1. Introduction
In intensive and semi-intensive aquaculture management models, the expenditure of artificial feed accounts for 40–60% of the total culture cost [
1]. The quality of feed formulas is of great importance to the growth of cultured organisms. For example, protein provides essential amino acids in the growing process, lipids provide essential fatty acids, starch provides energy and acts as a feed adhesive, and vitamins and minerals play an important role in physiological and biochemical metabolic processes. Therefore, the appropriate trophic components of feed, and the nutritional requirements and cost-effectiveness of the cultured species, must be considered in the use of feed [
2]. Protein is the costliest component of artificial feed formulas, as well as being a major trophic factor that sustains life and influences the growth performance of aquatic organisms. Ref. [
3] indicated that fish meal was used as the main protein source in feeds for carnivorous fishes. As the fish meal had a good amino acid composition, high nutrient digestibility, and low anti-nutritional factor, feeds should be mixed with 50–60% fish meal to meet the nutritional requirements of carnivorous fishes. Ref. [
4] suggested that, as global fish production increases rapidly and fishery resources decline, the price of fish meal rises continuously, causing artificial aquaculture costs to escalate. The use of fish meal in the aquatic feed industry often suffers from an unstable supply and price fluctuations. The anchoveta fishery in Peru is the source of the majority of the global fishmeal and fish oil supplies. Overall, 2021 has been a positive year for the fishmeal industry, as the annual production quantity of fishmeal in Peru reached 3.67 million tonnes in 2021, up by 12 percent compared to 2020. Fishmeal prices peaked in 2022, at USD 1600 per tonne (CIF Peru, 65% protein). They have since remained more or less stable [
5]. In addition to the cost of fish meal, the cost of soybean, another protein source used for aquatic feed, has increased year by year [
6,
7]. As the consumption of soybean and fish meal is expected to be limited due to human consumption in the future, the search for alternative protein sources remains a topic of discussion amongst researchers and within the aquatic feed manufacturing industry.
Insect meal protein has recently been increasingly discussed in relation to the nutrition of aquatic and livestock feeds [
8]. Insect meal protein is not a new protein source, but as fish meal prices have risen recently, and as vegetable protein is mostly consumed by humans, insect meal protein has provided a new direction for aquatic and livestock feeds [
9]. Insects belongs to the Arthropoda family, the largest class of the animal kingdom. Most insects have a short life span and are easy to culture. In terms of human food, insects are regarded as a staple food in a number of Southeast Asian countries [
10]. Insects can provide a quality protein source, making them attractive in the application of feed. Aquafeed has a higher protein demand than livestock feed. However, numerous reports indicate that from 7% to as high as 68% of the protein ingested by aquatic organisms are not absorbed [
11]. Given this, research on aquafeed is focusing on finding appropriate feed substitutes and improving the nutrient absorption efficiency of aquatic animals. Amongst insect proteins, black soldier fly has several major advantages over other insect species. The species is polyphagous and uses well-defined substrates, producing insects of a defined quality of macro- and micro-nutrients [
12]. Fish meal protein can be replaced with 50% and 48% black soldier fly (
Hermetia illucens L.) larvae meal protein without adverse effects on the weight gain of European sea bass,
Dicentrarchus labrax, and yellow catfish,
Pelteobagrus fulvidraco, respectively [
13,
14]. The partial substitution of dietary fish meal protein with black soldier fly larvae meal protein has also been successfully implicated within various fish species such as rainbow trout,
Oncorhynchus mykiss [
15]; Atlantic salmon,
Salmo salar [
16]; Nile tilapia,
Oreochromis niloticus [
17]; marron,
Cherax cainii [
18]; and African catfish,
Clariass gariepinus [
19].
Butyric acid is a type of carboxylic acid with the molecular formula CH
3-CH
2-CH
2-COOH. It is often used in the domain of veterinary medicine, especially with ruminants. In livestock production, butyric acid is used for promoting the growth of cattle [
20]. Research on animal nutrition has found that butyric acid can promote microbial fermentation in the colon to digest fibrous matters such as cereal flour, inulin, and psyllium [
21]. The effects of butyric acid can be divided into intraintestinal and extraintestinal effects. The intraintestinal effects include regulation of the epithelial transport system, an improvement in the inflammation and oxidative states of the intestinal mucosa, an enhancement in the mucosal barrier, and the regulation of visceral sensitivity and mobility [
22,
23]. The extraintestinal effects of butyric acid are largely unknown. Butyric acid is a short-chain fatty acid produced by colonic microbes, especially by the microbiota of the proximal end of the colon, and it is one of the main energy sources of colonic cells. Another primary function of butyric acid is to enhance the absorption and anti-secretion capacity of the intestinal mucosa [
21].
In the aquaculture process, the overuse of antibiotics to control disease results in a number of problems, such as degraded immunosuppression, the production of antibiotic drug-resistant strains, and excessive antibiotic residue in animal products [
24]. Ref. [
25] indicated that butyric acid is a short-chain fatty acid and has a remarkable effect on maintaining the intestinal health of organisms. Many researchers have recognized the successful use of synthetic sodium butyrate or butyric acid to promote growth and to stimulate the immune system. For example, Ref. [
26] mentioned that the addition of 1% butyric acid glyceride to the feed can significantly enhance the growth and immunoreaction of yellowfin seabream (
Acanthopagrus latus) fingerlings. Ref. [
27] indicated that the addition of 5 g/kg of diet butyric acid to their feed can significantly enhance the growth and immunity parameters of barramundi (
Lates calcarifer). Ref. [
26] indicated that the addition of 1% butyric acid glyceride to their feed can significantly enhance the hematological parameters and lipid peroxidation enzymes of yellowfin seabream. These findings show that butyric acid is a promising feed additive in aquaculture. Many studies have indicated that butyric acid, butyric acid glyceride, and sodium butyrate can significantly influence organism growth performance, the efficiency of feed utilization, body composition, intestinal microflora, tissue morphosis of the intestinal villi, digestive enzymes, oxidation resistance, haematogenic immunity, immune gene expression, and the resistance to disease of fishes and shrimps [
28,
29]. Therefore, this study explored the influence of substituting fish meal protein with insect meal protein and the addition of butyric acid on the growth, immunity, antioxidation, and intestinal villi of jade perch.
2. Materials and Methods
2.1. Experimental Diets
Approximately 210,000 black soldier fly eggs were obtained from Kunyi Biotech (Chiayi City, Taiwan), which were reared at National Chiayi University (NCYU; Chiayi City, Taiwan). The eggs were hatched and grown in empty containers (140 cm × 100 cm × 50 cm) indoors, and the temperature was maintained at 22–25 °C. Three days after hatching, the larvae were fed with soybean meal (crude protein: 38.4% and crude lipid: 17.26%; TTET Union Corporation, Tainan City, Taiwan). For the formulation of the fish’s diet, black soldier flies in the pupal stage were dried and homogenized.
Six isonitrogenous (31% crude protein) and isolipidic (8% crude lipid) diets were formulated to replace 0% (FM), 50% (FBM) and 100% (BMB) of fish meal protein with the protein from the black soldier fly meal. The treatment groups were mixed with 0% and 1% sodium butyrate, respectively. The dry matter of the experimental feed was mechanically pulverized and mixed. The dry feed was then mixed with 30% distilled water and made into feed pellets with a diameter of 2.5 mm using an automatic extruder. The feed pellets were dried in an oven at 60 ℃ until the moisture content was at about 10% and then stored in a refrigerated chamber at −40 ℃. The experimental feed composition is shown in
Table 1.
Table 2 shows the main fatty acid and amino acid compositions of the experimental feed. The main fatty acids of the different treatment groups were C16:0, C18:2 n-6, and C20:4 n-6. The n-3 highly unsaturated fatty acid proportion of the FM and FMB groups was 18.44%; the n-3 highly unsaturated fatty acid content of the FBM and FBMB groups was 11.03%; the n-3 highly unsaturated fatty acid content of the BM and BM + butyric acid (BMB) groups was 3.62%. In terms of amino acid composition, the FM, FMB, FBM, and FBMB groups have higher leucine, lysine, and arginine contents. The BM and BMB groups had a higher methionine content. The essential amino acid content in the experimental feed decreased as the substitution amount of fish meal increased in the fish feed.
2.2. Experimental Fish
The fingerling jade perch used in this experiment were provided by the fish hatchery in Pingtung County. The fries were packaged in the hatchery in the morning and transported in a truck to the experimental greenhouse of the Department of Aquatic Biology at Chiayi University. After the fries adapted to the water temperature of the experimental site, they were placed in a 300 L fiberglass-reinforced plastic (FRP) bucket. All the animal experiments conformed to the principles of the use and care of experimental animals of National Chiayi University’s Biosafety Committee (approval no. NCYU-IACUC-11101). In the raising period, the fries were fed with commercial feed (Marine fish larvae feed No. 3, Shye Yih Feeding Co., Ltd., Kaohsiung city, Taiwan) once per day for one week. At the beginning and end of the experiment, the feeding of the experimental fish was stopped for 24 h, during which time the fish digested the feed and excreted the waste from their digestive tracts. The individuals were then weighed after the body surface water was removed. The experiment was divided into six treatment groups, and each treatment group had three tank replicates. At the beginning of the experiment, juvenile jade perch weighing 7.3 g on average were selected and randomly allocated to 18 FRP buckets (57 × 35 × 30 cm), with a count of 20 fish per bucket. The fish were fed manually twice per day (09:00 and 15:00), and the feed quantity was 5% of the body weight. The fish were weighed once every two weeks, and the daily feed quantity was modified according to the individual weights. The experiment lasted for eight weeks. The experiment was performed in natural light. During the experimental period, the water quality parameters were maintained at a temperature of 26–28 °C, a pH of 7.5–7.6, NH3-N ≤ 0.05 mg·L−1, and dissolved oxygen ≥ 6.0 mg·L−1. The weight gain percentage (WG), protein efficiency ratio (PER), feed conversion ratio (FCR) and survival rate were calculated according to the following equations: WG (%) = 100 × (Wt − W0)/W0, PER = body weight gain/crude protein intake, FCR = feed intake (g)/weight gain (g), Feed intake (g/fish) = dry feed (g) given/number of fish, and survival (%) = 100 × (final number of fish/initial number of fish), where W0 is the initial mean body weight (g), Wt is the final mean body weight (g), and t (day) is the feeding period.
2.3. Sampling
At the end of trial, the feeding of all fish was stopped for 24 h to prepare the fish for the taking of muscle, intestinal tract, and blood samples. Three individuals were taken from each bucket (nine in each group) and anesthetized with 1% tricaine methane sulfonate (MS222, Sigma-Aldrich, St. Louis, MO 68178, USA). Afterwards, blood was collected from the caudal vein without using an anticoagulant, stored at room temperature for 30 min, and centrifuged (5000× g, 15 min) to separate the serum. The serum samples were stored in a refrigerated chamber at −20 °C before their biochemical indexes were analyzed. After the blood sampling, the hepatic and muscle tissues were sampled and stored at −80 °C directly before the composition analysis. The intestinal tract was taken out carefully, and the anterior intestinal tract was sampled and stored in formalin solution (10% Formalin solution, neutral buffered, Sigma-Aldrich) to evaluate its histomorphology.
2.4. Biochemical Measurement of the Serum
The alanine aminotransferase (ALT (mU/mL)) was analyzed using a reagent kit (Alanine Aminotransferase (ALT) Activity Assay Kit (Colorimetric) MET-5123, Cell Biolabs, Inc. Arjons Drive, San Diego, CA 92126, USA). For the analytic procedure, 50 μL of the sample, 50 μL of the diluted pyruvate standard, and 100 μL of a mixed reagent (147 μL ALT enzyme mix + 250 μL ALT substrate mix + 5 μL horseradish peroxidase) (100 μL of the prepared reaction reagent) were put in a 96-well microtiter plate in turn. The samples were determined using a spectrophotometric microplate reader with the setting of an absorbance value of 540–570 nm. The aspartate aminotransferase (AST) activity was analyzed using a reagent kit (Aspartate Aminotransferase (AST) Activity Assay Kit, MAK055, Sigma-Aldrich). For the analytic procedure, 50 μL of the sample and 100 μL of a reaction standard solution (80 μL AST assay buffer + 2 μL AST enzyme mix + 8 μL AST Developer + 10 μL AST substrate) were put in a 96-well microtiter plate in turn, reacted at 37 °C for two to three minutes, and determined using a spectrophotometric microplate reader with the setting of an absorbance value of 450 nm.
2.5. Lipid Peroxidation Enzyme Activity Analysis
A 2 g liver sample was placed in liquid nitrogen and immediately stored in a refrigerator at −80 °C for subsequent analyses. The superoxide dismutase (SOD) was analyzed in accordance with methods of [
30]. The glutathione peroxidase (GPx) was determined using a colorimetry determination reagent kit (ab102530). A 100 mg tissue sample was added with a phosphate buffer solution (PBS), reaction mix solution, and cumene hydroperoxide solution, sequentially. The absorbance value was determined using a microplate reader with 340 nm being set as the measurement standard. The catalase (CAT) was analyzed using a commercially available Catalase Assay Kit (No. 707002, Cayman Chemical, East Ellsworth Road Ann Arbor, Michigan 48108, USA). A 20 mg tissue sample was mixed with 100 μL of an assay buffer, 30 μL of methanol, 20 μL of a diluted hydrogen peroxide solution, 30 μL of potassium hydroxide and 30 μL of catalase purpald, sequentially. The absorbance value was determined using a microplate reader, using a standard of 540 nm. Thiobarbituric acid-reactive substances (TBARS) in the tissues were measured using a modified version of the method of [
31]. In brief, tissues were homogenized with a 20% trichloroacetic acid extracting solution containing 1% butylated hydroxytoluene (BHT) and incubated with 50 mM of thiobarbituric acid (TBA). The samples were then placed in a boiling water bath for 10 min and centrifuged at 4000 rpm. The optical density of the solution was then measured at 532 nm. TBARS were expressed as a micromole of malondialdehyde (MDA) per gram of tissue using a molar extinction coefficient of 1.56 × 105 M
−1 cm
−1.
2.6. Hematological Analysis
After the experiment was completed, three individuals were removed from each of the three buckets (nine fish each group) for hematological analysis. Blood was collected from the caudal vein, and eighteen tubes of about 1 mL of whole blood for each tube were collected from each group and examined using a blood analyzer (Sysmex XP-300, San Tung Instrument Co., Ltd., 651-0073 Hyogo Prefecture Shingo City, Japan). The investigated items included the RBC count, HGB, and Hct content; these three variables were used to calculate the mean corpuscular volume (MCV), mean corpuscular hemoglobin (MCH) content, and mean corpuscular hemoglobin concentration (MCHC).
2.7. Intestinal Tract Section
For the fixing process, the fish intestinal tract was taken from the fish body and divided into three equal parts (the anterior, intermediate, and posterior intestines) according to the total length. These parts were then soaked in a 10% neutral formalin (10% Formalin solution, neutral buffered, Sigma-Aldrich) fixing solution for 24 h. The parts were embedded in an embedding box after dehydration and cut up into pieces sized 3–5 mm, after which they were put in an embedding box and dehydrated according to the alcohol concentration gradient (50, 60, 70, 80, 90, 95, 100%). The xylene and paraffin solutions were changed in the order of the following ratios (all xylene, 2:1, 1:1, 1:2, and all paraffin). After the dehydration process was finished, the embedding box was opened, and the intestinal tract tissue was taken out. The intestinal tract tissue was put in a paper folded mold; afterwards, it was placed to stand in the embedding box vertically, filled with paraffin liquid and cooled to form a solid paraffin block. The section was stained after embedding, and the paraffin block with the embedded tissue was trimmed. The microtome section was 5 μm thick. The sectioned tissue wax strip was unfolded in a 42 °C distilled water bath, taken out using a microscope slide and dried in an incubator at 37 °C. After staining, an appropriate amount of Canada balsam (Sigma-Aldrich) was dripped onto the slide. A coverslip was picked up using a pair of forceps and dipped in xylene before being placed over the slide. Afterwards, the slide covered with the coverslip was air-dried and placed under a microscope (CX23RTFS2, Olympus, Yuan Li Instrument Co., Ltd. Yang-Guang St. 114 Taipei, Taiwan) for observation. The length and width of the villi were calculated using the built-in software of the camera (OCCA, HUSL2.0).
2.8. Fatty Acid Composition (% Total Fatty Acids) Analysis
The fatty acid composition was analyzed using gas–liquid chromatography (HP5890II plus). The chromatographic column used is an HP-INNOWax capillary column measuring 30 m × 0.247 mm × 0.5 μm, made in the USA, and hydrogen was used as the transport gas. The flow velocity was 2 mL/min, the split ratio was 12:1, and the temperature rose from 150 °C to 240 °C at a rate of 2 °C/min. The injector and detector temperatures remained at 250 °C and 260 °C, respectively. For the fatty acid identification, the retention time (RT) of the samples was compared with the retention time of the fatty acid methyl ester standard (Nu-Check Merck Ltd., Tiding Blvd. Neihu District. Taipei 11493, Taiwan).
2.9. Amino Acid Analysis
The sample was freeze-dried and defatted, after which 19.5 mg of the sample was put in a sample bottle, mixed with 1 mL of a 6N-HCl solution containing 1% phenol, charged with nitrogen for about one minute to remove air, and then quickly covered with aluminum foil. The bottle mouth was sealed with fire immediately, after which the sample bottle was kept in an oven for 24 h at 105 °C for acid hydrolysis. Afterwards, the bottle was taken out and cooled at room temperature, the seal was broken off, and the contents were dried in a vacuum drying dish at 70 °C. A 1 mL amount of 0.01 N was put in the sample bottle for redissolution and then filtered with a 0.22 μm syringe filter into a test tube. The sample was diluted 1000 times. The diluted sample and o-phythalaldehyde (OPA) were added at a ratio of 1:1 at room temperature and vibrated for 30 s, after which the amino acid content was analyzed using high-performance liquid chromatography (HPLC).
2.10. Statistical Analysis
The experiment data were tested using the one-way analysis of variance and the Statistical Analysis System (SAS-Windows 10) software to check whether there were significant differences among the experimental groups. When there was a difference in the average value (p < 0.05), the significance of the intergroup difference was analyzed using Duncan’s new multiple range test.
4. Discussion
In this study, the experimental feed’s nutrient composition changed as the amount of black soldier fly meal added to it was increased. Furthermore, the highly unsaturated fatty acid and total essential amino acid contents decreased as more black soldier fly meal was added to the feed, possibly because of the media in which black soldier fly are bred. Similar phenomena have been reported in other studies. For example, Ref. [
14] used chicken manure to breed black soldier flies and then produced meal from them, fed the meal to yellow catfish in a feeding experiment, and discovered that the black soldier fly meal could substitute for 34% of fish meal as a protein source. Ref. [
32] employed a peanut bran medium to breed black soldier flies, produced meal from them, and fed the meal to yellow catfish; the experimental results revealed that this meal could substitute for only 12% of fish meal as a protein source. Ref. [
33] produced black soldier fly meal from flies feeding on food waste, fed yellow catfish with this meal, and reported that it could substitute for only 14% of fish meal as a protein source. Also using food waste to breed black soldier flies, Ref. [
34] and Ref. [
33] have produced meal from the flied and fed this meal to white shrimps in their experiments; the meal they produced could substitute for 23.5% and 10% of fish meal as a protein source, respectively. In the present study, increases in the amount of black soldier fly meal added to the feed in the place of fish meal may have reduced the content of essential amino acid, resulting in an unbalanced amino acid composition and changing the content of highly unsaturated fatty acid in the feed. Such changes in nutrient composition undermined the jade perch fingerlings’ growth performance. Furthermore, anti-nutritional factors are compounds that reduce the absorption of nutrients, such as phytic acid in soybeans [
35]. Therefore, in this study, black soldier flies may contain antinutrients, which is likely caused by the different chemical compositions of the soybean meal on which the insects feed. In summary, although black soldier fly meal is a favorable protein source, its suitability for use in aquaculture feed depends on how the black soldier flies are bred.
Extensive research and discussions have been conducted regarding the performances of alternative ingredients to fish meal. However, related research has predominantly focused on whether the nutrient compositions of such alternatives meet the needs of aquatic organisms, without discussing how nutrient absorption can be improved for these organisms. Intestinal health is critical for the digestion and absorption of nutrients, the resistance to pathogenic micro-organisms, the influence of food antigens on organisms, and the secretion of hormones involved in the regulation of antimicrobial peptides and food intake [
36]. Ref. [
37] suggested that butyric acid can provide energy to epithelial cells, substantially increase cell proliferation, and improve the colonic barrier function. Ref. [
38] noted that a black soldier fly meal protein content higher than 5.3% in feeds caused damage to fish intestinal villi, created vacuoles in the hepatopancreas, and reduced lipid accumulation in tissues. This may result from the chitin existing in black soldier fly meal. Chitin is widely distributed within insects, and chitin polysaccharides account for approximately 20% of the dry weight of insect shells [
39]. Ref. [
38] indicated that chitin and its derivatives were reported to play a significant role in decreasing fatty acid synthesis as well as decreasing the digestibility of crude protein.
In the present study, butyric acid was added to a variety of feed formulas for the feeding experiment, which revealed a significantly reduced intestinal villi length (
p < 0.05) when black soldier fly meal without supplemented butyric acid was used as a substitute for fish meal in the feed. However, the addition of butyric acid significantly improved the growth of the jade perch fingerlings, their intestinal villi length, and their antioxidant enzyme activity (
p < 0.05). These results verified the benefits of adding butyric acid to feed and thus were consistent with the finding of Ref. [
40], namely that adding 1.3–1.5 mg/kg of sodium butyrate nanoparticles to their feed increased the surface area of the intestinal villi of Nile tilapia (
Oreochromis niloticus) fingerlings, thereby improving their growth performance. Ref. [
41] and [
42] have reported that adding 2 g/kg of butyric acid to their feed can improve the growth of grass carp (
Ctenopharyngodon idellus). Similar growth improvement was achieved by Ref. [
37] by adding 3 g/kg of butyric acid to the feed of sea bream (
Sparus aurata). However, Ref. [
43] added 500 mg/kg of butyric acid to the feed of grass carp (
Ctenopharyngodon idella) and observed no effect of the butyric acid on the grass carp’s growth; nevertheless, butyric acid was found to promote the growth of healthy bacteria in the intestines. Ref. [
41] and Ref. [
44] added an acidifier to the feed of Nile tilapia fingerlings that weighed 26 g, and reported that the acidifier significantly improved the growth of healthy intestinal microbiota and reduced the numbers of pathogenic bacteria. The present study’s growth parameters and intestinal tissue sections revealed that the study groups that consumed the feeds containing butyric acid had significantly longer intestinal villi than did those that consumed the feeds not containing butyric acid. Furthermore, the longer villi increased the intestines’ absorptive surface area, which in turn enhanced these groups’ nutrient absorption and growth performance.
Regarding feed performance, the FM group’s protein efficiency ratio (1.8%) was significantly higher than those of the FBM (1.3%) and BM (1.2%) groups. This finding indicated a greater protein efficiency in jade perch fingerlings when fish meal was the main protein source. Among the groups that consumed feeds containing butyric acid, the FMB group had the highest protein efficiency ratio (2.5%;
p < 0.05). However, no significant difference was noted between the protein efficiency ratios of the FBMB and FM groups, possibly because of the addition of butyric acid. Ref. [
45] indicated that butyric acid can inhibit harmful bacteria and promote the reproduction of beneficial bacteria after entering bacterial cells. Butyrate can also induce the synthesis of intestinal epithelial mRNA and protein, thus maintaining intestinal health, accelerating the proliferation of intestinal villus, and promoting nutrient absorption. This finding is exemplified by the study’s intestinal tissue sections, which showed an increased length in the anterior intestinal villi (26.16 mm) and indicating greater intestinal absorption in the FMB group. This observation is consistent with the finding of Ref. [
46], namely that butyric acid promoted nutrient digestion and absorption by increasing the number of epithelial cells in the fish intestine. The intestine is the organ where nutrient absorption primarily occurs in fish; nutrients are transported in and out of intestinal cells through the brush border as well as specific transport proteins located outside the intestinal cell membrane [
47,
48]. Accordingly, the length of intestinal villi is closely associated with intestinal health; good intestinal health is necessary for efficient nutrient absorption to promote growth in organisms [
49].
The nutrient composition of a diet affects the construction of intestinal villi, especially protein sources and their amino acid compositions. Many histological studies have been investigating the impact of various dietary protein sources and unbalanced amino acid composition in fish including rainbow trout [
50], gilthead sea bream [
51], and common carp [
52]. The partial amino acid deficiency in black soldier fly meal protein-based diets (BM and BMB) adversely affected the fish intestinal epithelium. Therefore, the histological effects on the intestine observed in this study may be partly explained by an amino acid imbalance in black soldier fly meal. The experimental results of this study revealed that, with regards to the amino acid composition balance in diets, adding butyric acid significantly increased the length of the anterior intestinal villi and thus benefited the intestinal health and nutrient absorption of the jade perch fingerlings.
Changes in blood parameters, which are sensitive to the nutrient composition of feed, may serve as a critical reference for assessing the health and physiological status of fish [
53]. Ref. [
54] highlighted that the HGB and Hct of fish decreased when the amount of nutrients was insufficient, thereby proving that blood parameters are effective indicators of fish health. In the present study, adding butyric acid to the feed significantly increased the RBC count, the HGB, and the Hct of the jade perch fingerlings. This result is consistent with those of other studies on fish. For example, Ref. [
40] added 1–2 mg/kg of butyric acid nanoparticles to the feed of Nile tilapia and observed a significantly increased RBC count, HGB concentration, Hct, and white blood cell count. Ref. [
41] added 2–3 g/kg of sodium butyrate to the feed of European seabass fingerlings and observed increases in the HGB, Hct, RBC count, MCHC, and white blood cell count. In the present study, the feeds containing butyric acid significantly increased the blood parameter values of the jade perch fingerlings, thereby demonstrating the health benefits of butyric acid to these fingerlings.
According to Ref. [
55], changes in serum ALT and AST activities are associated with hepatic steatosis. The present study revealed that the jade perch fingerlings consuming the butyric-acid-containing feeds had significantly higher ALT and AST activities in the serum than did those consuming the feeds not containing butyric acid. Moreover, no significant differences were noted in the serum ALT and AST activities of the fingerlings consuming the feeds where the fish meal was replaced with black soldier fly meal and those consuming the feeds that contained fish meal as the sole protein source. The present results revealed that adding butyric acid to the feeds may have stimulated the fingerlings’ liver to some extent. However, no comprehensive discussion has been conducted regarding whether butyric acid causes hepatic damage in aquatic organisms. Ref. [
40] conducted a feeding experiment by adding 2 mg/kg of butyric acid to the feed of Nile tilapia initially weighing 25.3 g and observed no hepatic damage in this Nile tilapia. Presenting a contrasting finding, Ref. [
40] added 2 g/kg of butyric acid to the feed of largemouth bass (
Micropterus salmoide) with an initial weight of 12.3 g and noted increased ALT and AST activities in the liver, which was consistent with histopathological changes. Accordingly, butyric acid’s damage to the liver may vary depending on the species and size of fish, the alternative protein sources used, and the environmental conditions. Several studies have reported that specific antimicrobial peptides and immunologically active substances in insect meal may improve the immunocompetent and antioxidant capacities of organisms. For example, Ref. [
56] found that adding maggot meal to the feed of black carp significantly increased the SOD and CAT activities and reduced the MDA content in the serum and liver of the black carp. Similarly, Ref. [
57] substituted maggot meal for fish meal in the feed of yellow catfish and demonstrated that when 20% of fish meal was replaced with maggot meal, the catfish exhibited decreased MDA content and increased SOD activity in the serum. This finding is inconsistent with the present study’s finding that substituting black soldier fly meal for more than 50% of the fish meal content in the feed resulted in an increased MDA content and decreased antioxidant enzyme activity in the liver. Ref. [
38] conducted a study on carp and found that the carp’s serum MDA content increased with the percentage of fish meal substituted with defatted black soldier fly meal as the feed’s protein source. Accordingly, an appropriate amount of black soldier fly meal may improve the antioxidant capacity of fish, whereas an excessive amount could lead to negative outcomes, such as increased oxidative stress. Sodium butyrate administration increased antioxidant gene expression, such as the SOD, CAT, GPx, GST and GR genes, and consequently these enzyme activities increased in the intestines of fish, which led to lower ROS formation in the intestinal tissues, thereby reducing oxidative stress [
58,
59]. Ref. [
60] suggested that excessive ROS could exacerbate increased MDA activity leading to lipid peroxidation, which decomposes and damages deoxyribonucleic acid, proteins, and the cytoplasm, resulting in cellular structural injury in organisms. When experiencing oxidative damage, an organism responds physiologically by increasing the activities of such antioxidant enzymes as SOD, CAT, and GPx [
61]. These enzymes protect organisms from the oxidative stress caused by free radicals [
62]. The present study verified the effectiveness of butyric acid in weakening the relationship between oxidant enzymes and lipid peroxidation indicators in jade perch fingerlings. Regarding the oxidative stress and lipid peroxidation induced in the process of replacing fish meal with black soldier fly meal, increasing the percentage of fish meal substituted with black soldier fly meal significantly decreased the SOD, CAT, and GPx activities and significantly increased the MDA content (
p < 0.05). According to Ref. [
63], antioxidant enzyme activity is negatively correlated with lipid peroxidation because antioxidant enzymes act against the ROS generated from oxidative stress. In the present study, the jade perch fingerlings that consumed feed containing butyric acid exhibited higher SOD, CAT, and GPx activities and lower MDA content than did those that consumed feed not containing butyric acid. This finding verified the benefit of butyric acid in inhibiting oxidation. In a two-way ANOVA, the interaction between the feed’s protein source composition and butyric acid content was found to significantly influence the antioxidant enzyme and lipid peroxidation indicators. Ref. [
64] argued that organic acid can increase the antioxidant responses of aquatic animals; this argument has been verified in multiple fish species, including grass carp [
42], Nile tilapia [
65], and Pengze crucian carp [
66]. In this study, the jade perch fingerlings that consumed the feeds containing butyric acid were more resistant to oxidative stress, which indicated that they were healthier compared with those that consumed the feeds not containing butyric acid.