Skip to main content

Thank you for visiting nature.com. You are using a browser version with limited support for CSS. To obtain the best experience, we recommend you use a more up to date browser (or turn off compatibility mode in Internet Explorer). In the meantime, to ensure continued support, we are displaying the site without styles and JavaScript.

Drivers of ecological assembly in the hindgut of Atlantic Cod fed a macroalgal supplemented diet

Abstract

It is difficult to disentangle the many variables (e.g. internal or external cues and random events) that shape the microbiota in the gastrointestinal tract of any living species. Ecological assembly processes applied to microbial communities can elucidate these drivers. In our study, farmed Atlantic cod (Gadus morhua) were fed a diet of 10% macroalgae supplement (Ulva rigida [ULVA] or Ascophyllum nodosum [ASCO] or a non-supplemented control diet [CTRL]) over 12 weeks. We determined the influence of ecological assembly processes using a suite of null-modelling tools. We observed dissimilarity in the abundance of common OTUs over time, which was driven by deterministic assembly. The CTRL samples showed selection as a critical assembly process. While dispersal limitation was a driver of the gut microbiome for fish fed the macroalgae supplemented diet at Week 12 (i.e., ASCO and ULVA). Fish from the ASCO grouping diverged into ASCO_N (normal) and ASCO_LG (lower growth), where ASCO_LG individuals found the diet unpalatable. The recruitment of new taxa overtime was altered in the ASCO_LG fish, with the gut microbiome showing phylogenetic underdispersion (nepotistic species recruitment). Finally, the gut microbiome (CTRL and ULVA) showed increasing robustness to taxonomic disturbance over time and lower functional redundancy. This study advances our understanding of the ecological assembly and succession in the hindgut of juvenile Atlantic cod across dietary treatments. Understanding the processes driving ecological assembly in the gut microbiome, in fish research specifically, could allow us to manipulate the microbiome for improved health or resilience to disease for improved aquaculture welfare and production.

Introduction

Aquaculture has become the fastest-growing food sector this century, surpassing over 82 million tonnes of seafood production in 20181 contributing >45% of the global seafood production1. At present, however, Atlantic cod (Gadus morhua) is primarily harvested through capture fisheries owing to species-specific production bottlenecks in aquaculture, leading to reduced profitability2,3. Such bottlenecks include poor larval survival rates4, early sexual maturation (reduced fillet yield)5, and reduced fish growth6. A review of these challenges is noted here7. An avenue that is being increasingly explored is the addition of aquafeed ingredients from a variety of natural sources that provide additional health benefits to the growing fish (e.g., macroalgae supplements8,9,10, immunostimulants11,12, pre- and probiotics13,14). In conjunction with such diet supplements, it is apparent that the impact of these feeds on the gut microbiome and fish health should be considered.

The fish gut microbiome is increasingly used to elucidate fish condition15, response to environmental conditions16 and changing diet17,18 and has been extensively reviewed elsewhere15,19,20. It is a tantalising goal to use the information yielded by microbial ecology to manipulate a particular fish species’ gut microbiome for improved welfare and growth in a commercial setting. To be tenable, we need to understand the gut microbiome beyond a descriptive analysis of the species found within a specific condition. Taking an example from our previous work, over twelve weeks, we fed Atlantic cod juveniles (G. morhua) a diet of 10% macroalgal supplement either Ascophyllum nodosum (ASCO) or Ulva rigida (ULVA) species, or a control non-amended diet21. We showed that temporal pressures outweighed the response to diet supplementation, with the gut microbiome of all fish consuming the different diets converging. It is unclear if this shift resulted from natural community succession in the developing hindgut microbiome of the juvenile farmed fish or other factors. Indeed, little is known about the gut microbiome development in cod, with a limited number of studies that have only reported on the larval phase22 or wild adults23. Moreover, the microbial communities within the gut face various driving forces from the host, environmental factors, and individual species interactions, for example.

Ecological theory has been used to describe the mechanisms that shape community assembly. It is more typically applied to macroorganisms (e.g., fish species24) or a population of macroorganisms within a specific environment (e.g., shore communities25). This approach is increasingly being used in microbial ecology26,27,28 to determine underlying rules driving the assembly and dynamics of microbial communities, which is particularly challenging29. The gut microbiome is a complex and dynamic ecosystem subject to fluctuating abiotic and biotic conditions. Authors have noted that founder (priority) effects can play a key role in the community assembly and succession, i.e., the species that first colonise will alter the environment and determine the resulting community structure30,31. The colonisation of that first species may be random like a lottery30, or determined via resource availability and species traits32,33. Assembly processes are broadly described as either random (stochastic) or non-random (deterministic)29. Researchers have noted that four assembly processes can occur in microbial communities: neutral and stochastic processes (e.g., probabilistic events such as births, deaths, mutations and ecological drift34) or non-probable events driven from niche or deterministic forces (e.g., environmental conditions, species interactions, and traits). Neutral theory differs from niche-based theory in assuming that all species are equal in functional traits, demographic rates, and the environment does not select. A range of tools have been described to determine the underlying mechanisms of microbial community assembly. Many of these rely on ‘null models’. A null modelling approach considers randomising the original community structure and then, through a statistical framework, compares microbiome properties between the original and randomised communities to elucidate a particular ecological phenomenon. The randomised community is generated to mimic a community without the force of a specified assembly process35. Deviations from the null model can then be used to predict the processes occurring in the real community.

Microbial community assembly mechanisms themselves remain relatively underexplored within fish gut studies. A recent review by Derome and Filteau (2020) summarises the work that has been published so far and offers a perspective on future directions36. Exploring these mechanisms may provide a realistic opportunity to manipulate the gut microbiome to improve commercial fish conditions, increase disease resilience, and mitigate stress under aquaculture conditions. Therefore, in the present study, the aims are to implement a suite of ‘null-modelling’ tools to understand the microbial ecological assembly mechanisms in the gut of Atlantic cod (G. morhua) in an experimental feeding trial over twelve weeks. Specifically, we aim to determine: (i) whether the microbial community was driven by stochastic, deterministic forces, niche, or neutral effects, (ii) the influence of specific ecological processes on microbial diversity, (iii) colonisation and community succession mechanisms and finally, (iv) the resilience of the gut microbial function to taxonomic perturbation. We hypothesised that the gut microbiome would demonstrate deterministic and niche-based assembly linked to host development, that this would outweigh environmental variables such as feed type, and that individuals with poorer growth (ASCO_LG) from a subset of fish that found the diet unpalatable, would demonstrate vulnerabilities to taxonomic perturbation. Our work has significant importance with respect to fish gut microbiome research. More broadly, this work is relevant to areas where manipulating the microbial community through novel feed additives and functional supplements is desired.

Results

It was evident that there were strong temporal pressures on the hindgut microbial community of juvenile Atlantic cod (G. morhua), with a change in the microbial community composition over the 12-week trial. Dissimilarity in community composition was highly significant across time points (Beta-diversity Bray-Curtis dissimilarity matrix - p = 0.001). The OTUs that best correlated with the temporal community dissimilarities were Proteobacteria, Bacteroidetes and Firmicutes species. Proteobacteria spp. (OTU_3130 + OTU_307 - Photobacterium spp. and OTU_2746 - Vibrio sp.) which were associated with Week 0 to Week 8 (Fig. 1). While Bacteroidetes spp. (OTU_9 + OTU_3586 - Bacteroides spp. and OTU_41 + OTU_37 - Rikenella spp.) and Firmicutes spp. (OTU_1855 + OTU_174 + OTU_33 - Ruminococcaceae spp., OTU_2624 - Lachnoclostridium sp. and OTU_23 - Tyzzerella sp.) correlated with Week 12 samples (Fig. 1). The OTU subset that most explained the dissimilarity pattern included all these OTUs except OTU_37 – Rikenella sp. (R = 0.902). Notably, a temporal shift in OTUs was not observed in the ASCO_LG individuals.

Fig. 1: Temporal dissimilarity of the gut microbiota of Atlantic cod.
figure 1

Dissimilarity is explained by Proteobacteria species at Week 0/Week 8 and Bacteroidetes and Firmicutes species at Week 12. The points represent grouped samples with ‘Time’ denoted by colour; 0 (red), 8 (green), 12 (orange), and dietary treatments denoted by symbols. Deviance in ordination space is explained by 24.5%. PERMANOVA (sources of variability explained by dissimilarities between samples) showed that variation accounted for by Treatment Groups; R2 = 0.098, ***p = 0.001 and variation accounted for by Time-Point; R2 = 0.08644, ***p = 0.001.

Predictive functional analysis using PICRUSt2 revealed that some of the detected microbial metabolism pathways had significantly changed (greater than Log2 fold) from Week 0 to Week 12 (Supplementary Fig. 1). This included pathways related to lysine biosynthesis and degradation and methane metabolism detected at Week 12, which were not found at Week 0.

What microbial community assembly mechanisms are shaping the microbiome of juvenile Atlantic cod (Gadus morhua), and how are these influenced by macroalgal feed supplements?

Now that we have established the shift in microbial community dynamics over time, we wanted to determine what assembly mechanisms could drive this change. First, we used Hill-based dissimilarity indices combined with a Raup-Crick null model37,38,39 to determine the nature of assembly patterns in pair-wise temporal comparisons (stochastic or deterministic assembly). The temporal dissimilarity observed above was corroborated here, with high dissimilarity (qd values > 0.65) between Week 0 and each Week 8 treatment (Fig. 2a). Dissimilarity was lower between the Week 8 and Week 12 comparisons (CTRL and ULVA) but remained high. However, the ASCO_N and ASCO_LG groups showed less dissimilarity over time with qd values < 0.5 between Week 8 and Week 12, as compared to the other temporal comparisons. When we consider how the empirical dissimilarity values compare to the null expectation, we observe at a diversity order of 0 (q = 0) that values are close to the null expectation and therefore shaped by random assembly. While, at higher diversity orders (q ≥ 1), empirical dissimilarity values differ greatly from the null expectation and are therefore shaped by deterministic forces.

Fig. 2: Microbial community assembly in the gut microbiota of Atlantic cod.
figure 2

The presence/absence of OTUs from Week 0 to Week 8 and Week 8 to Week 12 treatments are shaped by random microbial community assembly (at q = 0; empirical values are close to the null expectation). When we increase the importance of OTU relative abundance then assembly is shaped by deterministic processes (q ≥ 1; empirical values far greater than the null expectation). The solid lines show hill-based dissimilarity (qd) and the null expectation is shown by dashed lines. The diversity order (q) curve can be interpreted as follows; q = 0 considers OTU presence/absence, q = 1 OTUs are weighted according to relative abundance, and at q > 1 = increased weighting is given to highly abundant OTUs. Arrows at q = 0, 1, and 2 reflect the distances between the empirical dissimilarity observations and the null expectation at these key points in the diversity order curve (q). Colours reflect the pair-wise comparison tested. a shows comparisons between Week 0 and Week 8, and b shows comparisons between Week 8 and Week 12.

Subsequently, we implemented the beta-null deviation model34,40 considering both abundances and phylogenetic distance (Generalised Unifrac dissimilarity measure). We found that the hindgut microbiota showed an increasing contribution of neutral assembly processes (Fig. 3a). Week 12 treatment groups were significantly more neutral than Week 0 (p < 0.05), except for the ASCO_LG samples, which showed an increase towards niche assembly processes over time. Next, we applied the quantitative process estimates measure41,42, which assesses the percentage contribution of various assembly processes within treatment groups. At Week 0, dispersal limitation (limited dispersal or historical contingency), variable selection (diverging communities), and homogenising selection (converging communities) accounted for 39, 18, and 7%, respectively, of the assembly processes (Fig. 3b). Undominated assembly (i.e., moderate dispersal and weak selection) accounted for 36% at Week 0. In the control group [CTRL], variable selection increased to 60% at Week 8. At Week 12, variable selection and undominated equated 50% contribution to community assembly in the CTRL treatments. In contrast, the macroalgal diet treatments showed substantial dispersal limitation (25–48%), 40–70% undominated process (weak selection and moderate drift) and low variable selection (4–14%) at Week 12. This was particularly apparent in the ASCO_LG fish, where dispersal limitation accounted for 70% of community assembly at Week 8 and 48% at Week 12. Homogenising selection and homogenising dispersal were not critical assembly processes in the cod hindgut microbiome observed here.

Fig. 3: Quantification of microbial community assembly in the gut microbiota of Atlantic cod.
figure 3

a The hindgut microbiota of juvenile Atlantic cod is increasingly shaped by neutral assembly processes over time irrespective of dietary treatment, except for the ASCO_LG samples. In the boxplots, center value lines indicate the median, boxes indicate the lower/upper quartiles (25%/75%) and lines extending parallel from the boxes (whiskers) show the variability outside the upper and lower quartiles. Lines connecting categories shows significant relationships (pairwise t-test) with *(p < 0.05), **(p < 0.01), or ***(p < 0.001). b The percentage contribution of assembly processes varies over time and across dietary treatments. Variable selection increased in the CTRL samples. Dispersal limitation increased in both ASCO treatments. In comparison, the ULVA treatment showed an increased contribution of undominated processes.

How do priority effects (competitive lottery model), and species succession (phylogenetic recruitment) effects influence the juvenile Atlantic cod (Gadus morhua) microbiome?

There were ten clades (groups of taxa) within the cod hindgut microbiome that had OTUs, which were “lottery winners” (>90% abundance of that clade)—Table 1. According to the threshold described by Verster and Borenstein30, four clades displayed strong “lottery-like” assembly behaviour with winners were observed in nearly all samples (winner prevalence >0.75 and winner diversity >0.25). These clades were Alistipes, Cetobacterium, Fusobacterium, and Tyzzerella genera (Table 1). Over time, this behaviour changed with both winner prevalence and winner diversity decreasing. For example, the Alistipes clade with high prevalence (>0.75) and high diversity (>0.5) at Week 0, decreased from three OTUs (OTU_34, OTU_20, and OTU_3429) to a single OTU at Week 8 (OTU_3429) and a different single OTU at Week 12 (OTU_62). The Bacteroides clade showed near lottery-like status at Week 0 with a high prevalence (>0.75) and diversity of 0.2 at Week 0, winner diversity decreased from two OTUs (OTU_9 and OTU_2969) to one OTU at Week 12 (OTU_9). In contrast, Rikenella and Lachnoclostridium clades (with >50 prevalence) showed low diversity initially with a single OTU winning (i.e., OTU_41 Rikenella sp. and OTU_2624 Lachnoclostridium sp.). The diversity of winning OTUs increased over time with the addition of an OTU per clade (i.e., OTU_37 Rikenella sp. and OTU_130 Lachnoclostridium sp.) at Week 12. Many of the remaining clades showed low diversity, with a single OTU indicated as a ‘winner’. There was an overlap between the taxonomy of OTUs that best correlated with the temporal community dissimilarities (Fig. 1) and lottery winners. Tyzzerella, Lachnoclostridium, Bacteroides, Rikenella species (Week 8 and Week 12) had lottery-like behaviour (Table 1), while Photobacterium or Vibrio species did not conform to the lottery schema.

Table 1 Genera with operational taxonomic units (OTUs) showing lottery-like behaviour in the hindgut microbiota of Atlantic cod.

We implemented the phylogenetic recruitment model to examine the temporal assembly trends in species succession. The hindgut microbial communities from the CTRL and ULVA dietary fish groups were slightly neutral tending towards phylogenetic underdispersion with values of D > 0 or <0 (Fig. 4). In contrast, in the hindgut of the ASCO_N fish species recruitment showed phylogenetic overdispersion (D > 0; D = ~0.45), while species recruitment within the ASCO_LG group showed strong phylogenetic underdispersion (D < 0; D = ~−0.55). This suggests that the ASCO_LG group is relatively more nepotistic than the other categories considered.

Fig. 4: Microbial species succession in the gut microbiota of juvenile Atlantic cod.
figure 4

The hindgut microbiome of juvenile Atlantic cod fed that ASCO diet showed temporal phylogenetic underdispersion (ASCO_LG) and temporal phylogenetic overdispersion (ASCO_N). The CTRL and ULVA treatments varied from slightly neutral to underdispersed. Each violin plot shows the distribution of Dispersion estimates (D) given by logistic error model bootstraps. We have used a 95% bootstrapped confidence interval (with 2000 bootstraps), as shown by the error bars within the plot.

How stable is the hindgut microbiome to taxonomic perturbation?

Finally, we used the taxa-function robustness measure to determine the robustness of the cod hindgut microbiome to perturbation. This considers two important values; Attenuation—high attenuation indicates strong robustness due to functional overlap and Buffering—high values indicate functions are balanced across the communities. Attenuation values increased over time from 2.2 at Week 0 to 2.7 at Week 12. Attenuation was highest in the ASCO treatments at Week 12 (Fig. 5a). Treatments at Week 8 and Week 12 were significantly different (Supplementary Table 1: Tukey HSD p < 0.005). Buffering values were in the range of 1.9–2.05 and no temporal or treatment effects were noted (Fig. 5b). Eng and Borenstein43 identified five key gene distribution features (GDF) that can account for differences in robustness. When we implemented this measure to compare time and treatment groups, Week 0 microbial communities were clustered towards increased unique function abundance and higher average functional redundancy (Fig. 5c). The ASCO_LG Week 8 and Week 12 samples, and to some extent the ULVA samples clustered towards increased average genome size, genome size variability, and average functional dissimilarity (Fig. 5c). Note, we have performed this analysis again comparing Week 0, Week 8, and Week 12 groups (excluding ASCO samples) and observed a similar pattern (Supplementary Fig. 2).

Fig. 5: How robust is the gut microbiota of Atlantic cod to taxonomic perturbation?
figure 5

a Potential robustness to perturbation magnitude (attenuation) increased over time in the hindgut of juvenile Atlantic cod, with highest values in the ASCO_LG dietary treatment. In the boxplots, center value lines indicate the median, boxes indicate the lower/upper quartiles (25%/75%) and lines extending parallel from the boxes (whiskers) show the variability outside the upper and lower quartiles. Lines connecting categories shows significant relationships (pairwise t-test) with *(p < 0.05), **(p < 0.01), or ***(p < 0.001). b Potential buffering capacity towards functional perturbation was relatively stable over time and across treatment groups. In the boxplots, center value lines indicate the median, boxes indicate the lower/upper quartiles (25%/75%) and lines extending parallel from the boxes (whiskers) show the variability outside the upper and lower quartiles. Lines connecting categories shows significant relationships (pairwise t-test) with *(p < 0.05), **(p < 0.01), or ***(p < 0.001). c The microbial communities in the hindgut of juvenile Atlantic cod were separated according to variation in gene distribution features (GDF) between Week 0 and Week 8/12 macroalgal dietary treatments. The points represent grouped samples with ‘Time’ denoted by symbols and dietary treatments denoted by colours; Week 0 (blue), CTRL (red), ULVA (green), ASCO_N (light orange), ASCO_LG (dark orange). The percent variance explained by each principal component is indicated on the axis labels. The line and box with the GDF name show the direction of the GDF vectors.

In general, the robustness (attenuation) of many specific functions increased over time from Week 0 to Week 12 (Supplementary Fig. 3). Functions were categorised into superpathways relating to metabolism and cell function. For example, the attenuation values of carbohydrate metabolism increased from ~1.0 at Week 0 to 2.2 at Week 12 (Supplementary Fig. 3). Focusing on the metabolism superpathways, when we compared metabolism function robustness across dietary treatments, the ASCO treatments were typically increased (Fig. 6). The dietary subgroup ASCO_LG had increased values for functional superpathways related to the excretory system, translation, transport, and catabolism (Supplementary Fig. 4). In contrast, the attenuation values for functional superpathways related to infectious diseases, cell growth and death, replication and repair increased over time, in all but the ASCO_LG samples (Supplementary Fig. 4). The buffering values for superpathway functions related to metabolism (metabolism of cofactors and vitamins, biosynthesis of other secondary metabolites) decreased over time and across all treatment groups, except ASCO_LG (Supplementary Fig. 5).

Fig. 6: How robust are specific functions in the gut microbiota of Atlantic cod?
figure 6

Potential robustness to specific functional superpathways related to metabolism and cell function were significantly increased over time. In the boxplots, center value lines indicate the median, boxes indicate the lower/upper quartiles (25%/75%) and lines extending parallel from the boxes (whiskers) show the variability outside the upper and lower quartiles. Lines connecting categories shows significant relationships (pairwise t-test) with *(p < 0.05), **(p < 0.01), or ***(p < 0.001).

Discussion

The fish gut microbiome is essential to systemic function, fish health44, immune support45, and digestive capacity46. However, the factors that govern the microbial community colonisation, assembly, and succession in fish species are poorly understood, in terms of both the ecological assembly mechanisms and development within the life cycle. Indeed, in our previous work21, we noted a shift in the hindgut microbial community dynamics of juvenile Atlantic cod over time. This shift was summarised in the current manuscript as a displacement in Proteobacteria (mostly Photobacterium spp.) with Bacteroidetes and Firmicutes species. Interestingly, this pattern was not observed in fish that found one of the experimental diets unpalatable (ASCO_LG). In this study, we endeavoured to determine the ecological processes that may shed light on this temporal convergence in the hindgut microbiome. We implemented a suite of ‘null-modelling’ approaches to determine what assembly processes were driving the microbial community dynamics in the hindgut of juvenile Atlantic cod. We then used the taxa-function robustness measure to assess the potential stability of the gut microbiome functions to taxonomic perturbation. Understanding such mechanisms is an important step towards managing the response to newly introduced aquafeed ingredients, improving welfare in commercial facilities or indeed conducting targeted manipulations of the microbiome for improved fish health.

We showed high temporal dissimilarity within the hindgut of juvenile Atlantic cod using the Hill-based dissimilarity and null model methodology of Modin et al.37. Interestingly, we further revealed that dissimilarity with respect to the presence or absence of OTUs was driven by random (stochastic forces) such as births, deaths or ecological drift34. However, we found that deterministic forces were driving dissimilarity in the abundances of OTUs (diversity order q > 1). Deterministic assembly processes include those which are shaped by environmental conditions (e.g., pH, nutrient availability), species interactions (e.g., competitive exclusion), or species traits (species genetics). Thus, in the cod hindgut microbiome, we observed dissimilarity in the abundance of common OTUs over time, which may be explained by selective-type pressures/conditions favouring the proliferation of particular species. This finding agrees with our hypothesis that the gut microbiome would demonstrate deterministic assembly. Deterministic factors here could also include selective pressures from the host, particularly during phases of development47. The gut microbiota of Atlantic cod within the larval phase is driven by selective pressures, associated with host intestinal development combined with some stochastic pressures48,49. Similar results were observed in Gibel Carp (Carassius auratus gibelio)50 and zebrafish (Danio rerio)47,51. The zebrafish studies notably cover the complete lifecycle (which is more practical given their shorter lifecycle). In our current study, fish were 366 days post-hatch, and it is estimated that wild Atlantic cod (from the Irish Sea) mature within two or three years of hatching52. Host pressures in the juvenile or adult cod gut are not widely described, a study design similar to that of Xiao et al.47 taking into account the complete life cycle of Atlantic cod could help elucidate these factors. The addition of proteomics to characterise the Atlantic cod gut responses during development would enable direct linkage of the microbiome to the host response.

Contrary to our hypothesis, we also observed a temporal trend from niche to neutral processes. This is consistent with Hayes et al.53, where the authors showed neutral processes dominated the gut microbiome in farmed Atlantic salmon (Salmo salar). Multiple processes can occur in a system given the complexity of the biology and interactions with the environment54. Indeed, the gut environment may add a first-pass deterministic pressure as only species capable of withstanding the gut conditions will proliferate over time55,56. This theory is perhaps further evidenced by the results from the hill-based method, where we found the presence of OTUs was driven by stochastic mechanisms, but abundances were deterministic in nature. We further quantified the contribution of different ecological processes. We discovered that dispersal limitation, variable selection and undominated (weak selection and moderate dispersal) were the primary ecological processes occurring in the cod gut microbiome. The contribution of these processes varied with respect to time and treatment. For example, variable selection increased at Week 8 for all groups and was the control group’s primary process at Week 12. Variable selection indicates strong selective pressures driving divergent shifts in species composition. However, variable selection was not a dominant process in the macroalgae treatments at Week 12. Yet, the communities in the CTRL, ULVA, and ASCO_N converged in taxonomic composition over the trial without evidence of homogenising selection.

In the macroalgal dietary treatments dispersal limitation was a core process in the hindgut, this effect was increased in the ASCO_LG fish that found the diet unpalatable. We have not directly cross-compared treatment groups, as each sample represents an individual fish, treatment groups were in separate tanks, and we had sacrificial temporal sampling thus direct dispersal would have been limited between these communities. As defined by Stegen et al.42, dispersal limitation indicates that a low dispersal rate is the primary cause of high compositional turnover (aiding ecological drift or stochastic processes), although the framework does not account for in situ diversification. This would occur where dispersal rates are low and new OTUs that evolve within a single taxon may only be present in one community. Given the gut structure whereby the digesta content is contained within the digestive tract (i.e., a semi-closed system), of individual fish, diversification could be an uncharacterised influence here.

The digestive system is a space-limited system, stochastic models such as the competitive lottery model can shed light on what species will be first to occupy the niche space and thus, manipulate the conditions for subsequent species. Clades that showed very strong lottery-like behaviour (Alistipes, Cetobacterium, Tyzzerella, and Fusobacterium), primarily only did so at Week 0. This indicated that there was a temporal effect and/or that the physical change from a commercial diet to in-house pellets may have impacted microbial competition for space in the hindgut. To fully elucidate this, earlier time points including the former diet would be required (Experiment started Day 366 post-hatch baseline before changing feed—Week 0). We observed overlap between the genera that correlated with the temporal community dissimilarities at Week 8 and Week 12 and lottery winners (Tyzzerella, Lachnoclostridium, Bacteroides, Rikenella) species. While Photobacterium (Week 0), which decreased over the course of the trial did not conform to the lottery schema. Photobacterium species have a high prevalence in many fish species, including wild cod populations23,57. Notably, Photobacterium was completely absent from lottery winners (i.e., no OTUs were > 90% within this clade in our samples). Species that do not conform to the competitive lottery schema are thought to be less specialised in their niche and co-exist with other species30, which would support the widespread distribution of Photobacterium across fish species19. This result aligns with the gene distribution features showing high functional redundancy at Week 0, whereby multiple taxa can carry out the same function. The prevalence of lottery winners (Bacteroidetes and Firmicutes) increased at Week 8/Week 12 (low functional redundancy/increased unique function). Members of the Bacteroidetes phylum, have been highlighted as highly flexible generalists and specialists58. Authors have noted that the gut microbiome in wild Atlantic cod had limited diversity and exhibited phylogenetic nepotism59. We noted similar, and this was particularly apparent in the ASCO_LG fish. In most of the tested community assembly methods, the ASCO_LG fish did not follow the same trend as the other dietary treatments, showing, for example, temporal trends towards strong phylogenetic underdispersion (more nepotism) and niche assembly. Thus, indicating that microbial community assembly patterns were disrupted in fish that displayed poorer growth rates and found the diet unpalatable. These microbial community assembly patterns may drive unexpected changes in fish condition and function60. This indicates that diet selection could play a role in the disruption of the microbiome development in farmed fish61.

The gut microbiome of any species is integral to the functioning of the system, microbial imbalance can lead to harmful impacts to the host in a condition called dysbiosis62. This occurs when the microbial community changes result in a change in function, leading to altered pathways, and the production of excess acids for example. However, the microbial taxonomic composition of a system can fluctuate without detectable changes to the inherent functioning. We observed taxonomic shifts in the hindgut microbial community over time, and changes in the predicted functional pathways. This may have been related to community imbalance or a natural succession of the communities. In gut microbial communities, the relationship between species taxonomic and functional profiles has been defined as the ‘taxa-function relationship’. This relationship can be viewed as a landscape containing the breadth of microbial taxa and inter-related functional capacities. Using such a landscape, the situations resulting in dysbiosis (microbial imbalance which is harmful to the host) can be assessed. We used the taxa-function robustness measure43 to calculate the breadth of taxonomic shifts (perturbations) and the community functional capacity. In our work, we showed that in the hindgut Atlantic cod microbiome, the microbial communities increased in robustness and functional stability over time, despite temporal taxonomic shifts. Robustness was particularly increased for functions involved in metabolism and cell regulation. Increased robustness in metabolism-based function and cell cycle functions, particularly in the ASCO treatments needs further investigation beyond predictive functions, as we speculate that this result would not necessarily correlate with increased resilience to disturbance. Functional analysis of microbial communities in complex systems, such as the gut has a greater utility than taxonomic profiles63.

There are some potential limitations to our study. In our analysis, we have not considered the source metacommunity (tank seawater). While research has suggested that changes in the gut microbiome of Atlantic cod larvae49 and common molly adults (Poecilia sphenops)64 can occur independently of the tank rearing water, it is an unaccounted-for variable in our present study. Authors have used changes in tank water to manipulate the microbiome of Atlantic cod larvae using ecological theory to improve survival rates using selection65. To use these tools in a controlled and predictable manner we must first unravel what assembly processes are occurring and how we can exploit the microbial interactions. Moreover, targeted manipulations of the gut microbiome with aquafeed ingredients, like probiotics, must consider the interaction between adherent and non-adherent gut microbial communities66, an aspect not explored in this study. Resolving these issues may offer an opportunity to use the gut microbiome to develop fish with the improved condition and immune competence for commercial use as in aquaculture or in wild population restocking programmes.

In summary, the ecological drivers of microbial community assembly in the gut microbiome are important factors to consider when linking microbial community composition and diversity to fish health and environmental parameters. We conclude that the microbiome in the gut of Atlantic cod (G. morhua) in an experimental feeding trial over a twelve-week period was under the influence of multiple assembly processes; stochastic forces shaping the presence or absence of OTUs, deterministic forces and a trend from niche to neutral processes. We quantified these processes as an increase in variable selection in the control diet (divergence in communities related to selective environmental conditions) over time. Dispersal limitation was a driver of the gut microbiome for fish fed the macroalgae supplemented diet at Week 12. Generalist Photobacterium species (Week 0) decreased over the course of the trial and were absent from the lottery model. There was overlap between the genera that were increasing over time and lottery winners (Tyzzerella, Lachnoclostridium, Bacteroides, Rikenella) species at Week 8/Week 12. This corresponded to a shift from high to low functional redundancy. The recruitment of new taxa overtime was altered in the ASCO groups (10% Ascophyllum nodosum supplement), with individuals who found the diet unpalatable exhibiting phylogenetic underdispersion (nepotistic recruitment of species). The ecological processes are summarised in Fig. 7. Finally, the gut microbiome showed increasing robustness to taxonomic disturbance over time, which was increased in the ASCO_LG individuals. These fish showed an altered microbiome, with increased susceptibility to functions related to infectious diseases and cell regulation and increased robustness of metabolism functions. Although our study focused on the juvenile cod gut microbiome, many of these findings are of broad interest in fish research, and indeed to the wider field of gut microbiome research. We highlight research areas that warrant further investigation in fish farming trials; (i) how the host influences ecological assembly over the complete life cycle of Atlantic cod (G. morhua), (ii) increased investigation into gut functional pathways, particularly in response to stress and (iii) microbial network analysis to elucidate the interactions between source water, feed source, adherent, and non-adherent bacteria. These should be subsequently followed up with targeted and informed microbial manipulation experiments. This invaluable information would allow for better animal health management (for Atlantic cod in particular), to increase the resilience of farmed species, particularly towards the use of functional feed additives, such as prebiotics and probiotics for improved gut health.

Fig. 7: Summary of our key findings on microbial assembly in the Atlantic cod hindgut.
figure 7

The schematic figure was created with Biorender.com and shows the changes in community and assembly over time (Week 0, Week 8, and Week 12) and across treatments (Week 0, CTRL, ULVA, ASCO_N, and ASCO_LG).

Methods

Juvenile Atlantic cod (G. morhua) were hand-graded (123 ± 7 g, SD) and randomly allocated to one of nine experimental tanks (three tanks per treatment and 60 fish per tank). Fish were acclimated for one week on a commercial fishmeal diet (Amber Neptun, Skretting, Stavanger, Norway), noted as the Week 0 sampling phase. Then tanks were assigned to the following diets, a 10% dietary macroalgae supplement (either Ulva rigida [ULVA] or Ascophyllum nodosum [ASCO] species) or a control diet for basal comparison, i.e., no algal addition [CTRL]. At Week 8 within the feed trial, a subgroup of the ASCO fish displaying ‘reduced growth rates were observed and were likely due to reduced acceptance of the feed21. We, therefore, subcategorised this group as [ASCO_LG], and the remaining fish with ‘normal’ growth was referred to as [ASCO_N]. The feed trial was carried out for twelve weeks.

Sample collection, DNA extraction and 16S rRNA amplicon sequencing

Fish were removed from the tanks at Week 0, Week 8 and Week 12 and euthanised with an overdose of tricaine methanesulphonate solution (MS222, Pharmaq, Overhalla, Norway). The brain was then destroyed to confirm death according to regulations for animal welfare (EU Directive 2010/63/EU). We then removed the last 10–15% of the digestive tract and placed in sterile microcentrifuge tubes. There were 67 fish gut samples arising from eight fish at Week 0, 28 fish at Week 8 (6 CTRL, 9 ULVA, 8 ASCO_N, 5 ASCO_LG) and 31 fish at Week 12 (8 CTRL, 8 ULVA, 8 ASCO_N, 7 ASCO_LG). Variability in sample numbers was due to some fish not having sufficient gut content for eventual analysis. Samples were transported to the National University of Ireland Galway on dry ice and stored at −80 °C. DNA extractions from hindgut digesta per sample were carried out by phenol-chloroform extraction with an additional bead-beating step using Lysing Matrix E tubes (MP Biomedical, Illkirch-Graffenstaden, France)21,67. Sample DNA and DNA from a negative extraction control (nuclease-free water, Qiagen, Venlo, The Netherlands) were sent to the Research Technology Support Facility at Michigan State University (Michigan, USA) for sequencing. Amplicon sequencing of the 16 S rRNA gene targeting the V4 hypervariable region was performed using the universal primer set [515 f/806r68]. Sequencing was carried out using the Illumina technology using a standard flow cell and 500 cycle v2 reagent cartridge (Illumina Inc., Hayward, California, USA).

Ethics approval and consent to participate

The feeding trial was carried out in 2014 at the Carna Research Station, Carna, Co. Galway, Ireland, a Health Products Regulatory Authority (HPRA) licensed institution. All personnel involved in the feed trial work were Laboratory Animal Safety Trained Ireland (LAST-Ireland) with individual authorisation as per our previous publication21.

Bioinformatics

The methods to generate all microbial data (e.g., operational taxonomic units (OTUs), phylogenetic trees and biom. files) are given in Supplementary Methods.

Subset analysis

For finding key microbial species that contribute to beta-diversity between samples over time we used the “BVSTEP” routine69. This method reduces the abundance table down to the subset of OTUs which can roughly still explain the same beta-diversity pattern as the full OTU table, therefore finding the key OTUs. Briefly, the method calculates the Bray-Curtis distance between samples using all the OTUs and records it as original distances. It then permutes through the subset of OTUs, and for each permutation, it calculates the Bray-Curtis distances between the samples again and correlates these distances against the original recorded distances until subsets are obtained that explain roughly the same beta diversity as the full set of OTUs. To run this algorithm, bvStep() (from the sinkr package) was used70. After obtaining the subset of OTUs, we used R’s ‘Vegan’ package71, particularly the bioenv () function to regress the subsets on top of the principal coordinate analysis (PCOA) plot.

Microbial community assembly

Hill-numbers dissimilarity indices (q d)

Hill numbers are a set of indices parameterised by q representing the diversity order which determines the weight given to the relative abundance of OTUs in a community. Modin et al.37 derived the beta-diversity equivalent of hill numbers (qd) as a dissimilarity index of diversity order where qd values are scaled between 0 (similar) and 1 (dissimilar). The authors used this approach to illustrate how OTU abundance contributes to the dissimilarity between communities. Here, we compared qd at q = 0 (presence/absence, i.e., Jaccard index), q = 1 (OTUs abundances are weighted i.e., Bray-Curtis) and q = >1 (OTUs with greater relative abundance have increased weighting). Further, a randomisation scheme was applied and repeated many times to obtain the null distribution for the dissimilarities across this scale between communities. These null distributions when compared to the observed dissimilarity (qd) reveal ecological insights, i.e., if the values are similar, the observed dissimilarity can be explained by stochastic factors, and if higher or lower than the null expectation, then there are likely deterministic factors that favour different or similar microbial taxa in two categories. These indices and null distributions were calculated using the qdiv Python software37.

Beta-null model

Beta-null deviation measures were calculated according to Tucker et al. and Lee et al.34,40. The method first calculates the pairwise observed dissimilarities (βobs) between samples using the Generalised Unifrac dissimilarity measure. By preserving the alpha diversity in the observed samples, random communities are generated (999 randomisations) to calculate the beta diversity measure again for these communities (βnull) and then the deviation from the observed dissimilarities are recorded. The average of the deviations gives a numerical value that differentiates between niche (values further from 0) and neutrally structured communities (values nearer to 0). We have done this separately for each treatment group on a temporal basis (Week 0, CTRL_08, ULVA_08, ASCO_N_08, ASCO_LG_08, CTRL_12, ULVA_12, ASCO_N_12, and ASCO_LG_12).

Quantitative process elements

Quantitative process elements (QPE) were used to assess the influence of ecological processes based on the conceptual framework of Vellend et al.72 and implemented according to Stegen et al.41,42. This framework provides a quantitative measure of the influence of selection and dispersal pressures on microbial community structure. Selection considers deterministic selective pressure which results in divergent (variable selection), or convergent (homogenous selection) communities often considered over time. While dispersal considers the spatial movement of species where the increased movement of species results in convergent communities (homogenising dispersal), or limited movement of species results in divergent communities through drift (dispersal limitation). The authors also included the category ‘Undominated’ to describe the situation whereby neither selection nor dispersal processes dominate. The framework considers the phylogenetic distance and phylogenetic turnover between closely related OTUs in pairwise samples28. This is achieved using the abundance-weighted β-mean-nearest taxon distance (βMNTD)73. To determine how this varied from the null expectation, randomisations were employed whereby the abundances and species names were shuffled across phylogenies to provide a null value41. This was replicated 999 times to give the null distribution. The deviation between the null distribution and the observed βMNTD value = β-nearest taxon index (βNTI). If the observed βMNTD value is significantly greater (βNTI > 2) or less (βNTI < − 2) than the null expectation, the community is assembled by Variable or Homogeneous Selection, respectively. For the remaining with no significant deviation, in the next step, Raup-Crick was used with the inclusion of OTU relative abundance38 termed RCbray. RCbray values were compared to the null expectation and the resulting deviation determined the influence of dispersal (RCbray > 0.95). Values of RCbray > −0.95 indicate Homogenising Dispersal (transport between microbiomes leading to establishment), while values of RCbray > +0.95 indicate Dispersal Limitation. In the latter, this may indicate ‘true’ effects of dispersal limitation (i.e., limited transport across microbiomes and stochastic events) and/or historical contingency. In cases where values were <0.95 the communities were ‘Undominated’, i.e., not dominated by a sole ecological process (weak selection and moderate drift).

Competitive lottery model

We applied the competitive lottery model as outlined in Verster and Borenstein30 which is based on the theory of Sale74 first proposed for fish populations. The theory is based on the idea that there is competition between colonising species within a niche and only a single species can ‘win’ in the space (strong priority effect). This ‘winner’ is chosen at random (stochastic process) with an analogy drawn to a ‘lottery’. In microbial ecology this scheme determines clade-based assembly, i.e., within a taxonomic group (a genus), we can determine if the group follows lottery-like behaviour and if so what OTUs ‘win’. A winning species/OTU is defined as a clade member with >90% abundance [see Verster and Borenstein30 for details on how this threshold was determined]. Then the diversity of lottery winners was calculated using Shannon diversity index of the winners across samples (how often each OTU occurs as a winner in samples where lottery-like behaviour was observed). Diversity was normalised between 0 and 1 to account for differences in lottery winners. Values approaching 0 indicate that a single OTU is dominating that specific genus in all samples, while values approaching 1 indicate an even distribution of winning OTUs within a genus.

Phylogenetic recruitment model

The phylogenetic recruitment model75 was then used to describe the order in which new species are detected in the cod hindgut microbiome over time. In this model, the Dispersion parameter (D) is calculated based on the probability of detection of new species on temporal scales by fitting a logistic error model on changes in phylogenetic diversity (PD) estimates. As opposed to the previous models, time-series dependency is assumed. The value of D determines the primary recruitment mechanisms, where D = 0 indicates that all species have an equiprobable chance of recruitment. If D > 0 then taxa that are more phylogenetically divergent (to the taxa detected in previous time-points) are preferentially added to the community (overdispersion). In contrast, if D < 0 then taxa that are more phylogenetically similar (to the taxa detected in previous time-points) are preferentially added to the community (underdispersion).

Functional analysis and taxa-function robustness

Functional analysis

The functional potential was obtained as KEGG orthologs (KO) and pathway predictions by using Phylogenetic Investigation of Communities by Reconstruction of Unobserved States (PICRUSt2)76 and the Quantitative Insights into Microbial Ecology (QIIME2) plugin77 using the parameters --p-hsp-method pic --p-max-nsti 2. To find KEGG enzymes/MetaCyc pathways that are significantly different between different categories, we used DESeqDataSetFromMatrix() function from DESeq278 package with the adjusted P-value significance cut-off of 0.05 and log2 fold change cut-off of 2. This function uses a negative binomial general linear model to obtain maximum likelihood estimates for OTUs log fold change between two conditions. Then Bayesian shrinkage is applied to obtain shrunken log-fold changes subsequently employing the Wald test for obtaining significances. For KEGG orthologs that were at least log2 fold significant, we used iPath379 to give an overview of KEGG pathways for microbial metabolic function.

Taxa-function robustness

Following the procedure of Eng and Borenstein43, the taxa-function robustness measure of the cod hindgut microbial communities was calculated. The principle of the taxa-function robustness measure is to perturb an individual sample several times (100 perturbations) and then calculate a two-dimensional profile of taxonomic shift versus functional shift. To create the taxonomic profiles, weighted Unifrac dissimilarities were calculated across samples and simulated perturbations. To obtain predicted functional profiles, the authors calculated the KEGG Orthology (KO)roups for the whole green genes database (gg_13_5) along with KO copy numbers provided as a reference database (https://github.com/borenstein-lab/robustness), which can be used if the OTUs follow the green genes nomenclature. For the functional profiles, cosine dissimilarities were calculated across samples and simulated perturbations. After obtaining the taxonomic and functional shifts (both denoted as t) for a given sample, a relationship between taxonomic perturbation magnitude and functional profile shift is assumed to behave individually as \(f = \frac{1}{{e^a}}t^b\) and fitted using the linear regression model on natural log transformed data: \(\ln \left( f \right) = - a + b\ln (t)\). In the equation, f. denotes the expected shift in functional profile and we can estimate a (termed as “attenuation” coefficient describing the expected rate at which increases in the taxonomic perturbation magnitude are expected to increase functional profile shifts) and b (termed as “buffering” coefficient indicating how large a perturbation must be before a functional profile shift becomes noticeable). The coefficients thus serve as proxies (robustness factors) to summarise the property of a sample to withstand perturbation. These were calculated for all the samples in the dataset. Additionally, the main gene distribution features (GDFs) across the genomes of species in a community, were then displayed as a PCOA plot. Further details can be found in Eng and Borenstein43.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

The raw sequences are available in the SRA database under Bioproject Submission PRJNA636649.

References

  1. FAO. The State of World Fisheries and Aquaculture 2020. Sustainability in action. Rome. https://doi.org/10.4060/ca9229en (2020).

  2. Nardi, G., Prickett, R., Meeren, T., van der, Boyce, D. & Moir, J. Atlantic cod aquaculture: Boom, bust, and rebirth? J. World Aquac. Soc. 52, 672–690 (2021).

    Article  Google Scholar 

  3. Kjesbu, O. S., Taranger, G. L. & Trippel, E. A. Gadoid mariculture: development and future challenges. ICES J. Mar. Sci. 63, 187–191 (2006).

    Article  Google Scholar 

  4. Vadstein, O., Attramadal, K. J. K., Bakke, I. & Olsen, Y. K-selection as microbial community management strategy: a method for improved viability of larvae in aquaculture. Front. Microbiol. 9, https://doi.org/10.3389/fmicb.2018.02730 (2018).

  5. Karlsen, Ø., Norberg, B., Kjesbu, O. S. & Taranger, G. L. Effects of photoperiod and exercise on growth, liver size, and age at puberty in farmed Atlantic cod (Gadus morhua L.). ICES J. Mar. Sci. 63, 355–364 (2006).

    Article  Google Scholar 

  6. Taranger, G., Aardal, L., Hansen, T. & Kjesbu, O. Continuous light delays sexual maturation and increases growth of Atlantic cod (Gadus morhua L.) in sea cages. ICES J. Mar. Sci. 63, 365–375 (2006).

    Article  Google Scholar 

  7. Puvanendran, V. et al. Development of cod farming in Norway: Past and current biological and market status and future prospects and directions. Rev. Aquac. 14, 308–342 (2021).

  8. Wan, A. H. L., Davies, S. J., Soler-Vila, A., Fitzgerald, R. & Johnson, M. P. Macroalgae as a sustainable aquafeed ingredient. Rev. Aquac. 11, 458–492 (2019).

    Article  Google Scholar 

  9. Wan, A. H. L. et al. The inclusion of Palmaria palmata macroalgae in Atlantic salmon (Salmo salar) diets: effects on growth, haematology, immunity and liver function. J. Appl. Phycol. 28, 3091–3100 (2016).

    CAS  Article  Google Scholar 

  10. Niu, J. et al. Dietary values of macroalgae Porphyra haitanensis in Litopenaeus vannamei under normal rearing and WSSV challenge conditions: Effect on growth, immune response and intestinal microbiota. Fish. Shellfish Immunol. 81, 135–149 (2018).

    CAS  PubMed  Article  Google Scholar 

  11. Ringø, E., Erik Olsen, R., Gonzalez Vecino, J. L. & Wadsworth, S. Use of immunostimulants and nucleotides in aquaculture: a review. J. Mar. Sci.: Res. Dev. 02, (2011).

  12. Dawood, M. A., Koshio, S. & Esteban, M. Á. Beneficial roles of feed additives as immunostimulants in aquaculture: a review. Rev. Aquac. 10, 950–974 (2018).

    Article  Google Scholar 

  13. Gupta, S. et al. Macroalga-derived alginate oligosaccharide alters intestinal bacteria of Atlantic Salmon. Front. Microbiol. 10, https://doi.org/10.3389/fmicb.2019.02037 (2019).

  14. Azeredo, R. et al. The European seabass (Dicentrarchus labrax) innate immunity and gut health are modulated by dietary plant-protein inclusion and prebiotic supplementation. Fish. Shellfish Immunol. 60, 78–87 (2017).

    CAS  PubMed  Article  Google Scholar 

  15. Perry, W. B., Lindsay, E., Payne, C. J., Brodie, C. & Kazlauskaite, R. The role of the gut microbiome in sustainable teleost aquaculture. Proc. R. Soc. B: Biol. Sci. 287, 20200184 (2020).

    CAS  Article  Google Scholar 

  16. Dehler, C. E., Secombes, C. J. & Martin, S. A. M. Environmental and physiological factors shape the gut microbiota of Atlantic salmon parr (Salmo salar L.). Aquaculture 467, 149–157 (2017).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  17. Li, T. et al. Alterations of the gut microbiome of largemouth bronze gudgeon (Coreius guichenoti) suffering from furunculosis. Sci. Rep. 6, 30606 (2016).

  18. Riera, J. L. & Baldo, L. Microbial co-occurrence networks of gut microbiota reveal community conservation and diet-associated shifts in cichlid fishes. Anim. Microbiome 2, 36 (2020).

    PubMed  PubMed Central  Article  Google Scholar 

  19. Egerton, S., Culloty, S., Whooley, J., Stanton, C. & Ross, R. P. The Gut Microbiota of Marine Fish. Front. Microbiol. 9, https://doi.org/10.3389/fmicb.2018.00873 (2018).

  20. Gallo, B. D., Farrell, J. M. & Leydet, B. F. Fish gut microbiome: a primer to an emerging discipline in the fisheries sciences. Fisheries 45, 271–282 (2020).

    Article  Google Scholar 

  21. Keating, C. et al. Temporal changes in the gut microbiota in farmed Atlantic cod (Gadus morhua) outweigh the response to diet supplementation with macroalgae. Anim. Microbiome 3, 7 (2021).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  22. Lauzon, H. L. et al. Effects of bacterial treatment at early stages of Atlantic cod (Gadus morhua L.) on larval survival and development. J. Appl. Microbiol. 108, 624–632 (2010).

    CAS  PubMed  Article  Google Scholar 

  23. Riiser, E. S. et al. Single vibrionales 16S rRNA oligotype dominates the intestinal microbiome in two geographically separated Atlantic cod populations. Front Microbiol. 9 (2018).

  24. Mora, C., Chittaro, P. M., Sale, P. F., Kritzer, J. P. & Ludsin, S. A. Patterns and processes in reef fish diversity. Nature 421, 933–936 (2003).

    CAS  PubMed  Article  Google Scholar 

  25. Caro, A. U., Navarrete, S. A. & Castilla, J. C. Ecological convergence in a rocky intertidal shore metacommunity despite high spatial variability in recruitment regimes. Proc. Natl Acad. Sci. USA 107, 18528–18532 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  26. Pagaling, E. et al. Assembly of microbial communities in replicate nutrient-cycling model ecosystems follows divergent trajectories, leading to alternate stable states. Environ. Microbiol. 19, 3374–3386 (2017).

    CAS  PubMed  Article  Google Scholar 

  27. Vass, M., Székely, A. J., Lindström, E. S. & Langenheder, S. Using null models to compare bacterial and microeukaryotic metacommunity assembly under shifting environmental conditions. Sci. Rep. 10, 2455 (2020).

  28. Stegen, J. C., Lin, X., Konopka, A. E. & Fredrickson, J. K. Stochastic and deterministic assembly processes in subsurface microbial communities. ISME J. 6, 1653–1664 (2012).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  29. Zhou, J. & Ning, D. Stochastic community assembly: does it matter in microbial ecology? Microbiol Mol. Biol. Rev. 81, e00002-17 (2017). e00002-17.

    PubMed  PubMed Central  Article  Google Scholar 

  30. Verster, A. J. & Borenstein, E. Competitive lottery-based assembly of selected clades in the human gut microbiome. Microbiome 6, 186 (2018).

    PubMed  PubMed Central  Article  Google Scholar 

  31. Sprockett, D., Fukami, T. & Relman, D. A. Role of priority effects in the early-life assembly of the gut microbiota. Nat. Rev. Gastroenterol. Hepatol. 15, 197–205 (2018).

    PubMed  PubMed Central  Article  Google Scholar 

  32. Fukami, T. Historical contingency in community assembly: integrating niches, species pools, and priority effects. Annu. Rev. Ecol., Evolution, Syst. 46, 1–23 (2015).

    Article  Google Scholar 

  33. Urban, M. C. & Meester, L. D. Community monopolization: local adaptation enhances priority effects in an evolving metacommunity. Proc. R. Soc. B: Biol. Sci. 276, 4129–4138 (2009).

    Article  Google Scholar 

  34. Tucker, C. M., Shoemaker, L. G., Davies, K. F., Nemergut, D. R. & Melbourne, B. A. Differentiating between niche and neutral assembly in metacommunities using null models of β-diversity. Oikos 125, 778–789 (2016).

    Article  Google Scholar 

  35. Polunin, N. Ecosystem theory and application. (Wiley, 1986).

  36. Derome, N. & Filteau, M. A continuously changing selective context on microbial communities associated with fish, from egg to fork. Evolut. Appl. 13, 1298–1319 (2020).

    Article  Google Scholar 

  37. Modin, O. et al. Hill-based dissimilarity indices and null models for analysis of microbial community assembly. Microbiome 8, 132 (2020).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  38. Chase, J. M., Kraft, N. J. B., Smith, K. G., Vellend, M. & Inouye, B. D. Using null models to disentangle variation in community dissimilarity from variation in α-diversity. Ecosphere 2, 1–11 (2011).

  39. Raup, D. M. & Crick, R. E. Measurement of faunal similarity in paleontology. J. Paleontol. 53, 1213–1227 (1979).

    Google Scholar 

  40. Lee, S.-H., Sorensen, J. W., Grady, K. L., Tobin, T. C. & Shade, A. Divergent extremes but convergent recovery of bacterial and archaeal soil communities to an ongoing subterranean coal mine fire. ISME J. 11, 1447–1459 (2017).

    PubMed  PubMed Central  Article  Google Scholar 

  41. Stegen, J. C. et al. Quantifying community assembly processes and identifying features that impose them. ISME J. 7, 2069–2079 (2013).

    PubMed  PubMed Central  Article  Google Scholar 

  42. Stegen, J. C., Lin, X., Fredrickson, J. K. & Konopka, A. E. Estimating and mapping ecological processes influencing microbial community assembly. Front. Microbiol. 6 (2015).

  43. Eng, A. & Borenstein, E. Taxa-function robustness in microbial communities. Microbiome 6, 45 (2018).

    PubMed  PubMed Central  Article  Google Scholar 

  44. Bozzi, D. et al. Salmon gut microbiota correlates with disease infection status: potential for monitoring health in farmed animals. Anim. Microbiome 3, 30 (2021).

    PubMed  PubMed Central  Article  Google Scholar 

  45. Nayak, S. K. Role of gastrointestinal microbiota in fish. Aquac. Res. 41, 1553–1573 (2010).

    Article  Google Scholar 

  46. Ray, A. K., Ghosh, K. & Ringø, E. Enzyme-producing bacteria isolated from fish gut: a review. Aquac. Nutr. 18, 465–492 (2012).

    CAS  Article  Google Scholar 

  47. Xiao, F. et al. Host development overwhelms environmental dispersal in governing the ecological succession of zebrafish gut microbiota. npj Biofilms Microbiomes 7, 1–12 (2021).

    Article  Google Scholar 

  48. Vestrum, R. I., Attramadal, K. J. K., Vadstein, O., Gundersen, M. S. & Bakke, I. Bacterial community assembly in Atlantic cod larvae (Gadus morhua): contributions of ecological processes and metacommunity structure. FEMS Microbiol. Ecol. 96, https://doi.org/10.1093/femsec/fiaa163 (2020).

  49. Bakke, I., Coward, E., Andersen, T. & Vadstein, O. Selection in the host structures the microbiota associated with developing cod larvae (Gadus morhua): Ontogeny of cod larval microbiota. Environ. Microbiol 17, 3914–3924 (2015).

    PubMed  Article  Google Scholar 

  50. Li, X. et al. Composition of Gut Microbiota in the Gibel Carp (Carassius auratus gibelio) Varies with Host Development. Microb. Ecol. 74, 239–249 (2017).

    PubMed  Article  Google Scholar 

  51. Yan, Q., van der Gast, C. J. & Yu, Y. Bacterial community assembly and turnover within the intestines of developing zebrafish. PLoS ONE 7, e30603 (2012).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  52. Armstrong, M. J., Gerritsen, H. D., Allen, M., McCurdy, W. J. & Peel, J. A. D. Variability in maturity and growth in a heavily exploited stock: cod (Gadus morhua L.) in the Irish Sea. ICES J. Mar. Sci. 61, 98–112 (2004).

    Article  Google Scholar 

  53. Heys, C. et al. Neutral processes dominate microbial community assembly in Atlantic Salmon, Salmo salar. Appl. Environ. Microbiol. 86, https://doi.org/10.1128/AEM.02283-19 (2020).

  54. Ofiteru, I. D. et al. Combined niche and neutral effects in a microbial wastewater treatment community. Proc. Natl Acad. Sci. USA 107, 15345–15350 (2010).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  55. López Nadal, A. et al. Feed, microbiota, and gut immunity: using the Zebrafish model to understand fish health. Front. Immunol. 11, 114 (2020).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  56. Robinson, C. D. et al. Experimental bacterial adaptation to the zebrafish gut reveals a primary role for immigration. PLoS Biol. 16, e2006893 (2018).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  57. Le Doujet, T. et al. Closely-related Photobacterium strains comprise the majority of bacteria in the gut of migrating Atlantic cod (Gadus morhua). Microbiome 7, 64 (2019).

    PubMed  PubMed Central  Article  Google Scholar 

  58. Johnson, E. L., Heaver, S. L., Walters, W. A. & Ley, R. E. Microbiome and metabolic disease: revisiting the bacterial phylum Bacteroidetes. J. Mol. Med (Berl.) 95, 1–8 (2017).

    CAS  Article  Google Scholar 

  59. Riiser, E. S. et al. Switching on the light: using metagenomic shotgun sequencing to characterize the intestinal microbiome of Atlantic cod. Environ. Microbiol. 21, 2576–2594 (2019).

    CAS  PubMed  Article  Google Scholar 

  60. Tarnecki, A. M., Burgos, F. A., Ray, C. L. & Arias, C. R. Fish intestinal microbiome: diversity and symbiosis unravelled by metagenomics. J. Appl. Microbiol. 123, 2–17 (2017).

    CAS  PubMed  Article  Google Scholar 

  61. Parata, L., Mazumder, D., Sammut, J. & Egan, S. Diet type influences the gut microbiome and nutrient assimilation of Genetically Improved Farmed Tilapia (Oreochromis niloticus). PLoS ONE 15, e0237775 (2020).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  62. Petersen, C. & Round, J. L. Defining dysbiosis and its influence on host immunity and disease. Cell. Microbiol. 16, 1024–1033 (2014).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  63. Shanahan, F., Ghosh, T. S. & O’Toole, P. W. The healthy microbiome—what is the definition of a healthy gut microbiome? Gastroenterology 160, 483–494 (2021).

    PubMed  Article  Google Scholar 

  64. Schmidt, V. T., Smith, K. F., Melvin, D. W. & Amaral-Zettler, L. A. Community assembly of a euryhaline fish microbiome during salinity acclimation. Mol. Ecol. 24, 2537–2550 (2015).

    PubMed  Article  Google Scholar 

  65. Vestrum, R. I. et al. Rearing water treatment induces microbial selection influencing the microbiota and pathogen associated transcripts of Cod (Gadus morhua) Larvae. Front. Microbiol. 9, https://doi.org/10.3389/fmicb.2018.00851 (2018).

  66. Li, X. et al. The adherence and colonization of microorganisms in fish gastrointestinal tract. Rev. Aquac. 11, 603–618 (2019).

    CAS  Article  Google Scholar 

  67. Griffiths, R. I., Whiteley, A. S., O’Donnell, A. G. & Bailey, M. J. Rapid method for coextraction of DNA and RNA from natural environments for analysis of ribosomal DNA- and rRNA-based microbial community composition. Appl. Environ. Microbiol. 66, 5488–5491 (2000).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  68. Caporaso, J. G. et al. N. Ultra-high-throughput microbial community analysis on the Illumina HiSeq and MiSeq platforms. ISME J. 6, 1621–1624 (2012).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  69. Clarke, K. R. & Ainsworth, M. A method of linking multivariate community structure to environmental variables. Mar. Ecol. Prog. Ser. 92, 205–219 (1993).

    Article  Google Scholar 

  70. Taylor, M. Sinkr: A collection of functions featured on the blog’Me nugget’. R package version 1.0. Available at https://github.com/marchtaylor/sinkr (2014). Accessed May, 2021.

  71. Oksanen, J. et al. vegan: Community Ecology Package. R package version 2.5-7. https://CRAN.R-project.org/package=vegan (2020).

  72. Vellend, M. Conceptual synthesis in community ecology. Q. Rev. Biol. 85, 183–206 (2010).

    PubMed  Article  Google Scholar 

  73. Fine, P. V. A. & Kembel, S. W. Phylogenetic community structure and phylogenetic turnover across space and edaphic gradients in western Amazonian tree communities. Ecography 34, 552–565 (2011).

    Article  Google Scholar 

  74. Sale, P. F. Maintenance of high diversity in Coral reef fish communities. Am. Naturalist 111, 337–359 (1977).

    Article  Google Scholar 

  75. Darcy, J. L. et al. A phylogenetic model for the recruitment of species into microbial communities and application to studies of the human microbiome. ISME J. 14, 1359–1368 (2020).

    PubMed  PubMed Central  Article  Google Scholar 

  76. Douglas, G. M. et al. PICRUSt2 for prediction of metagenome functions. Nat. Biotechnol. 38, 685–688 (2020).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  77. Bolyen, E. et al. Reproducible, interactive, scalable and extensible microbiome data science using QIIME 2. Nat. Biotechnol. 37, 852–857 (2019).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

  78. Love, M. I., Huber, W. & Anders, S. Moderated estimation of fold change and dispersion for RNA-seq data with DESeq2. Genome Biol. 15, 550 (2014).

    PubMed  PubMed Central  Article  CAS  Google Scholar 

  79. Darzi, Y., Letunic, I., Bork, P. & Yamada, T. iPath3. 0: interactive pathways explorer v3. Nucleic Acids Res. 46, W510–W513 (2018).

    CAS  PubMed  PubMed Central  Article  Google Scholar 

Download references

Acknowledgements

We dedicate this paper to Dr Richard Fitzgerald, a dear colleague and friend, 1957–2016. The authors also kindly acknowledge all staff at the Carna Research Station, National University of Ireland Galway, Carna, Co. Galway, Ireland for their technical assistance during the feed trial. This study was part-funded by the EIRCOD (Cod Broodstock and Breeding) project, under the Sea Change Strategy with the support of the Marine Institute and the Marine Research Sub-programme of Ireland’s National Development Plan 2007–2013 co-funded by the European Regional Development Fund, and also NutraMara programme (Grant-Aid Agreement No. MFFRI/07/01) under the Sea Change Strategy with the support of Ireland’s Marine Institute and the Department of Agriculture, Food and the Marine. C.S. was funded by Science Foundation Ireland & the Marie-Curie Action COFUND under Grant Number 11/SIRG/B2159 and a Royal Academy of Engineering-Scottish Water Research Chair Grant Number: RCSRF1718643. UZI is supported by NERC, UK, NE/L011956/1.

Author information

Authors and Affiliations

Authors

Contributions

C.K. dissected the fish for microbiome sampling, DNA extraction optimisation and extractions on the gut content, bioinformatics, statistical analysis, and data interpretation. M.B.W. managed the feeding trial, coordinated sampling and data management of tank populations. J.H. and R.D. ran the feeding trial and assisted with sampling. S.W. ran the feeding trial and assisted with dissections for microbiome analysis. A.H.L.W. was responsible for seaweed identification and collection, designed the test diets and feed analysis. U.Z.I. wrote the analysis scripts and performed the microbiota bioinformatic and statistical analysis, and data interpretation with C.K. U.Z.I. and C.K. conceived the ecological assembly research question study. While C.J.S., R.F., M.B.W., S.J.D., and A.H.L.W. designed the experimental feeding-trial study. C.K. and U.Z.I. wrote the manuscript, which was reviewed and edited by all authors. R.F. was EIRCOD Project Coordinator. All authors made a substantial contribution towards the research study and all authors (except RF) approved the final manuscript.

Corresponding author

Correspondence to U. Z. Ijaz.

Ethics declarations

Competing interests

The authors declare no competing interests.

Additional information

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

Supplementary information

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as 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 images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Keating, C., Bolton-Warberg, M., Hinchcliffe, J. et al. Drivers of ecological assembly in the hindgut of Atlantic Cod fed a macroalgal supplemented diet. npj Biofilms Microbiomes 8, 36 (2022). https://doi.org/10.1038/s41522-022-00296-x

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://doi.org/10.1038/s41522-022-00296-x

Search

Quick links

Nature Briefing

Sign up for the Nature Briefing newsletter — what matters in science, free to your inbox daily.

Get the most important science stories of the day, free in your inbox. Sign up for Nature Briefing