# Response of Gut Microbiota, Digestive Enzyme Ability, and Immune Function to Starvation in the Oriental River PrawnMacrobrachium nipponense

Authors: Wenying Shen; Yin Qu; Han Zhang; Xiaodong Zhang; Freeman Bluefin Masell; Gang Ren
Journal: Aquaculture Nutrition
 (2022)

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## Abstract

In order to evaluate the interplay of nutritional status and the digestive capacity, immune function, and gut microbiota in the oriental river prawnMacrobrachium nipponense, a 14-day starvation trial was conducted to detect the effects of starvation on the activities of digestive enzymes and immune enzymes and the structure of prawn gut microbiota. The adult prawns were randomly assigned to a control group (F group) and starvation group (S group) with three replicates. The F group was normally fed with commercial diet, and the S group was starved for 14 days. The result showed that digestive enzyme activities of trypsin and lipase in the hepatopancreas of the S group were significantly lower than those of the F group after 4 d of starvation (P<0.05), while the activity of amylase significantly increased after 14 d of starvation (P<0.05). Moreover, the results of the histological analysis of prawn gut showed that both the height of epithelial cells and microvilli of intestine in the S group were obviously decreased than those in the F group (P<0.05) after 14 d of starvation. The activities of immune-related enzymes including superoxide dismutase, catalase, and acid phosphatase in the hepatopancreas of the S group significantly decreased after 4 d of starvation, and lysozyme activity of the F group was lower than that of the S group after 7 d of starvation (P<0.05). In addition, the results of Illumina high-throughput sequencing showed that a total of 14,285 OTUs were obtained and classified into 30 phyla, among which Actinobacteria and Proteobacteria were the predominant microflora in the intestinal microbial communities of both groups. However, the relative abundance of opportunistic pathogens was significantly increased in the S group, while the relative abundance of beneficial bacterium was decreased (P<0.05). The bacterial richness with the Chao estimator was significantly higher in the F group than in the S group (P<0.05). Both the results of principal coordinate analysis (PCoA) and nonmetric multidimensional scaling (NMDS) demonstrated that the intestinal microbiota of the F group was separate from those of the S group. The result of functional prediction of the metabolic pathways showed that the intestinal microbiota was enriched in the KEGG pathways of amino acid, carbohydrate, fatty acid, and lipid biosynthesis and degradation at level 2. This result implied that the microbiota of shrimp gut decreased nutrition metabolism under the stress of starvation. Meanwhile, comparing to the F group, the immune-related pathway of enterobacterial common antigen biosynthesis was markedly reduced in the S group (P<0.05). The result of redundancy analysis (RDA) further confirmed that the activities of digestive and immune enzymes were correlated with the microbial community structure. Finally, the structural equation modeling highlighted that changes in the activities of digestive and immune enzymes were directly related to the gut bacterial community and notably affected prawn growth.


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## Body

## 1. Introduction

Aquaculture species suffer from transient food deprivation caused by climate changes, migration, and reproduction and may also suffer from starvation due to feed cost reduction, stress of transportation, management of disease outbreaks, and water quality amelioration [1]. During the starvation period, animal metabolism is adapted to utilize fuel stores for surviving and maintaining body functions [2, 3]. It was reported that shrimp could regulate the digestion activity in response to short-term starvation [4]. The activities of the digestive enzymes could be significantly downregulated in shrimp during fasting periods, reducing the mechanochemical stimulators of the gastrointestinal tract [5] and drastically altering the morphological structure of the gastrointestinal tract [6]. The digestive enzyme activities of crustaceans under the stress of starvation depend on the duration of food deprivation. The protease activities in the juveniles of Fenneropenaeus chinensis were significantly decreased when exposed to food deprivation at different periods and then rapidly increased after food refeeding, but the changes of amylase and lipase activities exhibited opposite trends [7]. The activities of amylase, lipase, and pepsin were significantly lower in the starved group of Litopenaeus vannamei than in a normal fed group [8]. Because of the inconsistent results as mentioned above, it is necessary to further investigate the response of the digestive enzymes and their regulation mechanism under starvation stress in more shrimp species. Previous studies had demonstrated that starvation also affected the nonspecific immune activity of fishes. Starvation significantly promoted the lysozyme activities in the sea bass Dicentrarchus labrax and Pagellus bogaraveo [2] and the activities of antioxidative enzymes and such as superoxide dismutase (SOD) in Labeo rohita[9]. Nevertheless, little is known about the mechanism of starvation on immune activities of crustaceans. The intestinal microbes are a complex organ ecosystem and have a profound influence on nutrient metabolism, pathogen resistance, and immune system development [10]. Studies had found that the diet could shape the intestinal microbiota in the host [11, 12]. The changes in the gut microbial composition had marked effects on health, growth, and survival of farmed fishes and crustaceans [13]. However, the information on the relationship between feeding regimes and intestinal microbiota was still limited in crustaceans. Recent studies had shown that starvation stress affected the composition structure of intestinal microbiota [8], and the changes in the gut microbial community were related to digestive and immune enzyme activities, which subsequently affected the growth of L. vannamei [14].The oriental river prawnMacrobrachium nipponense is a nutritional and economic species of the decapod crustacean throughout China, Japan, and Vietnam [15]. Previous studies had proven that there was complete compensatory growth in this species following 2 or 4 d of starvation [16]. During the period of starvation, the activities of pepsin, tryptase, and lipase significantly decreased while the activity of amylase increased at 4 d, but the activities of immune-related enzymes SOD and CAT increased a little at 2 d and then decreased significantly at 8 d [5]. The effects of starvation on the composition of intestinal microbiota and the interplay among shrimp gut microbiota and digestive and immune enzyme activities in M. nipponense were still unclear. The aim of this study was to explore the effect of starvation stress on the changes and relationship among the activities of digestive and immune-related enzymes and the structure of gut microbiota in M. nipponense.


## 2. Materials and Methods

### 2.1. Rearing Procedures

All animal experiments were carried out under strict accordance with the Guide for the Care and Use of Laboratory Animal at Shaoxing University and were approved by the Bioethics Committee of Shaoxing University. Healthy prawns were obtained from a local freshwater farm in Shaoxing city (Zhejiang, China). Before the feeding trial, prawns were acclimated for one week and fed with commercial feed (Zhejiang Kesheng Feed Co., Ltd., Shaoxing, China) in round fiberglass tanks of 750 L. The composition of the feed (wet weight) contained 39.22% of crude protein, 6.25% of crude fat, 3.87% of crude fiber, 13.28% of crude ash, and 9.39% of moisture, and its gross energy was 4339 kcal kg-1. At the end of the acclimatization period, a total of 180 prawns with an average initial weight of 2.90±0.08 g and length of 6.31±0.11 cm were randomly assigned to two groups with three replicates. The feeding group (F group) was continuously fed, and the starvation group (S group) was continuously fasted during the experimental period of 14 d.


### 2.2. Sample Preparation

At the end of the experiment, the weight growth rate (WGR) of the different groups was calculated according to the following equation:WGR%=100×Wt−W0/W0, where Wt is the weight of prawns at the termination of the experiment and W0 is the weight of prawns at the start of the experiment.At the end of the experiment period of 14 d, ten individual prawns per tank were randomly chosen and aseptically dissected in an ice bath; then, their intestinal tissues were isolated. Subsequently, the midguts of five prawns were segmented into the same length and fixed with 10% formalin solution for 24 h before histological analysis. The whole guts of the other five prawns were directly frozen in liquid nitrogen, then stored at −80°C before microbiota analysis. At 0, 4, 7, 11, and 14 d after starvation, the hepatopancreas from three prawns of both groups was immediately extracted and pooled for the measurement of the digestive and immune-related enzyme activities. These tissues were homogenized in 10x volumes (original tissue weight/volume) of phosphate buffer saline (PBS) and centrifuged at 6000 g for 10 min at 4°C. The supernatant was harvested to measure the activities of the digestive enzyme including amylase (AMS), trypsin (TRY), and lipase (LPS) and the immune-related enzyme including superoxide dismutase (SOD), catalase (CAT), lysozyme (LZM), and acid phosphatase (ACP) with the commercial kits (Nanjing Jiancheng Bioengineering Institute, Nanjing, China), according to the manufacturers’ protocol. Total protein concentration was determined by the method of Coomassie Brilliant Blue G-250 with bovine serum albumin as a standard [17]. The enzyme-specific activities were expressed as U mg−1 protein.


### 2.3. Digestive and Immune Enzyme Activity Assays

Amylase activity (U mg-1 protein) was determined by the iodine-starch colorimetric method and defined as hydrolyzing 10 mg of starch with 1 mg tissue protein acting on the substrate within 30 min at 37°C. Lipase activity (U mg-1 protein) was defined as the amount of enzyme which consumes 1 μmol substrate when incubating with 1 mg tissue protein in 1 min at 37°C. Trypsin was measured by incubating the mixtures in a water bath at 37°C, and absorbance A1 and A2 were recorded at 253 nm after mixing for 0.5 min and 20.5 min, respectively. The ACP activities were measured using a disodium phenyl phosphate method [18]. One unit of ACP activity was defined as the production of 1 mg total protein to produce 1 mg phenol in 15 min at 37°C. The SOD activity was measured spectrophotometrically using the xanthine oxidase-cytochrome c method at the wavelength of 550 nm [19]. One unit of SOD activity was defined as the amount required to inhibit the rate of reduction of cytochrome c by 50% and determined as ng of SOD mg-1 protein in the supernatant fraction. The CAT activity was measured by the disappearance rate of H2O2 at 240 nm [20]. One unit of CAT activity is defined as the amount of enzyme catalyzing the degradation of 1 μmol of H2O2 min-1 and the specific activity corresponding to μmol transformation of substrate (H2O2) min-1 mg-1 protein. Lysozyme activity was measured with the turbidimetric method [21]. One unit of LZM activity was defined as the absorbance change in the cell suspension of Micrococcus luteus per min. Lyophilized M. flavus cells were resuspended in 2.0 mL of 0.05 M phosphate buffer (pH 6.2) at the concentration of 0.25 mg mL-1 and incubated at 30°C for 5 min, and then, 100 μL of the tissue supernatant was added to 2.0 mL of the suspension. The transmittance was measured after 5 s and 125 s at 540 nm. Lysozyme activity was defined as (T5-T125)/(S5-S125), where T was the sample transmittance and S was the standard transmittance.


### 2.4. Histological Assay

Gut segments were dehydrated with different gradients of alcohol concentration, cleaned in toluene, and embed in paraffin to make solid wax blocks. Then, the solid wax blocks were cut as continuous section blocks into sections 5μm thick using a rotary microtome. The prepared paraffin sections were stained by hematoxylin and eosin (H&E) and observed with a light microscope (Nikon Eclipse 80i, Tokyo, Japan). The epithelial cells and microvilli height of the gut were measured with a micrometer [22].


### 2.5. Gut DNA Extraction

The luminal contents of the gut were isolated, and the DNA of the total bacterial community were extracted using E.Z.N.A.™ Soil DNA Kit (Omega Bio-Tek, Norcross, USA) according to the manufacturer’s instructions. The quality of extracted DNA samples was measured using a NanoDrop spectrophotometer (Thermo Fisher Scientific, Waltham, MA, USA) and further confirmed by PCR amplification of the bacterial 16S rRNA gene.


### 2.6. Illumina High-Throughput Sequencing

The V3-V4 region of the 16S rRNA genes was amplified from the bacterial DNA template. The primers of 338F (5′-ACTCCTACGGGAGGCAGCA-3′) and 806R (5′-GGACTACHVGGGTWTCTAAT-3′) were used, which were modified with 7 bp barcodes to distinguish the PCR products. PCR amplification was performed according to the reported protocol of Shao et al. [23]. PCR products were detected by agarose gel electrophoresis and subsequently purified using an AxyPrep™ DNA gel extraction kit (Axygen, Hangzhou, China). Each purified PCR product was sequenced with Illumina high-throughput sequencing (Shanghai Personal Biotechnology Co., Ltd., Shanghai, China).


### 2.7. Processing of Illumina Sequencing Data

Raw FASTQ file reads were analyzed and quality-filtered. Operational taxonomic units (OTUs) were defined as sequences clustered with a threshold of 97% similarity using UCLUST [24]. Taxonomic richness estimators and community diversities were determined for each library in Mothur [25]. The species richness for each community was estimated based on OTU abundance matrices. Alpha diversity indices, Chao richness estimator, Shannon [26] and Simpson [27] diversity indexes, were used for assessing community diversity. Beta diversity indexes, including the principal coordinate analysis (PCoA) and nonmetric multidimensional scaling (NMDS), were performed to investigate the structural variation of microbial communities across samples using UniFrac distance metrics [28, 29]. The taxonomy compositions and abundances were visualized using GraPhlAn [30]. A Venn diagram was generated to represent the number of shared and unique species among groups and percentages (%) of OTUs. Normalized abundance was shown by heat map using pheatmap. Microbial functions were predicted with PICRUSt (version 1.1.0), based on high-quality sequences [31]. Predicted functional pathways were annotated by using the Kyoto Encyclopedia of Genes and Genomes (KEGG) at level 2 [32]. Redundancy analysis (RDA) was performed using Canoco 5.0 to reveal the effect of digestive and immune enzymes on bacterial communities, and the significant factor was chosen according to P value (P<0.05, [33]). To explore the interplay among shrimp digestion and immune enzyme activities, gut microbiota, and shrimp growth traits under starvation stress, the data matrix was fitted using structural equation modeling (SEM) based on the maximum-likelihood estimation method. The favorable model was confirmed using the nonsignificant x2 (chi-square) test (P>0.05), root of mean square residual (RMR<0.1), high goodness-of-fit index (GFI>0.90), and root-mean-square error of approximation (RMSEA<0.05). Only OTUs with IndValvalues>0.80 and significance<0.05 were selected as indicators for distinguishing starved and feeding shrimp, as described in a previous study [34].


### 2.8. Data Analysis and Statistics

The data of enzyme activities were presented as themean±standarddeviation (SD) and were analyzed with an unpaired t-test. The value of P<0.05 was set for the statistical significance level and P<0.01 for very significance level.


### 2.9. Accession Number

The raw data in this study had been deposited in the NCBI Sequence Read Archive database. The accession number is PRJNA778555.


## 2.1. Rearing Procedures

All animal experiments were carried out under strict accordance with the Guide for the Care and Use of Laboratory Animal at Shaoxing University and were approved by the Bioethics Committee of Shaoxing University. Healthy prawns were obtained from a local freshwater farm in Shaoxing city (Zhejiang, China). Before the feeding trial, prawns were acclimated for one week and fed with commercial feed (Zhejiang Kesheng Feed Co., Ltd., Shaoxing, China) in round fiberglass tanks of 750 L. The composition of the feed (wet weight) contained 39.22% of crude protein, 6.25% of crude fat, 3.87% of crude fiber, 13.28% of crude ash, and 9.39% of moisture, and its gross energy was 4339 kcal kg-1. At the end of the acclimatization period, a total of 180 prawns with an average initial weight of 2.90±0.08 g and length of 6.31±0.11 cm were randomly assigned to two groups with three replicates. The feeding group (F group) was continuously fed, and the starvation group (S group) was continuously fasted during the experimental period of 14 d.


## 2.2. Sample Preparation

At the end of the experiment, the weight growth rate (WGR) of the different groups was calculated according to the following equation:WGR%=100×Wt−W0/W0, where Wt is the weight of prawns at the termination of the experiment and W0 is the weight of prawns at the start of the experiment.At the end of the experiment period of 14 d, ten individual prawns per tank were randomly chosen and aseptically dissected in an ice bath; then, their intestinal tissues were isolated. Subsequently, the midguts of five prawns were segmented into the same length and fixed with 10% formalin solution for 24 h before histological analysis. The whole guts of the other five prawns were directly frozen in liquid nitrogen, then stored at −80°C before microbiota analysis. At 0, 4, 7, 11, and 14 d after starvation, the hepatopancreas from three prawns of both groups was immediately extracted and pooled for the measurement of the digestive and immune-related enzyme activities. These tissues were homogenized in 10x volumes (original tissue weight/volume) of phosphate buffer saline (PBS) and centrifuged at 6000 g for 10 min at 4°C. The supernatant was harvested to measure the activities of the digestive enzyme including amylase (AMS), trypsin (TRY), and lipase (LPS) and the immune-related enzyme including superoxide dismutase (SOD), catalase (CAT), lysozyme (LZM), and acid phosphatase (ACP) with the commercial kits (Nanjing Jiancheng Bioengineering Institute, Nanjing, China), according to the manufacturers’ protocol. Total protein concentration was determined by the method of Coomassie Brilliant Blue G-250 with bovine serum albumin as a standard [17]. The enzyme-specific activities were expressed as U mg−1 protein.


## 2.3. Digestive and Immune Enzyme Activity Assays

Amylase activity (U mg-1 protein) was determined by the iodine-starch colorimetric method and defined as hydrolyzing 10 mg of starch with 1 mg tissue protein acting on the substrate within 30 min at 37°C. Lipase activity (U mg-1 protein) was defined as the amount of enzyme which consumes 1 μmol substrate when incubating with 1 mg tissue protein in 1 min at 37°C. Trypsin was measured by incubating the mixtures in a water bath at 37°C, and absorbance A1 and A2 were recorded at 253 nm after mixing for 0.5 min and 20.5 min, respectively. The ACP activities were measured using a disodium phenyl phosphate method [18]. One unit of ACP activity was defined as the production of 1 mg total protein to produce 1 mg phenol in 15 min at 37°C. The SOD activity was measured spectrophotometrically using the xanthine oxidase-cytochrome c method at the wavelength of 550 nm [19]. One unit of SOD activity was defined as the amount required to inhibit the rate of reduction of cytochrome c by 50% and determined as ng of SOD mg-1 protein in the supernatant fraction. The CAT activity was measured by the disappearance rate of H2O2 at 240 nm [20]. One unit of CAT activity is defined as the amount of enzyme catalyzing the degradation of 1 μmol of H2O2 min-1 and the specific activity corresponding to μmol transformation of substrate (H2O2) min-1 mg-1 protein. Lysozyme activity was measured with the turbidimetric method [21]. One unit of LZM activity was defined as the absorbance change in the cell suspension of Micrococcus luteus per min. Lyophilized M. flavus cells were resuspended in 2.0 mL of 0.05 M phosphate buffer (pH 6.2) at the concentration of 0.25 mg mL-1 and incubated at 30°C for 5 min, and then, 100 μL of the tissue supernatant was added to 2.0 mL of the suspension. The transmittance was measured after 5 s and 125 s at 540 nm. Lysozyme activity was defined as (T5-T125)/(S5-S125), where T was the sample transmittance and S was the standard transmittance.


## 2.4. Histological Assay

Gut segments were dehydrated with different gradients of alcohol concentration, cleaned in toluene, and embed in paraffin to make solid wax blocks. Then, the solid wax blocks were cut as continuous section blocks into sections 5μm thick using a rotary microtome. The prepared paraffin sections were stained by hematoxylin and eosin (H&E) and observed with a light microscope (Nikon Eclipse 80i, Tokyo, Japan). The epithelial cells and microvilli height of the gut were measured with a micrometer [22].


## 2.5. Gut DNA Extraction

The luminal contents of the gut were isolated, and the DNA of the total bacterial community were extracted using E.Z.N.A.™ Soil DNA Kit (Omega Bio-Tek, Norcross, USA) according to the manufacturer’s instructions. The quality of extracted DNA samples was measured using a NanoDrop spectrophotometer (Thermo Fisher Scientific, Waltham, MA, USA) and further confirmed by PCR amplification of the bacterial 16S rRNA gene.


## 2.6. Illumina High-Throughput Sequencing

The V3-V4 region of the 16S rRNA genes was amplified from the bacterial DNA template. The primers of 338F (5′-ACTCCTACGGGAGGCAGCA-3′) and 806R (5′-GGACTACHVGGGTWTCTAAT-3′) were used, which were modified with 7 bp barcodes to distinguish the PCR products. PCR amplification was performed according to the reported protocol of Shao et al. [23]. PCR products were detected by agarose gel electrophoresis and subsequently purified using an AxyPrep™ DNA gel extraction kit (Axygen, Hangzhou, China). Each purified PCR product was sequenced with Illumina high-throughput sequencing (Shanghai Personal Biotechnology Co., Ltd., Shanghai, China).


## 2.7. Processing of Illumina Sequencing Data

Raw FASTQ file reads were analyzed and quality-filtered. Operational taxonomic units (OTUs) were defined as sequences clustered with a threshold of 97% similarity using UCLUST [24]. Taxonomic richness estimators and community diversities were determined for each library in Mothur [25]. The species richness for each community was estimated based on OTU abundance matrices. Alpha diversity indices, Chao richness estimator, Shannon [26] and Simpson [27] diversity indexes, were used for assessing community diversity. Beta diversity indexes, including the principal coordinate analysis (PCoA) and nonmetric multidimensional scaling (NMDS), were performed to investigate the structural variation of microbial communities across samples using UniFrac distance metrics [28, 29]. The taxonomy compositions and abundances were visualized using GraPhlAn [30]. A Venn diagram was generated to represent the number of shared and unique species among groups and percentages (%) of OTUs. Normalized abundance was shown by heat map using pheatmap. Microbial functions were predicted with PICRUSt (version 1.1.0), based on high-quality sequences [31]. Predicted functional pathways were annotated by using the Kyoto Encyclopedia of Genes and Genomes (KEGG) at level 2 [32]. Redundancy analysis (RDA) was performed using Canoco 5.0 to reveal the effect of digestive and immune enzymes on bacterial communities, and the significant factor was chosen according to P value (P<0.05, [33]). To explore the interplay among shrimp digestion and immune enzyme activities, gut microbiota, and shrimp growth traits under starvation stress, the data matrix was fitted using structural equation modeling (SEM) based on the maximum-likelihood estimation method. The favorable model was confirmed using the nonsignificant x2 (chi-square) test (P>0.05), root of mean square residual (RMR<0.1), high goodness-of-fit index (GFI>0.90), and root-mean-square error of approximation (RMSEA<0.05). Only OTUs with IndValvalues>0.80 and significance<0.05 were selected as indicators for distinguishing starved and feeding shrimp, as described in a previous study [34].


## 2.8. Data Analysis and Statistics

The data of enzyme activities were presented as themean±standarddeviation (SD) and were analyzed with an unpaired t-test. The value of P<0.05 was set for the statistical significance level and P<0.01 for very significance level.


## 2.9. Accession Number

The raw data in this study had been deposited in the NCBI Sequence Read Archive database. The accession number is PRJNA778555.


## 3. Result

### 3.1. Growth Performance, Digestive Enzyme Activity, and Intestinal Structure

After 14 d of starvation, the weight and the growth gain rate of the S group were significantly lower than those of the F group (Table1). The activities of trypsin and lipase in the hepatopancreas of the S group were significantly lower after 4 d of starvation (P<0.05). However, the activity of amylase in the hepatopancreas of the S group was significantly higher than that of the F group (P<0.05) at 14 d after starvation (Figure 1). The intestinal epithelial cells of the F group were closely connected, and their microvilli were abundantly and neatly arranged on the free surface of the epithelial cells. On the contrary, intestinal epithelial cells of the S group were shrunken or even disappeared and the height of epithelial cells and microvilli simultaneously decreased (Figure 2). The height of epithelial cells and microvilli of the midgut from the S group shrimps at 14 d after starvation (65.54±6.03 μm) were significantly lower than those from the F group (86.80±6.49 μm) (P<0.05).Table 1
Growth performance of prawn under the treatment of starvation and normal feeding.
Feeding groupStarvation groupW0 (g)2.89±0.082.89±0.08Wt (g)3.32±0.11∗2.59±0.16WGR (%)15.32±0.37∗−10.12±1.00Data are presented asmean±SD (n=10). Statistical significance is tested using an unpaired t-test (∗P<0.05). W0: initial weight; Wt: final weight; WGR: weight growth rate.Figure 1
The changes of digestive enzyme activities in the hepatopancreas ofM. nipponense after 14 d of starvation: (a) amylase (AMS); (b) lipase (LPS); (c) trypsin (TRY). Data are presented as mean±SD (n=6). Statistical significance is tested using an unpaired t-test (∗P<0.05).
(a)(b)(c)Figure 2
The changes of the intestinal histological structure inM. nipponense after 14 d of starvation by hematoxylin and eosin staining. Magnification is 400x, and the scale represents 50 μm. (a) Arrow shows that the epithelial cells were closely connected in the feeding group. (b) Arrow shows that the epithelial cells were shrunk or even disappeared in the starvation group. (c) Comparisons of the height of intestinal epithelial cells and microvilli in F (feeding) group and S (starvation) group. Results are presented as means±SD of ten observations for three samples in each groups. Statistical significance is tested using an unpaired t-test (∗P<0.05).
(a)(b)(c)


### 3.2. Immune Enzyme Activity

The activities of immune-related enzymes, SOD, CAT, LZM, and ACP, in the hepatopancreas of the S group were consistently decreased after starvation. The activities of SOD, CAT, and ACP in the S group were significantly lower at 4 d after starvation when comparing with those in the F group (P<0.05), and the decrease of LZM activity in the S group appeared at 7 d after starvation (P<0.05) when comparing with those in the F group (Figure 3). However, the change of LZM activity to starvation stress was slow compared to the changes of the activities of SOD, CAT, and ACP.Figure 3
The changes of immune enzyme activities in the hepatopancreas ofM. nipponense after 14 d of starvation: (a) superoxide dismutase (SOD); (b) catalase (CAT); (c) lysozyme (LZM); (d) acid phosphatase (ACP). Data are presented as mean±SD (n=6). Statistical significance is tested using an unpaired t-test (∗P<0.05).
(a)(b)(c)(d)


### 3.3. Intestinal Microbiota Richness and Diversity Analysis

A total of 338,779 high-quality sequences were obtained from 6 samples of the intestinal bacteria, ranging from 50,795 to 62,676. The good coverage ranged from 0.989 to 0.997, which suggested that the complete microbial communities presented in the samples were identified completely. The sequences were clustered into operational taxonomic units (OTUs), and each OTU represented a unique phylotype. Finally, a total number of 14,285 OTUs were identified in all samples, and the number of OTUs detected in each sample ranged from 1569 to 3129. The total number of OTUs in the F group was significantly higher than that in the S group (P<0.05) (Table 2), but 742 OTUs were shared by these two groups (Figure 4).Table 2
Sequencing, OTU classification information, and Good’s coverage in six samples.
SampleReadsPhylumClassOrderFamilyGenusSpeciesUnclassifiedTotalGood’s coverageS16267630155644509548129120810.994S25416821171487559632182021030.996S3561392199205446569173215690.997F1507951323011661030539108031250.994F253041132941012701565115027610.992F36196024218947697544121126560.989Figure 4
The distribution difference of the OTUs in the gut microbiota of the F group and the S group ofM. nipponense after 14 d of starvation by Venn diagram.Bacterial richness and diversity were estimated with Chao, Shannon, and Simpson indices, respectively. The Chao estimator of the F group was significantly higher than that of the S group (P<0.05), but the two groups showed no significant difference in the Shannon or Simpson index (P>0.05, Table 3). The analysis of beta diversity by both PCoA and NMDS showed that samples of the F group were separated from those of the S group, indicating the potential influence of different feeding regimes on intestinal microbiota (Figure 5).Table 3
Data from Illumina high-throughput sequencing yields bacterial diversity and richness based on operational taxonomic units (OTU), estimated OTU richness (Chao), and diversity index (Shannon & Simpson) for the intestinal bacterial diversity analysis ofM. nipponense in two groups.
Diversity indexFeeding groupStarvation groupRichness estimatorsChao2942.67±187.70∗1969.33±327.39Diversity estimatorsShannonSimpson8.24±0.570.98±0.027.31±0.460.95±0.02Data are presented asmean±SD (n=3). Statistical significance is tested using an unpaired t-test (∗P<0.05).Figure 5
Beta diversity analysis of the gut microbiota of the F group and the S group ofM. nipponense after 14 d of starvation: (a) principal coordinate analysis (PCoA); (b) nonmetric multidimensional scaling (NMDS) of Bray-Curtis distances. F: feeding group; S: starvation group.
(a)(b)


### 3.4. Bacterial Community Analysis and Comparison

In this study, total OTUs of bacterial community in all samples were classified into 30 phyla. The top 20 most abundant OTUs were shown in the taxonomic composition of intestinal microbiota at the phylum level (Figure6), in which Actinobacteria and Proteobacteria were the predominant microflora phylum in the bacterial communities of both groups, and they accounted for 44.06±13.80% and 39.44±11.21% in the F group, respectively, and 39.06±12.00% and 35.82±3.77% in the S group, respectively. Firmicutes, Tenericutes, Bacteroidetes, and Chlamydiae were also abundant in all samples. The abundance of Bacteroidetes in the S group was significantly higher than that in the F group (P<0.05).Figure 6
The abundance changes of the intestinal bacteria ofM. nipponense at the phylum level after 14 d of starvation. Statistical significance is tested using an unpaired t-test (∗P<0.05).The heat map of intestinal bacterial abundance in intestines at the genus level showed that the abundance of harmful bacteria and potential harmful bacteria, such asAcinetobacter [35], Streptococcus [36], Enterococcus [37], and Rhodococcus [38], in the S group were larger than those in the F group (P<0.05), while the abundance of beneficial bacteria enriched in feeding prawns, such as Microbacterium [39], Rhodobacter ([40, 41]. [42]), and Anoxybacillus [43], were larger than in the S group (P<0.05) (Figure 7). These results indicated that comparing to feeding prawns, starved ones had more opportunistic pathogenic bacteria but less beneficial bacteria in the intestine.Figure 7
The abundance changes of the intestinal bacteria ofM. nipponense at the genus level after 14 d of starvation by heat map. Phylogenetic positions are projected by the OTUs, and the taxa of OTUs are listed on the right. Color intensity indicates the relative enrichment of OTUs. F: feeding group (F1-F3); S: starvation group (S1-S3).


### 3.5. Functional Prediction of Intestinal Microbiota

To compare the functional potentials of the intestinal microbiota between feeding and starved prawns, functional content was predicted in the KEGG database at level 2. Functional prediction showed that thirteen pathways including amino acid biosynthesis, cofactor, prosthetic group, electron carrier, vitamin biosynthesis, nucleoside and nucleotide biosynthesis, fatty acid and lipid biosynthesis, carbohydrate biosynthesis, cell structure biosynthesis, aromatic compound degradation, nucleoside and nucleotide degradation, fermentation, and TCA cycle were enriched in the intestinal microbiota after starvation (Figure8). Meanwhile, the predicted nutrition metabolism of glycolysis V was significantly enriched in the S group (P<0.05). Moreover, the degradation of glucose, fucose, lactose, galactose, sucrose and rhamnose, L-arginine and L-ornithine degradation, peptidoglycan, and L-tryptophan biosynthesis were significantly decreased when the S group was compared with the F group (P<0.05). This result implied that the gut microbiota of prawns adapted to the stress of starvation by decreasing nutrition metabolism to a certain degree. The immune system pathway of enterobacterial common antigen biosynthesis was markedly reduced in starved prawns (P<0.05) (Figure 9). Nevertheless, for the terms of digestive-related metabolism (amino acid, carbohydrate, fatty acid, and lipid biosynthesis and degradation) and immune-related metabolism functions (antibiotic resistance, methanol oxidation to carbon dioxide, and phospholipases), there was no significant difference in the F and S groups (P>0.05, Table 4).Figure 8
Relative abundance of functional pathways of the intestinal microbiota inM. nipponense. Pathways were predicted in the KEGG database at level 2.Figure 9
The changes of the KEGG pathways of intestinal bacteria inM. nipponense after 14 d of starvation. Pillars in the right column indicate significant increase, while those in the left column indicate significant decrease in the starvation group as compared with the feeding group in abundances of the corresponding pathways. F: feeding group; S: starvation group.Table 4
Relative abundance of digestive-related metabolism and immune-related metabolism functions in the starvation and feeding groups.
Feeding group (%)Starvation group (%)Amino acid biosynthesis14.73±0.2014.14±0.32Carbohydrate biosynthesis4.76±0.024.76±0.32Fatty acid and lipid biosynthesis8.14±0.827.96±0.18Amino acid degradation1.20±0.181.18±0.25Carbohydrate degradation1.87±0.231.95±0.27Fatty acid and lipid degradation0.72±0.030.79±0.17Antibiotic resistance0.01±0.090.21±0.31Methanol oxidation to carbon dioxide0.03±0.000.06±0.03Phospholipases0.011±0.010.01±0.07Note: there was no significant difference in two groups (P>0.05).


### 3.6. The Interplay among Prawn Gut Bacterial Community, Digestive and Immune Enzyme Activity, and Growth

Redundancy analysis (RDA) was performed to examine the relationships among microbial community structures, digestive enzyme activities, and immune enzyme activities (Figure10(a)). The result showed that the composition of the intestinal bacterial flora in the S group had significant difference with that in the F group after 14 d of starvation. Meanwhile, the changes were potentially related to immune indicators SOD (R2=0.436, P value = 0.188), LZM (R2=0.437, P value = 0.175), ACP (R2=0.434, P value = 0.207), and CAT (R2=0.424, P value = 0.201) and digestive indicators TRY (R2=0.424, P value = 0.214), LPS (R2=0.459, P value = 0.162), and AMS (R2 = 0.465, P value = 0.166). In the RDA space, only AMS was negatively correlated with the microbial community structure in starved prawns, but the other indicators expressed positively with the microbial community structure. These indicators had an impact on the diversity and species composition of the bacterial flora of the S group.Figure 10
(a) The relationships between microbial community structures and digestive enzyme activity and the immune enzyme activity of the starvation group and the feeding group inM. nipponense with redundancy analysis (RDA). F: feeding group; S: starvation group. (b) The structural equation model (SEM) shows the interplay among the intestinal bacterial community, immune enzyme activity, digestive enzyme activity, and weight gain rate of M. nipponense. Numbers on the arrow are standardized paths calculated by Pearson correlation coefficient. Arrow widths show the strength of the causal relationship. R2 of all paths (>0.8, P<0.05) indicated that the structural equation model analysis of variance results was statistically significant.
(a)(b)The structural equation modeling (SEM) revealed the interplay among the gut bacterial community, digestive and immune enzyme activities, and weight gain rate (Figure10(b)). The results indicated that changes of digestive and immune enzyme activities were directly related to the gut bacterial community and notably affected prawn growth.


## 3.1. Growth Performance, Digestive Enzyme Activity, and Intestinal Structure

After 14 d of starvation, the weight and the growth gain rate of the S group were significantly lower than those of the F group (Table1). The activities of trypsin and lipase in the hepatopancreas of the S group were significantly lower after 4 d of starvation (P<0.05). However, the activity of amylase in the hepatopancreas of the S group was significantly higher than that of the F group (P<0.05) at 14 d after starvation (Figure 1). The intestinal epithelial cells of the F group were closely connected, and their microvilli were abundantly and neatly arranged on the free surface of the epithelial cells. On the contrary, intestinal epithelial cells of the S group were shrunken or even disappeared and the height of epithelial cells and microvilli simultaneously decreased (Figure 2). The height of epithelial cells and microvilli of the midgut from the S group shrimps at 14 d after starvation (65.54±6.03 μm) were significantly lower than those from the F group (86.80±6.49 μm) (P<0.05).Table 1
Growth performance of prawn under the treatment of starvation and normal feeding.
Feeding groupStarvation groupW0 (g)2.89±0.082.89±0.08Wt (g)3.32±0.11∗2.59±0.16WGR (%)15.32±0.37∗−10.12±1.00Data are presented asmean±SD (n=10). Statistical significance is tested using an unpaired t-test (∗P<0.05). W0: initial weight; Wt: final weight; WGR: weight growth rate.Figure 1
The changes of digestive enzyme activities in the hepatopancreas ofM. nipponense after 14 d of starvation: (a) amylase (AMS); (b) lipase (LPS); (c) trypsin (TRY). Data are presented as mean±SD (n=6). Statistical significance is tested using an unpaired t-test (∗P<0.05).
(a)(b)(c)Figure 2
The changes of the intestinal histological structure inM. nipponense after 14 d of starvation by hematoxylin and eosin staining. Magnification is 400x, and the scale represents 50 μm. (a) Arrow shows that the epithelial cells were closely connected in the feeding group. (b) Arrow shows that the epithelial cells were shrunk or even disappeared in the starvation group. (c) Comparisons of the height of intestinal epithelial cells and microvilli in F (feeding) group and S (starvation) group. Results are presented as means±SD of ten observations for three samples in each groups. Statistical significance is tested using an unpaired t-test (∗P<0.05).
(a)(b)(c)


## 3.2. Immune Enzyme Activity

The activities of immune-related enzymes, SOD, CAT, LZM, and ACP, in the hepatopancreas of the S group were consistently decreased after starvation. The activities of SOD, CAT, and ACP in the S group were significantly lower at 4 d after starvation when comparing with those in the F group (P<0.05), and the decrease of LZM activity in the S group appeared at 7 d after starvation (P<0.05) when comparing with those in the F group (Figure 3). However, the change of LZM activity to starvation stress was slow compared to the changes of the activities of SOD, CAT, and ACP.Figure 3
The changes of immune enzyme activities in the hepatopancreas ofM. nipponense after 14 d of starvation: (a) superoxide dismutase (SOD); (b) catalase (CAT); (c) lysozyme (LZM); (d) acid phosphatase (ACP). Data are presented as mean±SD (n=6). Statistical significance is tested using an unpaired t-test (∗P<0.05).
(a)(b)(c)(d)


## 3.3. Intestinal Microbiota Richness and Diversity Analysis

A total of 338,779 high-quality sequences were obtained from 6 samples of the intestinal bacteria, ranging from 50,795 to 62,676. The good coverage ranged from 0.989 to 0.997, which suggested that the complete microbial communities presented in the samples were identified completely. The sequences were clustered into operational taxonomic units (OTUs), and each OTU represented a unique phylotype. Finally, a total number of 14,285 OTUs were identified in all samples, and the number of OTUs detected in each sample ranged from 1569 to 3129. The total number of OTUs in the F group was significantly higher than that in the S group (P<0.05) (Table 2), but 742 OTUs were shared by these two groups (Figure 4).Table 2
Sequencing, OTU classification information, and Good’s coverage in six samples.
SampleReadsPhylumClassOrderFamilyGenusSpeciesUnclassifiedTotalGood’s coverageS16267630155644509548129120810.994S25416821171487559632182021030.996S3561392199205446569173215690.997F1507951323011661030539108031250.994F253041132941012701565115027610.992F36196024218947697544121126560.989Figure 4
The distribution difference of the OTUs in the gut microbiota of the F group and the S group ofM. nipponense after 14 d of starvation by Venn diagram.Bacterial richness and diversity were estimated with Chao, Shannon, and Simpson indices, respectively. The Chao estimator of the F group was significantly higher than that of the S group (P<0.05), but the two groups showed no significant difference in the Shannon or Simpson index (P>0.05, Table 3). The analysis of beta diversity by both PCoA and NMDS showed that samples of the F group were separated from those of the S group, indicating the potential influence of different feeding regimes on intestinal microbiota (Figure 5).Table 3
Data from Illumina high-throughput sequencing yields bacterial diversity and richness based on operational taxonomic units (OTU), estimated OTU richness (Chao), and diversity index (Shannon & Simpson) for the intestinal bacterial diversity analysis ofM. nipponense in two groups.
Diversity indexFeeding groupStarvation groupRichness estimatorsChao2942.67±187.70∗1969.33±327.39Diversity estimatorsShannonSimpson8.24±0.570.98±0.027.31±0.460.95±0.02Data are presented asmean±SD (n=3). Statistical significance is tested using an unpaired t-test (∗P<0.05).Figure 5
Beta diversity analysis of the gut microbiota of the F group and the S group ofM. nipponense after 14 d of starvation: (a) principal coordinate analysis (PCoA); (b) nonmetric multidimensional scaling (NMDS) of Bray-Curtis distances. F: feeding group; S: starvation group.
(a)(b)


## 3.4. Bacterial Community Analysis and Comparison

In this study, total OTUs of bacterial community in all samples were classified into 30 phyla. The top 20 most abundant OTUs were shown in the taxonomic composition of intestinal microbiota at the phylum level (Figure6), in which Actinobacteria and Proteobacteria were the predominant microflora phylum in the bacterial communities of both groups, and they accounted for 44.06±13.80% and 39.44±11.21% in the F group, respectively, and 39.06±12.00% and 35.82±3.77% in the S group, respectively. Firmicutes, Tenericutes, Bacteroidetes, and Chlamydiae were also abundant in all samples. The abundance of Bacteroidetes in the S group was significantly higher than that in the F group (P<0.05).Figure 6
The abundance changes of the intestinal bacteria ofM. nipponense at the phylum level after 14 d of starvation. Statistical significance is tested using an unpaired t-test (∗P<0.05).The heat map of intestinal bacterial abundance in intestines at the genus level showed that the abundance of harmful bacteria and potential harmful bacteria, such asAcinetobacter [35], Streptococcus [36], Enterococcus [37], and Rhodococcus [38], in the S group were larger than those in the F group (P<0.05), while the abundance of beneficial bacteria enriched in feeding prawns, such as Microbacterium [39], Rhodobacter ([40, 41]. [42]), and Anoxybacillus [43], were larger than in the S group (P<0.05) (Figure 7). These results indicated that comparing to feeding prawns, starved ones had more opportunistic pathogenic bacteria but less beneficial bacteria in the intestine.Figure 7
The abundance changes of the intestinal bacteria ofM. nipponense at the genus level after 14 d of starvation by heat map. Phylogenetic positions are projected by the OTUs, and the taxa of OTUs are listed on the right. Color intensity indicates the relative enrichment of OTUs. F: feeding group (F1-F3); S: starvation group (S1-S3).


## 3.5. Functional Prediction of Intestinal Microbiota

To compare the functional potentials of the intestinal microbiota between feeding and starved prawns, functional content was predicted in the KEGG database at level 2. Functional prediction showed that thirteen pathways including amino acid biosynthesis, cofactor, prosthetic group, electron carrier, vitamin biosynthesis, nucleoside and nucleotide biosynthesis, fatty acid and lipid biosynthesis, carbohydrate biosynthesis, cell structure biosynthesis, aromatic compound degradation, nucleoside and nucleotide degradation, fermentation, and TCA cycle were enriched in the intestinal microbiota after starvation (Figure8). Meanwhile, the predicted nutrition metabolism of glycolysis V was significantly enriched in the S group (P<0.05). Moreover, the degradation of glucose, fucose, lactose, galactose, sucrose and rhamnose, L-arginine and L-ornithine degradation, peptidoglycan, and L-tryptophan biosynthesis were significantly decreased when the S group was compared with the F group (P<0.05). This result implied that the gut microbiota of prawns adapted to the stress of starvation by decreasing nutrition metabolism to a certain degree. The immune system pathway of enterobacterial common antigen biosynthesis was markedly reduced in starved prawns (P<0.05) (Figure 9). Nevertheless, for the terms of digestive-related metabolism (amino acid, carbohydrate, fatty acid, and lipid biosynthesis and degradation) and immune-related metabolism functions (antibiotic resistance, methanol oxidation to carbon dioxide, and phospholipases), there was no significant difference in the F and S groups (P>0.05, Table 4).Figure 8
Relative abundance of functional pathways of the intestinal microbiota inM. nipponense. Pathways were predicted in the KEGG database at level 2.Figure 9
The changes of the KEGG pathways of intestinal bacteria inM. nipponense after 14 d of starvation. Pillars in the right column indicate significant increase, while those in the left column indicate significant decrease in the starvation group as compared with the feeding group in abundances of the corresponding pathways. F: feeding group; S: starvation group.Table 4
Relative abundance of digestive-related metabolism and immune-related metabolism functions in the starvation and feeding groups.
Feeding group (%)Starvation group (%)Amino acid biosynthesis14.73±0.2014.14±0.32Carbohydrate biosynthesis4.76±0.024.76±0.32Fatty acid and lipid biosynthesis8.14±0.827.96±0.18Amino acid degradation1.20±0.181.18±0.25Carbohydrate degradation1.87±0.231.95±0.27Fatty acid and lipid degradation0.72±0.030.79±0.17Antibiotic resistance0.01±0.090.21±0.31Methanol oxidation to carbon dioxide0.03±0.000.06±0.03Phospholipases0.011±0.010.01±0.07Note: there was no significant difference in two groups (P>0.05).


## 3.6. The Interplay among Prawn Gut Bacterial Community, Digestive and Immune Enzyme Activity, and Growth

Redundancy analysis (RDA) was performed to examine the relationships among microbial community structures, digestive enzyme activities, and immune enzyme activities (Figure10(a)). The result showed that the composition of the intestinal bacterial flora in the S group had significant difference with that in the F group after 14 d of starvation. Meanwhile, the changes were potentially related to immune indicators SOD (R2=0.436, P value = 0.188), LZM (R2=0.437, P value = 0.175), ACP (R2=0.434, P value = 0.207), and CAT (R2=0.424, P value = 0.201) and digestive indicators TRY (R2=0.424, P value = 0.214), LPS (R2=0.459, P value = 0.162), and AMS (R2 = 0.465, P value = 0.166). In the RDA space, only AMS was negatively correlated with the microbial community structure in starved prawns, but the other indicators expressed positively with the microbial community structure. These indicators had an impact on the diversity and species composition of the bacterial flora of the S group.Figure 10
(a) The relationships between microbial community structures and digestive enzyme activity and the immune enzyme activity of the starvation group and the feeding group inM. nipponense with redundancy analysis (RDA). F: feeding group; S: starvation group. (b) The structural equation model (SEM) shows the interplay among the intestinal bacterial community, immune enzyme activity, digestive enzyme activity, and weight gain rate of M. nipponense. Numbers on the arrow are standardized paths calculated by Pearson correlation coefficient. Arrow widths show the strength of the causal relationship. R2 of all paths (>0.8, P<0.05) indicated that the structural equation model analysis of variance results was statistically significant.
(a)(b)The structural equation modeling (SEM) revealed the interplay among the gut bacterial community, digestive and immune enzyme activities, and weight gain rate (Figure10(b)). The results indicated that changes of digestive and immune enzyme activities were directly related to the gut bacterial community and notably affected prawn growth.


## 4. Discussion

The stability and functional activities of gut microbiota are important to the host health. Gut microbiota enhanced the metabolic capabilities, modulated gastrointestinal development, balanced the immune response, and protected against pathogens for the host [44]. However, the relationship among starvation, digestion, immune activities, and intestinal microbiota community was rarely conducted in crustaceans. The studies showed that the change of gut bacterial community was directly related to digestive and immune enzyme activities under starvation stress in L. vannamei [8, 14]. In this present study, the difference of intestinal microbiota between starved and fed M. nipponense was studied using the method of high-throughput sequencing for the first time to elucidate the interplay among shrimp gut microbiota and digestive and immune enzyme activities after starvation.The activity of digestive enzymes in aquaculture species was affected by growth, diet composition, natural feeding habits, and genetics [45, 46]. Therefore, digestive enzyme activities might reflect digestion physiology and nutritional changes under adverse environmental conditions [47]. In the present study, the digestive activities of trypsin and lipase in starved prawns were lower than those in normal fed prawns. A few studies had shown that crustaceans could adapt to starvation stress by reducing the digestive activity in the shrimps L. vannamei [8, 48] and the crayfish Procambarus clarkii [46]. The changes of the digestive enzyme activities in shrimps reflected the availability of energy and nutrients; one possible reason for this phenomenon was that no food peristalsis mechanically stimulated the shrimp’s entire digestive tracts, thereby reducing the secretion of digestive enzymes [49]. Alternatively, the depression of digestive activity could attenuate the utilization of energy reserves, thereby affording an adaptation strategy for animals to deal with food-depriving conditions and to prevent damage or death [4]. However, the contrary results were found in fish and shrimps as well. Researches had shown that the amylase activities in the hepatopancreas of common carp increased significantly after starvation [50], and trypsin and α-glucosidase activities in the hepatopancreas were significantly higher in starved shrimps than in fed ones under short-term starvation in Penaeus monodon [51]. Starvation triggered amino acid catabolism in digestive gland cells of the hepatopancreas and increased the specific activities of amylase, protease, trypsin, and chymotrypsin in L. vannamei [52]. In this present study, the activity of amylase exhibited an opposite trend with those of lipase and trypsin, which increased significantly after 14 d of starvation. This result agreed with previous studies performed on M. nipponense [5]. We suspected that it might be related with omnivorous feeding habits of M. nipponense. In addition, this view was further supported by the results of significant enrichment of glycolysis V in starved prawns (Figure 9). Maintenance of high levels of digestive enzyme activity even after the lack of feed might assure the utilization and absorption of the remaining food [50] and a relatively quick metabolic recovery when food becomes available [53].The immune statuses of crustaceans were tightly linked with environmental factors [54, 55], diet supplementation [56, 57], and starvation [8]. The activities of SOD and CAT in M. nipponense decreased significantly with the rising of ROS under the stress of starvation [5] or sublethal concentration of nitrite [55]. In this study, the immune enzyme activities of SOD, CAT, LZM, and ACP in the hepatopancreas of starved prawns decreased and were consistently significantly lower than those of feeding ones (Table 4). The reduction of immune activities indicated that these enzymes might have been inhibited as a transitory response to food shortage [5]. By contrast, LZM, ACP, and SOD activities were consistently increased in starved L. vannamei [8], the CAT activity increased markedly in the hepatopancreas, and a contrary trend was observed in the hemolymph after white shrimp was exposed to ambient nitrite [54]. Reduction in the activities of digestive and immune enzymes under starvation might be an adaptation to feed scarcity and energy maintenance [52].Dietary and food availability play a predominant role to shape the structure of animal gut microbial. Starvation is a major factor determining host gut microbiota [58]. In this study, the community structures of gut microbiota including the total number of OTUs and bacterial richness were significantly changed in the prawns after 14 d of starvation, while the Shannon and Simpson diversity indices were not significantly affected by starvation (Tables 2 and 3). In L. vannamei, the Shannon and Simpson indexes of gut microbiota were greatly changed under starvation stress [8]. Meanwhile, beta diversity in terms of PCoA and NMDS showed that the feeding group samples clustered separately from the starvation group samples, which indicated that feed deprivation limited the adaptive potential of the microbiota [58].In the present study, the dominant microbiota phyla inM. nipponense gut were Actinobacteria and Proteobacteria, followed by Firmicutes, Tenericutes, Bacteroidetes, and Chlamydiae. The abundance of Actinobacteria and Proteobacteria was similar in the S group and the F group. It was not consistent with the results of previous studies conducted in M. nipponense, in which Proteobacteria was the most dominant bacteria in the intestine, followed by Firmicutes, Tenericutes, Bacteroidetes, Cyanobacteria, and Actinobacteria [59]. The result was also different in other shrimps such as Macrobrachium rosenbergii [60], L. vannamei [8, 23, 61], and black tiger shrimp [62]. Firmicute was the dominant phyla in humans and many land mammals [63–66]. In the present study, the relative abundance of Firmicutes in M. nipponense was relatively low, which were 4.41% in feeding prawns and 10.81% in starved ones. Similar result has also been found in L. vannamei [8, 23], which could be attributed to differences in phylogeny, living environment, and dietary habits. Research showed that Proteobacteria and Firmicutes were the dominant microflora in the intestinal flora of healthy Procambarus clarkii [67] and were also used as indicators of fish health [68]. In this study, the abundance of Bacteroidetes in the S group was significantly higher than that in the F group. Moreover, the difference in dominant bacteria in starvation and feeding groups at the genus level was also found. There were more abundant harmful bacteria and potential harmful bacteria in starved prawns, while more beneficial bacteria were enriched in feeding prawns. The reduced immune system pathway, immune enzyme activity, and gut microbial diversity and increased quantities of potentially pathogenic bacteria indicated that starved prawns were more susceptible to pathogen infection.Recently, many studies focused on the functional prediction of intestinal microbiota in shrimps. The severe changes of culture environmental conditions, diet composition, and health status could cause great difference on the metabolism functions of shrimp intestinal microbiota [8, 69–72]. When suffering the stress of starvation and white feces syndrome simultaneously, L. vannamei remarkably decreased the functional pathways involved in carbohydrate and protein digestion, glycan biosynthesis, and lipid and enzyme metabolism [8]. In the present study, the predicted nutrition metabolism involved in glycolysis V was significantly enriched after starvation. Meanwhile, partial carbohydrate and amino acid metabolism and the pathways involved in immunity significantly decreased in starved prawns (Table 4). Nevertheless, the main nutrition-related metabolism functions including amino acid, carbohydrate, fatty acid, and lipid biosynthesis and degradation and immune-related metabolism functions including antibiotic resistance, methanol oxidation to carbon dioxide, and phospholipases were not significantly changed by starvation. Similarly, the dietary replacement did not reduce the significant difference in intestinal bacterial nutrition-related metabolism functions in L. vannamei [23]. These results implied that the gut microbiota of prawns could adapt to starvation by decreasing its metabolism level, but the short-term feed deprivation was insufficient to significantly change metabolism functions of intestinal microbiota in M. nipponense.Gut microbiota had crucial effects on maintaining the mucosal structure, immunity, nutrition, and metabolism [12, 66]. Food deprivation or restriction was associated with alterations in the epithelial gut barrier [73]. In the present study, the significant decrease in the height of epithelial cells and microvilli in the S group suggested that starvation quickly damaged the structure of the prawn intestine, which might induce the change of the microbiota living environment. The increased abundance of Bacteroidetes, which possessed genes for a large number of enzymes involved in carbohydrate utilization [66, 74, 75], in starved prawns might be related to the increased activity of amylase, which was involved in glycolysis V metabolism. The results of redundancy analysis (RDA) showed a positive correlation between immune-related enzymes of SOD, CAT, LZM, and ACP; digestive enzymes of TRY and LPS, except AMS; and microbial community structure in starved prawns. The suppressed digestion and immune activities of starved prawns might be matched with the gut microbial richness and functions. It was supposed that energy homeostasis was kept under starvation condition by exploiting microbiota-derived sources of carbon and nitrogen as nutrients [76]. The result of SEM further revealed that there was a close correlation among prawn digestion and immune activities, gut microbiota, and growth traits. A similar result has also been found in L. vannamei [8].


## 5. Conclusions

In summary, the present study indicated that the changes of digestive and immune enzyme activities under the starvation condition were directly related to the gut bacterial community, which in turn affected the growth traits of prawns. Feed deprivation significantly changed the bacteria richness of the prawn gut microbiota. The increased abundance of Bacteroidetes in starved prawns might be related to the increased activity of amylase and glycolysis V metabolism. The starved prawns were more prone to be invaded by pathogens as evidenced by reduction of immune enzyme activity, the immune system pathway, and more abundant opportunistic pathogens. These results revealed the relationship among digestive enzymes, immune enzyme activities, and gut microbiota under starvation stress inM. nipponense.



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*Source: 6836727-2022-05-29.xml*