Skip to main content

Current basis and future directions of zebrafish nutrigenomics


This review investigates the current state of nutrigenomics in the zebrafish animal models. The zebrafish animal model has been used extensively in the study of disease onset and progression and associated molecular changes. In this review, we provide a synopsis of nutrigenomics using the zebrafish animal model. Obesity and dyslipidemia studies describe the genomics of dietary-induced obesity in relation to high-fat/high-calorie diets. Inflammation and cardiovascular studies describe dietary effects on the expression of acute inflammatory markers and resulting chronic inflammatory issues including atherosclerosis. We also evaluated the genomic response to bioactive dietary compounds associated with metabolic disorders. Carbohydrate metabolism and β-cell function studies describe the impacts of high-carbohydrate dietary challenges on nutritional programming. We also report tumorigenesis in relation to dietary carcinogen exposure studies that can result in permanent genomic changes. Vitamin and mineral deficiency studies demonstrate transgenerational genomic impacts of micronutrients in the diet and temporal expression changes. Circadian rhythm studies describe the relation between metabolism and natural temporal cycles of gene expression that impacts health. Bone formation studies describe the role of dietary composition that influences bone reabsorption regulation. Finally, this review provides future directions in the use of the zebrafish model for nutrigenomic and nutrigenetic research.


Nutrigenomics and nutrigenetics

The intake of specific food items and specific nutrients, or their absence from the diet, has long been related to the manifestation of disease states in humans and animals [1]. As we have gained an understanding of the roles of more specific nutrients and nutrient levels needed to maintain normal life function and prevent deficiency- or toxicity-related diseases, we now understand important nutrient-gene interactions (nutrigenomics) and how variation in individual genetics affects nutrient requirements and tolerances, requiring personalized diet recommendations (nutrigenetics).

Nutrigenomics can be defined as two alternate mechanisms of nutrient-gene interactions [2]. First, dietary components can act to alter gene expression or act as cofactors within metabolic systems. The impacts of these interactions of dietary components and genes are temporary and rely on the presence of the dietary component with effects modulated by the availability and storage of these components. These effects are more readily observed in poorly stored nutrients such as water-soluble vitamins. Second, there are longer-lasting impacts on a gene by diet interactions such as dietary components that alter mutation rates and result in essentially permanent genome alterations, or components that alter genome methylation patterns resulting in heritable alterations of the genome [3,4,5]. The ability to make personalized dietary recommendations based on a person’s individual genome could be considered an “ultimate goal” in the clinical application of nutrigenomic research, similar to the goal of personalized medicine [6]. To better understand these complex networks of nutrient and gene interactions, researchers can use modern “omics” technologies as well as novel high-throughput translational models. One increasingly more commonly utilized model for this type of experimentation is the zebrafish.

Danio rerio

The zebrafish species Danio rerio has become the third most utilized NIH animal model behind mice and rats [7]. There are important reasons for its utilization, both logistical and translational. Aside from a fast development time and easy and cost-efficient husbandry, the fully sequenced and annotated genome shows high similarity to humans, even accounting for a historical whole-genome duplication event in teleosts [8]. An abundance of molecular techniques has been developed for the model including CRISPR, GFP models, and Cre-Lox models [9,10,11]. Perhaps most important to nutrigenomics research is the similarity in how zebrafish metabolize and deposit dietary fat [12]. A high-fat diet was found to affect adipose gene expression (as measured by microarray) more similarly between humans and zebrafish than between humans and mice or rats [12]. This indicated a potential for better translational research into metabolic syndrome using this model, to be discussed later in detail below.

Nutrition-related studies

Obesity and dyslipidemia

Obesity has been a growing concern in the western world, and now worldwide. The age-standardized prevalence of obesity was 39.6% between 2015 and 2016 [13]. Obesity is often associated with several comorbidities including cardiovascular disease, diabetes, hypertension, and dyslipidemia [14]. Individuals with an obese phenotype display dysregulation of multiple genes [15]. These genes have been reported to be involved with metabolic processes and inflammatory responses.

Animals that over ingest calories (usually via a high-carb or high-fat diet) leading to stored adipose are considered models of dietary-induced obesity (DIO) and can be utilized to better understand physiological or molecular events that occur as a result of obese phenotypes [16]. The first seminal research for zebrafish DIO was reported by Oka et al. [12]. This study investigated DIO by over- or underfeeding Artemia (a live diet commonly used in zebrafish culture), or by caloric restriction following overfeeding. Overfeeding zebrafish (feeding ad libitum) resulted in an increase of fish BMI (measured as g weight/cm2 length by the investigators), plasma triglycerides, and hepatic steatosis in both males and females. Along with these metrics of growth and metabolic health, 168 genes were dysregulated. Following caloric restriction, fish weight and plasma triglycerides decreased significantly and 97 genes that had been dysregulated were normalized. Genes that were affected by overfeeding were in ontologies of blood coagulation, triglyceride metabolism, platelet activation, fatty acid metabolism, and cholesterol efflux. Comparisons of genes with expressions changed by DIO in zebrafish, rats, mice, and humans show a strong similarity in metabolic pathways involved among these species.

Landgraf et al. examined the effects of increased dietary calories leading to an obese phenotype by overfeeding either a high-fat diet (HFD-OF) or a normal fat diet (NFD-OF) [17]. This was evaluated only in adult male zebrafish and following 8 weeks both treatments gained weight and had increased percent body fat compared to a non-overfed control group (NFD). The HDF-OF, however, added on less body weight and no difference in body fat percentage compared to NFD-OF. HDF-OF showed differences in markers of metabolic health, namely increased fasting blood glucose, plasma triglycerides, and cholesterol compared to NFD-OF or NFD. Following from changes in blood glucose, there was an increased ratio of Thr 307 (human Thr 308 ortholog site) pAKT/AKT by western blot in the liver suggesting early insulin resistance [18]. Expression of pparg and lpl, lipid metabolism genes in the adipose, and srebf1, which regulates cholesterol biosynthesis in the liver, was reduced in the HFD-OF compared to the NFD-OF. Expression of fabp11a, lipid metabolism gene, and col1a1a, a collagen gene contributing to fibrosis [19] in the liver, was increased in HDF-OF compared to NFD-OF. This study demonstrates the effectiveness of the zebrafish model for investigating different metabolic and body composition phenotypes induced by different diets. Current evidence strongly supports ppar isoforms present having similarity in regulating mechanism for lipid metabolism as well as high structural similarity (67–74% identity) among humans, mice, and zebrafish [20]. High dietary linolenic acid increased expression of fabp2 in the intestine and fabp3 in the liver [21]. These genes are predicted to be regulated via ppar isomers.

As an alternative to evaluating zebrafish with a DIO phenotype, fasting experiments can be used to determine how energy and nutrients are allocated and absorbed. Fasting in humans has shown to have health benefits in obese individuals with either caloric restriction or intermittent fasting [22]. In addition to proven clinical benefits, studies of human fasting have provided a better understanding of genes that regulate energy intake and allocation. The same may be true for use of the zebrafish model. Zebrafish fasted for 3 weeks had reductions in weight, blood glucose, and liver glycogen, cholesterol, triglycerides, and phospholipids [23]. Fasted zebrafish also showed changes in the gene expression of srebp1+2, mtor, ampk, and crebp3l3, all known regulators of cellular energy and growth. Activity of proteins related to protein and sugar metabolism was also affected. Most effects were significantly ameliorated following a refeeding period, while some only trended towards the initial prefasting state. Similar zebrafish studies have evaluated dietary restriction (DR). DR, with either restricted calories, macronutrients, or feed-timing restriction, is one of the only known potent cross-species intervention that extends the life span [24, 25]. Arslan-Ergul et al. provided a control or calorie-restricted diet to either young (8–8.5 months) or old (26–32.5 months) zebrafish [26]. The calorie-restricted diet decreased body weight for both age groups and shortened telomere length of young zebrafish in the spleen and brain.

Inflammation and cardiovascular disease

Normal acute inflammation responses are localized, typically in response to tissue damage or infection [27]. Capillary dilation, heat, redness, cytokine and/or chemokine release, swelling, and leukocyte infiltration are all characteristics of this response. In contrast, chronic low-grade systemic inflammation is debilitating independently but can be caused by poor metabolic health [28].

The effects of diet in inflammatory response are one of debate within the nutrition community, and especially in the role of dietary lipids [29]. The lipid composition of the diet affects markers of inflammation in zebrafish. Fish provided an isocaloric diet of differing n3:n6 ratio (1:2, 1:5, or 1:8) had decreased expression of vitellogenin (males only), c-reactive protein, and serum amyloid A as the ratio of n3:n6 in the diet increased [30]. Zebrafish provided the highest n3:n6 ratio also had the highest body weight in females, but the lowest adiposity in both males and females. Diets formulated with a low n3:n6 ratio and high levels of w6 arachidonic acid (ARA) resulted in increased oxidative stress and lipid peroxidation [31]. The metabolomic analysis showed a lower whole body n3:n6 fatty acid ratio in relation to higher levels of eicosanoids. Though ARA-derived eicosanoids are considered proinflammatory, no markers of inflammatory response were reported in these fish.

Dietary-induced obesity in zebrafish has been shown to impact inflammatory pathways. Comparative transcriptomics of visceral white adipose in zebrafish and mammals (rats, mice, and humans) show that genes responsible for blood coagulation and platelet activation are dysregulated in obesity [12]. Regulators of these genes include il-6, il-1β, and apoh, which act as proinflammatory cytokines leading to chronic inflammation. These cytokines also play a role in the initiation and promotion of certain types of cancers. Forn-Cuní et al. [32] reported the impact of dietary-induced obesity on the liver transcriptome following an injection of an inflammatory stimulus (lipopolysaccharide). Comparisons between non-obese zebrafish receiving inflammatory stimuli and non-obese controls showed increased expression of pamp, tlr5b, proinflammatory cytokines il-1β and il-8, and chemokines cxcl-c1c and cxcl-11 l. Injection of inflammatory stimuli in obese zebrafish showed none of the changes compared to obese controls. These data suggest an inability in obese fish to support an appropriate inflammatory response when a stimulus for such a response is present. One of the genes displaying increased expression in obese zebrafish compared to non-obese controls was tac4. This gene is still categorized as unknown function in zebrafish, but a paralog of this gene has a role in chronic inflammation [33]. Karanth et al. studied the impact of isocaloric and isonitrogenous diets of either 4% or 12% lipid diets on atherosclerotic cardiovascular disease [34]. The 12% lipid diet resulted in higher body weight and body length in male, but not female zebrafish. The activity of the enzyme HMGCR was reduced in both males and females fed the 12% lipid diet. HMGCR is involved in LDL clearance and is a potent target for pharmacological inhibitory intervention to reduce cardiovascular-related mortality [35].

In aquaculture, fish meal is a common ingredient which serves as a protein source; however, attempts to replace this source with a more cost-effective, available, and purported eco-friendly protein source, such as soy, are being considered [36]. Inclusion of dietary soy has stimulated research into the growth and health effects of fish protein replacement by soy sources, especially inflammatory responses due to the immunogenic effects of soy components. Hedrera et al. created diets using different protein sources of either fish meal, fish and soybean meal, fish meal and soy protein isolate, or fish meal and soy saponins [37]. Diets containing soybean meal or saponins resulted in increased neutrophil infiltration into the intestines and increased expression of the inflammatory cytokine il-8. All diets containing soy components increased il-1β expression as well. Fuentes et al. also formulated diets of fish meal, fish meal with low and high content soy protein isolate, or fish meal with low and high content of soy saponins [38]. These diets showed that there are dose thresholds for inflammatory impacts of soy diet components. The diets with high inclusion of soy diet components resulted in increased granulocyte number in regions of the digestive tract and increased proinflammatory cytokines and peroxidases. Both studies use larval stage (5–10 dpf) zebrafish, but these effects of soy dietary components are shown to persist in later life. Early exposure to these dietary components modulates exposure in adulthood in a type of nutrient programming in which the zebrafish model can be used to investigate further [39]. Ulloa et al. investigated the impacts of plant (a mix of soy protein, wheat gluten, and corn gluten) and fish protein diets on zebrafish growth and expression genes related to muscle growth [40]. Muscle expression of igf2a was decreased and myogenin and mrf4 increased in males provided the plant protein diets, while female expression was not changed. Differences in growth-related genes were also found among isolated zebrafish families in response to plant and fish protein diets.

Cholesterol content is high in western diets and contributes to increased circulating cholesterol and risk of atherosclerosis and coronary heart disease [41, 42]. In Yoon et al., zebrafish provided a high-cholesterol diet that showed inflammatory responses and increased il-1β expression, but only in reproductive adults [43]. Reproductive adults in a study by Progatzky et al. [44] fed a high-cholesterol diet did show an inflammatory response, but no significant change in il-1β expression. This raises questions as to the pathways required for an inflammatory response to be produced and if dietary cholesterol impacts inflammation directly or via a non-canonical, inflammatory-regulating pathway in zebrafish. We should point out that there were differences in the feeding regime used in these studies. Cholesterol can contribute along with other dietary compounds to an inflammatory response. Aspartame provided in the zebrafish diet resulted independently in inflammation in the liver and brain, determined by oil-red O and hematoxylin staining [45]. When provided a diet that contained high cholesterol and aspartame, a synergistic increase in inflammatory responses was observed in these tissues. A high-cholesterol diet altered the lipid profile of zebrafish 5 to 14 days post-fertilization with a 70-fold increase in oxidized cholesterol esters [46]. A homogenate prepared from these zebrafish increased murine macrophage cell surface area and resulted in increased phosphorylation of ERK1+2, AKT, and JNK. Stoletov et al. [47] studied high-cholesterol diets to understand inflammation and arterial lipid accumulation. A high-cholesterol diet resulted in increased circulating cholesterol, altered lipoprotein profile, and increased macrophage activity in transplanted murine myeloid cells. High cholesterol also increased PLA2 activity, which is associated with increased CVD risk in humans by an unknown mechanism [48]. A high-cholesterol diet increased circulating cholesterol, triglycerides, and glucose and raised cholesterol-ester transfer protein (CETP) activity compared to a control diet [49]. Inclusion of a high-cholesterol diet with dried acai, a potent anti-oxidant berry of the acai palm, decreased circulating cholesterol and glucose compared to the high-cholesterol diet alone and fully returned CETP activity to the lower activity level of the control diet. Higher CETP activity is related to cardiovascular disease in some populations [50]. Pharmacological treatments to inhibit CETP activity in clinical trials have had many negative results or are ongoing [51]. Two cholesterol maintenance drugs commonly prescribed, ezetimibe and simvastatin, ameliorate the high circulating levels of cholesterol that occurs in zebrafish when they are fed a high-cholesterol diet [52], further supporting the use of zebrafish in translational research.

Bioactive dietary compounds

Zebrafish have recently been used to explore dietary bioactive compounds that impact disease onset and progression. Anserine and creatine, reported as anti-obesity therapeutics from mice studies [53, 54], were proffered to overfed zebrafish DIO models to explore hepatic gene expression leading to lipid metabolism alterations in obese phenotypes with related comorbidities [55]. These bioactive food compounds ameliorated the impact of an obesogenic diet on symptoms of metabolic disorders such as high blood glucose, dyslipidemia, and hepatic steatosis and normalized expression changes of genes related to lipid metabolism. When zebrafish were provided an obesogenic diet of increased calories and containing green tea extract (GTE), protective effects were observed [56]. In both males and females, visceral and total body fat increased when fish were provided an obesogenic diet, but the inclusion of GTE reduced visceral and total body fat increases. Males and females both increased total body weight on the obesogenic diet, but only females decreased in total body weight compared to DIO fish when GTE was included in the diet. The highest dietary inclusion of GTE in females increased liver expression of the lipid catabolism gene acox1, acadm, and ppara and decreased socs3 adipose expression, which affects leptin levels. Another study on the effects of GTE showed females provided a high-fat diet supplemented with GTE had increased citrate synthase and 3-hydroxyacyl-coenzyme A dehydrogenase activity compared to females fed a high-fat diet without GTE supplementation [57]. Zebrafish provided an obesogenic diet with the inclusion of Campari tomatoes (high in lycopene and beta-carotene) showed reduced weight gain and reduced triglycerides [58]. Expression of a number of genes relating to lipid metabolism, carbohydrate transport, and cell cycling, among others, was altered in the liver. Peels of the Japanese citrus fruit Yuzu (Citrus junos), which contains several bioactive compounds, also impacted DIO fish by reducing triglycerides and hepatic steatosis [59]. In the liver pparab and its targets acox1 and acadm were upregulated, and in adipose pparg, acox1, and adipoqb, which regulate adipose differentiation, were also upregulated in fish provided an obesogenic diet with Yuzu fruit peel supplementation compared to fish given a non-supplemented obesogenic diet. Caffeine has been shown to ameliorate the hepatic effects of overfeeding and decreases weight, circulating triglycerides, and steatosis [60]. Caffeine also regulated expression of lipogenesis genes aco, srebp1, acc1, cd36, and ucp2; endoplasmic reticulum stress genes perk, ire1, atf6, and bip; inflammatory cytokines genes il-1β and tnfa; and autophagy genes atg12 and beclin-1.

Carbohydrate metabolism and β-cell function

Fang et al. evaluated impacts of a high-carbohydrate (60% maltodextrin), low-protein dietary challenge in early life time-periods (larval stages between 3 and 10 days post hatch), and nutritional programming effects at 16 weeks with a high-carbohydrate low-protein dietary challenge (35% maltodextrin) [61]. In early life dietary challenges, expression of carbohydrate metabolism-related genes including gk, pk, g6pase, amy, pepck, and sglt-1 was differentially regulated in an age- and dietary-dependent manner. The dietary challenges at 16 weeks suggest metabolic programming by the initial high carbohydrate exposure. Both gene expression of all prior evaluated genes (except for g6pase) and activities of their respective enzymes were dependent upon initial exposure to differing dietary challenge. Rocha et al. [62] examined the consequences of early high carbohydrate exposure modulates later response by injecting zebrafish embryo yolks at 1-dpf with glucose or a saline vehicle and at 24-dpf they were provided a high-carbohydrate diet. Zebrafish that had received the 1-dpf glucose injection had decreased pkl and increased hk1 expression in viscera and increased 6pfk expression in muscle, all of which are related to alterations in gluconeogenesis. Seiliez et al. also looked at diets with differing protein and carbohydrate ratio by refeeding with either a high-protein, low-carbohydrate diet (HPLC) or a low-protein, high-carbohydrate diet (LPHC) following a 72-h starvation period [63]. Refeeding with LPHC increased hepatic gk and pk expression compared to HPLC refeeding and decreased expression of muscle acca, which functions in lipid metabolism.

In zebrafish, carbohydrate metabolism can be affected by the route of exposure. Different methods of studying the impact of carbohydrate metabolism changes exist. Exposure can be accomplished by diet, glucose injection, or a transdermal exposure to a high glucose environment, all of which can result in hyperglycemia [64,65,66]. Though non-dietary studies are less directly relevant to nutrigenomics, changes in gene regulation are important and some can be discussed due to the relevant regulatory changes and nutritional programming in metabolic disorders and due to the lack of a current dietary model for insulin resistance in zebrafish. Blood glucose has been shown to increase with exposure to a high-glucose environment [67]. Following removal from a high-glucose environment, blood glucose was maintained high during a 7-day wash-out period in clean system water. Treatment with the drugs glimepiride and metformin, popular clinical treatments for type 2 diabetes, reduced blood glucose back to normal levels. Along with increasing blood glucose, transdermal glucose exposure increased insra-1, insrb-1, and insrb-2 expression in the skeletal muscle. Another study showed the drug glipizide also proved effective at reducing elevated blood glucose caused by transdermal exposure [68]. Larval exposure to transdermal glucose reduced the expression of pepck and increased expression of insa. Injection of the diabetogenic drug streptozocin reduces insulin secretion and blood glucose levels, mimicking type-1 diabetes with zebrafish recovering from these effects within 14 days of injections ending [69]. Though recovery from environmental glucose exposure occurs, differences in genome-wide CpG island methylation changes and expressions persist. Caudal fin amputation following environmental glucose exposure shows that regeneration of the tissue is compromised, and new tissue has similar changes in expression and methylation patterning considered to be metabolic memory.

The function of β-cells of the pancreas is very important for carbohydrate metabolism and these cells respond to dietary challenges in zebrafish. Maddison et al. provided media with high amounts of either glucose or lipid (from locally sourced egg yolks) to larval stage fish either intermittently or persistently [70]. Either diet provided persistently increased the number of β-cells by initiating differentiation of precursor cells. The high glucose and high lipid exposure acted via different mechanisms to initiate differentiation, with the mTOR pathway being required for the response to the glucose-rich diet and the IGF-1 signaling being required for the response to the lipid-rich diet. Ninov et al. [71]. found similar results for excess nutrient availability for larval zebrafish by providing diets containing higher carbohydrate and lipid content which resulted in increased β-cell proliferation and in differentiation of progenitor cells in the pancreatic duct. The mechanism for these nutrient-driven changes was shown to be mTOR dependent. This persistent overnutrition effect on β-cell number is also supported by Michel et al. who utilized a high lipid exposure protocol [72].

Another study looking at steatosis formation used 5–7 dpf larval zebrafish exposed to either 4% glucose or 4% fructose treatments [73]. The fructose treatment resulted in increased steatosis and micrograph examination showed dilated endoplasmic reticulum, a sign of ER stress, and a “less distinct” mitochondrial membrane. The fructose treatment also increased expression genes related to lipogenesis (cidec, lipin1, lipin2, and srebpf1), inflammation (tnfa, irf2a, and nfkb), oxidative stress (gpx and trxr2), and ER stress (ddit3). Treatment with rapamycin to inhibit mTOR ameliorated the hepatic steatosis and all the genetic expression changes except for irf2a and nfkb.

Tumorigenesis and dietary carcinogen exposure

Methyl mercury is an environmental contaminant that can enter the body by multiple pathways including dietary contamination. Exposure to methyl mercury-tainted feed for 25 days resulted in differential gene expression patterns in zebrafish skeletal muscle [74]. Expression was altered in genes affecting general cell metabolism, lipid metabolism, cell cycle regulation, and ribosomal components involved in protein synthesis. The multiple ribosomal genes evaluated in this study had expression changes correlated to colorectal carcinoma, adenocarcinomas, and DNA integrity, though not in the skeletal muscle [75,76,77,78].

Polycyclic aromatic hydrocarbons (PAHs) are another class of environmental contaminants that can enter the body via dietary exposure. A diet contaminated by PAHs decreased survival and increased formation of global neoplasms with bile duct epithelial being the most susceptible [79]. Expression of the gene cyp1a, which is related to both circadian rhythm and detoxification, increased following ingestion of the PAH contaminated diets [80]. Expression of ahr2, which codes for a receptor that binds aromatic compounds, was unaffected by the PAH-contaminated diets except at the highest concentration where repression was observed [81]. Zebrafish consuming feed contaminated with TCDD (dioxin) resulted in dose- and time-dependent bioaccumulation and formation of lesions in multiple organs [82]. Microarray produced expression changes related to several genetic ontologies and pathways including cardiac fibrosis, lipid transport, metabolic processes, DNA replication, as well as cardiac, renal, and liver necrosis among others. A diet containing the 2,4-dimethoxybenzaldehyde (DMBA) resulted in a dose-dependent increase in weight, neoplasm formation, and mortality [83]. A diet contaminated with the carcinogen methylnitronitrosoguanidine showed no impact on zebrafish weight, survival, or neoplasm formation [84]. This was different from the profound effects of transdermal exposure or injection that formed neoplasms at a low dosage.

Vitamin and mineral deficiency

Retinoic acid (RA), one of the forms of vitamin A, was supplemented in diets for adult zebrafish [85]. Adult female zebrafish were initially fed a control diet and then transferred to either control, RA-supplemented diet, control diet and DEAB (which inhibits de novo RA synthesis), or control diet and DEAB with the RA supplement. All females that were treated with DEAB had reduced egg production 5 days after the diets were changed suggesting low RA levels inhibit egg production. The RA-supplemented diet maintained egg production similar to the control diet until 9 days after the diet was changed, and suggested an over supplementation of RA inhibits egg production. In male zebrafish testes, but not female ovaries, the RA supplemented diet decreased raldh2 expression, an enzyme that synthesizes retinal acid from retinol, and increased cyp26a, an enzyme that converts retinoic acid to polar metabolites for excretion [86, 87].

Zebrafish are one of the few species that lack gluconolactone oxidase that converts gluconolactone to ascorbic acid, though zebrafish need vitamin C for many processes [88]. Kirkwood et al. formulated diets deficient in vitamin C, vitamin E (tocopherol), and both vitamin E and vitamin C [89]. Both vitamins have antioxidant activity and can provide a sparring effect on each other. The vitamin C-deficient diet resulted in increased oxidative stress and increased AMPD enzyme activity, necessary for purine nucleotide synthesis and cellular energy [90]. Levels of several metabolites also changed in response to the vitamin C-deficient diet including metabolites related to amino acids and amino acid derivatives, carnitine metabolism, glutathione synthesis, glycerophospholipid synthesis, and purine metabolism. Aside from the role of vitamin E in vitamin C sparing, the response of parental vitamin E in offspring has been studied in zebrafish. Miller et al. provided a commercial lab diet, a diet with vitamin E supplementation, or a diet deficient in vitamin E to reproductive age adults [91]. Offspring from adults on the vitamin E-deficient diet had increased malformations at 2 and 3 days post fertilization and lower levels of tissue vitamin E. Microarray showed 2656 genes differentially expressed between the offspring of the vitamin E-deficient and vitamin E-supplemented diets. Several biological processes were altered including embryonic development, cell development, tissue development, cell growth, and cell cycle.

Zinc supplementation in the system water and the diet significantly increased body zinc and caused differential expression of 525 genes in zebrafish gills [92]. Genes related to transcription factors and steroid hormone receptors were enriched, impacting multiple pathways related to growth. Temporal transcriptome analysis showed that gene expression changes occurred immediately following transfer to water containing elevated levels of zinc, and the response to dietary zinc supplementation was maximal by day 7. By day 14, most of the genes impacted by zinc supplementation returned to basal expression levels. Beaver et al. provided zinc-deficient diets to zebrafish and looked at the impact on their offspring [93]. Embryos produced by those receiving the zinc-deficient diets had increased embryonic mortality and malformations of the snout and eyes. They also showed altered expression of genes related to metal homeostasis (znt8, znt9, and mtf1), diabetes and pancreatic development (insa, pax4, and pax5), and DNA methylation (dnmt4, and dnmt6). All of these show a temporally dependent expression change. These alterations of expression, especially those that impact DNA methylation and organ development, can have lasting impacts and shows the importance of zebrafish as models for maternal and offspring dietary studies. Diets supplemented with sodium selenite pentahydrate increased body selenium levels in male and female zebrafish after 7 days and altered the selenoproteome of the brain [94]. Selenoproteome alterations were strongly dependent on time and additional qRT-PCR shows differences between sexes.

Circadian rhythms

Recently, zebrafish have been used alongside more traditional animal models to understand circadian rhythms. Circadian rhythms are driven by primarily endogenous molecular events, occurring in 24-h cycles, which can be impacted by environmental factors such as energy intake and light exposure. Zebrafish held under a 24-h constant light exposure, as compared to the typical 14-h:10-h light and dark cycle, have an altered expression of genes that are important in maintaining circadian cycles such as clock, per1, per2, and cry1a [95]. Clock, per1, and cry1a are also dysregulated by providing the animals with a high-fat diet. High-fat diet also altered the expression of several ppar isoforms and lpl, while a continuous light cycle only altered pparbd expression. These results demonstrate the value of the zebrafish model to understand intersecting molecular pathways between circadian rhythms and metabolic disorders.

Bone Formation

High-fat diets in zebrafish affect bone formation [96]. Calcein staining showed decreased bone mineralization around the border of the scales. The activity of alkaline phosphatase is decreased and the activity of tartrate-resistant acid phosphatase is increased. Expression of thfrsf11 and thfrsf11/thfrsf11b ratio are both increased, which suggests impacts on bone reabsorption. Along with these changes in bone formation, zebrafish on the high-fat diet treatment exhibited decreased adiponectin and increased leptin, weight, BMI, and advanced glycation end products.


The case for the importance of the zebrafish model in nutrigenomic studies is substantial. Zebrafish models have been developed for almost any human disease in which nutrition is a confounding factor. The results in these studies are easily translatable to other animal models or human intervention trials for a wide array of public health concerns.

As the zebrafish model continues to be utilized in nutrigenomic studies, certain considerations will maximize effectiveness and create new avenues for investigation. Defined reference diets, similar to those used in rodents, are being developed to enhance experimental rigor and reproducibility. Currently, many labs rely on commercially available diets that can have unknown composition and differing sourced ingredients. These ingredients can contain undetected or unreported bioactive dietary components. The zebrafish community will benefit from an increased understanding of the nutritional needs of zebrafish [97], and additional research and education should be forthcoming.

Manipulation of diet content is an important tool to investigate diet-related physiology and molecular changes. Age-related responses to dietary content should also be considered in current and future studies. Studies of reproduction performed at various age structures and using various feed management strategies can yield different results. Alsop et al. bred females every few days to observe egg production following vitamin A supplementation [85]. Reproductive output was lower in zebrafish fed smaller rations compared to those fed large rations [98]. Ages at which diets were provided varied substantially among these studies. Temporal transcriptome studies reported by Zheng et al. demonstrated the importance of timing on genomic outcomes [92]. Thus, understanding the complexity of nutrigenomic outcomes in response to nutrient and non-nutrient-related manipulations will allow us to further clarify the role of nutrients in metabolic processes related to normal and disease states of zebrafish health.

Lastly, the value of zebrafish nutrigenetics studies has been enhanced by the high throughput nature of the model. Zebrafish have been used for drug discovery and forward genetic screens, and for novel gene functions and impacts of genetic variation [99, 100]. Similar screening of dietary components that function differentially in specific genotypes is not only possible but scientifically necessary and highly valuable. Parks et al. investigated the effects of diet on over 100 inbred strains of mice, yielding important information on single nucleotide differences in diet response. Similar study designs can be performed in the zebrafish model with less logistic effort to discover novel diet-responsive alleles [101]. Recently, single nucleotide polymorphisms of several growth factor genes were identified following the consumption of plant protein diets and were implicated as novel targets for future investigation [102]. Large-scale transposon insertion and targeted gene-editing techniques that have recently been used with zebrafish also provides means of novel gene discovery and of how gene variants can alter responses to diet.

The value of the zebrafish as a nutrigenomic model is just now being discovered. We hope that more studies will focus on the use of the zebrafish model for gene-diet interactions, and we believe that this information will be translatable to human health.

Availability of data and materials

Not applicable


  1. 1.

    Simopoulos AP. Nutrigenetics/nutrigenomics. Annu Rev Public Health. 2010;31:53–68.

    PubMed  Article  Google Scholar 

  2. 2.

    Trujillo E, Davis C, Milner J. Nutrigenomics, proteomics, metabolomics, and the practice of dietetics. J Am Diet Assoc. 2006;106(3):403–13.

    CAS  PubMed  Article  Google Scholar 

  3. 3.

    Jirtle RL, Skinner MK. Environmental epigenomics and disease susceptibility. Nat Rev Genet. 2007;8(4):253.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  4. 4.

    Huang S. Histone methyltransferases, diet nutrients and tumour suppressors. Nat Rev Cancer. 2002;2(6):469.

    CAS  PubMed  Article  Google Scholar 

  5. 5.

    Guengerich FP. Influence of nutrients and other dietary materials on cytochrome P-450 enzymes. Am J Clin Nutr. 1995;61(3):651S–8S.

    CAS  PubMed  Article  Google Scholar 

  6. 6.

    Fenech M, et al. Nutrigenetics and nutrigenomics: viewpoints on the current status and applications in nutrition research and practice. Lifestyle Genomics. 2011;4(2):69–89.

    CAS  Google Scholar 

  7. 7.

    Lieschke GJ, Currie PD. Animal models of human disease: zebrafish swim into view. Nat Rev Genet. 2007;8(5):353.

    CAS  PubMed  Article  Google Scholar 

  8. 8.

    Howe K, et al. The zebrafish reference genome sequence and its relationship to the human genome. Nature. 2013;496(7446):498.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  9. 9.

    Sassen W, Köster R. A molecular toolbox for genetic manipulation of zebrafish. Advances in Genomics and Genetics. 2015;2015(1):151–63.

    Google Scholar 

  10. 10.

    Hwang WY, et al. Efficient genome editing in zebrafish using a CRISPR-Cas system. Nat Biotechnol. 2013;31(3):227.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  11. 11.

    Bernardos RL, Raymond PA. GFAP transgenic zebrafish. Gene Expr Patterns. 2006;6(8):1007–13.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  12. 12.

    Oka T, et al. Diet-induced obesity in zebrafish shares common pathophysiological pathways with mammalian obesity. BMC Physiol. 2010;10(1):21.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  13. 13.

    Hales CM, et al. Trends in obesity and severe obesity prevalence in US youth and adults by sex and age, 2007-2008 to 2015-2016. Jama. 2018;319(16):1723–5.

    PubMed  PubMed Central  Article  Google Scholar 

  14. 14.

    Pi-Sunyer FX. Comorbidities of overweight and obesity: current evidence and research issues; 1999.

    Google Scholar 

  15. 15.

    MacLaren RE, et al. Association of adipocyte genes with ASP expression: a microarray analysis of subcutaneous and omental adipose tissue in morbidly obese subjects. BMC Med Genet. 2010;3(1):3.

    Google Scholar 

  16. 16.

    Li S, et al. Assessment of diet-induced obese rats as an obesity model by comparative functional genomics. Obesity. 2008;16(4):811–8.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  17. 17.

    Landgraf K, et al. Short-term overfeeding of zebrafish with normal or high-fat diet as a model for the development of metabolically healthy versus unhealthy obesity. BMC Physiol. 2017;17(1):4.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  18. 18.

    Liu, H., et al., Increased basal level of Akt-dependent insulin signaling may be responsible for the development of insulin resistance. American Journal of Physiology-Endocrinology and Metabolism, 2009.

  19. 19.

    Mogler C, et al. Hepatic stellate cell-expressed endosialin balances fibrogenesis and hepatocyte proliferation during liver damage. EMBO molecular medicine. 2015;7(3):332–8.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  20. 20.

    Den Broeder, M.J., et al., Zebrafish as a model to study the role of peroxisome proliferating-activated receptors in adipogenesis and obesity. PPAR research, 2015. 2015.

  21. 21.

    Venkatachalam AB, Sawler DL, Wright JM. Tissue-specific transcriptional modulation of fatty acid-binding protein genes, fabp2, fabp3 and fabp6, by fatty acids and the peroxisome proliferator, clofibrate, in zebrafish (Danio rerio). Gene. 2013;520(1):14–21.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  22. 22.

    Anton SD, et al. Flipping the metabolic switch: understanding and applying the health benefits of fasting. Obesity. 2018;26(2):254–68.

    PubMed  Article  PubMed Central  Google Scholar 

  23. 23.

    Craig PM, Moon TW. Fasted zebrafish mimic genetic and physiological responses in mammals: a model for obesity and diabetes? Zebrafish. 2011;8(3):109–17.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  24. 24.

    Piper MD, et al. Dietary restriction and aging: a unifying perspective. Cell Metab. 2011;14(2):154–60.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  25. 25.

    Lee, C. and V. Longo, Dietary restriction with and without caloric restriction for healthy aging. F1000 Research, 2016. 5.

  26. 26.

    Arslan-Ergul A, et al. Short-term dietary restriction in old zebrafish changes cell senescence mechanisms. Neuroscience. 2016;334:64–75.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  27. 27.

    Ferrero-Miliani L, et al. Chronic inflammation: importance of NOD2 and NALP3 in interleukin-1β generation. Clin Exp Immunol. 2007;147(2):227–35.

    CAS  PubMed  PubMed Central  Google Scholar 

  28. 28.

    Blüher M. The distinction of metabolically ‘healthy’from ‘unhealthy’obese individuals. Curr Opin Lipidol. 2010;21(1):38–43.

    PubMed  Article  CAS  PubMed Central  Google Scholar 

  29. 29.

    Innes JK, Calder PC. Omega-6 fatty acids and inflammation. Prostaglandins Leukot Essent Fat Acids. 2018;132:41–8.

    CAS  Article  Google Scholar 

  30. 30.

    Powell ML, et al. Effects of the dietary ω3: ω6 fatty acid ratio on body fat and inflammation in zebrafish (Danio rerio). Comparative medicine. 2015;65(4):289–94.

    CAS  PubMed  PubMed Central  Google Scholar 

  31. 31.

    Adam A-C, et al. High dietary arachidonic acid levels induce changes in complex lipids and immune-related eicosanoids and increase levels of oxidised metabolites in zebrafish (Danio rerio). Br J Nutr. 2017;117(8):1075–85.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  32. 32.

    Forn-Cuní G, et al. Liver immune responses to inflammatory stimuli in a diet-induced obesity model of zebrafish. J Endocrinol. 2015;224(2):159–70.

    PubMed  Article  CAS  Google Scholar 

  33. 33.

    Metwali A, et al. Cutting edge: hemokinin has substance P-like function and expression in inflammation. J Immunol. 2004;172(11):6528–32.

    CAS  PubMed  Article  Google Scholar 

  34. 34.

    Karanth S, et al. Polyunsaturated fatty acyl-coenzyme As are inhibitors of cholesterol biosynthesis in zebrafish and mice. Dis Model Mech. 2013;6(6):1365–77.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  35. 35.

    Baigent, C., et al., Efficacy and safety of more intensive lowering of LDL cholesterol: a meta-analysis of data from 170,000 participants in 26 randomised trials. 2010, Elsevier.

  36. 36.

    New, M.B. and U.N. Wijkström, Use of fishmeal and fish oil in aquafeeds: further thoughts on the fishmeal trap. FAO Fisheries Circular (FAO), 2002.

  37. 37.

    Hedrera MI, et al. Soybean meal induces intestinal inflammation in zebrafish larvae. PLoS One. 2013;8(7):e69983.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  38. 38.

    Fuentes-Appelgren P, et al. Effect of the dietary inclusion of soybean components on the innate immune system in zebrafish. Zebrafish. 2014;11(1):41–9.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  39. 39.

    Perera E, Yúfera M. Soybean meal and soy protein concentrate in early diet elicit different nutritional programming effects on juvenile zebrafish. Zebrafish. 2016;13(1):61–9.

    CAS  PubMed  Article  Google Scholar 

  40. 40.

    Ulloa PE, et al. Growth response and expression of muscle growth–related candidate genes in adult zebrafish fed plant and fishmeal protein–based diets. Zebrafish. 2013;10(1):99–109.

    CAS  PubMed  Article  Google Scholar 

  41. 41.

    Mattson F, Erickson B, Kligman A. Effect of dietary cholesterol on serum cholesterol in man. Am J Clin Nutr. 1972;25(6):589–94.

    CAS  PubMed  Article  Google Scholar 

  42. 42.

    McNamara DJ. Dietary cholesterol and atherosclerosis. Biochimica Et Biophysica Acta (Bba)-Molecular And Cell Biology Of Lipids. 2000;1529(1-3):310–20.

    CAS  Google Scholar 

  43. 43.

    Yoon Y, et al. High cholesterol diet induces IL-1β expression in adult but not larval zebrafish. PLoS One. 2013;8(6):e66970.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  44. 44.

    Progatzky F, et al. Dietary cholesterol directly induces acute inflammasome-dependent intestinal inflammation. Nat Commun. 2014;5:5864.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  45. 45.

    Kim J-Y, Seo J, Cho K-H. Aspartame-fed zebrafish exhibit acute deaths with swimming defects and saccharin-fed zebrafish have elevation of cholesteryl ester transfer protein activity in hypercholesterolemia. Food Chem Toxicol. 2011;49(11):2899–905.

    CAS  PubMed  Article  Google Scholar 

  46. 46.

    Fang L, et al. Oxidized cholesteryl esters and phospholipids in zebrafish larvae fed a high cholesterol diet macrophage binding and activation. J Biol Chem. 2010;285(42):32343–51.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  47. 47.

    Stoletov K, et al. Vascular lipid accumulation, lipoprotein oxidation, and macrophage lipid uptake in hypercholesterolemic zebrafish. Circ Res. 2009;104(8):952–60.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  48. 48.

    Kiechl S, et al. Oxidized phospholipids, lipoprotein (a), lipoprotein-associated phospholipase A2 activity, and 10-year cardiovascular outcomes: prospective results from the Bruneck study. Arterioscler Thromb Vasc Biol. 2007;27(8):1788–95.

    CAS  PubMed  Article  Google Scholar 

  49. 49.

    Kim J-Y, et al. Grape skin and loquat leaf extracts and acai puree have potent anti-atherosclerotic and anti-diabetic activity in vitro and in vivo in hypercholesterolemic zebrafish. Int J Mol Med. 2012;30(3):606–14.

    CAS  PubMed  Article  Google Scholar 

  50. 50.

    Barter PJ, et al. Cholesteryl ester transfer protein: a novel target for raising HDL and inhibiting atherosclerosis. Arterioscler Thromb Vasc Biol. 2003;23(2):160–7.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  51. 51.

    Di Bartolo B, et al. CETP inhibition in CVD prevention: an actual appraisal. Curr Cardiol Rep. 2016;18(5):43.

    PubMed  Article  PubMed Central  Google Scholar 

  52. 52.

    Baek, J.S., et al., Ezetimibe and simvastatin reduce cholesterol levels in zebrafish larvae fed a high-cholesterol diet. Cholesterol, 2012. 2012.

  53. 53.

    Rooney K, et al. Creatine supplementation alters insulin secretion and glucose homeostasis in vivo. Metabolism-Clinical and Experimental. 2002;51(4):518–22.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  54. 54.

    Takahashi Y, et al. The suppressive effect of salmon muscle extracts containing anserine on lipid accumulation in rats fed with high fat diet. Nippon Suisan Gakkaishi (Japan). 2008.

  55. 55.

    Shimada Y, et al. E2F8 promotes hepatic steatosis through FABP3 expression in diet-induced obesity in zebrafish. Nutrition & metabolism. 2015;12(1):17.

    Article  CAS  Google Scholar 

  56. 56.

    Hasumura T, et al. Green tea extract suppresses adiposity and affects the expression of lipid metabolism genes in diet-induced obese zebrafish. Nutrition & metabolism. 2012;9(1):73.

    Article  Google Scholar 

  57. 57.

    Meguro S, Hasumura T, Hase T. Body fat accumulation in zebrafish is induced by a diet rich in fat and reduced by supplementation with green tea extract. PLoS One. 2015;10(3):e0120142.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  58. 58.

    Tainaka T, et al. Transcriptome analysis of anti-fatty liver action by Campari tomato using a zebrafish diet-induced obesity model. Nutrition & metabolism. 2011;8(1):88.

    CAS  Article  Google Scholar 

  59. 59.

    Zang L, et al. Effects of Yuzu (Citrus junos Siebold ex Tanaka) peel on the diet-induced obesity in a zebrafish model. J Funct Foods. 2014;10:499–510.

    CAS  Article  Google Scholar 

  60. 60.

    Zheng X, et al. Caffeine reduces hepatic lipid accumulation through regulation of lipogenesis and ER stress in zebrafish larvae. J Biomed Sci. 2015;22(1):105.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  61. 61.

    Fang L, et al. Programming effects of high-carbohydrate feeding of larvae on adult glucose metabolism in zebrafish, Danio rerio. Br J Nutr. 2014;111(5):808–18.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  62. 62.

    Rocha F, et al. Glucose metabolism and gene expression in juvenile zebrafish (Danio rerio) challenged with a high carbohydrate diet: effects of an acute glucose stimulus during late embryonic life. Br J Nutr. 2015;113(3):403–13.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  63. 63.

    Seiliez I, et al. Postprandial regulation of growth-and metabolism-related factors in zebrafish. Zebrafish. 2013;10(2):237–48.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  64. 64.

    Gleeson M, Connaughton V, Arneson L. Induction of hyperglycaemia in zebrafish (Danio rerio) leads to morphological changes in the retina. Acta Diabetol. 2007;44(3):157–63.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  65. 65.

    Eames SC, et al. Blood sugar measurement in zebrafish reveals dynamics of glucose homeostasis. Zebrafish. 2010;7(2):205–13.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  66. 66.

    Olsen AS, Sarras MP Jr, Intine RV. Limb regeneration is impaired in an adult zebrafish model of diabetes mellitus. Wound Repair Regen. 2010;18(5):532–42.

    PubMed  PubMed Central  Article  Google Scholar 

  67. 67.

    Capiotti KM, et al. Persistent impaired glucose metabolism in a zebrafish hyperglycemia model. Comp Biochem Physiol B: Biochem Mol Biol. 2014;171:58–65.

    CAS  Article  Google Scholar 

  68. 68.

    Elo B, et al. Larval zebrafish as a model for glucose metabolism: expression of phosphoenolpyruvate carboxykinase as a marker for exposure to anti-diabetic compounds. J Mol Endocrinol. 2007;38(4):433–40.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  69. 69.

    Olsen AS, et al. Heritable transmission of diabetic metabolic memory in zebrafish correlates with DNA hypomethylation and aberrant gene expression. Diabetes. 2012;61(2):485–91.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  70. 70.

    Maddison LA, Chen W. Nutrient excess stimulates β-cell neogenesis in zebrafish. Diabetes. 2012;61(10):2517–24.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  71. 71.

    Ninov N, et al. Metabolic regulation of cellular plasticity in the pancreas. Curr Biol. 2013;23(13):1242–50.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  72. 72.

    Michel M, et al. Leptin signaling regulates glucose homeostasis, but not adipostasis, in the zebrafish. Proc Natl Acad Sci. 2016;113(11):3084–9.

    CAS  PubMed  Article  Google Scholar 

  73. 73.

    Sapp V, et al. Fructose leads to hepatic steatosis in zebrafish that is reversed by mechanistic target of rapamycin (mTOR) inhibition. Hepatology. 2014;60(5):1581–92.

    CAS  PubMed  Article  Google Scholar 

  74. 74.

    Cambier S, et al. Serial analysis of gene expression in the skeletal muscles of zebrafish fed with a methylmercury-contaminated diet. Environ Sci Technol. 2009;44(1):469–75.

    Article  CAS  Google Scholar 

  75. 75.

    Luo M-J, Lai M-D. Identification of differentially expressed genes in normal mucosa, adenoma and adenocarcinoma of colon by SSH. World J Gastroenterol. 2001;7(5):726.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  76. 76.

    Lin Y-M, et al. Molecular diagnosis of colorectal tumors by expression profiles of 50 genes expressed differentially in adenomas and carcinomas. Oncogene. 2002;21(26):4120.

    CAS  PubMed  Article  Google Scholar 

  77. 77.

    Barnard GF, et al. Gastric and hepatocellular carcinomas do not overexpress the same ribosomal protein messenger RNAs as colonic carcinoma. Cancer Res. 1993;53(17):4048–52.

    CAS  PubMed  Google Scholar 

  78. 78.

    Kim SH, Lee JY, Kim J. Characterization of a wide range base-damage-endonuclease activity of mammalian rpS3. Biochem Biophys Res Commun. 2005;328(4):962–7.

    CAS  PubMed  Article  Google Scholar 

  79. 79.

    Larcher T, et al. Chronic dietary exposure of zebrafish to PAH mixtures results in carcinogenic but not genotoxic effects. Environ Sci Pollut Res. 2014;21(24):13833–49.

    CAS  Article  Google Scholar 

  80. 80.

    Carmona-Antoñanzas G, et al. Light-and clock-control of genes involved in detoxification. Chronobiol Int. 2017;34(8):1026–41.

    PubMed  Article  CAS  Google Scholar 

  81. 81.

    Billiard SM, et al. Binding of polycyclic aromatic hydrocarbons (PAHs) to teleost aryl hydrocarbon receptors (AHRs). Comp Biochem Physiol B: Biochem Mol Biol. 2002;133(1):55–68.

    Article  Google Scholar 

  82. 82.

    Liu Q, et al. Histopathologic alterations associated with global gene expression due to chronic dietary TCDD exposure in juvenile zebrafish. PLoS One. 2014;9(7):e100910.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  83. 83.

    Spitsbergen JM, Buhler DR, Peterson TS. Neoplasia and neoplasm-associated lesions in laboratory colonies of zebrafish emphasizing key influences of diet and aquaculture system design. ILAR J. 2012;53(2):114–25.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  84. 84.

    Spitsbergen JM, et al. Neoplasia in zebrafish (Danio rerio) treated with N-methyl-N'nitro-N-nitrosoguanidine by three exposure routes at different developmental stages. Toxicol Pathol. 2000;28(5):716–25.

    CAS  PubMed  Article  Google Scholar 

  85. 85.

    Alsop D, et al. Retinoid requirements in the reproduction of zebrafish. Gen Comp Endocrinol. 2008;156(1):51–62.

    CAS  PubMed  Article  Google Scholar 

  86. 86.

    Thatcher JE, Isoherranen N. The role of CYP26 enzymes in retinoic acid clearance. Expert Opin Drug Metab Toxicol. 2009;5(8):875–86.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  87. 87.

    Duester G. Retinoic acid synthesis and signaling during early organogenesis. Cell. 2008;134(6):921–31.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  88. 88.

    Dabrowski, K., Ascorbic acid in aquatic organisms: status and perspectives. 2000: CRC press.

  89. 89.

    Kirkwood JS, et al. Vitamin C deficiency activates the purine nucleotide cycle in zebrafish. J Biol Chem. 2012;287(6):3833–41.

    CAS  PubMed  Article  Google Scholar 

  90. 90.

    WAARDE AV. Operation of the purine nucleotide cycle in animal tissues. Biol Rev. 1988;63(2):259–98.

    PubMed  Article  PubMed Central  Google Scholar 

  91. 91.

    Miller GW, et al. The influences of parental diet and vitamin E intake on the embryonic zebrafish transcriptome. Comparative Biochemistry and Physiology Part D: Genomics and Proteomics. 2014;10:22–9.

    CAS  Google Scholar 

  92. 92.

    Zheng D, et al. Dynamic transcriptomic profiles of zebrafish gills in response to zinc supplementation. BMC Genomics. 2010;11(1):553.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  93. 93.

    Beaver LM, et al. Adverse effects of parental zinc deficiency on metal homeostasis and embryonic development in a zebrafish model. J Nutr Biochem. 2017;43:78–87.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  94. 94.

    Benner MJ, et al. Sex-specific transcriptional responses of the zebrafish (Danio rerio) brain selenoproteome to acute sodium selenite supplementation. Physiol Genomics. 2013;45(15):653–66.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  95. 95.

    Kopp R, et al. Bringing obesity to light: Rev-erbα, a central player in light-induced adipogenesis in the zebrafish? Int J Obes. 2016;40(5):824.

    CAS  Article  Google Scholar 

  96. 96.

    Carnovali M, et al. Metabolic and bone effects of high-fat diet in adult zebrafish. Endocrine. 2018;61(2):317–26.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  97. 97.

    Watts SA, Powell M, D'Abramo LR. Fundamental approaches to the study of zebrafish nutrition. ILAR J. 2012;53(2):144–60.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  98. 98.

    Fowler LA, M. W, Dennis LN, Berry RJ, Powell ML, Watts SA. Influence of commercial and laboratory diets on growth, body composition, and reproduction in the zebrafish Danio rerio. Zebrafish. 2019; In Press.

  99. 99.

    Muto A, et al. Forward genetic analysis of visual behavior in zebrafish. PLoS Genet. 2005;1(5):e66.

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  100. 100.

    Stern HM, Zon LI. Cancer genetics and drug discovery in the zebrafish. Nat Rev Cancer. 2003;3(7):533.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

  101. 101.

    Parks BW, et al. Genetic control of obesity and gut microbiota composition in response to high-fat, high-sucrose diet in mice. Cell Metab. 2013;17(1):141–52.

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  102. 102.

    Ulloa PE, et al. RNA sequencing to study gene expression and SNP variations associated with growth in zebrafish fed a plant protein-based diet. Mar Biotechnol. 2015;17(3):353–63.

    CAS  PubMed  Article  PubMed Central  Google Scholar 

Download references


The authors acknowledge the participation of members of the Watts laboratory, Anna Grace Ballard, Jenna Alkhatib, and Siddhartha Brahma, PhD for discussions on the manuscript.


The authors acknowledge support from the NIH Nutrition Obesity Research Center (P30DK056336) and the Animal Models Core (Aquatic Animal Research Core).

Author information




MBW did the primary writing of the manuscript and SAW provided editing and writing. Both authors read and approved the final manuscript.

Corresponding author

Correspondence to Michael B. Williams.

Ethics declarations

Ethics approval and consent to participate

Not applicable

Consent for publication

Not applicable

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (, 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 ( applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Williams, M.B., Watts, S.A. Current basis and future directions of zebrafish nutrigenomics. Genes Nutr 14, 34 (2019).

Download citation


  • Zebrafish
  • Nutrition
  • Diet
  • Nutrigenomics
  • Nutrigenetics
  • Gene Interactions