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. 2016 Apr 18;2016:8305073. doi: 10.1155/2016/8305073

Roe Protein Hydrolysates of Giant Grouper (Epinephelus lanceolatus) Inhibit Cell Proliferation of Oral Cancer Cells Involving Apoptosis and Oxidative Stress

Jing-Iong Yang 1, Jen-Yang Tang 2,3,4, Ya-Sin Liu 1, Hui-Ru Wang 5, Sheng-Yang Lee 6,7, Ching-Yu Yen 6,8,*, Hsueh-Wei Chang 5,9,10,11,*
PMCID: PMC4852358  PMID: 27195297

Abstract

Roe protein hydrolysates were reported to have antioxidant property but the anticancer effects were less addressed, especially for oral cancer. In this study, we firstly used the ultrafiltrated roe hydrolysates (URH) derived from giant grouper (Epinephelus lanceolatus) to evaluate the impact of URH on proliferation against oral cancer cells. We found that URH dose-responsively reduced cell viability of two oral cancer cells (Ca9-22 and CAL 27) in terms of ATP assay. Using flow cytometry, URH-induced apoptosis of Ca9-22 cells was validated by morphological features of apoptosis, sub-G1 accumulation, and annexin V staining in dose-responsive manners. URH also induced oxidative stress in Ca9-22 cells in terms of reactive oxygen species (ROS)/superoxide generations and mitochondrial depolarization. Taken together, these data suggest that URH is a potential natural product for antioral cancer therapy.

1. Introduction

Oral cancer is the sixth most common cancer in the world [1, 2]. Although some oral tumor markers had been identified for detection [3], the oral cancer risk was unable to be reduced due to its nontherapeutic function. Oral carcinogenesis is a complex and long-term multifocal process [4]. Therefore, the drugs with chemoprevention are still needed for antioral cancer therapy.

Fish protein hydrolysates from cobia (Rachycentron canadum) [5, 6], tilapia (Oreochromis spp.) [7], grass carp (Ctenopharyngodon idellus) [8], fresh water carp (Catla catla) [9], and other species [10] exhibited the antioxidant property. Furthermore, the roe protein hydrolysates from defatted skipjack (Katsuwonous pelamis) [11], Channa striatus, Labeo rohita [12], Cyprinus carpio, and Epinephelus tauvina [13] had been found to possess the antioxidant property. These antioxidant properties may have the health promoting effects, such as anti-inflammation and antibacterial [14, 15]. However, the anticancer effect of roe protein hydrolysates-derived antioxidants may have different properties and is less addressed.

Drugs and natural products with the antioxidant effects also reported to inhibit cancer cell proliferation. For example, the grape seed extracts [16], red algal methanol extract [17, 18], and red algal ethanol extract [19] had been reported to be antiproliferative to oral cancer cells. Accordingly, the possible antiproliferative effect of roe protein hydrolysates is warranted for further investigation.

Recently, the protein hydrolysates of fish [20, 21], marine [22, 23], and plant [24] sources have been applied to cancer therapy study. For example, fish protein hydrolysates were found to inhibit proliferation of human breast cancer (MCF-7/6 and MDA-MB-231) cells [20]. Fractions from loach protein hydrolysates prepared by papain digestion have been reported to have the antioxidant and antiproliferative activities against colon (Caco-2) cancer cells [21]. Antioxidant and antiproliferative activities also have been reported in protein hydrolysate of blood clam (Tegillarca granosa) muscle against prostate, lung, and cervical cancer cells [22], bioactive peptides from enzymatic hydrolysate of oyster (Saccostrea cucullata) against colon cancer cells [23], and bioactive peptides from chickpea (Cicer arietinum L.) against breast cancer cells [24]. However, the performance of these protein hydrolysates in oral cancer cells remains unclear.

Giant grouper is the largest specie of groupers in Taiwan. The diameter of a fresh roe is from 2 to 3 mm. Due to its fast growth and high price, giant grouper currently is regarded as a favorite species for marine culture in Taiwan [25]. However, during the massive seed production, a large number of roes have been collected because they failed to hatch. To make the use of the protein byproduct, the enzymatic hydrolysis can be implemented to enhance the bioactivities of the roe protein hydrolysates.

Therefore, the subject of this study is to examine the possible antiproliferative function of fish roe hydrolysates of giant grouper (Epinephelus lanceolatus) against oral cancer cells and explore its detailed mechanisms in terms of cell viability, cell cycle analysis, apoptosis, reactive oxygen species (ROS)/superoxide generations, and mitochondrial membrane potential.

2. Materials and Methods

2.1. Preparation of Defatted Roe

Fresh fish roes of giant groupers (E. lanceolatus) were obtained from farm ponds in Pingtung, Taiwan, during July 2013. The samples were placed in ice and transported to the Department of Seafood Science, Kaohsiung Marine University, within 1 h. The whole roes were cleaned using cool water (4°C) and homogenized in a cool room. The homogenized roes were then freeze-dried. Afterward, lipids of the dried roe powders were extracted as described previously [26]. In brief, each 100 g freeze-dried homogenized roes were added to 300 mL hexane for 2 h fat extraction. This procedure was repeated three times. Moreover, the solvents were evaporated by vacuum concentration. The defatted roe protein samples were then freeze-dried. The defatted roe powders were kept in sealed polyethylene bag and then placed at −40°C until use.

2.2. Preparation of Roe Protein Hydrolysate

Roe protein hydrolysate (RPH) was prepared from defatted grouper roe powder using Protease N (Amano Pharmaceutical Co., Nagoya, Japan). The defatted sample (5 g dry matter) was suspended in a 250 mL of pH 8 phosphate buffer. The hydrolysis reaction was initiated by the ratio of Protease N/roe sample at 1 : 100 (w/w solid matter). The reaction was conducted at pH 8 and 50°C for 9 h. The enzymatic hydrolysis was ended by heating the mixtures at 90°C for 10 min to inactivate the protease activity. The solution containing hydrolysate was centrifuged at 5000 g for 10 min at 4°C (05PR-22 centrifuge, Hitachi, Tokyo, Japan). Then, the supernatants were desalted and lyophilized to dried RPH for storage at −40°C.

2.3. Preparation of Ultrafiltrates from RPH through Centrifugal Ultrafiltration Filters

The lyophilized RPH (obtained from 9 h Protease N hydrolysis) was subsequently dissolved in deionized distilled water. The solution containing RHP was processed through centrifugal ultrafiltration (UF) filters (Millipore, Bedford, MA, USA) as described previously [5]. RPH solution (12 mL) was first passed through a centrifugal filter with 10 kDa MWCO and then its permeate was passed through the UF membranes with 5 kDa MWCO. The permeates (ultrafiltrated roe hydrolysates, URH) with molecular size below 5 kDa were obtained. The URH filtrate was lyophilized and stored at −40°C until use.

2.4. Amino Acid Analysis of URH

The URH were hydrolyzed with 6 N HCl at 110°C for 24 h under vacuum. The amino acid analysis was performed using the Pico-Tag system (Waters, Milford, MA) as described [27].

2.5. Cell Cultures

Two human oral cancer cell lines (Ca9-22 and CAL 27) were available from the Japanese Collection of Research Bioresources (JCRB) Cell Bank (National Institute of Biomedical Innovation, Osaka, Japan) and the American Type Culture Collection (ATCC; Virginia, USA), respectively [28]. Cells were maintained in DMEM/F12 (3 : 2) medium (Gibco, Grand Island, NY, USA) supplemented with 10% fetal bovine serum (Gibco), 100 U/mL penicillin, 100 μg/mL streptomycin, and 0.03% glutamine under the humidified incubator at 37°C with 5% CO2.

2.6. Cell Viability

URH was dissolved in culture medium for cell treatment. Cells were plated at 4000 cells/well in 96-well plates. After plating overnight, cells were treated with URH at indicated concentrations (0, 0.25, 0.5, 0.75, 1, 1.5, 2, and 2.5 mg/mL) for 24 h. Then, cellular ATP level was analyzed by the ATP-lite Luminescence ATP Detection Assay System (PerkinElmer Life Sciences, Boston, MA, USA) according to the manufacturer's instructions [29]. Finally, the luminescence was detected using a microplate luminometer (CentroPRO LB 962; Berthold, ND, USA).

2.7. Cell Cycle Distribution

Cellular DNA was detected by propidium iodide (PI) (Sigma, St. Louis, MO, USA) [30]. In brief, 3 × 105 cells per well in 6-well plates were plated overnight. Cells were treated with 0, 0.5, 1, 1.5, 2, and 2.5 mg/mL of URH for 24 h. After harvest, cells were washed with PBS and fixed overnight with 70% ethanol. Finally, the cells were resuspended in 50 μg/mL PI in PBS for 30 min at 37°C in darkness. Cell cycle distribution was determined by a flow cytometer (BD Accuri™ C6; Becton-Dickinson, Mansfield, MA, USA) and a BD Accuri C6 Software (version 1.0.264).

2.8. Apoptosis by Annexin V/PI

The apoptosis-like (sub-G1) status was further examined by annexin V (Strong Biotect Corporation, Taipei, Taiwan)/PI as described [31]. In brief, 3 × 105 cells per well in 6-well plates were plated for 24 h. Cells were treated with the indicated concentrations of URH for 24 h. After drug treatment, cells were incubated with 100 μL binding buffer containing 2 μL of annexin-V-fluorescein isothiocyanate (FITC) stock (0.25 μg/μL) and 2 μL of PI stock (1 mg/mL) for 30 min. Finally, it was suspended with 400 μL PBS for analysis by a flow cytometer (BD Accuri C6) and its software.

2.9. Intracellular ROS

The fluorescent dye 2′,7′-dichlorodihydrofluorescein diacetate (DCFH-DA) was used to detect ROS [19]. 3 × 105 cells per well in 6-well plates in 2 mL medium were plated for 24 h. Cells were treated with different concentrations of URH for 6 h. After PBS washing, 100 nM DCFH-DA in PBS was added to cells in 6-well plates under an incubator for 30 min. After harvest, PBS washing, and centrifugation, cells were resuspended in 1 mL PBS for analysis by a flow cytometer (BD Accuri C6) and its software.

2.10. Intracellular Superoxide

MitoSOX™ Red mitochondrial superoxide indicator (Molecular Probes, Invitrogen, Eugene, OR, USA) was reported to be the fluorescent dye for mitochondrial superoxide [32]. Assessing mitochondrial redox status has been detected by flow cytometric methods [33]. With a slight modification, 3 × 105 cells per well in 6-well plates in 2 mL medium were plated for 24 h. Cells were treated with different concentrations of URH for 1 h. Subsequently, 5 μM MitoSOX was added to cells in 6-well plates under an incubator for 10 min. After harvest, PBS washing, and centrifugation, cells were resuspended in 1 mL PBS for analysis by a flow cytometer (BD Accuri C6) and its software.

2.11. Mitochondrial Membrane Potential (MMP)

MitoProbe™ DiOC2(3) assay kit (Invitrogen, Eugene, OR, USA) was used to measure MMP as described previously [34]. Briefly, 3 × 105 cells in 2 mL medium per well in 6-well plate were plated and incubated for 24 h. Cells were treated with URH treatment for 24 h. Subsequently, 50 nM DiOC2(3) was added per well under an incubator for 30 min. After harvest, cells were resuspended in 1 mL PBS for analysis by a flow cytometer (BD Accuri C6) and its software.

2.12. Statistical Analysis

The significance of differences was evaluated by Student's t-test in SigmaPlot 10 software (Systat Software Inc., San Jose, CA, USA). All data were compared with controls. ∗ and ∗∗, respectively, indicate p < 0.05 and p < 0.001 against control.

3. Results

3.1. Amino Acid Composition of URH

As shown in Table 1, the amino acid composition of URH indicates that URH was composed of full kind of amino acids after purification processes.

Table 1.

Amino acid composition∗ of URH.

Amino acid (%)
Asp + Asn 9.79
Glu + Gln 12.76
Ser 7.11
Gly 7.84
His 1.71
Arg 3.45
Thr 5.55
Ala 11.29
Pro 8.21
Tyr 2.49
Val 6.57
Met 1.67
Cys 0.31
Ile 4.79
Leu 7.58
Phe 2.66
Lys 6.21
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∗Data are the mean values of duplicate determinations expressed as milligram of amino acid per 100 mg of URH.

3.2. Antiproliferation of URH

With the cell viability (%) in terms of ATP content measurement (Figure 1), two oral cancer cells (Ca9-22 and CAL 27) at indicated concentrations of URH were dose-responsively decreased (p < 0.05–0.001 compared to the control). The IC50 values of URH at 24 h treatment for oral cancer Ca9-22 cells were 0.85 mg/mL and IC50 value was undetectable for CAL 27 cells.

Figure 1.

Figure 1

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Cell viabilities of two URH-treated oral cancer cells. Oral cancer (Ca9-22 and CAL 27) cells were treated with 0, 0.5, 0.75, 1, 1.5, 2, and 2.5 mg/mL of URH for 24 h incubation. The cell viability was measured by the ATP assay. Data, means ± SDs (n = 6). ∗ p < 0.05; ∗∗ p < 0.001 against control.

3.3. Morphology Change of URH

The cell morphology of URH-treated oral cancer Ca9-22 cells was shown in Figure 2. The morphological features of apoptosis, including apoptotic bodies and shrinkage of the cells, appeared at higher concentration of URH.

Figure 2.

Figure 2

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Cell morphology of URH-treated oral cancer Ca9-22 cells. Cells were treated with 0, 0.5, 0.75, 1, 1.5, 2, and 2.5 mg/mL of URH for 24 h incubation. Cell images were captured at 100x magnification.

3.4. Cell Cycle Disturbance of URH

As shown in Figure 3(a), the flow cytometry-based cell cycle distribution patterns of URH-treated oral cancer Ca9-22 cells were displayed. After URH treatment (Figure 3(b)), the sub-G1 (%) of URH-treated (0–2.5 mg/mL) Ca9-22 cells were dose-responsively increased (p < 0.001). In contrast, the G0/G1, S, and G2/M (%) of URH-treated Ca9-22 cells were dose-responsively decreased (p < 0.05–0.001).

Figure 3.

Figure 3

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The cell cycle changes of URH-treated oral cancer Ca9-22 cells. Cells were treated with 0, 0.5, 1, 1.5, 2, and 2.5 mg/mL of URH for 24 h. (a) Representative cell cycle distribution patterns of flow cytometry of URH-treated Ca9-22 cells. The cell cycle phases were labeled in each panel. (b) Quantification analysis for the cell cycle phases in Figure 3(a). Data, mean ± SD (n = 3). ∗ p < 0.05 and ∗∗ p < 0.001 against control.

3.5. Annexin V/PI-Based Apoptosis of URH

To further examine the role of apoptosis, the flow cytometry-based annexin V/PI patterns of URH-treated oral cancer Ca9-22 cells were performed (Figure 4(a)). As shown in Figure 4(b), the annexin V-positive intensities (%) for URH-treated (0–2.5 mg/mL) Ca9-22 cells were dose-responsively increased (p < 0.05–0.001).

Figure 4.

Figure 4

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Annexin V/PI-based apoptosis of URH-treated oral cancer Ca9-22 cells. Ca9-22 cells were treated with 0, 0.5, 1, 1.5, 2, and 2.5 mg/mL of URH for 24 h. (a) Representative results of flow cytometry-based annexin V/PI double staining of URH-treated Ca9-22 cells. Annexin V (+)/PI (+) and annexin V (+)/PI (−) were calculated as the apoptosis (+) in each panel. (b) Quantification analysis of apoptosis for URH-treated Ca9-22 cells in Figure 4(a). Data, mean ± SD (n = 3). ∗∗ p < 0.001 against control.

3.6. ROS Generation of URH

Since some apoptosis-inducible drugs were associated with ROS generation [35–38], the role of oxidative stress in URH-treated Ca9-22 cells was examined in terms of ROS detection. As shown in Figure 5(a), the flow cytometry-based ROS staining patterns of URH-treated Ca9-22 cells at 6 h incubation were displayed. As shown in Figure 5(b), the relative ROS-positive intensities (%) of URH-treated (0–2 mg/mL) Ca9-22 cells were dose-responsively induced (p < 0.05–0.001).

Figure 5.

Figure 5

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ROS generation of URH-treated oral cancer Ca9-22 cells. Cells were treated with 0, 0.5, 1, 1.5, and 2 mg/mL of URH for 6 h. (a) Representative ROS patterns of flow cytometry for URH-treated Ca9-22 cells. In each panel, the right side labeled with (+)% indicates the ROS-positive region. (b) Quantification analysis of relative ROS intensity in Figure 5(a). Data, mean ± SD (n = 3). ∗ p < 0.05 and ∗∗ p < 0.001 against control.

3.7. Superoxide Generation of URH

The role of oxidative stress in URH-treated Ca9-22 cells was examined in terms of superoxide detection. As shown in Figure 6(a), the flow cytometry-based superoxide staining (MitoSOX) patterns of URH-treated (0–2.5 mg/mL) Ca9-22 cells at 1 h incubation were displayed. As shown in Figure 6(b), the relative MitoSOX-positive intensities (%) of URH-treated (0–2.5 mg/mL) Ca9-22 cells were dose-responsively induced (p < 0.05–0.001).

Figure 6.

Figure 6

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Superoxide generation of URH-treated oral cancer Ca9-22 cells. (a) Ca9-22 cells treated with 0, 0.5, 1, 1.5, 2, and 2.5 mg/mL of URH for 1 h were stained with MitoSOX dye. The right side labeled with (+)% indicates the MitoSOX-positive region in each panel. (b) Quantification analysis of relative MitoSOX (+) fluorescent intensity (%). Data, mean ± SD (n = 3). ∗∗ p < 0.001 against control.

3.8. MMP of URH

The role of oxidative stress in URH-treated Ca9-22 cells was also examined in terms of MMP by flow cytometry. As shown in Figure 7(a), the MMP staining patterns of URH-treated Ca9-22 cells at 24 h incubation were displayed. As shown in Figure 7(b), the MMP-positive intensities (%) of URH-treated (0–2.5 mg/mL) Ca9-22 cells were dose-responsively decreased (p < 0.001) (Figure 7(b)).

Figure 7.

Figure 7

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MMP change of URH-treated oral cancer Ca9-22 cells. Cells were treated with 0, 0.5, 1, 1.5, 2, and 2.5 mg/mL of URH for 24 h. (a) Representative MMP patterns of flow cytometry for URH-treated Ca9-22 cells. In each panel, the horizontal line labeled with (+)% in the right side indicates the MMP-positive region. (b) Quantification analysis of MMP intensity ((+)%) in Figure 7(a). Data, mean ± SD (n = 3). ∗∗ p < 0.001 against control.

4. Discussion

Fish protein hydrolysates were well-known for the antioxidant property. Although most studies of fish protein hydrolysates had been reported, the possible anticancer effect was less addressed. In current study, we chose the Epinephelus lanceolatus-derived roe hydrolysates (URH) and validated their antiproliferative effect against oral cancer cells. We found that URH induced antiproliferation, sub-G1 accumulation, apoptosis, ROS generation, and mitochondrial depolarization of oral cancer cells.

In the current study, the fish roe protein hydrolysates-derived URH is the ultrafiltration fraction with low molecular weights (MW) (<5 kDa) and it showed that the IC50 values at 24 h treatment for oral cancer Ca9-22 cells were 0.85 mg/mL in terms of ATP assay. The IC30 (70% viability) values of URH at 24 h treatment for oral cancer Ca9-22 and CAL 27 cells were 0.5 and 1.5 mg/mL, respectively. Similarly, the muscle tissue-derived loach (Misgurnus anguillicaudatus) protein hydrolysates (LPH) prepared by papain digestion displayed differential antiproliferative activities against breast, colon, and liver cancer cells for different ultrafiltration fractions with different MW ranges [21]. Based on MTS assay, the IC50 values of LPH-III (MW ranging from 3 to 5 kDa) at 96 h treatment were 33, 15, and 22 mg/mL for breast (MCF-7), colon (Caco-2), and liver (HepG2) cancer cells, respectively. IC50 values of LPH-IV (MW ranging from <3 kDa) at 96 h treatment were 16, 10, and 13 mg/mL for MCF-7, Caco-2, and HepG2 cancer cells, respectively. Accordingly, the LPH fractions with the low MW ranging from <5 kDa (LPH-III and LPH-IV) have detectable IC50 values at 96 h treatment. In contrast, the IC50 values of the LPH fractions with the high MW (5–10 and >10 kDa) were undetectable. Therefore, antiproliferative activities against cancer cells may be varied with different ultrafiltration fractions with different MW ranges. Low MW protein hydrolysates seem to be more potential to anticancer cell proliferation.

The antiproliferative effect of several hydrolysates from different parts of the marine species had been reported in other cancer types such as breast [20], colon, and liver [39] cancers. For example, peptide-rich fish hydrolysates, derived from fresh filleting by-products or headed and gutted by-catches of blue whiting, exerted a significant antiproliferative activity at 1 mg/mL for 72 h treatment with growth inhibition of 22.3–26.3% on breast cancer MCF-7/6 cells and 13.5–29.8% on breast cancer MDA-MB-231 cells using MTS assay [20]. Because these protein hydrolysate studies mentioned above were derived from different parts and species of fishes and they were treated with different incubation times, it was suitable to compare their drug sensitivity between each other. In general, our experiment was performed in shorter treatment time and displayed the lower IC50 values of fish protein hydrolysates (URH) in inhibiting proliferation of oral cancer cells. It is also possible that drug sensitivity of fish protein hydrolysates in anticancer cell effect may be cancer cell-type dependent. Moreover, it was warranted for further investigation that the fish protein hydrolysates from roe and other parts may have different potentials for antiproliferation of oral cancer cells.

Protein hydrolysates from many species were reported to have the antioxidant property [5–13]. The dual roles of antioxidants can explain why protein hydrolysates with antioxidant property also display anticancer effect [40]. Oxidative stress had been reviewed to regulate the endoplasmic reticulum stress [41], autophagy [42], and apoptosis [43], leading to cell death. For exogenous antioxidants, it may behave like the double-edged swords in cellular redox state; that is, it is protective at physiologic doses but it is harmful at high doses [40]. In current study, we provided evidence for the apoptosis effect of URH in oral cancer Ca9-22 cells, such as sub-G1 accumulation and annexin V/PI staining (Figures 3 and 4), which were coupled with high ROS, superoxide generations, and mitochondrial depolarization; that is, the correlation values (R 2) are 0.8435, 0.6294, and 0.6782 for ROS (+), mitoSOX (+), and MMP (−) versus apoptosis (annexin V (+)), respectively, although the effect of lower doses of URH was not examined in our study. Similarly, the grape seed extract (GSE) displayed the normal proliferation at low doses but demonstrated the antiproliferation for oral cancer cells at high doses [16]. Moreover, GSE at high doses displayed high ROS generation and mitochondrial depolarization than those of the low doses [16]. Therefore, the differential oxidative stress may partly contribute the dual roles of antioxidants.

5. Conclusion

URH is the ultrafiltration fraction of fish roe protein hydrolysates with low MW. In current study, we firstly demonstrated that URH can inhibit cell proliferation of two oral cancer cells (Ca9-22 and CAL 27). URH also induced the characters of apoptosis of oral cancer cells such as apoptotic morphology change, sub-G1 accumulation, and annexin V/PI positive expression. This antiproliferative mechanism includes the ROS and superoxide generations and mitochondrial depolarization. Therefore, these results suggest that URH has an apoptosis-based anticancer potential for oral cancer therapy.

Acknowledgments

This work was supported by funds of the Ministry of Science and Technology (MOST 104-2320-B-037-013-MY3), the National Kaohsiung Marine University Research Project (NKMU-9910286), Kaohsiung Medical University “Aim for the Top Universities Grant, no. KMU-TP104PR02,” the National Sun Yat-sen University-KMU Joint Research Project (no. NSYSU-KMU 105-p002), the Kaohsiung Municipal Ta-Tung Hospital (kmtth-104-003), the Health and Welfare Surcharge of Tobacco Products, the Ministry of Health and Welfare, Taiwan, Republic of China (MOHW105-TDU-B-212-134005), and ChiMei-KMU Joint Project (104CM-KMU-02).

Competing Interests

The authors declare no competing interests.

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