- Research article
- Open Access
Development and validation of a mixed-tissue oligonucleotide DNA microarray for Atlantic bluefin tuna, Thunnus thynnus (Linnaeus, 1758)
© Trumbić et al. 2015
- Received: 12 August 2015
- Accepted: 12 November 2015
- Published: 25 November 2015
The largest of the tuna species, Atlantic bluefin tuna (Thunnus thynnus), inhabits the North Atlantic Ocean and the Mediterranean Sea and is considered to be an endangered species, largely a consequence of overfishing. T. thynnus aquaculture, referred to as fattening or farming, is a capture based activity dependent on yearly renewal from the wild. Thus, the development of aquaculture practices independent of wild resources can provide an important contribution towards ensuring security and sustainability of this species in the longer-term. The development of such practices is today greatly assisted by large scale transcriptomic studies.
We have used pyrosequencing technology to sequence a mixed-tissue normalised cDNA library, derived from adult T. thynnus. A total of 976,904 raw sequence reads were assembled into 33,105 unique transcripts having a mean length of 893 bases and an N50 of 870. Of these, 33.4 % showed similarity to known proteins or gene transcripts and 86.6 % of them were matched to the congeneric Pacific bluefin tuna (Thunnus orientalis) genome, compared to 70.3 % for the more distantly related Nile tilapia (Oreochromis niloticus) genome. Transcript sequences were used to develop a novel 15 K Agilent oligonucleotide DNA microarray for T. thynnus and comparative tissue gene expression profiles were inferred for gill, heart, liver, ovaries and testes. Functional contrasts were strongest between gills and ovaries. Gills were particularly associated with immune system, signal transduction and cell communication, while ovaries displayed signatures of glycan biosynthesis, nucleotide metabolism, transcription, translation, replication and repair.
Sequence data generated from a novel mixed-tissue T. thynnus cDNA library provide an important transcriptomic resource that can be further employed for study of various aspects of T. thynnus ecology and genomics, with strong applications in aquaculture. Tissue-specific gene expression profiles inferred through the use of novel oligo-microarray can serve in the design of new and more focused transcriptomic studies for future research of tuna physiology and assessment of the welfare in a production environment.
- Thunnus thynnus
- Tissue gene expression, genome mapping
Fish represent the oldest and most diverse vertebrate group, inhabiting every available aquatic environment . They display remarkable heterogeneity of life trait characteristics and occupy a historically important place in human culture as a source of nutritionally valuable food. Marked by genome duplication events, the diversification and adaptive radiation of fish represent an attractive evolutionary model to study ecological, behavioural and physiological aspects of biodiversity . Migratory tunas (family Scombridae, order Perciformes: suborder Scombroidei), are pelagic oceanodromous top predators, which display a set of extreme adaptations to life in a prey depauperate pelagic environment. They are obligate ram ventilators with streamlined bodies for rapid locomotion, have increased aerobic scope and metabolic rates that allow them to satisfy the energy needs of multiple high performance functions without compromise, including high digestive rates, increased somatic and gonadal growth and incredibly fast recovery from oxygen debt after exhaustive exercise compared to other teleosts [3, 4]. A key characteristic of tunas is their ability to retain metabolic heat in the brain, red muscle and viscera via vascular specialisations called rete mirabile, which comprise numerous juxtaposed arterial and venous vessels acting as a counter-current heat exchange system . This heterothermic physiology shares characteristics of both poikilothermic and homeothermic organisms and is considered to have developed in order to permit thermal niche expansion, especially in correlation with maintenance of central nervous system function  or to sustain a rise in aerobic capacity and muscular performance .
The largest of the tuna species, Atlantic bluefin tuna, Thunnus thynnus (Linnaeus, 1758), inhabits the North Atlantic Ocean and the Mediterranean Sea. Based on the observed homing behaviour to two major spawning grounds, the Gulf of Mexico and the Mediterranean Sea , the International Commission for the Conservation of Atlantic Tunas (ICCAT) recognises a smaller Western and larger Eastern population as separate management units divided by the 45°W meridian. Although the differentiation between these populations has been corroborated by genetic data [8, 9], results of electronic tagging reveal a complex ecology, with extensive trans-Atlantic migrations and mixing of individuals at the foraging and spawning grounds [10, 11], complicating T. thynnus stock management. In high demand for sushi and sashimi preparation in the Japanese market, both populations of T. thynnus are considered to be depleted and overfished [12–14]. While latest assessments report a reduction in fishing mortality and increase in spawning stock biomass, allowing for moderate catch quotas increase after a long time in 2015 , these populations remain under threat. Capture-based tuna aquaculture, developed in the Mediterranean Sea over the past two decades, relies on yearly population renewal from the wild, fattening fish to market size in 3 months to 2 years, but is not thought to be sustainable in the long run . Consequently, it is considered that only domestication of T. thynnus and development of high welfare aquaculture practices independent of wild resources can preserve the species for future generations. Extensive research efforts have been made regarding the control of T. thynnus reproduction in captivity [16, 17], a prerequisite for the development of a sustainable aquaculture industry. As evidenced from the Pacific bluefin tuna (T. orientalis) aquaculture development in Japan , the first bluefin tuna species successfully grown in captivity, a comprehensive approach will be required to solve many technical problems in order to meet this species’ physiological needs.
Large scale transcriptomic studies of important life trait characteristics, such as growth, maturation, environmental tolerance and disease resistance, can provide important knowledge concerning underlying molecular mechanisms and control elements, assisting in the development of welfare-centred and sustainable management strategies for aquaculture species, e.g. [19, 20]. With the increasing availability of high throughput sequencing technologies, development of the necessary tools and resources for broad-scale transcriptomics studies can be achieved in a relatively short period of time, even for species with a low level of background information . Until recently, publicly available genomic resources for T. thynnus have been relatively scarce, most being derived from a single EST (expressed sequence tag) sequencing project comprising adult liver, ovary and testis mRNA transcripts contributed by Chini et al. . This resource served as the basis for the construction of the first T. thynnus-specific oligonucleotide DNA microarray, which was employed for the description of the Gulf of Mexico T. thynnus gonad transcriptome . It was also utilised to profile the cardiac transcriptome response to temperature acclimation in congeneric T. orientalis , highlighting the applicability of such a tool for gene expression analyses in phylogenetically related species. The release of a genome for T. orientalis  opens new opportunities for tuna comparative genome studies and ongoing transcriptome characterisation projects.
The objectives of the current study were: 1) to contribute to and expand existing transcriptomics resources for studying T. thynnus, 2) to use the newly developed resource to design and validate a custom oligo-microarray, and 3) to employ the newly developed microarray to investigate functional differences in transcript expression among tissues. To this end, pyrosequencing technology was used to sequence adult mixed-tissue normalised cDNA library providing the template for the development of a custom 8 × 15 K Agilent oligo-microarray. The microarray was used to compare: gill, heart, liver, ovaries and testes of adult fish and to infer their respective transcriptional specificities. The derived transcriptome was also compared to T. orientalis genome.
Animal tissue collection and RNA extraction
All fish handling procedures were conducted in accordance with established standards for the care and use of animals of the Ethical committee for animal welfare at the Institute of Oceanography and Fisheries, Croatia. No specific permits were required as samples were collected during standard commercial operations without any form of experimental manipulation.
Atlantic bluefin tuna were reared in mid-Croatian offshore farm cages for two years. During the winter harvest of 2012, adult fish (curved fork length (mean ± SD) = 177 ± 9 cm; weight = 99 ± 14 kg) were sacrificed by pithing and samples of kidney, spleen, liver, gonads, gills, small intestine, heart (apex ventriculi), red and white skeletal muscle, skin scrapes and whole blood, were dissected and preserved in RNAlater stabilisation solution (Qiagen, UK) at −20 °C, after overnight storage at +4 °C. In addition, liver and kidney samples from juvenile moribund fish with signs of septicaemia were available from another study  and were included in a normalised cDNA library preparation to increase the diversity of the sequenced transcriptome.
Between 30 – 40 mg of each of the tissues were homogenised separately in 1 mL of TRI Reagent (Sigma-Aldrich, UK) by 2 × 35 s disruption runs on a Mini-Beadbeater-24 (BioSpec Products, Inc, USA) and total RNA was extracted according to manufacturer’s instructions. The RNA precipitation step was modified to include a high-salt solution as recommended for polysaccharide- and proteoglycan-rich sources . Integrity of total RNA preparations was assessed by ethidium bromide agarose gel electrophoresis and purity and concentration by spectrophotometry (NanoDrop ND-1000, Thermo Scientific, USA).
Normalised cDNA library preparation and sequencing
A mixed RNA sample comprising equal amounts (5 μg) derived from all sampled tissues, except ovaries, was created from one female, one male and one moribund juvenile specimen and purified using RNeasy columns (Qiagen, UK). Because T. thynnus ovaries showed a significantly increased proportion of the small RNA fraction comprising tRNA and 5S RNA, as previously found in amphibians [28, 29] and several other teleosts [30, 31], poly(A) + RNA was first isolated from the ovarian total RNA population using a Poly(A) Purist kit (Ambion, UK) and subsequently 200 ng of the isolated mRNA were included in the pool. For normalisation, the MINT kit (Evrogen, Russia) was initially used to construct a full-length-enriched double stranded cDNA library from 1.5 μg of the tissue RNA mixture, according to manufacturer’s protocol. The TRIMMER kit (Evrogen, Russia) was used to normalise 1 μg of cDNA starting material, applying the duplex-specific nuclease (DSN) method . The final normalised and amplified cDNA library was purified using a MinElute PCR Purification Kit (Qiagen, UK) and ranged in size from 0.25 to 3 kb, as visualised on a 1.5 % agarose/ethidium bromide gel.
GS FLX Titanium library preparation and sequencing were performed by the Edinburgh Genomics facility (University of Edinburgh, UK). Approximately 5 μg of normalised cDNA were used for generating a 454 sequencing library using the GS FLX Titanium Rapid Library Preparation kit (Roche Applied Science, UK), following manufacturer’s instructions. Sequencing was performed using The Genome Sequencer™ (GS) Titanium FLX instrument (Roche Applied Science, UK). Bases were called with 454 software and reads trimmed to remove adapter sequences.
Data filtering and assemblies
Low-quality reads (Phred score < 30) were filtered out and PRINSEQ v0.20  was used to remove PCR duplicates and low complexity sequences. Two complementary sequence read assembly methods were chosen for this study: WGS-assembler 7.0  and Mosaik-aligner v2.1  to assemble the contigs based on the Genbank archived T. thynnus EST database . Subsequently, to lower the redundancy resulting from de-novo assemblies, TRF 4.07b  was used to remove all transcripts shorter than 500 bases or exhibiting repetition, with entropy above 1.
Sequence annotation and functional assignments
The longest coding DNA sequences were determined for each transcript using the command-line program getorf from the EMBOSS v6.6.0 package . ESTScan v2  was then used to confirm transcript coding regions and determine sequence orientation. The BLAST algorithm  was used for sequence similarity searches against public databases. The coding sequences of the predicted transcripts were annotated using BLASTP searches against the GenBank Reference Proteins database , with an expectation value (e-value) cut-off of 10−4, minimum similarity of at least 60 %, and minimum alignment length of 33 amino acids. Additionally, the transcripts were annotated using BLASTN searches against the annotated EST T. thynnus database . The inferred annotations were used to retrieve Gene Ontology (GO) annotation for molecular function, biological process and cellular component . To avoid redundant functional assignments, the best-rated similarity hit with at least one GO annotation was chosen. A custom pipeline converted GO terms to GO Slim terms, using the Protein Information resource and Generic GO Slim files . Kyoto Enyclopedia of Genes and Genomes (KEGG) database  was used to infer functional annotation of the sequences through KAAS (KEGG Automatic Annotation Server)  using single-directional best hit method for ESTs. Sequences with assigned KO (KEGG Orthology) identifiers were categorised into functional groups according to the KEGG BRITE hierarchy, excluding human diseases.
Generated sequence data was compared with two perciform fish genomes that have been publicly released: Thunnus orientalis (Pacific bluefin tuna; NCBI Assembly GCA_000418415.1;), and Oreochromis niloticus (Nile tilapia, NCBI Assembly GCA_000188235.2). The 133,062 contigs (684,497,465 bp) of T. orientalis and the 77,755 (927,696,114 bp) of O. niloticus genomes were downloaded and BLASTN  was used to search for similar transcripts. Default parameters were used for BLASTN searches, with the following exceptions to account for the divergence and short length of the sequences available: minimum alignment size 80 nt, minimum percentage of sequence identity 25 %, maximum e-value 0.001 and low complexity mask on. Results were displayed using a hive plot .
T. thynnus microarray design
Transcripts with a significant match to a reference protein were chosen for microarray probe design. In addition, 57 publicly available full mRNA sequences from the T. thynnus nucleotide (NCBI) database were also included. Sixty-mer oligonucleotide probes were designed using the eArray (Agilent Technologies, UK) online probe design tool with Base Composition and Best Probe Methodologies, 3’bias and sense orientation. Two probes were designed for each target transcript. After initial screening, unique probes showing no cross-hybridisation potential were selected to produce an 8 × 15 K Agilent custom oligo-DNA microarray design format (Agilent Design ID = 038391), comprising 15,208 user defined features and 536 Agilent positive and negative controls. Target transcripts (N = 6,439) with best annotation were represented with two probes on the array and the remainder (N = 2,190) with a single probe. In all, 6,287 unique proteins were annotated. For calculation of the multiplicative detrending step implemented within the Agilent Feature extraction software 35 probes were replicated five times.
For microarray validation, five metabolically distinct tissues were chosen from adult T. thynnus: gill, heart, liver, testes and ovaries (4 biological replicates per tissue). A total of 20 arrays (4 replicates x 5 tissues) were assayed in the final common reference pool design, with the pool comprising a contribution from each biological sample. Amplified and fluorescently labelled cRNA (complimentary RNA) for microarray hybridisations was prepared in accordance with the Two-Color Microarray-Based Gene Expression Analysis - Low Input Quick Amp Labelling Protocol v6.6 (Agilent Technologies, USA). The cDNA synthesis was initiated with 150 ng of total RNA from each tissue sample, this being primed with an Oligo dT – T7 RNA polymerase promoter. Subsequently, T7 RNA polymerase incorporated Cyanine 3 (Cy3) or Cyanine 5 (Cy5) – CTPs into a growing chain of antisense cRNA. Amplified cRNA was purified using the GeneJET RNA Purification Kit (Thermo Scientific, UK) following the manufacturer’s RNA Cleanup Protocol and was further quality-checked by spectrophotometry (NanoDrop ND-1000, Thermo Scientific, USA) and agarose gel electrophoresis. Following amplification and purification, 300 ng of each Cy3 labelled test and 300 ng of Cy5 labelled reference pool cRNA were mixed together and incubated with Fragmentation and Hybridization buffers according to manufacturer’s instructions. Competitive hybridisations were carried out in a rotary oven (Agilent Technologies, UK) over 17 h at 65 °C and 10 rpm. Following Agilent standard protocols, the slides were subsequently washed in Wash Buffer 1, Wash Buffer 2, acetonitrile and Agilent Stabilization and Drying solution, the latter to reduce ozone-induced decay of Cy5 signal. Slides were stored in light proof box and scanned within 1 h of washing.
Microarray data analyses
Scanning was conducted using an Axon Genepix 4200A scanner with Genepix Pro 6.1 image acquisition software (Molecular Devices, UK) with 60 % red and 90 % green laser power at 5 μm resolution. Saturation tolerance was set to 0.05 % and automatic photo-multiplier tube (auto-PMT) gain used to achieve similar mean intensities of Cy3 and Cy5 signals. Acquired data were exported and processed using the Agilent Feature Extraction software (v18.104.22.168) to obtain background-subtracted signals, as well as other spot statistics and quality metrics. Scan data were analysed using GeneSpring GX v12 (Agilent Technologies, UK). Baseline transformation was not employed and data were normalised using a Lowess model. Principal component analysis (PCA) was conducted to visually inspect the distribution of gene expression variance among arrays within and between experimental conditions. Following removal of Agilent control features, stringent quality filtering involved removal of saturated and non-uniform features, population outliers and features that were not significantly positive with respect to the local background.
One-way ANOVA unequal variance (Welch) (p < 0.05) was applied to preselect features showing potential differences in gene expression between tissues. Unsupervised network analysis was conducted on identified features using Biolayout Express 3D , using a Pearson coefficient of correlation as a similarity measure and threshold over 0.94. The network graph was clustered into distinct patterns of gene expression using a Markov clustering algorithm (MCL) with inflation value set to 2.0 and smallest cluster allowed being 10, to achieve optimal granularity of clusters and focus only on larger areas of high connectivity .
Functional gene set analyses were performed on the entire list of quality filtered entities based on KEGG KO identifiers. During the analyses, gene expression profiles were collapsed into 3,222 unique KOs using the median method. Tests were run to identify significantly up- and down- regulated pathways for each tissue and their pairwise combinations against all other samples using Generally Applicable Gene-set Enrichment (GAGE) analyses , implemented as R/Bioconductor package , which is robust to small datasets with different sample sizes. A default FDR q-value of 0.1 was used as a cut-off. Pathways were subsequently grouped into KEGG functional categories and the difference between the counts of up- and down- regulated pathways in each category hierarchically clustered and displayed as a heatmap.
Ten transcripts from different Biolayout derived clusters showing tissue-specific and diverse expression profiles, and spanning a wide range of fold change (FC) values, were chosen for RT-qPCR validation. Three additional genes were tested to serve as internal controls (reference genes): elongation factor-1α (elf-1α) , beta-actin (actb)  and a transcript showing a stable expression profile across the experimental conditions, annotated as FtsJ methyltransferase domain containing 2 (ftsjd2), from the microarray. Primer3  software was used to design primers for the selected sequences with at least one in the pair overlapping the target hybridisation area of the microarray 60-mer probe. Complementary DNA (cDNA) was synthesised from 2 μg of the same total RNA extractions used for the microarray experiment employing the High Capacity cDNA Reverse Transcription Kit (Applied Biosystems, UK). The synthesis was primed with 1.5 μl of random hexamer primers supplied with the kit and 2.5 μM anchored-oligo (dT)20 (Eurofins, Germany) per 20 μl reaction. DNase treatment was not performed prior to cDNA synthesis as it may result in RNA degradation . Instead, minus RT (RT-) controls (reverse transcriptase replaced with water) were created to control for the presence of genomic DNA in the extractions.
Real-time PCR assays (20 μl) were performed on a Mastercycler ep realplex2 (Eppendorf, Germany) using Luminaris Color HiGreen qPCR Master Mix (Thermo Scientific, UK), in duplicate with 25 × cDNA template dilutions and 0.3 μM of each primer, according to the following thermal profile: 50 °C for 2 min (Uracil-DNA Glycosylase pre-treatment), 95 °C for 10 min, followed by 40 cycles of denaturation at 95 °C for 15 s, annealing at 60 °C for 30 s and elongation at 72 °C for 30 s. After amplification a melting curve analysis was performed from 55 °C to 95 °C at 0.5 °C increments for 15 s each to verify single product amplification. The presence of the correct size of PCR product was also verified by agarose gel electrophoresis. Six-point standard curves of a 4 × dilution series of a pool of all starting cDNAs were run with every assay to determine primer-specific efficiencies. A standard curve was used to extrapolate non-normalised relative copy numbers for each gene and the BestKeeper application  was used to inspect the suitability of reference genes for normalisation.
To compare the fit between qPCR and microarray fold changes (FCs), we calculated the concordance correlation coefficient (CCC) as well as other regression metrics previously described by Miron et al. . The statistical significance of individual targets’ expression profiles was examined on the combined qPCR and microarray data for each gene, coded by their respective percentile ranks, using a nonparametric Kruskal-Wallis test implemented in R software.
Pyrosequencing and transcriptome assembly
Statistics of the assembled T. thynnus sequences
Number of reads
Mean read size
Total size of reads
After assembly (no singletons)
Number of transcripts
Total size of transcripts
After assembly (singletons only)
Number of transcripts
Total size of transcripts
After filtering (>500 b)
Number of transcripts
Total size of transcripts
Functional inference by searching against public databases
The assembled transcripts were annotated using BLASTP and BLASTN searches against the RefSeq Proteins  and EST databases respectively . The results indicated that out of 33,105 transcripts, 11,065 (33.4 %) showed significant similarity to known proteins or gene transcripts in the RefSeq Proteins database. To evaluate the T. thynnus coverage of the assembled transcripts, the 10,163 EST available for T. thynnus were aligned to the 33,105 transcript sequences generated in this study and vice versa. In total, 4,939 (48.6 %) of all T. thynnus ESTs aligned to at least one transcript, whereas 4,394 (13.3 %) of the new transcripts had at least one corresponding T. thynnus EST. This demonstrates that the strategy employed captured some of the existing data  and added new information to T. thynnus database.
Results of microarray transcriptional inference and qPCR validation
Size and tissue specificity of the first six gene expression clusters of T. thynnus obtained by MCL algorithm in Biolayout Express 3D
Eight transcripts representative of the six largest Biolayout clusters were chosen for the purpose of qPCR validation, taking into account their functional relevance and FC span (see Additional file 4 for details): aquaporin 3b aqp3b (Gill), sarcoplasmic reticulum calcium-ATPase 2 atp2a2a (Heart), complement C4-like c4, coagulation factor V f5 (Liver), exosome component 2 exosc2, pescadillo pes (Ovary), somatolactin sl (Testis) and mediator complex subunit 6 med6 (Ovary/Testis). Transcripts specific to particular tissue clusters show high expression in only that tissue, such that examination of expression gives low values for all other tissues. Thus two additional transcripts, biliverdin reductase B blvrb and prohibitin 2 phb2, were chosen as exemplars showing expression across a range of tissues. This ensured that the microarray validation did not comprise only tissue specific transcripts. However, as functional interpretation of results focuses on tissue-specific signatures, these two transcripts are not specifically discussed. Three reference genes were tested, actb, elf-1α, previously used in T. thynnus qPCR experiments [23, 26, 50], and a candidate from this microarray study, ftsjd2, which subsequently did not show stable expression profiles according to BestKeeper tool, exceeding the recommended quantification cycle (Cq) standard deviation of one . This was not unexpected as we were comparing different tissues of adult fish; however, the variation was systematically attributed only to ovarian tissue, which was characterised by a very different total RNA population. Hence, non-normalised (normalised to total RNA used for cDNA synthesis) and normalised data (normalised to geometric mean of actb, elf-1α and ftsjd2 = TEF) were further compared to microarray results. For all information pertinent to RT-qPCR validation of microarray results see Additional file 4.
Agreement between qPCR and microarray data
Functional interpretation of tissue-specific expression profiles
In contrast to the gills, the ovaries showed over-representation of glycan biosynthesis and metabolism, folding, sorting and degradation, as well as cell growth and death, nucleotide metabolism, transcription, translation, replication and repair (Fig. 7). Primary oocyte growth is characterised by intense transcriptional activity and the presence of abundant ribosomes in highly granulated ooplasm [64, 65]. Maternal factors, protein and RNA species, are produced at this time and serve to support embryo development until the zygotic genome is activated . Our analyses also suggest these processes are coupled with RNA degradation and mRNA surveillance pathways, crucial for maintenance of the integrity of transcriptional activity. Expression of a pescadillo (pes) homologue, important for early embryonic development in zebrafish , cell cycle progression and 60S ribosomal subunit synthesis [67, 68], and a transcript corresponding to exosome component 2 (exosc2) of the exosomal complex, comprising several 3′-5′ exoribonucleases involved in mRNA, 5.8S rRNA and small RNA processing , were confirmed as ovary-specific cf. other tested tissues (Fig. 6). These processes could also reflect the fact that the specific total RNA population of T. thynnus ovary seems to be dominated by the 5S RNA fraction, thus resembling the oocyte RNA complement of African clawed frog Xenopus laevis , Iberian ribbed newt Pleurodeles waltl  and a number of teleost species [30, 31]. It is believed that the 5S fraction is stored with aminoacyl-tRNAs in 7S and/or 42S ribonucleoprotein particles in the ooplasm and is progressively transferred, starting with vitellogenesis, into ribosomes by the end of oocyte differentiation . This observation concurs well with our samples being taken during winter when the most advanced oocyte stage found in T. thynnus ovaries is perinucleolar . Other typical ovarian transcripts were also present in ovary-specific Cluster 1 (see Additional file 3), including the aquaporin 1a homologue, previously detected in T. thynnus ovaries [22, 23] and involved in the process of oocyte hydration prior to ovulation, which is necessary for providing buoyancy in pelagic fish eggs [64, 71]. A major driving force of this water influx is the osmotic pressure produced by oocyte yolk protein cleavage by lysosomal proteases termed cathepsins. Cathepsins B, D and L have been implicated in this process in fish [64, 72]. Gardner et al.  found transcripts similar to cathepsin S, L and cathepsin Z precursor differentially expressed in ovarian relative to testis tissue in T. thynnus and postulated that the species likely uses different cathepsin proteases for this purpose. In this study, expression profiles of different cathepsin-like transcripts (A, L, F, S, Z) were detected across tissue clusters (see Additional file 3) with transcripts similar to cathepsin A and S placed in the ovary-specific Cluster 1, thus supporting this hypothesis.
Testes displayed a number of transcripts in common with ovaries leading to a separate, shared “gonad-specific” cluster using Biolayout Express 3D (Cluster 5). This cluster was characterised by the presence of transcripts generally important for germline development. These included a subunit of mediator complex (med6), which is a transcriptional co-activator of RNA polymerase II that is particularly important for expression of developmentally regulated genes . Fanconi anaemia complementation group 1 (fanci) was also present, part of the DNA repair mechanism employed during homologous recombination in meiosis , as well as Piwi-like 2 (piwil2) homologue, essential for the germline integrity via transposable element repression and gonad development . Analysis of ovary- and testis-associated transcripts as a single amalgamated group (ovary + testis) did not reveal any new additional pathways relative to separate analysis of the two tissues (see Additional file 6). A further Biolayout cluster comprised largely testis-specific transcripts (Cluster 6). Testis-associated pathways (Fig. 7) were more similar to those of other inspected tissues than to ovaries, however there was an overlap. Shared pathways were associated with nucleotide metabolism, replication, repair and translation. Some of the transcriptional differences between ovaries and testes have been identified for T. thynnus . A similar transcript to one found differentially expressed in this previous study, was present here in the testis-specific Cluster 6; a component of t-complex tcte1, important for molecular interaction between sperm and egg zona pellucida . This was also identified as testis-specific in rainbow trout by Rolland et al., when compared to ovary, liver, muscle, gill and brain transcripts . Intestinal fatty acid binding protein 2 (fabp2), suggested to play a role in sex dependent energy balance in T. thynnus , was found in heart-specific Cluster 2 (see Additional file 3) with its expression markedly elevated in testes compared to ovaries. The presence of several typically pituitary hormone transcripts, growth hormone (gh) and somatolactin (sl), were also apparent in the testis-specific cluster. The expression profile for somatolactin was re-investigated with qPCR and joint analysis of both datasets statistically confirmed (p < 0.05) this observation (Fig. 6). Both hormones are members of the growth hormone/prolactin family and are implicated in pleiotropic functions such as somatic growth, osmoregulation, lipid metabolism and reproduction [78, 79]. Extra-pituitary expression of growth hormone has been demonstrated in mammals and chicken testes , as well as fish  being localised to spermatogonia and primary spermatocytes in chicken and Sertoli cells surrounding the germ cells in Japanese eel. It has a paracrine role during spermatogenesis, stimulating proliferation of spermatogonia. This mitotic phase of spermatogenesis occurs in Mediterranean T. thynnus between October and January , corresponding to the collection period for our samples. Accordingly, a germ cell line marker vasa homologue (vasa), a putative RNA helicase found to be expressed in Pacific bluefin tuna spermatogonia , was also found to be up-regulated in testes of T. thynnus examined here. Primarily expressed in the pituitary gland, somatolactin mRNA has been detected across various tissues, including gonads in fish [84, 85]. These findings suggest T. thynnus testes actively transcribe gh and sl, warranting further investigation, especially in the context of reproductive cycle in both gonads.
During their spawning migrations, tuna utilise perigonadal mesenteric fat deposits as a source of metabolic energy for reproductive maturation and active swimming, which are primarily processed by the liver [82, 86]. In this study the T. thynnus liver was functionally characterised by lipid, amino acid and carbohydrate metabolism, fat digestion and absorption, bile secretion, metabolism of cofactors and vitamins, xenobiotic biodegradation and immune system (Fig. 7), consistent with the basic metabolic role of this organ  and agreeing with previous findings for the liver of T. thynnus . Among the transcripts showing predominant expression in the liver, members of a haem-containing superfamily of cytochrome P450 mono-oxygenases, involved in metabolic biotransformation of xenobiotics and lipids often associated with liver , were found (see Additional file 3). The liver is also a key production site for coagulation and complement proteolytic cascade components, mediators of blood clotting and elements of the innate immune system. Two representative transcripts, homologues of blood coagulation factor V (f5), pivotal proteins in maintaining haemostasis with dual pro-coagulant and anti-coagulant activities in humans , and complement component C4 (c4), which plays a crucial role in the classical and lectin pathways of complement activation as a subunit of the C3 convertase , were found to be significantly up-regulated in the liver compared to other tissues (Fig. 6).
Tuna cardiac function has been the subject of extensive investigation, as the heart operates at ambient temperature while supporting high metabolic rates and endothermic physiology . Tuna have large hearts that function at close to maximum stroke volumes and depend, more than other teleosts, on oxygen consuming fatty acid oxidation as a fuel source, similar to mammals [62, 91]. Mitochondria isolated from skipjack tuna ventricles have a higher capacity to oxidise lactate than other metabolites, suggesting that lactate is also an alternative fuel source, especially during high intensity swimming when blood lactate is elevated . These processes were well represented in the pathways and functional categories assigned to T. thynnus heart (apex ventriculi) compared to gill, liver and gonads in this study. Lipid (fatty acid degradation), energy (oxidative phosphorylation), carbohydrate metabolism (pyruvate metabolism, glycolysis/gluconeogenesis) and circulatory system (cardiac muscle contraction) were most prominent categories in functional contrasts displayed for the heart in Fig. 7. The ability to maintain cardiac performance during temperature acclimation, especially to cold, has been linked at the transcriptomic and functional level to Ca2+-dependent excitation-contraction coupling (EC) in T. orientalis [24, 93]. Up-regulation of sarcoplasmic reticulum calcium-ATPase 2 (atp2a2a or serca2) homologue, vital for Ca2+ removal from cytosol into sarcoplasmic reticulum in vertebrates , has been identified in T. thynnus heart-specific Cluster 2 (Fig. 6 and see Additional file 3).
Amalgamating transcripts by pairs of tissues (e.g. gill + liver, gill + heart, gill + testis etc.), in order to resolve shared and unique pathways, showed pairings which included gill, heart and liver to be most informative and revealed functional signatures shared between these tissues. For instance, the most pronounced feature in Fig. 7 is the up-regulation of metabolism of other amino acids, β-alanine metabolism specifically (see Additional file 6), found exclusively for the heart + liver combination. β-Alanine is produced in vertebrate liver and is used as a rate-limiting precursor for synthesis of histidine-containing dipeptides such as carnosine and anserine in skeletal muscle, heart and brain [95, 96]. These compounds are involved in intracellular pH buffering by tissues exhibiting high dependence on anaerobic glycolytic metabolism in which lactic acid is generated, such as fast-twich white skeletal muscle in fish . High levels of histidine-containing dipeptides have been recorded for skipjack tuna white muscle, with anserine largely exceeding carnosine . Aside from strong buffering capacity, carnosine has also been found to exhibit antioxidant, pro-contractile, chelating and anti-glycating properties and it is considered that β-alanine diet supplementation can have protective cardiac effects due to increased levels of carnosine . Other important pathways mediating environmental and physiological adaptation were also identified. HIF-1 (hypoxia inducible factor) signalling pathway was found to be up-regulated in gill + heart and heart + liver combinations. Hif is a transcriptional factor governing the physiological response to hypoxia that induces a wide range of changes in energy metabolism, red blood cell formation, vascularisation, oxygen transport and apoptosis . Regulation of hif-1α has been reported in haemaotopoietic and gas-exchange organs in T. orientalis as a result of cold temperature acclimation . ABC transporter systems were found to be up-regulated in gill + heart and gill + liver combinations (see Additional file 6). The ATP-binding cassette (ABC-transporters) are trans-membrane spanning proteins involved in substrate translocation across membranes and form the basis of multi-xenobiotic resistance mechanism in aquatic animals, with high detoxification relevance. They also participate in transport of lipids, ions and other metabolites and have been attributed various tissue-specific roles . Finally, insulin signalling pathway was found common to all pairwise combinations of gill, heart and liver (see Additional file 6). Exerting its effect through insulin receptors and associated effector signalling cascade actively transcribed in various peripheral organs, insulin has been implicated in wide range of processes in fish, including vital carbohydrate and lipid metabolism, appetite regulation, growth and development .
Sequence data generated from a novel mixed-tissue T. thynnus cDNA library provides an important transcriptomic resource that can be further employed for study of various aspects of T. thynnus ecology and genomics, with strong applications in aquaculture. We have developed and validated a new and flexible gene expression profiling tool, in the form of a 15 K oligonucleotide DNA microarray, which produced biologically relevant information agreeing with prior observations made in the literature, providing external validation for our new resource. The resolved expression profiles of gill, heart, liver and gonads provide a useful starting point for exploring gene expression patterns in T. thynnus and for planning new transcriptomic studies. The oligo-microarray can also be further expanded to include un-annotated transcripts from the generated library with the aim of extending their functional characterisation through correlation with annotated entities. It is important to keep in mind that even tissue specific profiles can be population dependent , warranting further research on captive and wild tuna populations.
Availability of supporting data
The raw sequence data have been submitted to the EBI Sequence Read Archive (SRA) study PRJEB7253 (http://www.ebi.ac.uk/ena). The microarray design and data are available in the EBI ArrayExpress database (www.ebi.ac.uk/arrayexpress) under accession numbers A-MTAB-553 and E-MTAB-3412, respectively.
This study was supported by the Business Innovation Croatian Agency (BICRO) Proof of Concept (POC) grant: MikroTuna - a new diagnostic tool for monitoring disease in tuna farms (PoC_01_07-U-1), Unity Through Knowledge Fund (UKF): Development of a Health Genomic Profile for the captive Atlantic bluefin tuna (Thunnus thynnus) (23/08) and a Fellowship for Doctoral Students to ŽT from the Croatian Science Foundation.
The authors would like to express their gratitude to Leon Grubišić and Rino Stanić for help with sample acquisition and Stephen S. Carmichael for help and valuable advice with sequence data and microarray design.
The authors acknowledge the support of the MASTS pooling initiative (The Marine Alliance for Science and Technology for Scotland) in the completion of this study. MASTS is funded by the Scottish Funding Council (grant reference HR09011) and contributing institutions.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- FishBase. World Wide Web electronic publication. www.fishbase.org. Accessed Aug 2014.
- Volff J-N. Genome evolution and biodiversity in teleost fish. Heredity. 2005;94:280–94.View ArticlePubMedGoogle Scholar
- Brill RW. Selective advantages conferred by the high performance physiology of tunas, billfishes, and dolphin fish. Comp Biochem Physiol Part A Physiol. 1996;113:3–15.View ArticleGoogle Scholar
- Block BA, Stevens ED, editors. Tuna: Physiology, Ecology, and Evolution. San Diego: Academic; 2001.Google Scholar
- Block BA, Finnerty JR, Stewart AF, Kidd J. Evolution of endothermy in fish: mapping physiological traits on a molecular phylogeny. Science. 1993;260:210–4.View ArticlePubMedGoogle Scholar
- Block BA, Finnerty JR. Endothermy in fishes: a phylogenetic analysis of constraints, predispositions, and selection pressures. Environ Biol Fishes. 1994;40:283–302.View ArticleGoogle Scholar
- Rooker JR, Secor DH, De Metrio G, Schloesser R, Block BA, Neilson JD. Natal homing and connectivity in Atlantic bluefin tuna populations. Science. 2008;322:742–4.View ArticlePubMedGoogle Scholar
- Carlsson J, McDowell JR, Carlsson JEL, Graves JE. Genetic identity of YOY bluefin tuna from the eastern and western Atlantic spawning areas. J Hered. 2007;98:23–8.View ArticlePubMedGoogle Scholar
- Boustany AM, Reeb CA, Block BA. Mitochondrial DNA and electronic tracking reveal population structure of Atlantic bluefin tuna (Thunnus thynnus). Mar Biol. 2008;156:13–24.View ArticleGoogle Scholar
- Block BA, Teo SL, Walli A, Boustany A, Stokesbury MJ, Farwell CJ, et al. Electronic tagging and population structure of Atlantic bluefin tuna. Nature. 2005;434:1121–7.View ArticlePubMedGoogle Scholar
- Walli A, Teo SLH, Boustany A, Farwell CJ, Williams T, Dewar H, et al. Seasonal movements, aggregations and diving behavior of Atlantic bluefin tuna (Thunnus thynnus) revealed with archival tags. PLoS One. 2009;4, e6151.PubMed CentralView ArticlePubMedGoogle Scholar
- Fromentin J-M, Powers JE. Atlantic bluefin tuna: population dynamics, ecology, fisheries and management. Fish Fish. 2005;6:281–306.View ArticleGoogle Scholar
- MacKenzie BR, Mosegaard H, Rosenberg AA. Impending collapse of bluefin tuna in the northeast Atlantic and Mediterranean. Conserv Lett. 2009;2:25–34.View ArticleGoogle Scholar
- Taylor NG, McAllister MK, Lawson GL, Carruthers T, Block BA. Atlantic bluefin tuna: a novel multistock spatial model for assessing population biomass. PLoS One. 2011;6, e27693.PubMed CentralView ArticlePubMedGoogle Scholar
- ICCAT. Report of The Standing Committee on Research and Statistics (SCRS). ICCAT: Madrid, Spain; 2014.Google Scholar
- Mylonas CC, De La Gándara F, Corriero A, Ríos AB. Atlantic bluefin tuna (Thunnus Thynnus) farming and fattening in the Mediterranean Sea. Rev Fish Sci. 2010;18:266–80.View ArticleGoogle Scholar
- Rosenfeld H, Mylonas CC, Bridges CR, Heinisch G, Corriero A, Vassallo-Aguis R, et al. GnRHa-mediated stimulation of the reproductive endocrine axis in captive Atlantic bluefin tuna, Thunnus thynnus. Gen Comp Endocrinol. 2012;175:55–64.View ArticlePubMedGoogle Scholar
- Sawada Y, Okada T, Miyashita S, Murata O, Kumai H. Completion of the Pacific bluefin tuna Thunnus orientalis (Temminck et Schlegel) life cycle. Aquac Res. 2005;36:413–21.View ArticleGoogle Scholar
- Taggart JB, Bron JE, Martin SAM, Seear PJ, Høyheim B, Talbot R, et al. A description of the origins, design and performance of the TRAITS-SGP Atlantic salmon Salmo salar L. cDNA microarray. J Fish Biol. 2008;72:2071–94.PubMed CentralView ArticlePubMedGoogle Scholar
- Nielsen J, Pavey S. Perspectives: gene expression in fisheries management. Curr Zool. 2010;56:157–74.Google Scholar
- Ekblom R, Galindo J. Applications of next generation sequencing in molecular ecology of non-model organisms. Heredity. 2011;107:1–15.PubMed CentralView ArticlePubMedGoogle Scholar
- Chini V, Cattaneo AG, Rossi F, Bernardini G, Terova G, Saroglia M, et al. Genes expressed in Blue Fin Tuna (Thunnus thynnus) liver and gonads. Gene. 2008;410:207–13.View ArticlePubMedGoogle Scholar
- Gardner LD, Jayasundara N, Castilho PC, Block B. Microarray gene expression profiles from mature gonad tissues of Atlantic bluefin tuna. Thunnus thynnus in the Gulf of Mexico BMC Genomics. 2012;13:530.PubMedGoogle Scholar
- Jayasundara N, Gardner LD, Block BA. Effects of temperature acclimation on Pacific bluefin tuna (Thunnus orientalis) cardiac transcriptome. Am J Physiol Regul Integr Comp Physiol. 2013;305:R1010–20.View ArticlePubMedGoogle Scholar
- Nakamura Y, Mori K, Saitoh K, Oshima K, Mekuchi M, Sugaya T, et al. Evolutionary changes of multiple visual pigment genes in the complete genome of Pacific bluefin tuna. Proc Natl Acad Sci U S A. 2013;110:11061–6.PubMed CentralView ArticlePubMedGoogle Scholar
- Lepen Pleić I, Secombes CJ, Bird S, Mladineo I. Characterization of three pro-inflammatory cytokines, TNFα1, TNFα2 and IL-1β, in cage-reared Atlantic bluefin tuna Thunnus thynnus. Fish Shellfish Immunol. 2013;36:98–112.View ArticleGoogle Scholar
- Chomczynski P, Mackey K. Short technical reports. Modification of the TRI reagent procedure for isolation of RNA from polysaccharide- and proteoglycan-rich sources. Biotechniques. 1995;19:942–5.PubMedGoogle Scholar
- Picard B, Wegnez M. Isolation of a 7S particle from Xenopus laevis oocytes: a 5S RNA-protein complex. Proc Natl Acad Sci U S A. 1979;76:241–5.PubMed CentralView ArticlePubMedGoogle Scholar
- Van den Eynde H, Mazabraud A, Denis H. Biochemical research on oogenesis. RNA accumulation in the oocytes of the newt Pleurodeles waltl. Development. 1989;106:11–6.PubMedGoogle Scholar
- Mazabraud A, Wegnez M, Denis H. Biochemical research on oogenesis. RNA accumulation in the oocytes of the newt Pleurodeles waltl. Dev Biol. 1975;44:326–32.View ArticlePubMedGoogle Scholar
- Cerio O, Rojo-Bartolomé I, Bizarro C, Ortiz-Zarragoitia M, Cancio I. 5S rRNA and accompanying proteins in gonads: powerful markers to identify sex and reproductive endocrine disruption in fish. Environ Sci Technol. 2012;46:7763–71.View ArticleGoogle Scholar
- Zhulidov PA, Bogdanova EA, Shcheglov AS, Vagner LL, Khaspekov GL, Kozhemyako VB, et al. Simple cDNA normalization using kamchatka crab duplex-specific nuclease. Nucleic Acids Res. 2004;32, e37.PubMed CentralView ArticlePubMedGoogle Scholar
- Schmieder R, Edwards R. Quality control and preprocessing of metagenomic datasets. Bioinformatics. 2011;27:863–4.PubMed CentralView ArticlePubMedGoogle Scholar
- Myers E, Sutton G, Delcher A, Dew I, Fasulo D, Flanigan M, et al. A whole-genome assembly of Drosophila. Science. 2000;287:2196–204.View ArticlePubMedGoogle Scholar
- Lee W-P, Stromberg MP, Ward A, Stewart C, Garrison EP, Marth GT. MOSAIK: a hash-based algorithm for accurate next-generation sequencing short-read mapping. PLoS One. 2014;9, e90581.PubMed CentralView ArticlePubMedGoogle Scholar
- NCBI Thunnus thynnus EST database. http://www.ncbi.nlm.nih.gov/nucest/?term=thunnus. Accessed 6 Oct 2013.
- Benson G. Tandem repeats finder: a program to analyze DNA sequences. Nucleic Acids Res. 1999;27:573–80.PubMed CentralView ArticlePubMedGoogle Scholar
- Rice P, Longden I, Bleasby A. EMBOSS: the European Molecular Biology Open Software Suite. Trends Genet. 2000;16:276–7.View ArticlePubMedGoogle Scholar
- Iseli C, Jongeneel C, Bucher P. ESTScan: a program for detecting, evaluating, and reconstructing potential coding regions in EST sequences. Proc / Int Conf Intell Syst Mol Biol ISMB. 1999;138–148.Google Scholar
- Altschul S, Gish W, Miller W, Myers E, Lipman D. Basic local alignment search tool. J Mol Biol. 1990;215:403–10.View ArticlePubMedGoogle Scholar
- RefSeq: NCBI Reference Sequence Database. http://www.ncbi.nlm.nih.gov/refseq. Accessed 6 Oct 2013.
- Ashburner M, Ball C, Blake J, Botstein D, Butler H, Cherry J, et al. Gene ontology: tool for the unification of biology. The Gene Ontology Consortium Nat Genet. 2000;25:25–9.PubMedGoogle Scholar
- Bekaert M. SlimIt. p. Creative Commons Attribution 3.0 License. http://www.isalmon.eu/slimit/. Accessed 6 Oct 2013.
- Kanehisa M, Goto S. KEGG: Kyoto Encyclopedia of Genes and Genomes. Nucleic Acids Res. 2000;28:27–30.PubMed CentralView ArticlePubMedGoogle Scholar
- Moriya Y, Itoh M, Okuda S, Yoshizawa AC, Kanehisa M. KAAS: an automatic genome annotation and pathway reconstruction server. Nucleic Acids Res. 2007;35(Web Server issue):W182–5.PubMed CentralView ArticlePubMedGoogle Scholar
- Krzywinski M, Birol I, Jones SJ, Marra MA. Hive plots--rational approach to visualizing networks. Brief Bioinform. 2012;13:627–44.View ArticlePubMedGoogle Scholar
- Theocharidis A, van Dongen S, Enright AJ, Freeman TC. Network visualization and analysis of gene expression data using BioLayout Express 3D. Nat Protoc. 2009;4:1535–50.View ArticlePubMedGoogle Scholar
- Luo W, Friedman MS, Shedden K, Hankenson KD, Woolf PJ. GAGE: generally applicable gene set enrichment for pathway analysis. BMC Bioinformatics. 2009;10:161.PubMed CentralView ArticlePubMedGoogle Scholar
- Gentleman RC, Carey VJ, Bates DM, Bolstad B, Dettling M, Dudoit S, et al. Bioconductor: open software development for computational biology and bioinformatics. Genome Biol. 2004;5:R80.PubMed CentralView ArticlePubMedGoogle Scholar
- Morais S, Mourente G, Ortega A, Tocher JA, Tocher DR. Expression of fatty acyl desaturase and elongase genes, and evolution of DHA:EPA ratio during development of unfed larvae of Atlantic bluefin tuna (Thunnus thynnus L.). Aquaculture. 2011;313:129–39.View ArticleGoogle Scholar
- Untergasser A, Cutcutache I, Koressaar T, Ye J, Faircloth BC, Remm M, et al. Primer3--new capabilities and interfaces. Nucleic Acids Res. 2012;40, e115.PubMed CentralView ArticlePubMedGoogle Scholar
- Pfaffl MW. Quantification Strategies in Real-Time PCR. In A-Z of Quantitative PCR. Edited by Bustin SA. La Jolla, CA, USA: International University Line; 2004:87–112.Google Scholar
- Pfaffl MW, Tichopad A, Prgomet C, Neuvians TP. Determination of stable housekeeping genes, differentially regulated target genes and sample integrity: BestKeeper -Excel-based tool using pair-wise correlations. Biotechnol Lett. 2004;26:509–15.View ArticlePubMedGoogle Scholar
- Miron M, Woody OZ, Marcil A, Murie C, Sladek R, Nadon R. A methodology for global validation of microarray experiments. BMC Bioinformatics. 2006;7:333.PubMed CentralView ArticlePubMedGoogle Scholar
- Gilles A, Meglécz E, Pech N, Ferreira S, Malausa T, Martin J-F. Accuracy and quality assessment of 454 GS-FLX Titanium pyrosequencing. BMC Genomics. 2011;12:245.PubMed CentralView ArticlePubMedGoogle Scholar
- Chow S, Nakagawa T, Suzuki N, Takeyama H, Matsunaga T. Phylogenetic relationships among Thunnus species inferred from rDNA ITS1 sequence. J Fish Biol. 2006;68:24–35.View ArticleGoogle Scholar
- Su AI, Wiltshire T, Batalov S, Lapp H, Ching KA, Block D, et al. A gene atlas of the mouse and human protein-encoding transcriptomes. Proc Natl Acad Sci U S A. 2004;101:6062–7.PubMed CentralView ArticlePubMedGoogle Scholar
- Morey JS, Ryan JC, Van Dolah FM. Microarray validation: factors influencing correlation between oligonucleotide microarrays and real-time PCR. Biol Proced Online. 2006;8:175–93.PubMed CentralView ArticlePubMedGoogle Scholar
- Evans DH, Piermarini PM, Choe KP. The multifunctional fish gill: dominant site of gas exchange, osmoregulation, acid–base regulation, and excretion of nitrogenous waste. Physiol Rev. 2005;85:97–177.View ArticlePubMedGoogle Scholar
- Uribe C, Folch H, Enriquez R, Moran G. Innate and adaptive immunity in teleost fish: a review. Vet Med. 2011;56:486–503.Google Scholar
- Brill RW, Bushnell PG. The cardiovascular system of tunas. In: Block BA, Stevens ED, editors. Tuna: Physiology, Ecology, and Evolution, vol. 19. San Diego: Academic; 2001. p. 79–120.View ArticleGoogle Scholar
- Bushnell PG, Brill RW. Oxygen transport and cardiovascular responses in skipjack tuna (Katsuwonus pelamis) and yellowfin tuna (Thunnus albacares) exposed to acute hypoxia. J Comp Physiol B. 1992;162:131–43.View ArticlePubMedGoogle Scholar
- Cerdà J, Finn RN. Piscine aquaporins: an overview of recent advances. J Exp Zool. 2010;313A:623–50.View ArticleGoogle Scholar
- Babin PJ, Cerdà J, Lubzens E, editors. The Fish Oocyte From Basic Studies to Biotechnological Applications. Dordrecht, The Netherlands: Springer; 2007.Google Scholar
- Abascal FJ, Medina A. Ultrastructure of oogenesis in the bluefin tuna, Thunnus thynnus. J Morphol. 2005;264:149–60.View ArticlePubMedGoogle Scholar
- Allende ML, Amsterdam A, Becker T, Kawakami K, Gaiano N, Hopkins N. Insertional mutagenesis in zebrafish identifies two novel genes, pescadillo and dead eye, essential for embryonic development. Genes Dev. 1996;10:3141–55.View ArticlePubMedGoogle Scholar
- Kinoshita Y, Jarell AD, Flaman JM, Foltz G, Schuster J, Sopher BL, et al. Pescadillo, a novel cell cycle regulatory protein abnormally expressed in malignant cells. J Biol Chem. 2001;276:6656–65.View ArticlePubMedGoogle Scholar
- Oeffinger M, Leung A, Lamond A, Tollervey D. Yeast Pescadillo is required for multiple activities during 60S ribosomal subunit synthesis. RNA. 2002;8:626–36.PubMed CentralView ArticlePubMedGoogle Scholar
- Allmang C, Kufel J, Chanfreau G, Mitchell P, Petfalski E, Tollervey D. Functions of the exosome in rRNA, snoRNA and snRNA synthesis. EMBO J. 1999;18:5399–410.PubMed CentralView ArticlePubMedGoogle Scholar
- Corriero A, Desantis S, Deflorio M, Acone F, Bridges CR, De la Serna JM, et al. Histological investigation on the ovarian cycle of the bluefin tuna in the western and central Mediterranean. J Fish Biol. 2003;63:108–19.View ArticleGoogle Scholar
- Fabra M, Raldúa D, Bozzo MG, Deen PMT, Lubzens E, Cerdà J. Yolk proteolysis and aquaporin-1o play essential roles to regulate fish oocyte hydration during meiosis resumption. Dev Biol. 2006;295:250–62.View ArticlePubMedGoogle Scholar
- Carnevali O, Carletta R, Cambi A, Vita A, Bromage N. Yolk formation and degradation during oocyte maturation in seabream Sparus aurata: involvement of two lysosomal proteinases. Biol Reprod. 1999;60:140–6.View ArticlePubMedGoogle Scholar
- Kwon JY, Park JM, Gim BS, Han SJ, Lee J, Kim YJ. Caenorhabditis elegans mediator complexes are required for developmental-specific transcriptional activation. Proc Natl Acad Sci U S A. 1999;96:14990–5.PubMed CentralView ArticlePubMedGoogle Scholar
- Titus TA, Yan Y-L, Wilson C, Starks AM, Frohnmayer JD, Canestro C, et al. The Fanconi anemia/BRCA gene network in zebrafish: Embryonic expression and comparative genomics. Mutat Res. 2009;668:117–32.PubMed CentralView ArticlePubMedGoogle Scholar
- Zhou Y, Wang F, Liu S, Zhong H, Liu Z, Tao M, et al. Human chorionic gonadotropin suppresses expression of Piwis in common carp (Cyprinus carpio) ovaries. Gen Comp Endocrinol. 2012;176:126–31.View ArticlePubMedGoogle Scholar
- Juneja R, Agulnik SI, Silver LM. Sequence divergence within the sperm-specific polypeptide TCTE1 is correlated with species-specific differences in sperm binding to zona-intact eggs. J Androl. 1998;19:183–8.PubMedGoogle Scholar
- Rolland AD, Lareyre J-J, Goupil A-S, Montfort J, Ricordel M-J, Esquerré D, et al. Expression profiling of rainbow trout testis development identifies evolutionary conserved genes involved in spermatogenesis. BMC Genomics. 2009;10:546.PubMed CentralView ArticlePubMedGoogle Scholar
- Kaneko T, Hirano T. Role of prolactin and somatolactin in calcium regulation in fish. J Exp Biol. 1993;184:31–45.Google Scholar
- Pérez-Sánchez J. The involvement of growth hormone in growth regulation, energy homeostasis and immune function in the gilthead sea bream (Sparus aurata): a short review. Fish Physiol Biochem. 2000;22:135–44.View ArticleGoogle Scholar
- Harvey S, Baudet M-L, Murphy A, Luna M, Hull KL, Aramburo C. Testicular growth hormone (GH): GH expression in spermatogonia and primary spermatocytes. Gen Comp Endocrinol. 2004;139:158–67.View ArticlePubMedGoogle Scholar
- Miura C, Shimizu Y, Uehara M, Ozaki Y, Young G, Miura T. Gh is produced by the testis of Japanese eel and stimulates proliferation of spermatogonia. Reproduction. 2011;142:869–77.View ArticlePubMedGoogle Scholar
- Abascal F, Megina C, Medina A. Testicular development in migrant and spawning bluefin tuna (Thunnus thynnus (L.)) from the eastern Atlantic and Mediterranean. Fish Bull. 2004;102:407–17.Google Scholar
- Nagasawa K, Takeuchi Y, Miwa M, Higuchi K, Morita T, Mitsuboshi T, et al. cDNA cloning and expression analysis of a vasa-like gene in Pacific bluefin tuna Thunnus orientalis. Fish Sci. 2009;75:71–9.View ArticleGoogle Scholar
- Yang BY, Arab M, Chen TT. Cloning and characterization of rainbow trout (Oncorhynchus mykiss) somatolactin cDNA and its expression in pituitary and nonpituitary tissues. Gen Comp Endocrinol. 1997;106:271–80.View ArticlePubMedGoogle Scholar
- Lynn SG, Shepherd BS. Molecular characterization and sex-specific tissue expression of prolactin, somatolactin and insulin-like growth factor-I in yellow perch (Perca flavescens). Comp Biochem Physiol Part B Biochem Mol Biol. 2007;147:412–27.View ArticleGoogle Scholar
- Mourente G, Megina C, Díaz-Salvago E. Lipids in female northern bluefin tuna (Thunnus thynnus thynnus L.) during sexual maturation. Fish Physiol Biochem. 2002;24:351–63.View ArticleGoogle Scholar
- Wolf JC, Wolfe MJ. A brief overview of nonneoplastic hepatic toxicity in fish. Toxicol Pathol. 2005;33:75–85.View ArticlePubMedGoogle Scholar
- Andersson T, Förlin L. Regulation of the cytochrome P450 enzyme system in fish. Aquat Toxicol. 1992;24:1–20.View ArticleGoogle Scholar
- Segers K, Dahlbäck B, Nicolaes GAF. Coagulation factor V and thrombophilia: Background and mechanisms. Thromb Haemost. 2007;98:530–42.PubMedGoogle Scholar
- Boshra H, Li J, Sunyer JO. Recent advances on the complement system of teleost fish. Fish Shellfish Immunol. 2006;20:239–62.View ArticlePubMedGoogle Scholar
- Moyes CD. Cardiac metabolism in high performance fish. Comp Biochem Physiol Part A Physiol. 1996;113:69–75.View ArticleGoogle Scholar
- Moyes C, Mathieu-Costello OA, Brill RW, Hochachka PW. Mitochondrial metabolism of cardiac and skeletal muscles from a fast (Katsuwonus pelamis) and a slow (Cyprinus carpio) fish. Can J Zool. 1992;70:1246–53.View ArticleGoogle Scholar
- Shiels H, Di Maio A, Thompson S, Block B. Warm fish with cold hearts: thermal plasticity of excitation–contraction coupling in bluefin tuna. Proc R Soc B Biol Sci. 2011;278:18–27.View ArticleGoogle Scholar
- Landeira-Fernandez AM, Castilho PC, Block BA. Thermal dependence of cardiac SR Ca2+-ATPase from fish and mammals. J Therm Biol. 2012;37:217–23.View ArticleGoogle Scholar
- Abe H. Role of histidine-related compounds as intracellular proton buffering constituents in vertebrate muscle. Biochem. 2000;65:757–65.Google Scholar
- McCarty MF, DiNicolantonio JJ. β-Alanine and orotate as supplements for cardiac protection. Open Hear. 2014;1, e000119.View ArticleGoogle Scholar
- Abe H, Brill R, Hochachka P. Metabolism of L-histidine, carnosine, and anserine in skipjack tuna. Physiol Zool. 1986;59:439–50.Google Scholar
- Nikinmaa M, Rees BB. Oxygen-dependent gene expression in fishes. Am J Physiol Regul Integr Comp Physiol. 2005;288:R1079–90.View ArticlePubMedGoogle Scholar
- Mladineo I, Block BA. Expression of Hsp70, Na+/K+ ATP-ase, HIF-1α, IL-1β and TNF-α in captive Pacific bluefin tuna (Thunnus orientalis) after chronic warm and cold exposure. J Exp Mar Bio Ecol. 2009;374:51–7.View ArticleGoogle Scholar
- Luckenbach T, Fischer S, Sturm A. Current advances on ABC drug transporters in fish. Comp Biochem Physiol Part C Toxicol Pharmacol. 2014;165:28–52.View ArticleGoogle Scholar
- Caruso MA, Sheridan MA. New insights into the signaling system and function of insulin in fish. Gen Comp Endocrinol. 2011;173:227–47.View ArticlePubMedGoogle Scholar
- Whitehead A, Crawford DL. Variation in tissue-specific gene expression among natural populations. Genome Biol. 2005;6:R13.PubMed CentralView ArticlePubMedGoogle Scholar