Comparative Transcriptome Analysis of Litopenaeus vannamei Reveals That Triosephosphate Isomerase-Like Genes Play an Important Role During Decapod Iridescent Virus 1 Infection

Decapod iridescent virus 1 (DIV1) results in severe economic losses in shrimp aquaculture. However, little is known about the physiological effect of DIV1 infection on the host. In this study, we found that the lethal dose 50 of DIV1-infected Litopenaeus vannamei after 48, 72, 96, and 156 h were 4.86 × 106, 5.07 × 105, 2.13 × 105, and 2.38 × 104 copies/μg DNA, respectively. In order to investigate the mechanisms of DIV1 infection, a comparative transcriptome analysis of hemocytes from L. vannamei, infected or not with DIV1, was conducted. The BUSCO analysis showed that the transcriptome was with high completeness (complete single-copy BUSCOs: 57.3%, complete duplicated BUSCOs: 41.1%, fragmentation: 0.8%, missing: 0.8%). A total of 168,854 unigenes were assembled, with an average length of 601 bp. Based on homology searches, Kyoto Encyclopedia of Genes and Genomes (KEGG), gene ontology (GO), and cluster of orthologous groups of proteins (KOG) analysis, 62,270 (36.88%) unigenes were annotated. Among them, 1,112 differentially expressed genes (DEGs) were identified, of which 889 genes were up-regulated and 223 genes were down-regulated after DIV1 infection. These genes were mainly annotated to the major metabolic processes such as fructose and mannose metabolism, carbon metabolism, and inositol phosphate metabolism. Among these metabolic pathways, the triosephosphate isomerase (TPI) family was the most eye-catching DEG as it participates in several metabolic processes. Three types of TPI, LvTPI-like, LvTPI-Blike, and LvTPI-Blike1, were obtained for gene silencing by RNA interference. The results showed that LvTPI-like and LvTPI-Blike1 silencing caused a high mortality rate among L. vannamei. However, LvTPI-like and LvTPI-Blike silencing reduced DIV1 replication in DIV1-infected L. vannamei. All the results indicated that TPI-like genes play an important role during DIV1 infection, which provides valuable insight into the infection mechanism of DIV1 in shrimp and may aid in preventing viral diseases in shrimp culture.

Decapod iridescent virus 1 (DIV1) results in severe economic losses in shrimp aquaculture. However, little is known about the physiological effect of DIV1 infection on the host. In this study, we found that the lethal dose 50 of DIV1-infected Litopenaeus vannamei after 48, 72, 96, and 156 h were 4.86 × 10 6 , 5.07 × 10 5 , 2.13 × 10 5 , and 2.38 × 10 4 copies/µg DNA, respectively. In order to investigate the mechanisms of DIV1 infection, a comparative transcriptome analysis of hemocytes from L. vannamei, infected or not with DIV1, was conducted. The BUSCO analysis showed that the transcriptome was with high completeness (complete single-copy BUSCOs: 57.3%, complete duplicated BUSCOs: 41.1%, fragmentation: 0.8%, missing: 0.8%). A total of 168,854 unigenes were assembled, with an average length of 601 bp. Based on homology searches, Kyoto Encyclopedia of Genes and Genomes (KEGG), gene ontology (GO), and cluster of orthologous groups of proteins (KOG) analysis, 62,270 (36.88%) unigenes were annotated. Among them, 1,112 differentially expressed genes (DEGs) were identified, of which 889 genes were up-regulated and 223 genes were down-regulated after DIV1 infection. These genes were mainly annotated to the major metabolic processes such as fructose and mannose metabolism, carbon metabolism, and inositol phosphate metabolism. Among these metabolic pathways, the triosephosphate isomerase (TPI) family was the most eye-catching DEG as it participates in several metabolic processes. Three types of TPI, LvTPI-like, LvTPI-Blike, and LvTPI-Blike1, were obtained for gene silencing by RNA interference. The results showed that LvTPI-like and LvTPI-Blike1 silencing caused a high mortality rate among L. vannamei.

INTRODUCTION
Litopenaeus vannamei is a widely cultured shrimp species all around the world, with a huge production per year (1). The development of farmed shrimp has led to high-density growth conditions, large-scale production, and unsanitary aquaculture wastewater discharge, resulting in disease overflow, ecological imbalance, and environmental deterioration. The shrimp industry is now faced with finding solutions for these serious problems (2,3). Over the past decades, diseases caused by various bacterial, fungal, parasitic, and viral species have significantly constrained the productivity of the L. vannamei industry (4). For a long time, the most concerning viruses were the white spot syndrome virus (WSSV), the Taura syndrome virus (TSV), and the infectious hypodermal and hematopoietic necrosis virus (IHHNV) (5). However, in 2014, the decapod iridescent virus 1 (DIV1) caused huge losses in farmed L. vannamei in Zhejiang Province in China. DIV1 was isolated and identified by Qiu et al. in 2017 (6). Since then, the prevention and the control of DIV1 have attracted much attention in shrimp culture.
In 1993, Lightner and Redman first discovered the iridescent virus in shrimp in Ecuador (7). In 2004, Tang et al. found the iridescent virus in Acetes erythraeus grown in Madagascar and, via sequencing, found that it was a new type of iridescent virus (Sergestid iridovirus, SIV) (8). In 2016, Xu et al. detected a new iridescent virus, Cherax quadricarinatus iridovirus (CQIV), from Cherax quadricarinatus on a farm in China (9). In 2017, Qiu et al. detected shrimp hemocyte iridescent virus (SHIV) from L. vannamei and determined that SHIV is a member of the new genus Xiairidovirus, which also belongs to the Iridoviridae family. The complete genome sequence of SHIV is 165,908-bp long with 34.6% G + C content and 170 open reading frames. Qiu et al. used intermuscular injection and reverse gavage methods to infect L. vannamei with SHIV, resulting in a 100% cumulative mortality rate. Results from the histopathological study using transmission electron microscopy of ultrathin sections and in situ hybridization indicated that SHIV mainly infects the hematopoietic tissue and hemocytes in the Pacific white shrimp (6). In 2019, the Executive Committee of the International Committee on Taxonomy of Viruses (ICTV) identified two virus isolates, SHIV and CQIV, as decapod iridescent virus 1 (DIV1) (10). Crustaceans in the coastal region of China, including L. vannamei, Fenneropenaeus chinensis, Exopalaemon carinicauda, and Macrobrachium rosenbergii, can all carry DIV1 (6,11,12). Until now, most of the studies on DIV1 focused on the virus itself or the histopathological changes in the host. Latest studies in 2020 based on transcriptome analysis showed that the phagosome and the MAPK signaling pathway were positively modified during DIV1 infection in C. quadricarinatus (13), while lysosome and phagosome were induced during DIV1 infection in Fenneropenaeus merguiensis (14). However, little is known about the mechanism of the host response to DIV1 infection.
Shrimp rely on their innate immune system to defend against invading viruses and microbes. Shrimp cells can recognize the invading virus via unique host pattern recognition proteins with pathogen-associated molecular patterns, which can activate the host immune response (15). The innate immune system includes the humoral immune system and the cellular immune system. The humoral responses are mediated by macromolecules in the hemolymph. Humoral responses are mainly divided into melanin synthesis by the prophenoloxidase system, the blood clotting system, and the generation of circulating antimicrobial peptides (16). The cellular immune response involves different types of hemocytes, which clear harmful substances in the hemolymph by defensive reactions such as phagocytosis and encapsulation (17). Recent studies confirmed that hemocytes are an important source of several humoral effector molecules, which are required in killing foreign invaders in shrimp (18,19). It is necessary to understand the immune system of shrimp in order to develop methods that can successfully control and reduce the loss of shrimp production due to infectious diseases. High-throughput RNA sequencing (RNA-Seq) is an efficient technology to analyze gene expression, discover transcripts, and select differentially expressed genes (DEGs) (20). This technology has been used to study the molecular basis of certain gene transcription processes (21). Ren et al. found several genes related to immunity through the transcriptome profiles of M. japonicus following infection with V. parahemolyticus or WSSV (22). Additional research into the function of these immune genes, such as caspase 4, integrin, crustin, ubiquitinconjugating enzyme E2, C-type lectin, and α 2 -macroglobulin, is required to understand the molecular interactions between V. parahemolyticus and WSSV in M. japonicus and to provide valuable information for preventing diseases (22). However, no information is available on the gene expression profiles of DIV1infected L. vannamei.
In the present study, the lethal concentration 50 (LD 50 ) of DIV1-infected L. vannamei was determined, and RNA-Seq was applied to compare the transcriptome difference between the DIV1-infected and non-infected L. vannamei. This study aims to gain a better insight into the DIV1-shrimp interaction and may help better understand the innate immune mechanism in shrimp, which would be beneficial to disease prevention in shrimp culture.

Shrimp Culture
The study protocol was approved by the ethics review board of the Institutional Animal Care and Use Committee in Guangdong Ocean University. L. vannamei (body weight 11.2 ± 2.4 g) was purchased from Hainan Zhongzheng Aquatic Science and Technology Co., Ltd., in Dongfang (Hainan, China). The shrimps were acclimatized for 1 week in 0.3-m 3 tanks with aerated and filtered seawater in East Island Marine Biological Research Base, Guangdong Ocean University in Zhanjiang, Guangdong, China. The holding seawater conditions were as follows: salinity at 28.5 ± 0.26 ‰, pH at 8.17 ± 0.01, and temperature at 29.3 ± 0.5 • C. Commercial feed was used to feed the shrimp three times a day. The shrimps were then randomly sampled and tested by PCR to ensure that they were free from WSSV, IHHNV, and DIV1 using the primers shown in Table S1.

LD 50 Test
DIV1 was obtained from a Peihua prawn farm in Wuchuan, Guangdong, China, and the virus was extracted from the infected tissue of L. vannamei, as conducted previously (23). The DIV1 inoculation was tested by PCR to ensure that it was not contaminated with the DNA of any other known crustacean virus (e.g., WSSV and IHHNV). DNA was extracted using the EasyPure Marine Animal Genomic DNA Kit (Transgen, Beijing, China). Extracted DNA was quantified using SimpliNano (GE Healthcare, US). The DNA samples of the pleopods were used to detect the viral loads by real-time PCR performed in a LightCycler (Roche) with the following program: denaturation at 95 • C for 30 s, followed by 40 cycles at 95 • C for 5 s and 60 • C for 30 s, using the primers qRT-DIV1-F, qRT-DIV1-R, and Taqman Probe (Table S1) (24). Toxicity tests were performed with the same method as in the study of WSSV in shrimp (25). Six groups of healthy L. vannamei were intramuscularly injected at the third abdominal segment with 50 µl of DIV1 supernatants at five concentrations (2.14 × 10 8 , 2.14 × 10 7 , 2.14 × 10 6 , 2.14 × 10 5 , and 2.14 × 10 4 copies/µg DNA) and phosphate-buffered saline (PBS; pH 7.4) as a control. Three replicates of 30 shrimps per replicate were used in each group. The conditions of the LD 50 test were the same as discussed in "Shrimp Culture" section. The cumulative mortality was recorded every 4 h for the LD 50 calculation. To investigate the copies of DIV1, total DNA was extracted from hemocyte, hepatopancreas, intestine, gill, and muscle of L. vannamei at 6, 12, 24, 48, and 72 h after DIV1 injection on the concentration at LD 50 48 h from infection.

Sample Collection
L. vannamei was intramuscularly injected with 50 µl of DIV1 supernatant based on LD 50 48 h after infection. L. vannamei injected with PBS was used as controls. At 48 h post-injection (hpi), the hemocytes from three shrimp were combined as one sample for transcriptome sequencing. The hemolymph was withdrawn into modified ACD anticoagulant solution, and the hemocytes were separated from plasma by centrifugation (3,000 × g for 5 min at 4 • C) (26). The hemocytes of L. vannamei were immediately frozen in liquid nitrogen and stored at −80 • C until RNA extraction. Three biological replicates were performed for the infection and the control groups, for a total of six samples. The extracted RNA was pooled for transcriptome sequencing.

RNA Extraction and Transcriptome Sequencing
Total RNA from the hemocytes of L. vannamei was isolated using TransZol Up Plus RNA Kit (Transgen, Beijing, China), and the RNA concentration was determined using SimpliNano (GE Healthcare, US). Fragmentation buffer was used to break the mRNA into short fragments. Using mRNA as a template, the firststrand cDNA strand was synthesized using random hexamers, followed by the addition of buffer, dNTPs, RNase H, and DNA polymerase I to synthesize the second-strand cDNA. Poly(A) was added to connect to the sequencing adaptor. Finally, the Illumina HiSeqTM platform was used to sequence the library at Guangzhou Sagene Biotech Co., Ltd. (Guangzhou, China).

Differential Expression Analysis and Functional Annotation
Log 2 (FC) was used as an indicator of the genetic transcriptome differences between the DIV1-infected and the control groups. Fragments per kilobase million was used as the measurement unit to estimate the expression level of each transcript in the study. False discovery rate (FDR) was also used to correct the calculated p-values (28). Genes with FDR ≤0.05 and |log 2 (FC)| >1 were considered to be DEGs. In addition, KEGG and GO were also used for DEGs pathway and GO enrichment analysis, respectively.

Validation of DEGs by qRT-PCR
To validate the transcriptome data, 2 µg of high-quality hemocyte RNA samples from the DIV1-infected group and the PBS control group was reverse-transcribed using the 5X All-in-One RT Master Mix (Applied Biological Materials, Vancouver, Canada) according to the manufacturer's protocol. The RNA concentration of the DIV1-infected group and the PBS control group was 120.48 and 156.64 µg/ml, respectively. A total of eight differentially expressed unigenes from the hemocyte transcriptome data of L. vannamei were selected for qPCR  Table S1. 2 − Ct method was used to calculate gene expression (29). The amplification efficiencies (E) were calculated using the formula provided by Bustin et al. (30). The expression level of each gene was normalized by EF1α (GenBank accession no. GU136229).

Knockdown of TPI of L. vannamei in vivo Expression by Double-Stranded RNA-Mediated RNA Interference
Three types of triosephosphate isomerase (TPI)-specific primer sequences were linked to the T7 promoter by using the T7 RiboMAX TM Express Large Scale RNA Production System (Promega) to synthesize double-stranded RNAs (dsRNAs) following the method as previously described (31). The primers used for the synthesis of dsRNAs are shown in Table S1. The experimental group was injected with dsRNA-LvTPI-likes (2 µg/g), while the control groups were injected with equivalent dsRNA-EGFP. RNA interference efficiency was investigated using qPCR. The hemocyte samples were taken from nine shrimp in each challenge group at 24 and 48 hpi, and three shrimp were pooled together. Total RNA was extracted and reverse-transcribed into cDNA for qPCR. LvEF1-α was used  as the internal control. The primer sequences are listed in Table S1.

Bioassay of DIV1 and PBS Challenge Tests in TPI-Knockdown L. vannamei
Healthy L. vannamei (7.12 ± 1.05 g, n = 40) received an intramuscular injection of dsRNA-LvTPI-like, dsRNA-LvTPI-Blike, dsRNA-LvTPI-Blike1, dsRNA-EGFP, or PBS. dsRNA was injected at a concentration of 2 µg/g shrimp. Four replicates (three replicates for mortality calculation and one for the sample collection) were analyzed for each group. After 48 h, the shrimp were injected again with 2.01 × 10 4 copies of DIV1 particles and mock-challenged with PBS as a control.
The shrimp were cultured in tanks with air-pumped circulating seawater and were fed with artificial diet three times a day at 5% of body weight for about 7 days following the infection. The mortality of each group was counted every 4 h. At 24 and 48 h after DIV1 challenge, the hepatopancreas, intestines,  gill, muscle, and hemocyte of shrimp were collected for viral load detection.

Statistical Analysis
Data are expressed as mean ± standard deviation (SD). Statistical analyses were performed using SPSS software (version 18.0), with one-way ANOVA using Duncan's test to evaluate whether the means were significantly different (P < 0.05). Differences between groups were analyzed by using the Mantel-Cox (logrank χ 2 test) method with the GraphPad Prism software. The formula for calculating the LD 50 of the virus is: where x i is the logarithm of the dose or concentration and ρ i is the mortality rate.  Figure 2. The shrimp mortality rate increased as the DIV1 concentration increased. Probit analysis showed that the LD 50 values for DIV1 determined are 3.91× 10 7 , 4.86 × 10 6 , 5.07 × 10 5 , 2.13 × 10 5 , 2.38 × 10 4 , and 2.38 × 10 4 copies/µg DNA for 24, 48, 72, 96, 120, 144, and 168 h after injection, respectively (Figure 2A). The copies of DIV1 in all the five detected tissues of infected L. vannamei were significantly increased at all the detected timepoints after injection ( Figure 2B).

De novo Assembly and Annotation of Unigenes
Six cDNA libraries from L. vannamei were sequenced on the Illumina HiSeqTM platform. As Table S2 shows, a total of 328,670,602 raw reads were generated, and 328,555,316 clean reads were left after removing the adapters filtering the low-quality sequences. Therefore, 163,056,696 clean reads were generated from 163,103,692 raw reads in the DIV1infected group, and 165,498,620 clean reads were generated from 165,566,910 raw reads in the control group. The whole de novo assembly reads, from six libraries, yielded a total length of 101,529,805 bp, with 168,854 unigenes and an N50 length of 807 bp. The clean read data were deposited to the NCBI Sequence Read Archive (SRA, http://www.ncbi.nlm.nih.gov/Traces/sra) with the accession number SRP252506. A detailed summary of the sequencing and the assembly results is shown in Table 1. The sequence length (nt) ranges from 200 to ≥3,000 nt, with the distribution shown in Figure 3A. The most abundant unigenes were clustered in a group with 200-400 nt in length. Based on BUSCO, we compared the transcriptome with 1,066 conserved arthropod genes. A total of 98.4% of the transcriptome (251 genes) were encoded as complete proteins. Among these genes, 57.3% (146 genes) were complete and single-copy BUSCOs, 41.1% (105 genes) were complete and duplicated BUSCOs, 0.8% (two genes) were fragmented BUSCOs, and 0.8% (two genes) were missing BUSCOs (Figure 3B).

Classification and Analysis of DEGs
To analyze and characterize the DEGs in L. vannamei following DIV1 infection, a cutoff false discovery rate (FDR) was set at <0.05 and a |log 2 ratio| ≥1 was employed as threshold. Based on this, 1,112 genes were observed to be dysregulated in DIV1infected group compared to the control, including 889 upregulated genes and 223 down-regulated genes. These DEGs were visualized by volcano plot in Figure 5.
The DEGs were further annotated with GO and KEGG databases. In the GO enrichment analysis, the 197 up-regulated and the 41 down-regulated genes expressed in the DIV1-infected group were enriched in several categories: biological process (106 up-regulated and 23 down-regulated), molecular function (38 up-regulated and 11 down-regulated), and cellular component (53 up-regulated and seven down-regulated) (Figure 6). For the KEGG pathway enrichment analysis, 121 DEGs were annotated into 108 pathways. Among them, metabolism was a crucial pathway. The category that contained the higher number of DEGs was "protein processing in endoplasmic reticulum." The top 20 KEGG enrichment pathways influenced by DIV1 infection are shown in Figure 7. KEGG analysis showed that 28 DEGs were presented in seven immune system pathways, including NOD-like receptor signaling pathway (four), MAPK signaling pathway (seven), Wnt signaling pathway (two), Toll-like receptor signaling pathway (two), phagosome (seven), RIG-I-like receptor signaling pathway (two), and p53 signaling pathway (four) ( Table 3). In these pathways, TPI genes received particular attention for their participation in several distinct pathways, such as fructose and mannose metabolism, glycolysis/gluconeogenesis, biosynthesis of amino acids, inositol phosphate metabolism, and carbon metabolism ( Table 4).

Validation of RNA-Seq Results by qRT-PCR
To further evaluate our DEG library, eight unigenes were randomly selected, including four up-regulated and four down-regulated DEGs for qPCR analysis. The amplification efficiency (E) of all unigenes and EF1α ranged from 95.2 to 98.2% (Table S1). As shown in Figure 8, the qPCR results showed significant, identical expression tendencies as the high-throughput sequencing data. However, some quantitative differences in the expression level were seen for Unigene064464, Unigene072846, Unigene027278, and Unigene040974. The qPCR analysis results, therefore, confirmed the expressions of DEGs which were detected in the high-throughput sequencing analysis.

Functional Analysis of LvTPI in L. vannamei During DIV1 Infection
Silencing of LvTPI-likes Led to L. vannamei Death According to the transcriptome information in this study and the genome information from NCBI, three full-length TPI types were obtained and named as LvTPI-like (accession no. MT123334), LvTPI-Blike (accession no. MT107901), and LvTPI-Blike1 (accession no. MN996302). The silencing efficiency was checked using qPCR. At 24 and 48 h post-dsRNA injection, the mRNA level of LvTPI-likes was remarkably downregulated in dsRNA-LvTPI-likes-treated shrimp (p < 0.05), whereas there was no suppressive effect on LvTPI-likes in the dsRNA-EGFP-treated group (Figure 9A). The L. vannamei started to die after dsRNA-LvTPI-like and dsRNA-LvTPI-Blike1 injection, with a cumulative mortality of 50 and 82.5% at 48 hpi, respectively. The final mortality rates at 144 hpi were 72.5 and 92.5% for the dsRNA-LvTPI-like and the dsRNA-LvTPI-Blike1 groups, respectively. However, there was no effect on the survival rate of L. vannamei by dsRNA-LvTPI-Blike injection ( Figure 9B).

LvTPI-like and LvTPI-Blike Suppression Did Not Affect the Survival Rates of L. vannamei but Reduced DIV1 Replication
Due to the mass death of L. vannamei when LvTPI-Blike1 was silenced, the function of LvTPI-like and LvTPI-Blike in DIV1-infected L. vannamei was investigated. The shrimp were challenged with DIV1 at 48 h post-dsRNA injection in the following experiments. As shown in Figure 9C, the cumulative survival rate in the dsRNA-LvTPI-Blike group was lower than those in the dsRNA-EGFP group. However, there was no significant difference between the cumulative survival rate of the dsRNA-LvTPI-like and dsRNA-LvTPI-Blike groups compared with the dsRNA-EGFP group during DIV1 infection. The final survival rates were 30.0, 11.1, and 28.95% for dsRNA-LvTPI-like, dsRNA-LvTPI-Blike, and dsRNA-EGFP groups, respectively. However, both dsRNA-LvTPI-like and dsRNA-LvTPI-Blike suppression reduced DIV1 replication. The virus copies in five tissues-hemocyte, hepatopancreas, intestine, gill, and muscle-were measured in shrimp at 24 and 48 h post-DIV1 infection in each double-stranded RNA silencing group. As shown in Figure 10, the DIV1 copy numbers for both the dsRNA-LvTPI-like and the dsRNA-LvTPI-Blike groups were not significantly different from that for the dsRNA-EGFP group at 24 hpi. At 48 hpi, the viral loads in the hemocyte, hepatopancreas, intestine, gill, and muscle of the dsLvTPI-Blike + DIV1 group was 3.10 × 10 2 , 1.75 × 10 3 , 1.34 × 10 3 , 2.64 × 10 3 , and 6.95 × 10 2 copies/µg DNA, respectively. The viral loads in all the detected tissues of the dsLvTPI-Blike + DIV1 group were significantly lower than those of the dsRNA-EGFP + DIV1 control group (p < 0.05). In the dsLvTPI-like + DIV1 group, the number of copies of DIV1 at 48 hpi decreased in the hemocyte and muscle but increased in the hepatopancreas, intestine, and gill, with a significantly different level only in the hepatopancreas.

DISCUSSION
DIV1 is a new disease prevalent in shrimp cultures in China. DIV1 mainly affects the hematopoietic tissue and the hemocytes of shrimp (6). The emergence of DIV1 poses a new biological risk to the shrimp farming industry (33). However, there are no reports on the harmful effects of DIV1 on L. vannamei until now. In this study, the toxicity of DIV1 for L. vannamei was measured at different time points, and a comparative transcriptome analysis of L. vannamei challenged by DIV1 was conducted. The results showed that several metabolisms and immune function signaling pathways participated in the L. vannamei response to DIV1. In addition, TPI genes play an outstanding role.
As an important parameter of virulence, LD 50 was often used to evaluate the effect of virus on shrimp. In crustaceans, the LD 50 of several disease-causing viruses including WSSV, IHHNV, and TSV have been reported (34)(35)(36); however, the LD 50 of DIV1 in shrimp has not been found. To our knowledge, this is the first report on the virulence of DIVI in crustaceans. The detection of DIV1 replication in LD 50 test showed that the copies of DIV1 in the hemocyte, hepatopancreas, intestine, gill, and muscle of infected L. vannamei were significantly increased at all the detected timepoints after injection. A consistent conclusion was confirmed by Qiu et al. A histological analysis of ultrathin sections imaged under transmission electron microscopy revealed that enveloped icosahedral virus-like particles were present in hemocytes localized to the hemal sinus, hepatopancreas, and muscle of L. vannamei infected by DIV1 (6). It can be inferred that the mortality of L. vannamei was the result of virus replication.
Transcriptome sequencing, a powerful tool in biological research, has been used to analyze the immune response to many shrimp pathogens (37). Xue et al. compared the transcriptome profiles in hemocytes of uninfected and WSSV-infected L. vannamei and found 1,179 immune-related unigenes (38). Zeng et al. performed transcriptome sequencing in the hepatopancreas of L. vannamei infected with TSV and found 1,311 differential genes, including a large number of immune-related genes (39).   (13). Our previous study in F. merguiensis found that DIV1 affected not only some immune-related pathways but also some metabolic pathways such as amino sugar and nucleotide sugar metabolism, glycolysis/gluconeogenesis, and inositol phosphate metabolism (14). However, the key factors that play important roles during DIV1 infection in these species are still unclear. Another notable result in our transcriptome analysis was that lots of DEGs annotated as TPI participated in several members of the top 20 KEGG enrichment pathways. TPI was known as an important factor which plays a role in both glycolysis and phospholipid biosynthesis in all organisms (43). TPI is an enzyme in the glycolytic pathway, which catalyzes the reversible Error bars represent ± SD of three replicates. Data were analyzed with the GraphPad Prism software using the log-rank (Mantel-Cox) method. All data are given in terms of means ± standard error (SE). Asterisks indicate significant differences. *P < 0.05 and **P < 0.01 (n = 3).
interconversion of dihydroxyacetone phosphate (DHAP) and the triose phosphate glyceraldehyde 3-phosphate (GAP) (44)(45)(46)(47). TPI is vital to an organism's response to external factors (48). Besides that, TPI could be used to develop vaccines against parasitic diseases in mammals (49,50). In shrimp, the only study in Exopalaemon carinicauda showed that TPI facilitated the replication of WSSV (51). In this study, three types of TPI genes (namely, LvTPI-like, LvTPI-Blike, and LvTPI-Blike1) were obtained in L. vannamei, and their functions during DIV1 infection were identified using RNAi. To our surprise, the results showed that the silence of LvTPI-like or LvTPI-Blike1 significantly reduced the survival rate of L. vannamei. This result can be attributed to the important role of TPI in both glycolysis and phospholipid biosynthesis, and the silence of LvTPI-like or LvTPI-Blike1 caused the metabolic disorders, affecting the normal life activities of L. vannamei (43). It is notable that LvTPI-Blike1 expression at 48 h post-dsRNA injection was not significantly lower than the control. That may be because the L. vannamei, in which LvTPI-Blike1 was knocked down, died before the detection time point. On these bases, only the survival rates of LvTPI-like and LvTPI-Blike knock-down L. vannamei after DIV1 infection were investigated. It was shown that the silence of LvTPI-like and LvTPI-Blike did not lead to a significant difference in shrimp survival, but the DIV1 copies were significantly reduced in all the detected tissues of LvTPI-Blike knock-down L. vannamei and the hemocytes and the muscle of LvTPIlike knock-down L. vannamei at 48 hpi. Similar results have been reported in the function analysis of immune genes in L. vannamei. Shi et al. showed that the cumulative mortality of L. vannamei after WSSV infection had no significant difference between laccase knockdown and the control groups, but the WSSV copies were significantly reduced in laccase knock-down L. vannamei (52). Similarly, the knockdown LvTube, LvPelle, and LvTAB2 did not affect the mortality of L. vannamei caused by WSSV infection, but could slow down the replication of WSSV in the infected L. vannamei (53,54). All these findings were in accordance with the viewpoint that host physiology could be taken over by the virus to support their replication, and the physiological disorder of the host is not conducive to the replication of the virus. In this study, the reduced DIV1 copies may probably be due to the physiological disorder caused by LvTPI-like or LvTPI-Blike silence. Considering the important role of TPI in metabolism, it can be speculated that a viralinduced Warburg effect could also be induced in DIV1-infected L. vannamei, which is similar to the effect of WSSV infection in shrimp (42). In E. carinicauda infected with WSSV, glycolysis was affected and TPI was up-regulated, which produced more GAP which became DHAP, which is necessary for the synthesis of phospholipids. The production of phospholipids then affected WSSV replication (51). However, the mechanism of TPI shrimp during DIV1 infection could not be clarified in this study. Further studies are needed. In addition, what could not be ignored was that the DIV1 copies were not significantly different in the hepatopancreas, intestines, and gill of LvTPI-like knock-down L. vannamei when compared with the control. It may be related to the functional specificity of the gene in different tissues. In any case, there is no doubt about the fact that TPI-like genes play an important role during DIV1 infection in L. vannamei.
In conclusion, we determined the LD 50 values of DIV1infected L. vannamei and found that TPI-like genes played an important role during DIV1 infection in L. vannamei. The results were helpful to better understand the immune response mechanism of disease resistance in shrimp, which could provide a theoretical basis for the prevention and the control of the viral disease in shrimp culture and be of great significance for promoting the health and the sustainable development of the shrimp industry.

DATA AVAILABILITY STATEMENT
The datasets presented in this study can be found in online repositories. The names of the repository/repositories and accession number(s) can be found in the article/Supplementary Material.