Granulin Secreted by the Food-Borne Liver Fluke Opisthorchis viverrini Promotes Angiogenesis in Human Endothelial Cells

Introduction

Infection with the fish-borne liver flukes Opisthorchis viverrini, Opisthorchis felineus, and Clonorchis sinensis remains a major public health problem in East Asia and Eurasia with >40 million cases. O. viverrini is endemic in regions of Thailand, Cambodia, Lao PDR, and Vietnam (1), and opisthorchiasis has been extensively studied in Thailand where ~8 million people are infected, calculated from nation-wide prevalence of 9.4% for the Thai population in 2001 (2, 3). Eating undercooked fish infected with the metacercariae stage of the fluke leads to infection in humans and other mammals, such as cats and dogs (1). The metacercarial stage of the parasite excysts in the duodenum and the juvenile fluke migrates into the bile ducts of the liver and matures over a month into an adult fluke, which grazes on biliary epithelia. The parasites are long lived, and often persist in the biliary tree for decades (1, 3). Fluke eggs are shed into the bile and exit with the fecal stream (1). Eggs that enter fresh water ecosystems can be ingested by the gastropod snail Bithynia siamensis (2, 4). The parasite develops within the snail, in turn releasing cercariae that seek out and penetrate the skin of a cyprinid fish, which encyst in the fish as a metacercaria, the infective stage for humans and other definitive host species (1).

Infection causes hepatobiliary disease, including cholangitis and periductal fibrosis (1). More problematically, both experimental and epidemiological evidence strongly implicates liver fluke infection in the etiology of cholangiocarcinoma (CCA), commonly known as bile duct cancer—one of the major liver cancer subtypes (1, 5). Up to 81% of liver cancers in the endemic Isaan region in north-eastern Thailand are CCA, which also suffers the world’s highest incidence of CCA—65 times the rate experienced in non-endemic regions (1, 5, 6). CCA is an adenocarcinoma that generally exhibits slow growth and which is diagnosed at advanced stage often with metastasis to distant sites due to proximity to lymphatic vessels (4). Unfortunately, prognosis is dismal at the advanced stage when the primary tumor is no longer amenable to liver resection. The mechanism(s) by which infection initiates genetic lesions that eventually culminate in CCA is unclear, but it likely involves biliary tract and systemic inflammation, inflammation associated endogenous and dietary nitrosation, and secretion of mitogens and other by the liver fluke.

One aspect of liver fluke infection that is potentially involved in malignant transformation is the excessive, unremitting wound healing in response to continued feeding by the parasites on bile duct tissue (2, 3, 5). We have shown that the granulin-like growth factor, Ov-GRN-1, secreted by the fluke is the dominant proliferative factor and is sufficient to drive wound healing (2, 7). A critical step in new tissue generation, including wound healing and tumor growth induced by the infection, is the stimulation of angiogenesis—the formation of new capillaries from pre-existing blood vessels or vasculogenic stem cells (8). New tissue requires angiogenesis to supply oxygen and nutrients, facilitate immune surveillance, and remove waste products (9). A complex interplay of growth factors and inhibitors regulates angiogenesis and imbalance can lead to disease (10). While angiogenesis does not itself initiate malignancy, it can promote tumor progression and metastasis (9, 11). Angiogenic cytokines, including fibroblast growth factor, vascular endothelial growth factor (VEGF), platelet-derived growth factor, and epidermal growth factor (9, 10), stimulate endothelial cells or precursors to proliferate and migrate, leading rapidly to new capillaries and blood vessel networks.

The tubule formation assay (TFA) provides an informative, convenient, rapid, and quantifiable approach to investigate angiogenesis (12). The TFA involves endothelial cell adhesion, migration, proteolysis, and tubule formation by the endothelial cells, which is initiated following seeding of the cells onto gelled basement matrix, the natural substrate of endothelial cell progenitors. The endothelial cells form capillary-like structures with a lumen (12). Recombinant Ov-GRN-1 (rOv-GRN-1) induces angiogenesis (blood vessel growth) in quail embryos in the chorioallantoic membrane (CAM) assay (2). However, the angiogenic potential of liver fluke granulin on human cells has not been determined. Herein, we report potent angiogenic and mitogenic activity of Ov-GRN-1 at nanomolar concentration on primary human umbilical vein endothelial cells (HUVECs) using both a high-throughput TFA with automated ImageJ-based analyses and with the xCELLigence system real-time cell assay.

Materials and Methods

Ov-GRN-1 Recombinant Production

Purification of rOv-GRN-1 was achieved using an AKTA10 purification system at 4°C (GE Healthcare) as previously described (2, 13). Briefly, BL21 E. coli bacterial pellet containing the rOv-GRN-1 expression plasmid was lysed with three freeze/thaw cycles followed by sonication. The resulting insoluble pellet was solubilized in urea-containing nickel binding buffer [8 M urea/300 mM NaCl/50 mM imidazole/50 mM sodium phosphate pH 8 (Sigma)]. The 0.22-µM-filtered supernatant was passed over 2 × 5 ml Histrap IMAC nickel columns (GE Healthcare) and washed with increasing imidazole concentrations and eluted with 500-mM imidazole in binding buffer. Refolding of urea-denatured rOv-GRN-1 was performed with 28 ml of G10 Sephadex resin on a XK16/20 column (GE Healthcare) with 7 ml applied at 100 µg/ml and eluted with 150-mM NaCl, 50-mM sodium phosphate, pH 6. A 120-ml Superdex 30 XK16/60 column (GE Healthcare) was used to fractionate rOv-GRN-1 monomer eluting at a folded size equivalent to ~1 kDa. Protein concentration was determined by a combination of microplate Bradford assay (Bio-Rad) according to the manufacturer’s instructions and optical density at 280 nm.

Human Umbilical Vein Endothelial Cells

Human umbilical vein endothelial cells pooled from donors (PromoCell, Heidelberg, Germany) were cultured in T75 tissue culture flasks in complete EGM-2 medium (PromoCell) at 37°C in a humidified atmosphere in 5% CO₂ in air. HUVECs were grown to ~80% confluence, after which the culture was trypsinized using the PromoCell Detach Kit (PromoCell). The cells investigated by tubule formation assay (TFA) were used from the third, fourth, or fifth passage only, with HUVEC passaged to ~80% confluence within 24 h of the TFA, as described (14).

Proliferation xCELLigence Assay

Cells were seeded at 5,000 cells per well in 200 µl of complete media (above) in E-plates (ACEA Biosciences, San Diego, CA, USA) and grown overnight while monitored with an xCELLigence DP system (ACEA Biosciences) which monitors cellular events in real time by measuring electrical impedance across interdigitated gold micro-electrodes integrated on the bottom of tissue culture plates. Cells were washed three times with PBS and replaced with 180 µl EGM-2 basal media (no growth factors or supplements) and incubated for a minimum of 6 h before further treatment. Treatments were prepared at 10 × concentrations and added to each well in a total volume of 20 µl. The xCELLigence DP recorded cell index readings every 15 min for 3 days after treatment. Cell index readings were normalized before treatment and cell proliferation ratios were determined from four biological replicates and represent the relative numbers of cells compared to control cells. A two-way ANOVA with Holm–Sidak’s multiple comparisons test was used to compare Ov-GRN-1 treatment to medium-alone control, with P ≤ 0.05 deemed significant.

Tubule Formation Assay (TFA)

Growth factor-reduced Matrigel (Corning, Corning, NY, USA) was plated into a 96-well μ-angiogenesis plate (ibidi, Planegg, Germany) at 10 μl/well, and incubated at 37°C in 5% CO₂ in air for 60 min as described (14). HUVECs were detached (above) and resuspended in complete endothelial cell growth medium 2 (EGM-2) (PromoCell), and seeded at 10,000 cells/well in medium supplemented with 10 µM sulforaphane (SFPH, Sigma) (negative control), 1.2 nM VEGF-165 (Novus Biologicals) (positive control), or 5, 10, 20, and 40 nM Ov-GRN-1. The ibidi plate was incubated for 12 h in a humidified atmosphere of 5% CO₂ in air at 37°C in a microscope stage top incubator (OKOLAB, Pozzuoli, Naples, Italy). At intervals, photomicrographs of cells and nascent and developed tubules were collected using a Leica DMi8 automated platform microscope under bright field at 2.5 × magnification, and Leica LASX software (Leica).

Analysis of Tubule Formation

Automated angiogenesis assessment was performed on TFA 490² pixel images by ImageJ (NIH) with the phase-contrast Angiogenesis Analyzer plugin tool as described (12, 15). Settings used were as follows: 10 pixel minimum object size; 25 pixel minimum branch size; 2,500 pixel artifactual loop size; 25 pixel isolated element size threshold; 30 pixel master segment size threshold; with iteration number of 3. The four output metrics (mesh count, segment count, segment length, and junction count) were either plotted directly or as a percentage relative to the medium-alone blank treatment (treatment measure divided by medium-alone measure). A two-way ANOVA with Holm–Sidak’s multiple comparisons test was used to compare Ov-GRN-1 treatment against medium-alone blank control for the four metrics with P ≤ 0.05 deemed significant.

Combining the four metrics into a single evenly weighted variable was accomplished through the calculation of Z standardized scores that were based on population values (16). The formula below generates the Z score and represented the distance between the raw score and the population mean in units of the SD. Population values were estimated from 39 treatment replicates.

$Z=(\text{treatment metric value}-\text{metric population mean})\text{/population standard deviation}$

The combined robust Z score (Z*) was generated for each replicate from the median Z score of the four metrics. Z* scores were plotted and Ov-GRN-1 treatments compared to medium-alone blank control using one-way ANOVA with Holm–Sidak’s multiple comparisons test, P ≤ 0.05 was considered to be statistically significant.

Results

To assess the influence of Ov-GRN-1 on HUVEC compared with other cell types, we analyzed HUVEC cellular proliferation and migration with the xCELLigence system. Treatment with Ov-GRN-1 induces proliferation in a range of cell types (2, 4, 17). Exposure of HUVEC to 5–20 nM Ov-GRN-1 showed a similar response (Figure 1). As the angiogenic assay with HUVECs would be assessed at 12 h, for proliferation, we focused on the first 24 h and noted minor (5–11%) non-significant increase above values of negative controls from 5 to 10 nM Ov-GRN-1 (Figure 1B). Twenty nanomolars were sufficient to induce a significant 14% increase in cell index from 4 h (*P < 0.05) that had expanded to 29% by 24 h (****P < 0.0001), indicative of proliferation (Figure 1B). Cell migration has also been reported with bile duct cells from Ov-GRN-1 treatment (2, 3). In contrast to induction of proliferation, our HUVEC tests with 10–100 nM Ov-GRN-1 using CIM e-plates (cell invasion and migration xCELLigence plates) did not reveal an increase in migration compared to controls (data not shown).

FIGURE 1

Figure 1. Cell proliferation induction by Ov-GRN-1 with human umbilical vein endothelial cells (HUVECs). (A) Normalized cell index (nCI) output of the xCELLigence system of treatments of 5–20 nM Ov-GRN-1 on HUVECs cells over 70 h. (B) nCI relative to medium only negative controls (0 nM Ov-GRN-1) from (A) is plotted to highlight the first 24 h after treatment. RM two-way ANOVA with Holm–Sidak’s multiple comparison test of Ov-GRN-1 treatment vs medium only control at each time point: ns = not significant; *P < 0.05; **P < 0.01; ***P < 0.001; ****P < 0.0001. Data points are average values of four biological replicates and have been nudged ±0.2–1 h to ensure that SE bars are visible.

The TFA angiogenesis was used to assess the ability of rOv-GRN-1 to induce capillary-like tubule structures from endothelial cells. The three main characteristics considered for angiogenic stimulation in the TFA are highlighted in Figure 2A—tubule “segments” branch at “junctions” and combine to enclose a “mesh.” Ten (10) micromolar SFPH negative control revealed an ablated tubule network, as reported in other studies (18), whereas positive control VEGF at 1.2 nM strongly stimulated a network of tubules compared to the medium only group (19) (Figure 2A).

FIGURE 2

Figure 2. Angiogenic screening with primary human umbilical vein endothelial cells. Cells are seeded and treatments applied at time zero. Images are taken at 12 h and assessed in ImageJ for angiogenic properties. (A) Representative images depict the control treatments at 50× magnification: medium only; anti-angiogenic negative control [10 µM sulfurophane (SFPH)]; pro-angiogenic positive control [1.2 nM vascular endothelial growth factor (VEGF)]. The VEGF zoom overlay shows the boxed VEGF section magnified with angiogenic features overlaid: A mesh (blue) is bordered by four tubule segments (red dotted lines) that join at four branching junctions (green circles). (B) Representative images of 5–40 nM Ov-GRN-1 treatments at 50× magnification. (C) Automated mesh count quantitation of control and Ov-GRN-1 treatments represent network complexity. The mean is marked as a horizontal bar with SE bars from 3 to 9 biological replicates plotted as circles.

The automated ImageJ angiogenesis plugin analysis measures both topological features that represent network complexity (meshes and branching junction points) and morphometric descriptors that are dimensional and considered the principal angiogenic in vitro response (tubule segment number and total tubule segment length) (8). Ov-GRN-1 treatments show a concentration dependent increasingly complex tubule mesh network (Figure 2). The mesh count raw data (Figure 2C) show that 40 nM Ov-GRN-1 increased the mesh count from the medium only control of 9.7–15.7 meshes—a highly significant (P < 0.0001) relative increase over the blank control of 62% (Figure 3A). In addition, 10 and 20 nM Ov-GRN-1 increased the mesh count to a lesser degree—35% increase (P < 0.01) and a 20% increase (non-significant), respectively. While the number of branching junctions (Figure 3B) increased slightly (13–18%) with 10–40 nM Ov-GRN-1 treatments, none of these changes were significantly different to the medium only control. The dimensional measures both showed slight increases of 8–18% with 10–20 nM but only significant increases from 40 nM Ov-GRN-1 treatment (Figures 3C,D). The number of tubule segments increased by 31% (P < 0.01) and the associated total length of the tubule segments increased by 27% (P < 0.05) to the medium only control. The 5 nM Ov-GRN-1 treatment showed almost no difference (non-significant minor reductions of 5–8%) for all four metrics relative to medium only controls.

FIGURE 3

Figure 3. Angiogenic metrics from Ov-GRN-1 treatments. ImageJ was used to quantify 12-h time point images for various characteristics of the tubule networks. Treatments consist of the blank control (medium only); anti-angiogenic negative control [10 µM sulforaphane (SFPH)]; pro-angiogenic positive control [1.2 nM vascular endothelial growth factor (VEGF)]; and 5–40 nM Ov-GRN-1 treatments and are plotted relative to the blank (medium only) control treatment. (A) Topological features representing an increase in complexity of the tubule network are measured by the relative number of meshes and (B) branching junctions. (C) Dimensional descriptors of the networked tubules include the number of tubule segments and (D) the total combined length of the tubule segments. All panels: two-way ANOVA with Holm–Sidak’s multiple comparisons test to compare Ov-GRN-1 treatment to medium only blank control: ns = not significant; *P < 0.05; **P < 0.01; ****P < 0.0001. The mean is marked as a horizontal bar with SE bars from 3 to 9 biological replicates plotted as circles. Dotted line crosses the medium only blank 100% value.

To assess the angiogenic potential of Ov-GRN-1 treatments the four metrics were converted to Z-scores and combined into a single median robust Z score (Z*) for each replicate (Figure 4). The Z* score incorporates differences from the total population mean and population variation. This dimensionless variable is a useful equally weighted mechanism to combine metrics with different means and variations into a single composite variable for statistical comparisons. Comparing the Z* scores to the medium only controls (Figure 4) showed 10–40 nM Ov-GRN-1 induced increased angiogenesis but only 10 and 40 nM showed significant increases (P < 0.05 and P < 0.001, respectively). As noted with the four separate metrics, 5 nM Ov-GRN-1 did not stimulate angiogenesis.

FIGURE 4

Figure 4. Angiogenic induction from Ov-GRN-1 treatments. Converting the four angiogenic metrics (meshes, junctions, segments, and segment length) to dimensionless Z-scores allows a pooled median value for each replicate (Z* score) to be generated. This enables the total angiogenic effect to be compared between groups. One-way ANOVA with Holm–Sidak’s multiple comparisons test to compare Ov-GRN-1 treatment to medium only blank control: ns = not significant; *P < 0.05; **P < 0.01; ***P < 0.001. The mean is marked as a horizontal bar with SE bars from 3 to 9 biological replicates plotted as circles. Dotted line crosses the medium only blank −0.28 Z* score.

Discussion

Angiogenesis describes the growth of new vasculature and is a process that has been the subject of significant historical interest due to its involvement in a spectrum of diseases (10, 20, 21). During development new blood vessels are essential and angiogenesis is rapid (9, 10). In the fully developed adult, as part of physiologic processes such as wound healing, angiogenesis is turned on, but only transiently (9, 10). Over a century ago, studies demonstrated that the mechanisms of tumor growth and spread are intimately linked to the formation of new blood vessels from pre-existing larger blood vessels (10). Subsequently, it was determined that as this process occurs, the “angiogenic switch” is almost always activated and remains on, causing normally quiescent vasculature to sustain expanding neoplastic growths (9).

Molecular angiogenic studies have focused on VEGF, as many angiogenic factors induce signals that result in blood vessel signaling that ultimately rely on VEGF (10, 21, 22). Recent reports focus on angiogenic signaling via VEGF-independent mechanisms and associated problems with VEGF inhibitors for cancer treatments (23–26). One such alternate pathway that is not blocked by VEGF inhibitors is driven by human progranulin, a growth factor comprised of 7.5 granulin active domains (24, 27). The individual human granulin units are difficult to produce actively (28) but Ov-GRN-1 is produced by liver flukes as a single unit, and is bioactive when purified from denatured bacterial recombinant expression systems and refolded (17). Previously, we have shown that Ov-GRN-1 is a potent growth factor that stimulates human cell proliferation, migration, avian angiogenesis, and ultimately mouse wound healing (3, 4, 7, 17). Ongoing research suggests the potential for beneficial therapies emanating from pathophysiological investigation of granulins, including anti-tumor action and promotion of wound healing (7, 29, 30).

The avian CAM assay is an informative in vivo model of angiogenesis (31). The CAM assay is based around blood vessel induction in avian embryos and results may not traverse phylogenetic boundaries and apply to mammalian systems. With this consideration ensuring the parasite growth factor Ov-GRN-1 stimulated human angiogenesis is a useful step toward developing therapeutics (2, 7, 10, 32). Herein, we focused on angiogenesis screening using HUVEC and the tubule formation assay (TFA) with automated imaging in real time (14). The TFA involves a range of the angiogenic processes that includes endothelial cell adhesion, migration, protease activity, and tubule formation (14). The advantages of the TFA to study angiogenesis are the ease of set up, short culture period, the ability to produce quantitative data, and its ease of adaptation toward high-throughput analysis. The automated TFA analysis allows comparison of both topological features that represent network complexity and morphometric dimensional descriptors that are considered the principal angiogenic in vitro response (8). This depth of analysis combined with the high-throughput capability allows a greater range of treatments to be tested than the labor-intensive and subjectively scored CAM assay.

Human liver epithelial cells (H69 bile duct cell line) hyper-proliferates at Ov-GRN-1 concentrations of 12 nM and above (7). Although the cell types were different, we note that Ov-GRN-1 is able to stimulate significant HUVEC proliferation and angiogenic stimulation at similar concentrations of at least 20 nM and 10 nM, respectively (Figures 1 and 4). Sample limitations restricted the Ov-GRN-1 TFA maximum concentration to 40 nM, but as the trend appeared to be dose dependent we predict that higher concentration would induce further angiogenesis, and plan to assess in the future. Mesh counts showed the most marked rise with a 62% highly significant increase (P < 0.0001) with 40 nM Ov-GRN-1, whereas the junction counts trended up (13–18%) but did not reach statistical significance (Figure 3). Whether the outcome related to the Ov-GRN-1 mechanism is not clear, but these phenomena may be an artifact of the TFA mechanics. A junction is the end point of at least three segments, and more may radiate from the connecting junction. Increased junction branching was evident with 40 nM Ov-GRN-1, a small increase in junctions (18%) but about double the increase in tubule segments (31%) was observed. The increase in segments can in turn enhance the mesh count, as a single segment tubule can grow across a mesh and split it into two smaller meshes; our estimated mesh numbers increased 62%. To explore this junction/mesh outcome further and delve into the angiogenic activity of Ov-GRN-1, we plan to test other aspects of angiogenesis, including apoptosis, and to employ three-dimensional cell culture systems that more closely reflect the in vivo situation (19, 33). Furthermore, future studies will explore the Ov-GRN-1 proliferative and signaling responses of HUVECs to compare with our previous work (2) that showed the transcriptional responses of Ov-GRN-1 treatment on the H69 bile duct cell line. The most relevant to Ov-GRN-1 transcriptional response to angiogenesis we observed in the H69 cells was the stimulation of CXCL1, 2, 5, and 8—chemokines that signal through CXCR2, a receptor with complex signaling interactions but often resulting in angiogenesis among other outcomes such as inflammation (22, 34).

Whereas the origin of helminth and host cell communication is unknown, the process likely evolved to facilitate parasitism (35). Metabolites participating in communication signaling may, however, contribute to carcinogenesis (1, 35). The close homology between liver fluke and human granulins may enable secreted Ov-GRN-1 to activate signaling pathways that promote angiogenesis and wound repair of bile ducts damaged by the activities of the parasite (4). The stimulation of wound healing potentially evolved for successful parasitism and a concomitant productive host–parasite relationship (2, 7). Other helminth parasites release mediators that promote angiogenesis, and from an evolutionary perspective, Opisthorchis-induced neovascularization may be beneficial to parasitism (35, 36). However, given that angiogenesis represents a hallmark of cancer, the angiogenic potency of Ov-GRN-1 may also contribute to liver fluke infection-induced malignancy (2, 30, 35).

The current findings confirmed potent angiogenic signaling of liver fluke with nanomolar levels of granulin and expand upon previous reports using an in vivo CAM assay (2). Liver fluke granulin likely contributes to the carcinogenicity of liver fluke infection in the human biliary tract (2, 35, 36). On the other hand, it also holds marked potential as a therapeutic wound-healing agent and as a vaccine against the liver fluke infection-induced cancer (2, 7, 35).

Author Contributions

Study conception: PB, MS, and AL; performed experiments: BH, SK, and VM; data analysis: AP, MS and BH; data presentation: MS; manuscript preparation: MS, BH, SK, and PB; manuscript editing: MS, AL, BH, SK, VM, and PB; Supervision: AP, PB and MS, and Funding acquisition: PB and AL.

Conflict of Interest Statement

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.

Acknowledgments

We thank Drs. Carolyn Cousin and Matty Knight for their support and advice. Support from award CA164719 from the National Cancer Institute, National Institutes of Health (NIH) is gratefully acknowledged. Part of this study was performed in the GW Nanofabrication and Imaging Center. The content is solely the responsibility of the authors and does not necessarily represent the official views of the NIH.

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