,30,31,32. These results thus suggested the possibility that tranilast might suppress tumour progression in NF1 patients.
The expression of TGF-β, IL-8, VEGF, and MMP2 genes was increased in sNF96.2 cells compared with normal human Schwann cells (HSCs) (Supplementary Fig. S4). However, transient depletion of neurofibromin by siRNA transfection did not significantly increase the expression of these genes in HSCs (Supplementary Fig. S4). These results suggested that chronic deficiency of neurofibromin may be indirectly related to angiogenesis.
Tranilast suppresses invasion and proliferation in NF1-mutated tumour cells
Our results suggested that tranilast inhibits EMT-like changes and angiogenesis-related gene expression and shows potential antitumour activity for NF1-mutated tumour cells. To test this scenario further, we again transplanted sNF96.2 cells into the brain of NOD/SCID mice and allowed the cells to form tumours. After 3 weeks, the mice were treated orally once a day for 8 weeks with tranilast (300 mg/kg) or vehicle. Immunohistochemical analysis revealed that tranilast treatment markedly inhibited migration of the vimentin-positive tumour cells into the host brain tissue (Fig. 6a), suggesting that tranilast suppresses sNF96.2 cell invasion in vivo. Although the sNF96.2 cell line was derived from a recurrent mass in an NF1 patient that was diagnosed as a malignant peripheral nerve sheath tumour, these cells generally show low tumourigenic activity in mice. We found that injection of sNF96.2 cells in subcutaneous tissue or in the sciatic nerve of immunodeficient mice did not result in tumour formation. Given that the cells reliably developed tumours when injected into the brain, we adopted this approach for our in vivo model.
To investigate the effects of tranilast in more detail, we established sNF96.2 cells that stably express green fluorescent protein (GFP) and then injected these sNF96.2-GFP cells into the brain of NOD/SCID mice. After 6 weeks, the brain was removed and thin slices of brain tissue were cultured in medium with or without tranilast for up to 5 days. Confocal fluorescence images revealed that tranilast inhibited sNF96.2-GFP cell growth and significantly suppressed cell migration into the brain tissue (Fig. 6b).
Effects of tranilast on NF1-mutated cells derived from clinical specimens
With the use of a previously described method33, we established neurofibroma cells and dedifferentiated fat (DFAT) cells from neurofibromas of NF1 patients. These cells expressed SOX10, S100, and CD90 (Supplementary Fig. S5), all of which are expressed in Schwann cells. We identified NF1 mutations in the patients by next-generation sequencing34. Peripheral blood specimens from patients 1 and 2 were positive for c.1466A>G, p.Tyr489Cys and c.3213_3214delAA, p.Ser1072Hisfs*16 mutations of NF1, respectively. The tumour specimen of patient 1 was also positive for c.6772C>T, p.Arg2258X of NF1. Culture of the patient-derived neurofibroma cells and DFAT cells in the presence of various concentrations of tranilast revealed that the drug suppressed the growth of the cells in a concentration-dependent manner (Fig. 7a,b). Immunoblot analysis revealed that tranilast also inhibited the expression of fibronectin in these cells (Fig. 7c), whereas quantitative RT-PCR analysis showed that it significantly attenuated the expression of genes for TGF-β1, VEGF, and MMP2 (Fig. 7d).
Knockdown of COL3A1 suppresses the proliferation of NF1-mutated cells
Both ECM and EMT-TFs are thought to be important in neurofibromas. Neurofibromas comprise various cell types including Schwann cells, fibroblasts, mast cells, and endothelial cells, all of which are embedded in abundant ECM. MMPs regulate the proliferation and infiltration of Schwann cells as well as contribute to the development of peripheral nerve sheath tumours35,36,37,38. In addition, the EMT-TF Twist has been found to be overexpressed in malignant peripheral nerve sheath tumours, and down-regulation of Twist expression inhibits cell chemotaxis39,40. We examined whether collagen type III might affect the proliferation of sNF96.2 cells by depleting the cells of COL3A1 mRNA by RNA interference. Transfection of the cells with a COL3A1 siRNA inhibited cell growth (Fig. 8a). Such depletion of COL3A1 also suppressed the growth of neurofibroma cells and DFAT cells derived from NF1 patients (Fig. 8b). These results thus suggested that collagen type III plays a role in maintenance of neurofibromin-deficient cells.
We established the tranilast-resistant neurofibroma cells derived from patient 1 that had been exposed to 250 µM tranilast for 20 days, and we found that the abundance of COL3A1 and SOX2 mRNAs was increased in the tranilast-resistant neurofibroma cells (Fig. 8c). Given that SOX2 is a key transcription factor in normal stem cells including pluripotent and tissue-specific stem cells41 and that it has been shown to be expressed in brain tumours and other cancers42, it is possible that the up-regulation of COL3A1 and SOX2 expressions may contribute to the development of resistance to tranilast treatment. We further examined the effect of COL3A1 depletion by siRNA transfection on the number and viability of tranilast-resistant neurofibroma cells from patient 1. The knockdown of COL3A1 markedly suppressed the proliferation of tranilast-resistant neurofibroma cells (Fig. 8d), suggesting that COL3A1 is a major ECM component affecting the proliferation of neurofibromin-deficient cells, however, the depletion of COL3A1 did not increase tranilast sensitivity.
Discussion
With the use of a cell-based drug screening assay, we have now identified tranilast as an inhibitor of the EMT. We further found that tranilast inhibited the expression of genes related to EMT signalling and angiogenesis in neurofibromin-deficient cells as well as suppressed the proliferation of such cells both in vitro and in vivo. Moreover, the growth-inhibitory effect of tranilast was more pronounced in neurofibromin-deficient cells than in intact cells. Our data thus suggest that tranilast may inhibit the growth of NF1-associated neurofibromas via suppression of EMT signalling and angiogenesis.
The EMT, in which epithelial cells acquire mesenchymal phenotypes, has been found to occur in various types of cancer, with activation of EMT signalling having been shown to promote cancer progression and metastasis43. EMT is associated with increased migratory capacity, invasiveness, resistance to apoptosis, and production of ECM components in cells44, and recent studies have indicated that activation of EMT signals also promotes malignancy of nonepithelial tumours13. Given that EMT signalling contributes to malignant traits of diverse tumour types, it is a potential therapeutic target. We performed a drug screening assay and thereby identified tranilast as an inhibitor of EMT in the human retinal pigment epithelial cell line ARPE-19. Depletion of neurofibromin by RNA interference in HeLa cells induced EMT signalling, and we found that such signalling was activated in NF1-mutated sNF96.2 cells. These results thus suggested that tranilast might suppress the formation or growth of NF1-associated neurofibromas.
Tranilast is an antiallergy drug that is also administered for the treatment of inflammatory diseases, keloids, and hypertrophic scars. It inhibits the release of chemical mediators from mast cells as well as the proliferation of and TGF-β1 and collagen production by fibroblasts21,45. In addition, tranilast has been shown to attenuate tumour growth, angiogenesis, migration, invasion, and metastasis through down-regulation of the TGF-β signalling pathway in breast, pancreatic, gastric, and prostate cancer as well as glioma cell lines46. TGF-β1 is a key trigger of the EMT program in both normal epithelial cells and cancer cells. In the present study, we determined the effects of tranilast on neurofibromin-deficient cells.
We found that tranilast suppressed the expression of mesenchymal markers in NF1-mutated sNF96.2 cells as well as in neurofibroma cells from NF1 patients. The abundance of mRNAs for various EMT-TFs, collagens, hyaluronan synthases, and integrins was also down-regulated by tranilast in sNF96.2 cells, suggesting that tranilast suppresses the mesenchymal characteristics of these cells. We also determined that tranilast suppressed the proliferation of both sNF96.2 cells and NF1 patient–derived cells, and that such growth suppression was more effective in HeLa and NIH3T3 cells depleted of neurofibromin than in intact cells. These results indicate that tranilast suppresses EMT signalling that is induced by neurofibromin deficiency and which gives rise to neurofibroma growth.
We detected the expression of collagen type III, an EMT-related ECM component, in neurofibroma specimens from NF1 patients. The expression of collagen type III in sNF96.2 cells was down-regulated at both the mRNA and protein levels by treatment with tranilast. Furthermore, we found that targeting of the collagen type III gene COL3A1 by RNA interference induced growth suppression both in sNF96.2 cells and in NF1 patient–derived cells. The expression of COL3A1 has previously been implicated in promotion of cell proliferation, metastasis, and invasion47,48,49. Tranilast may suppress the proliferation of neurofibromin-deficient cells by down-regulating mesenchymal phenotypes such as the production of ECM components. TGF-β1 induces transcriptional activation of COL3A1 in renal fibroblast cell lines50. In addition, tranilast was recently shown to suppress transcription of COL3A1 and CDK2 through regulation of the microRNA miR-29c in leiomyoma smooth muscle cells51. Tranilast might therefore have therapeutic potential for various benign tumours.
The expression of VEGF-A was found to be increased in cells undergoing TGF-β–induced EMT, and the extent of vascularization in tumours formed by MTΔECad mesenchymal cells correlated with the level of VEGF-A expression52, suggestive of a relation between EMT and tumour angiogenesis. We found that tranilast inhibited expression of the angiogenesis-related genes for TGF-β, IL-8, VEGF-A, and MMP2 in sNF96.2 cells. All of these angiogenic factors have been associated with tumour angiogenesis29,30,31,32. Tranilast may therefore inhibit the formation of tumour blood vessels by suppressing the expression of angiogenesis-related genes, with such activity possibly contributing to its antitumour effects. Angiogenesis has been shown to accompany the progression of NF1-associated neurofibromas53. We found that expression of the genes for TGF-β, IL-8, VEGF, and MMP2 was increased in NF1-mutated sNF96.2 cells compared with normal HSCs. However, transient depletion of neurofibromin by siRNA transfection did not increase the expression of these genes in HSCs, suggesting that chronic deficiency of neurofibromin is indirectly associated with angiogenesis. Angiogenesis is a potential therapeutic target for cancer. Many angiogenesis inhibitors, including bevacizumab, aflibercept, and ramucirumab, are thus administered as anticancer agents, and the development of new antiangiogenesis drugs is being actively pursued54,55,56,57,58,59,60. Such agents may prove effective for inhibition of neurofibroma growth. Our data also suggest that tranilast may inhibit vascularization, although further studies are required to confirm this possibility.
Finally, we found that the expression of COL3A1 and SOX2 was increased in tranilast-resistant neurofibroma cells, suggesting that the encoded proteins may give rise to resistance to tranilast treatment. The pluripotency-associated transcription factor SOX2 was recently shown to be expressed in a cell population manifesting properties of cancer stem cells or tumour-initiating cells and to be associated with drug resistance42. Attenuation of the expression of SOX2 or COL3A1 is therefore a potential approach to circumventing resistance to tranilast treatment. Inhibition of SOX2 expression has been shown to suppress cancer initiation and tumour cell proliferation, migration, invasion, and metastasis as well as to induce apoptosis in oligodendroglioma, lung cancer, breast cancer, and osteosarcoma cells61,62,63,64. Combined treatment with a SOX2 blocker and tranilast is therefore also a potential approach to inhibition of neurofibroma growth.
In summary, tranilast inhibited the expression of EMT- and angiogenesis-related genes associated with neurofibromin deficiency as well as suppressed the proliferation of neurofibromin-deficient cells both in vitro and in vivo. Our findings thus suggest that tranilast and other EMT inhibitors warrant further investigation as potential therapeutic agents for NF1-associated neurofibromas.
Methods
Cell lines and cell culture
ARPE-19 cells were obtained from American Type Culture Collection (ATCC) and were maintained in Dulbecco’s modified Eagle’s medium (DMEM)–F-12 (Sigma) supplemented with 10% fetal bovine serum (FBS), penicillin (100 U/ml), and streptomycin (100 µg/ml). sNF96.2, HeLa, and NIH3T3 cells were also obtained from ATCC and were maintained in DMEM supplemented with 10% FBS. HSCs were obtained from ScienCell Research Laboratories and were cultured in Schwann cell medium (SCM, ScienCell Research Laboratories).
Patients
Patients who met the NIH clinical diagnostic criteria for NF1 (Neurofibromatosis Conference Statement, 1988) were recruited. Tissue samples were obtained during tumour resection surgery at Keio University Hospital. Whole-blood specimens were also obtained for gene analysis. All patients provided written informed consent, and this aspect of the study was approved by the institutional review board of Keio University.
Preparation of tumour cells from NF1 patients
Neurofibroma cells and DFAT cells were established from neurofibromas of NF1 patients as described previously33. Tumor tissue was washed extensively with phosphate-buffered saline (PBS), minced in DMEM containing 0.1% collagenase (Sigma) and 2% bovine serum albumin (BSA, Sigma), and dissociated by incubation for 1 h at 37 °C with gentle shaking. The cell suspension was passed through a 100-µm cell strainer (Corning) to remove tissue debris. The cells were then washed three times with PBS by centrifugation at 135 × g for 3 min. The neurofibroma cells at the bottom of the tube and the floating stromal adipocytes were collected separately and purified by centrifugation three times. For establishment of DFAT cells, the stromal adipocytes were placed in a culture flask (Corning) filled with DMEM supplemented with 20% FBS, which generated a sealed environment, and the flask was then inverted and incubated at 37 °C in a humidified atmosphere of 5% CO2. Under this culture condition, the stromal adipocytes float up through the medium and adhere to the top inner surface (ceiling) of the flask. After 1 week, the cells were firmly attached to the ceiling and had transformed into fibroblast-like DFAT cells with no visible fat droplets. Both the neurofibroma cells and the DFAT cells were maintained in DMEM supplemented with 20% FBS at 37 °C in a humidified atmosphere of 5% CO2.
Focus formation assay
ARPE-19 cells were cultured in 96-well plates for 5 days and then exposed for 2 days to TNF-α (100 ng/ml, eBioscience) and TGF-β2 (5 ng/ml, eBioscience) in the absence or presence of SB431542 (10 µM, Calbiochem) or test drugs. They were then fixed for 30 min at room temperature with 4% paraformaldehyde in PBS, washed with PBS, incubated for 60 min at room temperature with Hoechst 33342 (Invitrogen) and phalloidin–Alexa Fluor 568 (Invitrogen) in PBS, and washed again with PBS. The cells were examined with a high-throughput image screening system (ImageXpress ULTRA, Molecular Devices) for quantitation of focus formation, with a focus being defined as a cell aggregate with an area of Hoechst 33342 fluorescence greater than a certain threshold. The fluorescence intensity of each focus was measured, and the percentage inhibition of focus formation by test drugs was determined as: 100 – [100 × (fluorescence intensity for all foci in the presence of the test drug)/(fluorescence intensity for all foci in the absence of the drug)]. The median inhibitory concentration for each drug was determined from the concentration-response curve.
RNA interference
NF1, COL3A1, and negative control (GAPD) siRNAs were obtained from Dharmacon and were introduced into cells by transfection with the Lipofectamine RNAiMAX reagent (Invitrogen). NIH3T3 cells were transfected with plasmids for NF1 shRNAs (pSUPER-NF1 249, 5′-GATCCCCCAAGGAGTGTCTGATCAACTTCAAGAGAGTTGATCAGACACTCCTTGTTTTTA-3′ and 5′-AGCTTAAAAACAAGGAGTGTCTGATCAACTCTCTTGAAGTTGATCAGACACTCCTTGGGG-3′; pSUPER-NF1 611, 5′-GATCCCCGGTTACAGGAGTTGACTGTTTCAAGAGAACAGTCAACTCCTGTAACCTTTTTA-3′ and 5′-AGCTTAAAAAGGTTACAGGAGTTGACTGTTCTCTTGAAACAGTCAACTCCTGTAACCGGG-3′) or a control plasmid with the use of the Lipofectamine 2000 transfection reagent (Thermo Fisher Scientific), and the cells were then subjected to selection with puromycin (3 µg/ml).
Quantitative RT-PCR analysis
Total RNA was extracted from cells with the use of an RNeasy Mini Kit (Qiagen), and portions (1 μg) of the isolated RNA were subjected to RT with a Transcriptor first-strand cDNA synthesis kit (Roche). The resulting cDNA was subjected to real-time PCR analysis with SYBR Premix ExTaq (TaKaRa) and a Thermal Cycler Dice RealTime System (TP800, TaKaRa). Primer sequences are listed in Supplementary Table S1. The amplification protocol comprised an initial incubation at 95 °C for 2 min followed by 40 cycles of 95 °C for 30 s and 60 °C for 30 s. The abundance of each target mRNA was normalized by that of hypoxanthine phosphoribosyltransferase 1 (HPRT1) mRNA.
Immunoblot analysis
Cells were collected and lysed in lysis buffer (2% SDS, 10% glycerol, 50 mM Tris-HCl (pH 6.8), 100 mM dithiothreitol). Equal amounts of total lysates were fractionated by SDS-polyacrylamide gel electrophoresis, and the separated proteins were transferred to a nitrocellulose filter and probed with primary antibodies to fibronectin (Santa Cruz Biotechnology), to N-cadherin (Santa Cruz Biotechnology), to collagen type I (Abcam), or to α-tubulin (Sigma-Aldrich). Immune complexes were detected with horseradish peroxidase–conjugated secondary antibodies (GE Healthcare and Dako), enhanced chemiluminescence reagents (ImmunoStar LD, Wako), and an LAS-3000mini instrument (GE Healthcare).
Fluorescence or immunofluorescence analysis
ARPE-19 cells cultured in 96-well plates were fixed for 30 min at room temperature with 4% paraformaldehyde in PBS, washed with PBS, and exposed for 1 h at room temperature to 3% BSA in PBS before incubation overnight at 4 °C with biotinylated HABP (5 µg/ml, Seikagaku) and 3% BSA in PBS. The cells were then washed with PBS, incubated for 60 min at room temperature with streptavidin–Alexa Fluor 488 (Invitrogen) and Hoechst 33342 in PBS containing 3% BSA, washed again with PBS, and imaged with a BZ-9000 fluorescence microscope (Keyence).
sNF96.2 cells cultured in 35-mm dishes were fixed for 15 min at room temperature with 4% paraformaldehyde in PBS, washed with PBS, and then permeabilized for 30 min at room temperature with 0.2% Triton X-100 in PBS. The cells were stained for 90 min at room temperature with antibodies to collagen type III (Abcam) diluted in PBS containing 1% BSA, washed with 0.2% Triton X-100 in PBS, incubated for 60 min at room temperature with Alexa Fluor 594–conjugated secondary antibodies (Invitrogen) in PBS containing 1% BSA, and washed again with 0.2% Triton X-100 in PBS. They were finally stained for 5 min with Hoechst 33342 in PBS containing 1% BSA, washed with 0.2% Triton X-100 in PBS, and imaged with a BZ-9000 fluorescence microscope (Keyence).
Cell viability assay
Cells were seeded at a density of 2.5 × 103 per well in 96-well plates and incubated for 24 h before exposure to various concentrations of tranilast (Calbiochem) for the indicated times. Cell viability was then assayed with a CellTiter-Glo Kit (Promega) and an EnVision Plate Reader (PerkinElmer).
Cell transplantation
sNF96.2 cells (1 × 106 cells in 2 µl of Hanks’ balanced salt solution) were injected as a single-cell suspension into the brain of 6-week-old female NOD/SCID mice (Charles River) that had been anesthetized by exposure to 1% to 3% isoflurane. After 3 weeks, the mice were treated by oral administration of tranilast (300 mg/kg) or vehicle (1% NaHCO3) once a day for 8 weeks. This aspect of the study was approved by the Animal Care and Use Committee of Keio University School of Medicine.
Tissue slice culture
Brain tissue slice culture was performed as previously described65. sNF96.2-GFP cells were injected into the brain of NOD/SCID mice as described above. After 6 weeks, the brain was removed and thin tissue slices were cultured in the presence of tranilast (750 µM) or DMSO vehicle. The slices were imaged with a Fluoview FV10i microscope (Olympus). The maximum tumour diameter and the maximum length of the invasion path were determined from the images.
Immunohistochemistry
Immunohistochemical staining was performed as described previously14 with antibodies to vimentin (Dako), to collagen type I (Abcam), to collagen type III (Abcam), to ZEB1 (Santa Cruz Biotechnology), or to SOX2 (R&D Systems).
Collagen type III ELISA
The collagen type III content of sNF96.2 cells was determined with the use of a Human Collagen Type III ELISA kit (Kamiya Biomedical Co.).
Statistical analysis
Data are presented as means ± s.d. and were analysed with Student’s unpaired t test. A P value of <0.05 was considered statistically significant.
Data availability
Representative data are provided in this published article and its Supplementary Information files. Other data sets generated during and/or analysed during the current study are available from the corresponding author on reasonable request.
All methods were performed in accordance with the relevant guidelines and regulations.
References
Shen, M. H., Harper, P. S. & Upadhyaya, M. Molecular genetics of neurofibromatosis type 1 (NF1). J. Med. Genet. 33, 2–17 (1996).
Bollag, G. et al. Loss of NF1 results in activation of the Ras signalling pathway and leads to aberrant growth in haematopoietic cells. Nat. Genet. 12, 144–148 (1996).
Rad, E. & Tee, A. R. Neurofibromatosis type 1: fundamental insights into cell signalling and cancer. Semin. Cell Dev. Biol. 52, 39–46 (2016).
Vincent, M. R. et al. von Recklinghausen disease: 130 years, in Neurofibromatosis Type 1 (eds Meena, U. & David, N. C.) 1–16 (Springer, 2012).
Monroe, C. L., Dahiya, S. & Gutmann, D. H. Dissecting clinical heterogeneity in neurofibromatosis type 1. Annu. Rev. Pathol. 12, 53–74 (2017).
Kiuru, M. & Busam, K. J. The NF1 gene in tumour syndromes and melanoma. Lab. Invest. 97, 146–157 (2017).
Weiss, B. et al. Sirolimus for progressive neurofibromatosis type 1-associated plexiform neurofibromas: a Neurofibromatosis Clinical Trials Consortium phase II study. Neuro-Oncol. 17, 596–603 (2015).
Weiss, B. et al. Sirolimus for non-progressive NF1-associated plexiform neurofibromas: an NF Clinical Trials Consortium phase II study. Pediatr. Blood Cancer 61, 982–986 (2014).
Widemann, B. C. et al. Phase II trial of pirfenidone in children and young adults with neurofibromatosis type 1 and progressive plexiform neurofibromas. Pediatr. Blood Cancer 61, 1598–1602 (2014).
Widemann, B. C. et al. Phase 2 randomized, flexible crossover, double-blinded, placebo-controlled trial of the farnesyltransferase inhibitor tipifarnib in children and young adults with neurofibromatosis type 1 and progressive plexiform neurofibromas. Neuro-Oncol. 16, 707–718 (2014).
Robertson, K. A. Imatinib mesylate for plexiform neurofibromas in patients with neurofibromatosis type 1: a phase 2 trial. Lancet Oncol. 13, 1218–1224 (2012).
Thiery, J. P., Acloque, H., Huang, R. Y. & Nieto, M. A. Epithelial-mesenchymal transitions in development and disease. Cell 139, 871–890 (2009).
Kahlert, U. D., Joseph, J. V. & Kruyt, F. A. E. EMT- and MET-related processes in nonepithelial tumours: importance for disease progression, prognosis, and therapeutic opportunities. Mol. Oncol. 11, 860–877 (2017).
Arima, Y. et al. Decreased expression of neurofibromin contributes to epithelial-mesenchymal transition in neurofibromatosis type 1. Exp. Dematol. 19, 136–141 (2010).
Takahashi, E. et al. Tumour necrosis factor-α regulates transforming growth factor-β-dependent epithelial-mesenchymal transition by promoting hyaluronan-CD44-moesin interaction. J. Biol. Chem. 285, 4060–4073 (2010).
O’Conner, J. W. & Gomez, E. W. Biomechanics of TGFβ-induced epithelial-mesenchymal transition: implications for fibrosis and cancer. Clin. Transl. Med. 3, 23 (2014).
Jung, H. Y., Fatter, L. & Yang, J. Molecular pathways: linking tumour microenvironment to epithelial-mesenchymal transition in metastasis. Clin. Cancer Res. 21, 962–968 (2015).
Guan, X. Cancer metastases: challenges and opportunities. Acta Pharm. Sin. B. 5, 402–418 (2015).
Hahn, J. M., McFarland, K. L., Combs, K. A. & Supp, D. M. Partial epithelial-mesenchymal transition in keloid scars: regulation of keloid keratinocyte gene expression by transforming growth factor-β1. Burns Trauma 4, 30 (2016).
Chen, Q. K., Lee, K., Radisky, D. C. & Neison, C. M. Extracellular matrix proteins regulate epithelial-mesenchymal transition in mammary epithelial cells. Differentiation 86, 126–132 (2013).
Azuma, H., Banno, K. & Yoshimura, T. Pharmacological properties of N-(3’,4’-dimethoxycinnamoyl) anthranilic acid (N-5’), a new anti-atopic agent. Br. J. Pharmacol. 58, 483–488 (1976).
Darakhshan, S. & Pour, A. B. Tranilast: a review of its therapeutic applications. Phamacol. Res. 91, 15–28 (2015).
Zoltan-Jones, A., Huang, L., Ghatak, S. & Toole, B. P. Elevated hyaluronan production induces mesenchymal and transformed properties in epithelial cells. J. Biol. Chem. 278, 45801–45810 (2003).
Toole, B. P., Zoltan-Jones, A., Misra, S. & Ghatak, S. Hyaluronan: a critical component of epithelial-mesenchymal and epithelial-carcinoma transitions. Cells Tissues Organs 179, 66–72 (2005).
Li, L. et al. Transforming growth factor-β1 induces EMT by the transactivation of epidermal growth factor signalling through HA/CD44 in lung and breast cancer cells. Int. J. Mol. Med. 35, 113–122 (2015).
Heldin, P., Basu, K., Kozlova, I. & Porsch, H. HAS2 and CD44 in breast tumourigenesis. Adv. Cancer Res. 123, 211–229 (2014).
Takehana, Y. et al. Suppression of laser-induced choroidal neovascularization by oral tranilast in the rat. Invest. Ophthalmol. Vis. Sci. 40, 459–466 (1999).
De Palma, M., Biziato, D. & Petrova, T. V. Microenvironmental regulation of tumour angiogenesis. Nat. Rev. Cancer 17, 457–474 (2017).
Carmeliet, P. Angiogenesis in life, disease and medicine. Nature 438, 932–936 (2005).
Ribatti, D. Mast cells and macrophages exert beneficial and detrimental effects on tumour progression and angiogenesis. Immunol. Lett. 152, 83–88 (2013).
Webb, A. H. et al. Inhibition of MMP-2 and MMP-9 decreases cellular migration, and angiogenesis in in vitro models of retinoblastoma. BMC Cancer 17, 434 (2017).
Koch, A. E. et al. Interleukin-8 as a macrophage-derived mediator of angiogenesis. Science 258, 1798–1801 (1992).
Nobusue, H. & Kano, K. Establishment and characteristics of porcine preadipocyte cell lines derived from mature adipocytes. J. Cell. Biochem. 109, 542–552 (2010).
Maruoka, R. et al. The use of next-generation sequencing in molecular diagnosis of neurofibromatosis type 1: a validation study. Genet. Test. Mol. Biomarkers 18, 722–735 (2014).
Jouhilahti, E. M., Peltonen, S., Heape, A. M. & Peltonen, J. The pathoetiology of neurofibromatosis 1. Am. J. Pathol. 178, 1932–1939 (2011).
Peltonen, J. et al. Cellular differentiation and expression of matrix genes in type 1 neurofibromatosis. Lab. Invest. 59, 760–771 (1988).
Muir, D. Differences in proliferation and invasion by normal, transformed and NF1 Schwann cell cultures are influenced by matrix metalloproteinase expression. Clin. Exp. Metastasis 13, 303–314 (1995).
Muir, D. et al. Tumorigenic properties of neurofibromin-deficient neurofibroma Schwann cells. Am. J. Pathol. 158, 501–513 (2001).
Miller, S. J. et al. Large-scale molecular comparison of human schwann cells to malignant peripheral nerve sheath tumor cell lines and tissues. Cancer Res. 66, 2584–2591 (2006).
Pytel, P. et al. Neoplasms with schwannian differentiation express transcription factors known to regulate normal schwann cell development. Int. J. Surg. Pathol. 18, 449–457 (2010).
Kondoh, H. et al. Historical perspectives, in Sox2 Biology and Role in Development and Disease (eds Kondoh, H. & Lovell-Badge, R.) 3–13 (Elsevier, 2016).
Wuebben, E. L. & Rizzino, A. The dark side of SOX2: cancer—a comprehensive overview. Oncotarget 8, 44917–44943 (2017).
Prieto-Garcia, E., Diaz-Garcia, C. V., Garcia-Ruiz, I. & Agulló-Ortuño, M. T. Epithelial-to-mesenchymal transition in tumour progression. Mes. Oncol. 34, 122 (2017).
Otsuki, Y., Saya, H. & Arima, Y. Prospects for new lung cancer treatments that target EMT signalling. Dev. Dyn. https://doi.org/10.1002/dvdy.24596 (2017).
Suzawa, H., Kikuchi, S., Arai, N. & Koda, A. The mechanism involved in the inhibitory action of tranilast on collagen biosynthesis of keloid fibroblasts. Jpn. J. Pharmacol. 60, 91–96 (1992).
Ammendola, M. et al. Targeting mast cells tryptase in tumour microenvironment: a potential antiangiogenetic strategy. Biomed. Res. Int. 2014, 154702 (2014).
Maehata, Y. et al. Type III collagen is essential for growth acceleration of human osteoblastic cells by ascorbic acid 2-phosphate, a long-acting vitamin C derivative. Matrix Biol. 26, 371–381 (2007).
Su, B. et al. Let-7d suppresses growth, metastasis, and tumour macrophage infiltration in renal cell carcinoma by targeting COL3A1 and CCL7. Mol. Cancer 13, 206 (2014).
Qiu, F. et al. miR-29a/b enhances cell migration and invasion in nasopharyngeal carcinoma progression by regulating SPARC and COL3A1 gene expression. PLoS One 10, e0120969 (2015).
Bertelli, R. et al. Cell-specific regulation of α1 (III) and α2 (V) collagen by TGF-β1 in tubulointerstitial cell models. Nephrol. Dial. Transplant. 13, 573–579 (1998).
Chuang, T. D. & Khorram, O. Tranilast inhibits genes functionally involved in cell proliferation, fibrosis, and epigenetic regulation and epigenetically induces miR-29c expression in leiomyoma cells. Reprod. Sci. 24, 1253–1263 (2017).
Fantozzi, A. et al. VEGF-mediated angiogenesis links EMT-induced cancer stemness to tumor initiation. Cancer Res. 74, 1566–1575 (2014).
Thomas, S. L. & De Vries, G. H. Angiogenic expression profile of normal and neurofibromin-deficient human Schwann cells. Neurochem. Res. 32, 1129–1141 (2007).
Hurwitz, H. et al. Bevacizumab plus irinotecan, fluorouracil, and leucovorin for metastatic colorectal cancer. N. Engl. J. Med. 350, 2335–2342 (2004).
Van-Cutsem, E. et al. Addition of aflibercept to fluorouracil, leucovorin, and irinotecan improves survival in a phase III randomized trial in patients with metastatic colorectal cancer previously treated with an oxaliplatin-based regimen. J. Clin. Oncol. 30, 3499–3506 (2012).
Spratlin, J. L. et al. Phase I pharmacologic and biologic study of ramucirumab (IMC-1121B), a fully human immunoglobulin G1 monoclonal antibody targeting the vascular endothelial growth factor receptor-2. J. Clin. Oncol. 28, 780–787 (2010).
Naveen, S. V. & Andrew, R. R. Anti-angiogenic therapy for cancer: current progress, unresolved questions and future directions. Angiogenesis 17, 471–494 (2014).
Garcia-Alfonso, P. et al. The role of antiangiogenic agents in the treatment of patients with advanced colorectal cancer according to K-RAS status. Angiogenesis 17, 805–821 (2014).
Li, C. et al. Discovery of novel anti-angiogenesis agents. Part 7: Multitarget inhibitors of VEGFR-2, TIE-2 and EphB4. Eur. J. Med. Chem. 141, 506–518 (2017).
Rathinavelu, A., Alhazzani, K., Dhandayuthapani, S. & Kanagasabai, T. Anti-cancer effects of F16: a novel vascular endothelial growth factor receptor-specific inhibitor. Tumour Biol. 39, 1010428317726841 (2017).
Favaro, R. et al. Sox2 is required to maintain cancer stem cells in a mouse model of high-grade oligodendroglioma. Cancer Res. 74, 1833–1844 (2014).
Xiang, R. et al. Downregulation of transcription factor SOX2 in cancer stem cells suppresses growth and metastasis of lung cancer. Br. J. Cancer 104, 1410–1417 (2011).
Wang, X. et al. SOX2 enhances the migration and invasion of ovarian cancer cells via Src kinase. PLoS One 9, e99594 (2014).
Ren, T. et al. Inhibition of SOX2 induces cell apoptosis and G1/S arrest in Ewing’s sarcoma through the PI3K/Akt pathway. J. Exp. Clin. Cancer Res. 35, 44 (2016).
Minami, N. et al. Organotypic brain explant culture as a drug evaluation system for malignant brain tumours. Cancer Med. 6, 2635–2645 (2017).
Acknowledgements
We thank T. Ozawa for providing NF1 shRNA vectors as well as S. Kuninaka, K. Miyamoto, and M. Hosonaga for technical assistance. This study was supported by the Translational Research Network Program and by Research on Applying Health Technology and Research on Rare and Intractable Diseases grants from the Japan Agency for Medical Research and Development (AMED).
Author information
Authors and Affiliations
Contributions
The study was designed by R.H., T.K., H.S., and Y.A. Method development, material preparation, and data analysis were performed by all authors. R.H. wrote the manuscript with contributions from H.S. and Y.A. All authors approved the manuscript before submission.
Corresponding author
Ethics declarations
Competing Interests
The authors declare no competing interests.
Additional information
Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Electronic supplementary material
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Harigai, R., Sakai, S., Nobusue, H. et al. Tranilast inhibits the expression of genes related to epithelial-mesenchymal transition and angiogenesis in neurofibromin-deficient cells. Sci Rep 8, 6069 (2018). https://doi.org/10.1038/s41598-018-24484-y
Received:
Accepted:
Published:
DOI: https://doi.org/10.1038/s41598-018-24484-y
This article is cited by
-
Tranilast-tyrosine hybrid molecule exhibits dual activity: suppression of epithelial-mesenchymal transition and induction of cytotoxicity in cancer cells
Medicinal Chemistry Research (2022)
-
Placental extract suppresses the formation of fibrotic deposits by tumor necrosis factor alpha and transforming growth factor beta-induced epithelial–mesenchymal transition in ARPE-19 cells
BMC Research Notes (2021)
-
Tumorigenesis in neurofibromatosis type 1: role of the microenvironment
Oncogene (2021)
-
The Role of Desmoplasia and Stromal Fibroblasts on Anti-cancer Drug Resistance in a Microengineered Tumor Model
Cellular and Molecular Bioengineering (2018)
Comments
By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.