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Formation of blood vessels, or angiogenesis, is crucial to cancer progression. Thus, inhibiting angiogenesis can limit the growth and spread of tumors. The natural polyphenol catechin has moderate anti-tumor activity and interacts with copper, which is essential for angiogenesis. Catechin is easily metabolized in the body and this limits its clinical application. We have recently shown that conjugation of catechin with dextran (Dextran-Catechin) improves its serum stability, and exhibits potent anti-tumor activity against neuroblastoma by targeting copper homeostasis. Herein, we investigated the antiangiogenic activity of Dextran-Catechin and its mechanism. We found that Dextran-Catechin displayed potent antiangiogenic activity in vitro and in vivo. We demonstrated Dextran-Catechin generates reactive oxygen species which in turns disrupts copper homeostasis by depleting the copper importer CTR-1 and copper trafficking ATOX-1 protein. Mechanistically, we showed that disrupting copper homeostasis by knockdown of either CTR-1 or ATOX-1 protein can inhibit angiogenesis in endothelial cells. This data strongly suggests the Dextran-Catechin potent antiangiogenic activity is mediated by disrupting copper homeostasis. Thus, compounds such as Dextran-Catechin that affects both tumor growth and angiogenesis could lead the way for development of new drugs against high copper levels tumors.
Blood supply plays a critical role in the growth and spread of cancer. The formation of blood vessels, or angiogenesis, can be stimulated by chemical signals secreted by tumors. The resulting new blood vessels feed growing tumors with oxygen and nutrients, allowing the cancer cells to metastasise1. The growth and spread of tumors can be inhibited by limiting angiogenesis, and numerous studies have demonstrated this through the use of antiangiogenic agents2–5.
Angiogenesis, and thus the activation of endothelial cells by angiogenic factors, play an essential role in tumor growth and progression. The essentiality of copper ions in humans has long been recognized, with the imbalance of its homeostasis causing neurodegenerative, cardiovascular diseases, bone metabolism disorders, and inflammatory responses6. Furthermore, copper ions have been found to play an important role in tissue remodeling by regulating the cross-linking of collagen7, and to enhance dermal wound healing via the promotion of the biosynthesis of vascular endothelial growth factor (VEGF) by keratinocytes and the regulation of endothelial cell survival, proliferation and migration8.
Previous studies have shown that the copper concentration in serum increases with cancer disease progression and correlates with tumor incidence and burden9. As mentioned, copper homeostasis is tightly regulate by the body, because of the toxicity of high plasmatic copper concentrations10. A key protein in regulating copper homeostasis is Antioxidant-1 (ATOX-1), which obtains copper via copper importer CTR-1 and transfers it to the copper transporter ATP7A that delivers copper to the secretory copper enzymes or exclude copper. More specifically, by regulating extracellular matrix modifying secretory copper enzyme, ATOX-1 plays an essential role in angiogenesis10. Depletion of copper, indeed, has been successful in inhibiting angiogenesis in a wide variety of cancer cell and xenograft systems, and several clinical trials using copper chelation treatment as either an adjuvant or primary therapy have been conducted11–13, including the CTR-1 silencing that inhibited angiogenesis by limiting copper entry into endothelial cells14. However, the biological basis linking the activity of antiangiogenic molecules and copper remains unclear.
Natural derived polyphenols, such as catechin, have anticancer and antiangiogenic activity but their low bioavailability has limited their clinical applications15–17. We have previously shown that the conjugation of Catechin with Dextran, here referred to as Dextran-Catechin, has led to higher serum stability and exhibits potent anti-tumor properties by targeting copper homeostasis in neuroblastoma18.
In this study, we tested the hypothesis that Dextran-Catechin has an antiangiogenic effect mediated by the disruption of copper homeostasis and thus inhibition of endothelial cell angiogenesis. Our results showed that Dextran-Catechin treatment exhibits potent antiangiogenic activity in human microvascular endothelial cells (HMEC-1) due to the production of reactive oxygen species (ROS), which in turn led to depletion of ATOX-1, an anti-oxidant and intracellular copper-transporting protein19. This study therefore highlights the potential of natural products with ROS-generating properties as novel therapeutics for the treatment of cancers that are dependent on high levels of copper to sustain their growth.
To determine the antiangiogenic property of Dextran-Catechin, we investigated the degree of angiogenesis by HMEC-1 cells after treatment with the Matrigel™ assay. The Matrigel™ assay measures the surface area of vascular structures formed by the endothelial cells, which indicates the extent of angiogenesis. We found a dose response between the concentration of Dextran-Catechin and the degree of angiogenesis, exhibiting lower angiogenesis activity at higher treatment concentration. Notably, there was significant decrease in angiogenesis at 10µg/ml (−42±6%, P<0.001) and 25µg/ml (−98±2%, P<0.0001, Fig. 1). These data demonstrate that Dextran-Catechin has potent antiangiogenic activity.
To determine if any antiangiogenic effect observed with Dextran-Catechin treatment was due to direct toxicity, cell viability of HMEC-1 cells was examined following treatment using a range of Dextran-Catechin concentrations. The IC50 of Dextran-Catechin was 76.1 (±6.3) and 24.9 (±0.3) µg/ml after 8h and 24h of treatment (See Supplementary Fig. 1). This suggests that Dextran-Catechin treatment was not toxic to HMEC-1 cells at low dose within 8h, which indicates that the anti-angiogenic effect seen in the Matrigel was not due to toxicity.
We recently demonstrated that Dextran-Catechin can disrupt copper metabolism in cancer cells18. Therefore, we postulated that a possible antiangiogenic mechanism of Dextran-Catechin is through the disruption the copper homeostasis in endothelial cells. Initially, to determine whether copper is important in the angiogenic activity of HMEC-1 cells, the main importer of copper, CTR-1, was suppressed using SiRNA. Suppression of CTR-1 has previously been shown to reduce intracellular copper levels20. To further validate the dependence of copper on angiogenesis, we utilised a commonly used copper chelator tetraethylenepentamine (TEPA) to restrict the availability of free copper to the cells.
As anticipated, we observed a significant reduction in angiogenesis following knockdown of CTR-1 (−69±7%, P<0.0001) in comparison with the control and non-silencing siRNA transfected HMEC-1 cells (Fig. 2). Similar to the results of the CTR-1 knockdown experiment, HMEC-1 cells with the TEPA treatment showed a significant reduction in angiogenesis (−30±1%, P<0.0001, Fig. 2). The concentration of TEPA that had shown antiangiogenic effect was found to be non-toxic to HMEC-1 cells (See Supplementary Fig. 2).
These results suggest that copper plays an important role in the promotion of angiogenesis and disrupting copper metabolism in endothelial cells reduces their angiogenic capabilities.
Catechin has been shown to act as a pro-oxidant in the presence of copper, which results in the production of ROS21. Hence, the interaction between Dextran-Catechin and the copper contained in the culture media will inevitably generate ROS. Using the cellular ROS detection kit, we found that the level of ROS in cell culture media increases dramatically after addition of Dextran-Catechin even at a low dose of 10μg/ml (Fig. 3a).
Subsequently, the level of ROS in HMEC-1 cells, which was induced by Dextran-Catechin, was evaluated at various time points. We noted that the level of ROS in HMEC-1 cells decreased over time in comparison to the control (Fig. 3b). The gradient decrease in ROS levels indicated that HMEC-1 cells activated mechanisms to compensate for the oxidative stress and prevent oxidative damage.
Given the role of copper, Dextran-Catechin and ROS, we sought to investigate the change in the levels of proteins that are involved in the prevention of oxidative damage, copper homeostasis and angiogenesis.
One of the proteins that are involved in both copper regulation and protection from oxidative damage is ATOX-1. ATOX-1 regulates copper trafficking within the cells, and importantly, it transports copper to the VEGF promoter22. Thus, we investigated the changes in ATOX-1 protein level after 24h Dextran-Catechin treatment and found a significant decrease of ATOX-1 protein at 10 and 25μg/ml (Fig. 4a). This decrease reflects the degradation of ATOX-1 to compensate for the increase in oxidative stress. VEGF-R2, the potent receptor for endothelial cell angiogenesis, and CTR-1 were downregulated in equal measure (Fig. 4a).
To determine the intracellular copper levels in HMEC-1 cells after Dextran-Catechin treatment, a spectrophotometric assay was used to measure the level of copper in the cell lysate. We found a significant increase in intracellular copper levels following treatment with 10µg/ml (P<0.05) and 25µg/ml (P<0.05) Dextran-Catechin for 24h (Fig. 4b). This is likely due to the reduction in copper trafficking capability of the cells to export copper after the lower levels of ATOX-1 proteins.
To determine the effect of ATOX-1 reduction on proteins that are involved in angiogenesis and copper homeostasis, we investigated the protein levels of VEGF-R2 and CTR-1 following ATOX-1 knockdown in HMEC-1 cells. We found that the VEGF-R2 and CTR-1 protein levels between the non-silencing siRNA control and the ATOX-1 knockdown cells showed no significant changes (Fig. 5a). This implies that the level of ATOX-1 did not directly affect VEGF-R2 and CTR-1 levels.
To determine the angiogenic effect of reduced ATOX-1 protein levels, the Matrigel™ assay was carried out using ATOX-1 knockdown HMEC-1 cells. The Matrigel™ assay revealed that the loss of this protein had resulted in a significant reduction in angiogenesis (−31±3%, P<0.0001) as compared to the control and non-silencing siRNA treated HMEC-1 cells (Fig. 5b). This suggested that ATOX-1 is also important in maintaining the angiogenic activity of HMEC-1 cells.
To determine the in vivo anti-angiogenic activity of Dextran-Catechin, we investigated the response of formation of blood vessels in a human neuroblastoma xenograft model18. After the 26day experimental period, tumor slices were stained for CD31 protein, which indicates the presence of endothelial cells. Vessels were only counted when it shows a clear morphological vascular structure with a visible lumen. There was a significant reduction of vessel observed in the 300µg/ml Dextran-Catechin treatment group (1.3±0.7 vessels, 8 fields per view counted) as compared to the saline control group (4.9±0.3 vessels, 8 fields per view counted, Fig. 6). The reduction in number of vessels observed in the tumor slices suggests that the Dextran-Catechin treatment exhibited anti-angiogenic activity in vivo.
ATOX-1 is an important protein that traffics copper from the importer protein CTR-1 to various locations. As a transporter, it brings copper ions to the VEGF promoter for the transcription of growth factors for angiogenesis, and to the copper exporter site for removal of excess copper22. ATOX-1 also acts as an anti-oxidant for the prevention of oxidative damage. However, ATOX-1 can only fulfil one of these roles at a single time, either as a copper transport protein or as an anti-oxidant23. The depletion of ATOX-1 in endothelial cells under oxidative stress has not been investigated prior to this study. However, the ATOX-1 scavenger activity of superoxide anion was reported before in yeast24. Here, we describe the depletion of ATOX-1 in endothelial cells following Dextran-Catechin treatment, to compensate for the effect of ROS and thus the prevention of oxidative damage.
As seen in the generation of ROS by Dextran-Catechin in the cell culture media, the higher the concentration of Dextran-Catechin treatment, the higher level of ROS is being generated. However, the amounts of ROS detected in the HMEC-1 cells showed the opposite trend whereby lower ROS level is being detected at a higher Dextran-Catechin concentration treatment. This occurs because the cells have to ability to prevent oxidative damage. In this mechanism, ATOX-1 plays an important role and is depleted to reduce the ROS level within the cells. Hence, after the treatment with Dextran-Catechin, lower protein level of ATOX-1 was detected in the HMEC-1 cells.
The depletion of ATOX-1 reduces the ability to transport copper within the endothelial cells, but also leads to the accumulation of copper ions within cells, as demonstrated in the Dextran-Catechin treated HMEC-1 cells. Despite the increased level of free intracellular copper following Dextran-Catechin treatment, these copper ions are not functional as they are unlikely to be transported to sites that assist in cellular functions such as the VEGF promoter due to reduction in the levels of ATOX-1. In the case of Dextran-Catechin treatment in endothelial cells, ATOX-1 protein level is reduced for the prevention of oxidative stress, less copper is transported to the VEGF promoter, thus preventing angiogenesis. The reduction in formation of vascular structures of the endothelial cells with reduced ATOX-1 following Dextran-Catechin treatment was simulated through the knock-down of ATOX-1.
VEGF receptors are crucial for the activation of angiogenesis, and the most important receptor in endothelial cell is the VEGF-R225. Here, we found that in HMEC-1 cells, the regulation of VEGF-R2 seems to be independent from the level of ATOX-1 protein as the knockdown of ATOX-1 had no effect on the VEGF-R2 protein levels. Nevertheless, we found that both the ATOX-1 and VEGF-R2 levels were markedly downregulated in the Dextran-Catechin treated HMEC-1 cells. This suggests that Dextran-Catechin is affecting both ATOX-1 and VEGF-R2 simultaneously. Thus for the first time, we demonstrated the potent antiangiogenic property of Dextran-Catechin (Fig. 7). Further studies will therefore be necessary to reveal other possible mechanisms of how Dextran-Catechin affects the VEGF and thus angiogenesis.
Unlike cancer cells, oxidative stress is well tolerated by normal cells due to their various ROS-salvaging systems26. Hence, the use of ROS-generating agents can potentially have anti-tumor and antiangiogenic activity. However, agents with ROS producing abilities as their only mechanism of action have been reported to show low clinical response and resistance in cancer when used for treatment26. This report suggests that anti-tumor or antiangiogenic agents with multiple modes of action are required to effectively combat cancer.
The finding in the in vivo model of neuroblastoma showing reduction in the number of vascular structures when they were treated with Dextran-Catechin furthers supports the anti-angiogenic effects of Dextran-Catechin reported in the in vitro experiments. The results from this study, combined with our previous study on Dextran-Catechin18, suggest that Dextran-Catechin exerts its anticancer and antiangiogenic properties by targeting copper homeostasis in tumor and endothelial cells. Furthermore, Dextran-Catechin also has minimal effect on the viability of non-malignant MRC-5 cells18, making it highly attractive as an anti-tumor agent with multiple modes of action. This study therefore highlights the potential of developing natural products that can disrupt copper homeostasis as a novel therapeutic approach for the treatment of cancers requiring high levels of copper to sustain growth and angiogenesis.
The experimental design and standard operating protocols were approved by the Children Cancer Institute of Australia UNSW; all methods were performed in accordance with the relevant guidelines and regulations. The animal study was approved by the Animal Ethics Committee at UNSW Australia (AEC# 14/36B).
HMEC-1 were grown in MCDB-131 medium (Invitrogen, Mount Waverley, Australia) supplemented with 10% fetal calf serum (FCS), 2mM L-glutamine, 1µg/mL hydrocortisone and 10ng/mL epithelial growth factor (BioScientific, Gymea, Australia). The cells were cultured on 0.1% gelatin-coated culture plates for all experiments, except for the MatrigelTM assay. The cell lines were maintained at 37°C in 5% CO2 as an adherent monolayer and were passaged upon reaching confluence using standard cell culture techniques.
Dextran-Catechin was synthesized and characterized as previously described27. (+)-Catechin hydrate and Dextran 6000kDa (Sigma Aldrich, NSW, Australia) were used for the synthesis of this conjugate. With the optimized synthesis protocol27, a conjugation of 19.9mg of Catechin per g of Dextran-Catechin was obtained. A stock solution of Dextran-Catechin 1mg/ml (1mg/ml refers to the concentration of catechin in the compound) was prepared in cell culture media MCDB-131 and stored at −20°C. The copper chelator tetraethylenepentamine (TEPA) was prepared at a concentration of 2 mg/ml in Milli-Q water (Sigma Aldrich, Castle Hill, NSW, Australia) and stored at −20°C.
The antiangiogenic properties of treated or protein knockdown cells were determined by using the Matrigel™ assay. Briefly, 24-well plates were coated at 4°C with 270µL of Matrigel™ solution (1:1 dilution in cell culture medium) and were allowed to solidify at 37°C for 1h before seeding. HMEC-1 cells were then seeded at 1×105 cells per well and allowed to adhere for 5min before treatment was initiated, or without treatment for the knockdown cells. For the treatment, HMEC-1 cells were treated with 1 to 25µg/mL of Dextran-Catechin or 20µg/mL of TEPA. HMEC-1 cells were transfected with the optimized conditions for knockdown of CTR-1 (siRNA B, 20nM) or ATOX-1 (siRNA C, 60nM) for 6hours and was incubated in fresh media for another 10hours prior to the Matrigel™ assay. Photographs were taken after 8hours using the 5X objective of an Axiovert 200M fluorescent microscope coupled to an AxioCamMR3 camera driven by AxioVision 4.8 software (Carl Zeiss, North Ryde, Australia). The total surface area of capillary tubes formed was measured in 5 view fields per well using AxioVision 4.8 software and Matrigel™ Assay Recognition Software (M.A.R.S) to quantitatively evaluate the vascular surface area of the structures formed.
HMEC-1 cells were seeded at 5×103 cells per well in 96-well plates to ensure full confluence (quiescence). The cells were treated 24h after seeding with a various concentration of Dextran-Catechin (5µg/ml to 55µg/ml) or TEPA (2µg/ml to 75µg/ml). After 8 or 24h of incubation, the media containing treatment was replaced with 10% AlamarBlue in fresh media. The metabolic activity was detected by spectrophotometric analysis by assessing the absorbance of AlamarBlue® (difference between 570nm and 595nm) using a Bio Rad multiplate reader. Cell viability was determined and expressed as the percentage of viability of untreated control cells. The determination of IC50 values was performed using GraphPad Prism 6 (San Diego, CA, USA).
HMEC-1 cells were seeded at 1.5×106 cells in 10cm cell culture dishes. The cells were treated 24h after seeding with 25µg/ml Dextran-Catechin. After 24h of treatment, the cells were washed with PBS and scraped in Milli-Q water. Protein levels were measured using standard BCA assay. The intracellular copper level was measured using the QuantiChrom™ Copper Assay Kit (BioAssay Systems, Hayward, CA, USA). Copper levels were determined according to manufacturer’s instructions by absorbance spectrophotometry at 359nm and normalized to the protein content.
To assess oxidative stress, a fluorogenic probe (CellROX® Green Reagent, Life Technologies, Vic Australia) designed to reliably measure reactive oxygen species (ROS) in live cells was used. HMEC-1 cells were plated in black 96-well plates with transparent bottoms at 5×104 cells per well. The cells were allowed to adhere onto the well for 24h before being incubated with various concentration of Dextran-Catechin for 30min, 1h or 6h. The measuring of oxidative stress is according to manufacturer’s instructions using a fluorometer (Wallac VICTOR, PerkinElmer, Massachusetts, USA).
HMEC-1 cells were plated into 6-well plates at a density of 1.25×106 cells/well, respectively. Cells were transfected for 6hours with two different siRNAs (Origene, Rockville, MD, USA) specific for CTR-1 (20nM, Catalog no. SR300931), or ATOX-1 (60nM, Catalog no. SR300333), or a scrambled non-silencing siRNA included in the kit, using Lipofectamine LTX reagent (Invitrogen, Carlsbad, CA, USA). Expression levels of CTR-1 and ATOX-1 protein were monitored for 24hours post-transfection using western blot analysis.
Whole cell extracts were separated by SDS-PAGE (12% poly-acrylamide gels) and transferred to a PVDF membrane using a transfer apparatus according to the manufacturer’s protocols (Bio-Rad). After incubation with 10% skim milk powder in TBST (10mM Tris, pH 8.0, 150mM NaCl, 0.5% Tween 20) for 60min, the membrane was washed once with TBST and incubated with antibodies against CTR-128 (1:500 dilution; rabbit anti-CTR-1, ab129067, Abcam, Melbourne, VIC, Australia), ATOX-1 (1:500 dilution; rabbit anti-ATOX-1, ab154179, Abcam, Melbourne, VIC, Australia), VEGF-R2 (1:1000 dilution; rabbit anti-VEGF-R2, 2479, Cell Signaling Technology, Danvers MA, USA), or GAPDH (1:10,000; mouse anti-GAPDH, Abcam, Cambridge, UK). Incubation with primary antibodies for CTR-1, ATOX-1 and VEGF-R2 was at 4°C overnight and at room temperature for 1h for GAPDH primary antibody. Membranes were washed and incubated with a 1:10,000 anti-rabbit/mouse dilution of horseradish peroxidase-conjugated anti-antibody for 90min. Blots were developed with the Amersham ECL Prime Western Blotting Detection Reagent (GE Healthcare Life Sciences, Rydalmere, Australia), developed in the dark room with X-ray films and analysed using QuanityOne (Version 4.6.9, Bio-Rad, Gladesville, NSW, Australia). CTR-1, ATOX-1, and VEGF-R2 protein expression were normalized to that of the housekeeping protein GAPDH. Blots and additional information about the antibodies are available in Supplementary Materials.
For this study, tumor samples were derived from the animals in our previous work18. Female BALB/c-Fox1nu/Ausb mice, six to eight-weeks old were injected subcutaneously into the right flank with 4×106 human IMR-32 cells suspended in 100μL Phosphate Buffered Solution (HBSS; Invitrogen) and growth factor–reduced Matrigel (BD Biosciences) at a 1:1 ratio. When tumors reached approximately 200mm3, mice were randomised into treatment (300µg/ml of Dextran-Catechin) and control (Saline) group (4 mice per group) and treated once per week for a total of 3 weeks. Tumor size was measured every 3 days using callipers. Tumor volume was calculated using the formula ½×L×W2, where L and W represent the longer and shorter dimension, respectively. Mice were euthanized once tumors reached 1,000mm3, at the time of sacrifice tumor tissue was collected and placed into 4% paraformaldehyde for histologic analysis.
Tissues were formalin fixed, paraffin embedded, and stained immunohistochemically for CD31. The paraffin sections were deparaffinised in xylene and rehydrated in gradient alcohol series. The sections were washed in milliQ water and heated in a microwave in citrate buffer (10mM, pH 6) for 3min and in an oven (104°C) for 15min for epitope retrival. Endogenous peroxidases were blocked using 3% H2O2 in methanol/H2O. Slides were incubated with normal goat serum (10% in PBS) for 1h and incubated with CD31 antibody (1:50 in 1% normal goat serum in PBS) at 4°C overnight. The slides were incubated with anti-rabbit biotinylated antibodies (1:50 in 1% normal goat serum in PBS) for 1h. Sections were washed and incubated with standard avidin-biotin complex (ABC, Vectastain ABC HRP kit, USA) for 45min. DAB (DAKO) was used as chromgen and counterstained was performed with hematoxylin (Vector). Photographic representations were taken randomly around the tumor at 40x magnifications.
All in vitro and in vivo experiments were performed at least in triplicate, statistical analysis were performed by using students t-test, and multiple statistical comparisons between different groups were performed by using one-way ANOVA. All statistical analyses were performed using GraphPad Prism 6 (GraphPad Software, Inc).
O.V. is thankful to the Cancer Institute New South Wales Development Career Fellowship. M.K. is thankful to the National Health and Medical Research Council (NHMRC) Program Grant (APP1091261); Cancer Council NSW Program Grant (PG16-01); NHMRC Principle Research Fellowship (APP1119152). M.K.’s research is conducted and funded in part by the Australian Research Council Centre of Excellence in Convergent Bio-Nano Science and Technology (project number CE140100036). E.Y. is thankful to the University of New South Wales for a Tuition Fee Scholarship (TFS) and to N.K. for a Living Allowance Scholarship. We also thank the University of New South Wales and the Australian Research Council for their financial support.
E.Y. and M.B. Conception and design, acquisition of data, analysis and interpretation of data, Statistical analysis, writing of the manuscript. E.P. Acquisition of data, analysis and interpretation of data, revision of the manuscript. K.K. and G.C. Technical assistance, proof-reading of the manuscript. M.K. Analysis and interpretation of data, proof-reading of the manuscript. N.K. and O.V. Obtained funding, conception and design, acquisition of data, analysis and interpretation of data, study supervision, revision of the manuscript. All authors discussed the results and commented on the manuscript.
The authors declare that they have no competing interests.
Eugene M. H. Yee, Miriam B. Brandl, Maria Kavallaris, Naresh Kumar and Orazio Vittorio contributed equally to this work.
Electronic supplementary material
Supplementary information accompanies this paper at doi:10.1038/s41598-017-07452-w
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