Characteristics, Functional Properties, and Antioxidant Activities of Water-Soluble Proteins Extracted from Grasshoppers, Patanga succincta and Chondracris roseapbrunner

Water-soluble proteins extracted from two species of grasshoppers, Patanga succincta (WSPP) and Chondracris roseapbrunner (WSPC), were characterized as well as their functional properties and antioxidant activities were investigated.)e extraction yield, on a wet weight basis, was 7.35% and 7.46% for WSPP and WSPC, respectively. )e most abundant amino acid in both proteins was glutamic acid, followed by aspartic, alanine, and leucine, in that order. )e electrophoretic study revealed that proteins with MW of 29, 42, 50, 69, and 146 kDa were the major protein components in WSPP and WSPC. FTIR analysis showed that those proteins remained their structural integrity. )e surface hydrophobicity at pH 7 of WSPC was higher than WSPP, but the sulfhydryl group content did not show significant difference between the proteins from two species. Both grasshopper proteins were mostly soluble in strong acidic and alkaline aqueous solutions with a minimum value at pH 4.)ose proteins exhibited poor emulsifying properties and foaming capacity, but they had greater foaming stability compared with bovine serum albumin (BSA) (p< 0.05). WSPC showed greater DPPH and ABTS scavenging activities and ferric-reducing antioxidant power (FRAP) than did WSPP (p< 0.05). )erefore, based on characteristics and functional properties, water-soluble proteins from both edible grasshoppers can be used as an ingredient in food applications.


Introduction
In 2050, the world population is estimated at more than 9 billion people, resulting in an additional need for food and feed outputs [1]. Conventional sources of protein will not be sufficient for the global human population, and alternative sources such as insects will be required [2]. Approximately 1,900 species of edible insects are traditionally consumed in many parts of the world, for example in Africa, Asia, and Latin America, and are considered as having potential to contribute to the world's food security [3]. In countryside of Northern and Northeastern ailand, people consume several species of insects including grasshoppers, crickets, beetles, silkworm pupae, and bamboo worm. Edible insects offer an important source of minerals, lipids, and above all proteins. Edible insects have higher crude protein content and have been reported to be a good source of essential amino acids [4]. Currently, most insect consumption is as a component ingredient of processed foods, and their successful utilization depends on fulfilling one or more functional requirements of good solubility, emulsion/foam capacity and stabilization, and gel formation [5,6]. Omotoso [7] evaluated the functional properties of the larvae of Pallid Emperor Moth (Cirina forda) and found that they had good solubility and emulsion properties. Yi et al. [8] reported poor foam and gelling properties of five different acid-extracted insect proteins, including those from a cricket (Acheta domesticus). Kim et al. [9] determined the effects of adding flour made from defatted mealworm larvae (Tenebrio molitor) and defatted silkworm pupae (Bombyx mori) and found that the added insect flours increased their cooking yield and hardness on emulsion sausages. Park et al. [10] also found that adding transglutaminase to silkworm pupae flour resulted in improved physicochemical properties of meat batter.
From previous reports, 32 insect species have been evaluated for their nutrition value in ailand [11]. eir protein content ranged from 6.12 to 25.88 g/100 g wet weight, and their fiber levels ranged from 1.00 to 12.42 g/100 g wet weight [12,13]. Yang et al. [14] reported polyunsaturated fatty acid content of 6 species of edible insects from ailand to range from 726 to 2883 mg/100 g and monounsaturated fatty acid content to range from 714 to 5889 mg/100 g. is leads to the fact that edible insects are a potential source of fat and protein, but there is limited information on the characteristics and functional properties of extracted edible protein from specific insects. e aim of this investigation was, therefore, to characterize and compare the functional properties as well as antioxidant activities of water-soluble proteins from two species of grasshoppers (P. succincta and C. roseapbrunner), commonly found in ailand, for their potential use as an alternative source of protein in food ingredients.

Materials. Frozen Bombay Locust (P. succincta) and
Spur-throated grasshopper (C. roseapbrunner) were obtained from a commercial supplier (Mr. BUC FOOD, Phra Nakhon Si Ayutthaya, ailand). ese two species were selected, because they are well known, cheaper, and easily available in ailand and are reported to have high protein content [11,15].

Samples Preparation.
e grasshopper samples were thawed and washed with running portable tap water, rinsed with distilled water, and drained using a plastic sieve for 1 h. e prepared samples were then stored in plastic containers at −20°C until further experiments.

Protein Extraction.
e grasshopper proteins were extracted using an adapted extraction method of Yi et al. [8].
e insects were first blended with cold water (4°C) at a ratio of 1 : 4 w/v for 15 min using a blender (MMB54G5S, BOSCH, Germany) and stirred overnight at 4°C using a magnetic stirrer, to ensure that the proteins were dissolved. e suspension was centrifuged at 12,500 × g for 30 min at 4°C. e upper layer, containing the lipid fraction, and undissolved debris layer were removed. e supernatant or middle layer was collected, freeze-dried, and referred to as "WSPP" and "WSPC" for the protein from P. succincta and C. roseapbrunner, respectively. Extractions were performed in triplicate, and the protein content of the extracts was measured by the Kjeldahl method [16].

Calculation of Extraction Yield and Efficiency.
e yields of WSPP and WSPC were calculated as a percentage of the weight of WSPP and WSPC in comparison with the weight of grasshoppers before extraction, as follows: Extraction efficiency was calculated as a percentage of the total protein extracted from P. succincta and C. roseapbrunner for WSPP and WSPC, respectively, in comparison with that of its protein content, which was determined by the Kjeldahl method [16]. e extraction efficiency of each WSPP and WSPC was calculated as follows: total extracted protein of WSPP or WSPC(g) total protein content of grasshoppers(g) × 100. (2)

Amino Acid Composition.
e amino acid compositions of WSPP and WSPC were determined by the Central Instrument Facility at Mahidol University, Bangkok, ailand. Analysis was performed using HPLC (Waters Alliance 2695 with heater, Jasco FP2020 fluorescence detector (EX: 250 and EM: 395 nm)) with a Hypersil Gold column C18 (4.6 × 150 mm, 3 µm) at 35°C. Amino acid standards (Sigma-Aldrich, USA) were used for calibration.

Sodium Dodecyl Sulfate-Polyacrylamide Gel Electrophoresis (SDS-PAGE)
. SDS-PAGE was performed according to the method of Laemmli [17] with slight modifications. e samples (3 g) were mixed with 27 mL of 5% (w/v) SDS, heated at 85°C for 1 h, and then centrifuged at 8,500 × g for 5 min at 25°C using a centrifuge (5804 R Eppendorf, Germany) to remove undissolved debris. e supernatant was collected and mixed at 1:1 (v/v) ratio with the sample buffer (0.5 M Tris-HCl, pH 6.8, containing 4% (w/v) SDS, 20% (v/v) glycerol and 0.3% (w/v) bromophenol blue) for nonreducing condition and in the presence of 10% (v/v) β-ME for reducing condition. Samples (15 µg protein, determined by the biuret method) were loaded onto a polyacrylamide gel made of 10% separating gel and 4% stacking gel and subjected to electrophoresis at a constant current of 20 mA/gel, using an electrophoresis apparatus (AE-6440, Atto Co., Tokyo, Japan). After electrophoresis, gels were fixed with a mixture of 50% (v/v) methanol and 10% (v/v) acetic acid for 45 min, followed by staining with 0.05% (w/v) Coomassie Blue R-250 in 15% (v/v) methanol and 5% (v/v) acetic acid overnight with constant shaking. Finally, gels were destained with the mixture of 30% (v/v) methanol and 10% (v/v) acetic acid until a clear background was obtained. e molecular weight protein standard markers, using Precision Plus Protein ™ Unstained Standard (10-250 kDa) (Bio-Rad, CA, USA), were run in the same manner and used to estimate the molecular weight of proteins. Gels were imaged using a scanner (MFC-L2700DW, Brother, UK), and band intensities were quantified with the public domain digital analysis software, ImageJ (ImageJ 1.51t, National Institutes of Health, Bethesda, USA).

Fourier Transform Infrared Spectroscopy (FTIR).
FTIR spectra of WSPP and WSPC were determined by Scientific Instrument Centre at King Mongkut's Institute of Technology Ladkrabang, Bangkok, ailand. Analysis was performed using a Nicolet Model Nicolet 6700 FT-IR Spectrometer ( ermo Scientific, Germany) from 400 to 4000 cm −1 with automatic signal gain at 25°C. e spectra were collected in 32 scans at a resolution of 4 cm −1 and evaluated against a background spectrum from a clean empty cell.

Determination of Surface Hydrophobicity (H 0 ).
Surface hydrophobicity of the protein samples was determined using a fluorescence probe 1-anilino-8naphthalenesulfonate (ANS) following the method described by Malik et al. [18] with some modifications. e protein solution was prepared at concentrations in the range of 0.05-0.5 mg/mL with a phosphate buffer (0.1 M, pH 7). 20 µL of ANS (8.0 mM in phosphate buffer 0.01 M, pH 7) was added to 4 mL of protein solution, vortexed, and kept in the dark for 15 min. Relative fluorescence intensity (RFI) of both the buffer (blank) and each protein solution (from the lowest to the highest concentration) was measured using a fluorescence spectrophotometer (F-2700 Hitachi, Japan) at 390 nm (excitation wavelength) and 480 nm (emission wavelength), with a scanning speed of 5 nm·s −1 . RFI of each dilution bank was subtracted from the corresponding protein solution with the fluorescence probe ANS to obtain the net RFI. e initial slope of the plot of standardized net RFI values versus % protein concentration was expressed as surface hydrophobicity.

Determination of Free and Total Sulfhydryl Group
Content.
e method used for determination of the sulfhydryl group content of WSPP and WSPC was adopted from Malik et al. [18] with some modifications. e protein solution (0.5% w/v) was prepared using a standard buffer pH 8.0 (0.086 M Tris 0.09 M glycine 4 mM Na 2 EDTA) for free sulfhydryl group determination and in the denaturing buffer (standard buffer plus 8 M urea and 0.5% w/v sodium dodecyl sulfate) for total sulfhydryl group determination. e samples were incubated at room temperature for 30 min. e mixture was then centrifuged (12,500 × g for 20 min at 25°C) and the supernatant collected for determination. To each 4 mL aliquot of supernatant 0.1 mL Ellman's reagent solution (5,5-dithiobis (2-nitrobenzoic acid): DTNB) (4 mg DTNB/mL buffer) was added, rapidly mixed, and allowed to stand for 15 min. e solution was then read at 412 nm in a UV-Vis spectrophotometer (Shimadzu UV 1800, Japan) against a blank. e blank was prepared by mixing 4 mL of the respective buffer with 0.1 mL of Ellman's reagent. In order to calculate micromoles of SH/g of protein, a molar extinction coefficient of 1.36 × 10 4 M −1 ·cm −1 was used.

Color Measurement.
e colors of WSPP and WSPC were determined using the ColourQuest XE colorimeter (Hunter Lab., Hunter Assoc. Laboratory, USA). e setting for the illuminant was D 65 source, and the observer was standard 10°. Calibration of the instrument was conducted with black and white calibration tiles. WSPP and WSPC were filled in a cuvette quartz path length 25 mm, and three observations were measured and expressed as CIE L * (lightness), a * (redness), and b * (yellowness) with 5 readings/sample.

pH Measurement.
One gram of WSPP and WSPC was mixed with 9 mL of distilled water and stirred at 100 rpm for 10 min. e pH value of the mixture was measured at room temperature in triplicate using an electronic pH meter (FE-20, Mettler-Toledo Instruments Co., Ltd., Switzerland).

Evaluation of Functional Properties
2.6.1. Protein Solubility. Protein solubility was measured according to the method of Nalinanon et al. [19] with slight modifications. e solubility of WSPP and WSPC was determined at pH 1 to 11. Briefly, the protein sample (50 mg) was dispersed in 8 mL of distilled water, and the pH of the mixture was adjusted to 1, 2, 3, 4, 5, 6, 7, 8, 9, 10, or 11 using 1 M HCl or 1 M NaOH. e dispersion was stirred for 30 min at room temperature, and the volume was adjusted to 10 mL prior to centrifugation at 6,000 × g for 10 min at 25°C. e supernatant was collected and subjected to protein determination using the biuret method [20]. BSA was used as a protein standard. Total protein content in the sample was determined from the soluble portion of the sample in 0.5 M NaOH, and relative solubility of the protein sample was calculated as follows: protein content in supernatant total protein content in sample × 100. (3)

Emulsifying Properties. Emulsion activity index (EAI)
and emulsion stability index (ESI) were determined according to the method of Pearce and Kinsella [21] with slight modifications. Two mL of soybean oil and 6 mL of protein solution (5 mg/mL) were homogenized (Model T25 basic; IKA) at 20,000 rpm for 1 min. An aliquot of the emulsion (50 µL) was pipetted from the bottom of the container at 0 and 10 min after homogenization and subsequently diluted 100-fold using 0.1% (w/v) SDS solution.
Each sample was mixed thoroughly for 10 s using a vortex mixer. A 500 of the resulting dispersion was measured using a spectrophotometer (UV-1800, Shimadzu, Japan). EAI and ESI were calculated as follows: where A � A 500 , DF � dilution factor (100), l � path length of cuvette (m), Φ � oil volume fraction, and C � protein concentration in the aqueous phase (g/m 3 ), where ΔA � A 0 −A 10 and t � 10 min.

Foaming Properties.
Foaming capacity (FC) and foam stability (FS) of protein samples were determined as described by Nalinanon et al. [19] with slight modifications. Solutions (35 mL) of each sample at 5 mg/mL protein concentration were transferred into a 100 mL cylinder. e solutions were homogenized by a homogenizer (Model T25 basic; IKA) at 16,000 rpm for 1 min at room temperature (∼25°C), and the samples were allowed to stand for 0 and 60 min. FC and FS were then calculated using the following equations: where V T is the total volume after whipping, V 0 is the original volume before whipping, and V 60 is the total volume after leaving at room temperature for 60 min.

Determination of Antioxidant Activities
2.7.1. DPPH Radical Scavenging Activity. DPPH radical scavenging activity was determined by DPPH assay as described by Murakami et al. [22] with slight modifications. Briefly, the reaction mixture contained 5.4 mL of WSPP or WSPC at different concentrations and 0.6 mL of 0.8 mM DPPH in 95 % ethanol. e mixture was incubated at room temperature for 30 min in dark, and then the absorbance of the resulting solution was measured at 517 nm in a UV-1800 spectrophotometer (Shimadzu, Japan). e control was prepared in the same manner except that distilled water was used instead of the sample. e percentage of DPPH • radical scavenging activity of the sample was calculated as follows: where A control is the absorbance of the assay without sample and A sample is the absorbance in the presence of the WSPP or WSPC. e sample concentration providing 50% inhibition (IC 50 ) was calculated using the graph by plotting scavenging activity percentage against sample concentration.

ABTS Radical Scavenging
Activity. ABTS radical scavenging activity was determined by ABTS assay as described by Rice-Evans et al. [23] with slight modifications. e ABTS radical (ABTS •+ ) was produced by reacting 7.4 mM ABTS stock solution with 2.45 mM potassium persulphate at a ratio of 1 : 1 (v/v). e mixture was allowed to react for 12-16 h at room temperature in the dark. is working solution of ABTS •+ solution was diluted with 95% ethanol at a ratio of 1 : 50 (v/v), in order to obtain an absorbance of 0.700 ± 0.020 at 734 nm. A fresh ABTS •+ solution was prepared for each assay. e reaction mixture contained 0.15 mL of WSPP or WSPC at different concentrations and 2.85 mL of ABTS •+ solution. e mixture was incubated at room temperature for 6 min in dark. en, the absorbance was measured at 734 nm using a UV-1800 spectrophotometer (Shimadzu, Japan). e control was prepared in the same manner except that distilled water was used instead of the sample. e percentage of ABTS •+ scavenging activity of the sample were calculated in the same manner as described in section 2.7.1. e IC 50 value was the inhibitory concentration at which ABTS •+ were scavenged by 50%.

Ferric-Reducing Antioxidant Power (FRAP).
FRAP was determined by the method described by Benzie and Strain [24]. FRAP reagent was freshly prepared by mixing 10 mM TPTZ (2,4,6-Tris(2-pyridyl)-s-triazine) in 40 mM HCl, 20 mM FeCl 3 , and 300 mM acetate buffer, pH 3.6 (1 : 1 : 10 v/v/v). A sample (0.1 mL) was mixed with 3 mL of FRAP reagent, and the mixture was left at room temperature for 8 min in the dark. e absorbance was measured at 593 nm using a UV-1800 spectrophotometer (Shimadzu, Japan). e blank was prepared in the same manner except that distilled water was used instead of the sample. A standard curve was prepared with Trolox ranging from 20 to 120 µg/mL. e antioxidant power of the samples was expressed as μg Trolox equivalent (TE)/g protein.

Statistical Analysis.
Extractions and all results were performed in triplicate (n � 9). All data were subjected to analysis of variance (ANOVA), and the differences between means were evaluated by Duncan's multiple range test. For pair comparison, t-test was used. SPSS statistic program (SPSS 11.0 for Windows, SPSS Inc., Chicago, USA) was used for data analysis.

Yield and Extraction Efficiency.
e yield and extraction efficiency of water-soluble protein from grasshoppers, WSPP and WSPC, are shown in Table 1. e proteins from both grasshoppers were simply extracted with distilled water. e yields of the resultant freeze-dried counterparts called WSPP and WSPC were 7.35 ± 0.19 and 7.49 ± 0.19% (wet weight basis), respectively. Clarkson et al. [25] found that protein yield in soluble locust fraction from L. migratoria was 9.83%. e difference in extraction yield was probably due to different preparations and extraction procedures. e crude protein contents determined by the Kjeldahl method of P. succincta and C. roseapbrunner were 15.07 and 17.40% (wet weight basis), respectively (data not shown), which is expressed in dry weight to be 65.55 and 71.75%, respectively. e protein content of those grasshoppers was lower than that previously reported in the whole freeze-dried locust and alkali-extracted defatted locusts (65.87 and 82.26% dry weight, respectively) [26]. Clarkson et al. [25] reported that crude protein content of L. migratoria was 50.79% (dry weight). e extraction efficiency of WSPP and WSPC were calculated to be 48.77 and 42.86%, indicating high efficacy of protein extraction. erefore, water-soluble protein might be one of the major protein components in grasshoppers and was suitable for protein extraction by water, an environment friendly method.

pH and Color.
e color and pH of WSPP and WSPC are shown in Table 1. WSPP and WSPC exhibited a faintly acidic pH with a value of 6.08 and 6.07, respectively. e color of WSPP and WSPC expressed as L * , a * , and b * values was 47.26, 6.04, and 16.80, respectively, for WSPP and 55.80, 5.48, and 18.20, respectively, for WSPC. e WSPC had a higher value than the WSPP for L * and b * , but lower values for a * , indicating more light green color in WSPC than WSPP. e green coloration could be due to a common green pigment identified in insects called insectoverdin [25]. Goodwin [27] postulated a mixture of two chromoproteins, one yellow component from carotenoids and the other a bile component (blue), creating the green color in the locust. However, a general observation of the visible color of both WSPP and WSPC tended to be brown, which could be attributed to melanin [28].

Surface Hydrophobicity and Sulfhydryl Content.
e surface hydrophobicity of WSPC and WSPP was found to be 22.59 ± 0.22 and 15.92 ± 0.21, respectively (Table 1). From the result, surface hydrophobicity of both insect proteins was lower than the previous report of Azagoh et al. [29]. ey reported that surface hydrophobicity of T. molitor larvae meal was 102.5. Aggregating proteins are more hydrophobic, and hydrophobic zones are buried inside the structure of proteins [30]. e surface hydrophobicity of protein extracted from edible insects has been shown to vary, depending on the extraction protocol [31]. Surface hydrophobicity might also be dependent on the size, conformation, amino acid composition, and sequence of a protein.
e total sulfhydryl content and free sulfhydryl content of WSPC (1.06 and 0.48 µmol/g) was comparable with WSPP (1.14 and 0.48 µmol/g) ( Table 1). is was expected from the amount of sulphur-containing amino acids found in both proteins. Differences in sulfhydryl content found in different proteins have been reported. Van der Plancken et al. [32] reported that total sulfhydryl content of untreated egg white solution was 58.5 µM/g protein. Malik et al. [18] found that the free and total sulfhydryl content of sunflower protein isolate was about 7.7 and 80.1 µmol/g. us, the quantity of free and total sulfhydryl content might be depended on the source of protein, part of animal, and species of samples.

Protein Patterns.
Protein patterns and molecular weight distribution of WSPP and WSPC analyzed by SDS-PAGE using 10% separating gel under reducing and nonreducing conditions are shown in Figure 1. ere was a wide range of molecular weights in the WSPP and WSPC ranging from lower 20 kDa to 250 kDa. Six major groups of protein bands under reducing condition were found to be more than  [26] reported that protein concentrate from Locusta migratoria included proteins in the range of 6-100 kDa. e characteristic bands (40, 50 and 100 kDa) of L. migratoria protein contained muscle protein tropomyosin and high amounts of tubulin, which are responsible for the formation of the microtue bules [26]. Zielińska et al. [33] reported that raw locust S. gregaria had protein band with molecular weight range between 29.0 and 44.3 kDa and 97.2 kDa, while boiled locust found low intensity of protein band at range 29.0-44.3 kDa and baked locust disappeared protein band. e differences in protein patterns under reducing and nonreducing conditions might be depended on species of insects, extraction method, and insects processing. Furthermore, protein functionalities and antioxidant activities are also governed by molecular weight distribution, amino acid composition and amino acid sequence of the protein itself [19].

Amino Acid Composition.
e amino acid compositions of WSPP and WSPC are presented in Table 2. Generally, both grasshopper proteins had similar amino acid profile. WSPP and WSPC composed of 15 amino acids of which 7 essential amino acids and 8 nonessential amino acids. Methionine, tryptophan and cysteine were not detectable, possibly due to they had very low ratio or were not present in the proteins studied. e predominant essential amino acids were leucine and lysine which are similar to those reported for Locusta migratoria [26], Tenebrio molitor larvae [29] and silkworm larvae protein isolates [34]. e amount of essential amino acids in WSPP and WSPC were sufficient to meet the adult nutritional requirements based on the FAO/WHO guidelines [1]. e predominant nonessential amino acids were glutamic acid, aspartic acid, alanine and arginine. Glutamic acid, aspartic acid, leucine and alanine were the major amino acid found in both WSPP and WSPC with descending amount in order. Glutamic acid was the most abundant amino acid in locust and grasshopper [35,36]. ese results are similar to those reported by Makkar et al. [35] for grasshoppers (glutamic acid 4.5-15.2 g/16 g nitrogen). ese differences might be due to the differences in the extraction method, species and source of insects. In general, protein functionality and bioactivity govern by its amino acid composition as well as amino acid sequence [37]. Both WSPP and WSPC contained higher amount of hydrophobic amino acids than hydrophilic amino acids. It has been shown that hydrophobic amino acids and one or more residues of histidine, proline, methionine, cysteine, tyrosine, tryptophan and phenylalanine can enhance the activities of the antioxidant peptides [5]. However, although both WSPP and WSPC had similar amino acid profile, they might have same or different molecular properties, functionalities and bioactive potentials which also depending on their amino acid sequence.

Relative Solubility.
e relative solubility (%) of WSPP and WSPC in the pH range of 1-11 was depicted in Figure 3. e result showed that WSPC generally had higher relative solubility than WSPP in all pHs tested. WSPP and WSPC were highly solubilized more than 85% in the pH range of 6-11, indicating that the protein in grasshopper can be solubilized at neutral to alkaline pH. At strong acidic condition (pH 1-2), the solubility of grasshopper proteins was relatively high with relative solubility of 73-78% and 88-90% for WSPP and WSPC, respectively. However, the solubility of those proteins decreased with increasing pH to 3 and 4. e lowest relative solubility was found at the pH 4 for both proteins, indicating their isoelectric pH (pI). is was due to a reduction in electrostatic repulsive forces between the proteins, leading to protein aggregation [29]. ese results correspond well with the protein from migratory locusts S. gregaria [44]. e pIs of migratory locust [26], edible meal worm and black soldier fly [45] were also found at pH 4. Additionally, the solubility of insect proteins was similar to those reported for several legumes, animal proteins and protein isolates [26,29,41,45,46].

Emulsifying Properties.
Emulsifying and foaming properties of WSPP and WSPC are shown in Table 3. e emulsion activity index (EAI) and emulsion stability index (ESI) of WSPP and WSPC ranged from 29.23 to 36.69 m 2 /g and 15.67 to 33.34 min, respectively. e EAI and ESI of those proteins were significantly lower than bovine serum albumin (BSA) (p < 0.05). Low emulsifying properties found in both insect proteins might be due to they contained high amount of low molecular weight components. When peptides are shorter and less globular, they will form less stable protein layers around the oil droplets that offer less resistance to coalescence or Ostwald ripening [47]. Adebowale et al. [48] reported an adequate emulsification but poor stability in whole giant African cricket (Gryllidae sp.) powder. In contrast, both high emulsion formation and stability in moth (Cirina forda) larva and silkworm (Bombyx Mori) powders have been report by [49]. Although WSPC exhibited greater EAI and ESI than WSPP, they had poor emulsifying properties when compared with BSA and  protein from locusts S. gregaria [44]. Emulsifying properties of other proteins have been determined and reported. Tirgar et al. [50] reported that EAI and ESI of flaxseed protein were 46.5 m 2 /g and 12.51 min, respectively. Hall et al. [51] reported EAI of 27 to 32 m 2 /g for cricket (G. sigillatus) protein hydrolysates. EAI and ESI of WSPP were similar to that found by Nalinanon et al. [19], who reported EAI and ESI for protein hydrolysate at concentration of 0.5% from ornate threadfin bream (Nemipterus sp.) muscle and DH10-30% using skipjack tuna (Katsuwonus sp.) pepsin digestion were 29.9 to 30.3 m 2 /g and 14.1 to 18.6 min, respectively. WSPC exhibited greater emulsifying properties than WSPP. is might be due to a greater surface hydrophobicity of WSPC had a positive effect on emulsification (Table 1). e ability of a protein to rapidly lower free energy of a newly created interface is controlled by (1) how rapidly it can adsorb to the interface and (2) how rapidly and easily it can undergo conformational rearrangement and reorientation at the interface [52]. e differences between the emulsion activity and emulsion stability are related to the amphiphilicity of the protein surface, protein contents (soluble and insoluble) and other components [44]. e lower ESI of WSPP and WSPC than BSA which could be attributed to partial denaturation of proteins and change in the distribution of molecular charge that exposes hydrophobic amino acid [44].

Foaming Properties.
Foam capacity (FC) and foam stability (FS) of WSPP and WSPC are shown in Table 3. WSPP and WSPC exhibited 8.57, 25.71% and 86.41, 98.72% for FC and FS, respectively. WSPC showed higher FC than WSPP, although the FC of those proteins were low when compared with BSA (81.23%) (p < 0.05). e result of FC from WSPC was similar to those reported by Adebowale et al. [48], for whole giant cricket (Gryllidae sp.) powder that had an FC of 6%, and Omotoso [7], who reported the FC from Cirina forda larvae powder as 7.1%. However, WSPC had lower FS than WSPP. e FS of WSPP and WSPC (∼80%) was significantly higher than that of BSA (67.41%) (p < 0.05), indicating the excellent capacity to stabilize foam against collapse. Generally, foam collapse takes place by any of these three mechanisms including (1) disproportionation of bubbles; (2) coalescence of bubbles due to instability of thin film between them; and (3) drainage of water from the surface of the bubbles down to the liquid layer, thereby leading to the removal of protein from film around the bubble [52]. Zielińska et al. [44] reported the FC of protein preparations with alkali extraction from locusts (S. gregaria) as 32% and FS was 6.17%. e differences between FC and FS of proteins may be due to the factors influencing foam formation including hydrophobic amino acid content, surface hydrophobicity, location of hydrophobic amino acid residues on the protein surface, presence of thiol groups, cations and anions, carbohydrates, and lipids [44]. Johnson and Zabik [53] explained that intermolecular proteinprotein interaction enhances the cohesive nature of the film, imparting stability and elasticity to the membrane. is interaction appears to be dependent on the presence of a high ratio of nonpolar/polar side chains in the protein [53]. Additionally, Nalinanon et al. [19] suggested that low MW peptide could not maintain well-ordered orientation of the molecule at the interface.

Antioxidant
Activities. Antioxidant activities as determined by ABTS, DPPH, and FRAP assays of WSPP and WSPC are shown in Table 4. WSPP and WSPC exhibited strong scavenging activities with IC 50 of 204.67 and 176.31 µg/mL for DPPH radical and 81.97 and 69.12 µg/mL for ABTS radical, respectively. Zielińska et al. [54] reported that the antiradical activities against DPPH • and ABTS •+ for the hydrolysates obtained after digestion of locusts L. migratoria were found to be 67 µg/mL and 25.9 µg/mL of their IC 50 , respectively. ese reports found less effective on DPPH • scavenging activity when compared with the present result (IC 50 of 176.31 to 204.67 µg/mL). Additionally, Zielińska et al. [33] reported that the protein hydrolysates prepared by alkali extraction from locusts (S. gregaria) exhibited IC 50 for DPPH • and ABTS •+ scavenging activities were 28.5 and 16.6 µg/mL, respectively. With high ABTS radical-scavenging activity, it was postulated that antioxidative compounds were most likely hydrophilic [19]. Also, with high DPPH radical-scavenging activity, the results obtained suggest that the grasshopper proteins contained amino acids or peptides that were electron donors and could react with free radicals to convert them to more stable products and terminate the radical chain reaction. e protein from various species of edible insects might give a different scavenging activity on DPPH • and ABTS •+ radicals. It might be depended on molecular weight of protein or peptide as well as its amino acid composition. Zhang et al. [55] postulated that peptides with large molecular weight have less antioxidant activity. Nalinanon et al. [19] found that peptides in hydrolysates from ornate threadfin bream muscle with various degree of hydrolysis (DH) might differently scavenge two different radicals, ABTS and DPPH radicals. In addition, the presence of hydrophobic sequences in the peptides could interact with  Journal of Chemistry lipid molecules and could scavenge by donating protons to lipid-derived radicals [5].
As per FRAP assay, WSPP and WSPC also presented reducing power on Fe 3+ of 22.26 and 27.59 µg TE/g protein. Similar results were obtained by Xia et al. [56] who reported that the antioxidant properties of the barley glutelin hydrolysates had ferric-reducing power values of 24.0 µg Fe 2+ /mg, respectively. Bousopha et al. [57] reported that collagen hydrolysate from pharaoh cuttlefish skin with 10-30% DH had ferric reducing power values of 23.50 to 26.50 µmolTE/g protein. e increase or decrease in ferricreducing power for protein hydrolysates may be related to the exposure of electron-dense amino acid side chain groups, such as polar or charged moieties during hydrolysis [58]. Compounds with higher reducing power were shown to have a better ability to donate electrons or hydrogen and serve as a significant indicator of their potential for use as an antioxidant [59].

Conclusion
e proteins from edible insects, P. succincta and C. roseapbrunner, could be effectively extracted by water. Based on physicochemical and functional properties as well as antioxidant activities, water-soluble proteins from both insects are beneficial for human nutrition and had potential use as a food ingredient. is opens up the possibility for these edible insect proteins to be used as in suitable food applications.

Data Availability
e data used to support the findings of this study are available from the corresponding author upon request.

Conflicts of Interest
e authors declare that there are no conflicts of interest regarding the publication of this article.