IMR Press / FBE / Volume 14 / Issue 3 / DOI: 10.31083/j.fbe1403016
Open Access Original Research
Does a Diet Rich in the Bacterium Rhodopirellula rubra Improve Daphnia magna Performance?
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1 Departamento de Biologia da Faculdade de Ciências da Universidade do Porto (FCUP), 4169-007 Porto, Portugal
2 Centro Interdisciplinar de Investigação Marinha e Ambiental (CIIMAR/CIMAR), 4450-208 Matosinhos, Portugal
3 Paralab, SA, 5040-535 Valbom, Portugal
4 CEBIMED - Faculdade de Ciências da Saúde da Universidade Fernando Pessoa (FCS-UFP), 5040-535 Valbom, Portugal
*Correspondence: scantunes@fc.up.pt (Sara C. Antunes); olga.lage@fc.up.pt (Olga M. Lage)
Academic Editors: Neven Zarkovic and Guoyao Wu
Front. Biosci. (Elite Ed) 2022, 14(3), 16; https://doi.org/10.31083/j.fbe1403016
Submitted: 22 December 2021 | Revised: 3 March 2022 | Accepted: 10 March 2022 | Published: 29 June 2022
Copyright: © 2022 The Author(s). Published by IMR Press.
This is an open access article under the CC BY 4.0 license.
Abstract

Background: In the wild various organisms contribute to daphnids diet. This study, intendeds to evaluate the potential of the concentration of Rhodopirellula rubra as a single or supplementary food source for Daphnia magna. Methods: Feeding assays were performed according to standard guidelines for chronic assays (21 days), and life-history parameters and several biomarkers (protein content, oxidative stress, energetic reserves and pigments) were measured. Five food regimens were conducted with 20 individual replicates (A - R. subcapitata; 0.2 - suspension of R. rubra at 0.2 arbitrary units (AU); 0.4 - suspension of R. rubra at 0.4 AU; 0.2+A - suspension of R. rubra at 0.2+alga; 0.2+A-suspension of R. rubra at 0.4 AU + alga). Additionally, the effects of three diets (A, 0.2, and 0.2+A) on the longevity of D. magna were assessed. Results: The five diets showed a different C, N, and carotenoids composition, with an increase in the mixed diets. The results confirmed that the mixed diets improved D. magna life-history parameters. A decrease in glycogen, and the increase of haemoglobin, protein, and gluthione-S-transferase (GST) were observed. Furthermore, D. magna fed with bacterial single diets, presented worsen life history parameters and a decrease in the protein content. An induction of oxidative stress response (increased catalase and GST), and a significant decrease in lipid peroxidation and an accumulation of glycogen and carotenoids were observed. Overall, an increase in the amount of R. rubra provided to D. magna, from 0.2 AU to 0.4 AU, negatively impacted daphnid performance. No significant effects on Daphnia longevity (a 110-day assay) were observed among the three diets tested. However, a significant survival percentage and fertility (cumulative offspring is more than twice) was observed when D. magna was fed with the mixed diet. Conclusions: Results demonstrated that different diets provided a nutritional diversified food to the daphnids that induced differences in D. magna performance. The mixed diets proved to be beneficial (with increase in offspring) on D. magna performance, independently of the bacterial concentration tested. When in single diet, bacterial concentration is not nutritionally sufficient to raise D. magna even when in increased concentration.

Keywords
life history
fecundity
carbon
nitrogen
proteins and carotenoids content
oxidative stress
haemoglobin
lipid peroxidation
1. Introduction

The freshwater crustacean species of the genus Daphnia is a versatile model organism that has long been used in several areas of research [1, 2, 3, 4, 5, 6, 7]. In addition, among the live zooplankton, Daphnia spp. are a valuable food for small freshwater fishes and are also used as an ingredient in the formulation of commercial foods [8, 9, 10]. Furthermore, Daphnia is recognized as a sentinel species of freshwater ecosystems because its decline is an indicator of environmental impacts [3]. This characteristic associated with parthenogenic reproduction, short life cycle, high fecundity, and easy laboratory maintenance, makes them commonly used tool in toxicity assessments [11, 12, 13, 14, 15, 16, 17]. Normally, these organisms are maintained in laboratory conditions during several generations for use in biological research. For the laboratory maintenance, one must consider several factors that influence the performance and the health of these organisms and the responses to experimental conditions tested. Diet, in terms of quality and quantity of food, is a predominant factor that impacts Daphniaperformance due to its effects on life-history parameters such as growth, reproduction, and survival [18, 19], and response in the presence of toxics [20, 21, 22]. The algae-based diet is standardized under laboratory conditions because of its sufficiency, reliability, and simplicity. However, reliance on a single carbon source can lead to fluctuations in Daphnia performance [23, 24]. Indeed, previous studies have shown that Cladocera’s exhibits different responses when subjected to different algae as food source [25, 26]. Jonczyk et al. [27] reviewed notions about culture and maintenance in the laboratory and suggested that survival and reproduction in Daphnia were improved on mixed diets comparatively to a single algal diet. In fact, several studies addressed the effects of mixed diets on Cladocera’s fitness [28, 29, 30], while others evaluate alternative food sources that complement and diversify their diet [31, 32].

Aquatic ecosystems have a considerable amount of bacteria which contribute to the diet of Daphnia spp. since they are non-selective filters. Previous studies conducted by Antunes et al. [33] and Marinho et al. [34, 35] already showed the potential of Planctomycetes, namely Rhodopirellula rubra, to be a good supplementary food source when used in association with the standard food source (the microalgae Raphidocelis subcapitata), and its capacity to improve Daphnia magna life history parameters and in providing pink coloration. The authors also observed that these effects of R. rubra were more relevant at the exponential growth phase than the stationary growth phase. Furthermore, D. magna performance with mixed diets with two different planctomycetes, R. rubra and Gemmata obscuriglobus, was also assessed. Even though G. obscuriglobus produces sterols, molecules fundamental in nutritional terms for D. magna, R. rubra induced a better D. magna performance [34]. Also, an increase of MUFAs content in D. magna fatty acid’ profile associated with the diet rich in R. rubra was found and the pink color displayed by bacteria was retained by mothers and observed in the offspring [35]. However, R. rubra showed not to be sufficient when used as a single food. In face of these results, one may question if the amount of bacterium provided as food has been sufficient for the welfare of D. magna as well as its ability to grow, reproduce and survive? Several studies reported that the amount of food affects growth, longevity, and reproduction in Daphnia spp. [18, 19, 36]. So, the question about bacterial concentration used in our previous studies for D. magna was raised. It is still unclear if the previous concentration of bacterium provided was sufficient regarding the nutritional value, and which are the physiological consequences of the increase of bacterial concentration on D. magna. In natural habitats, organisms are subject to wide seasonal variations in food concentration [37] in contrast to a constant food supply under laboratorial conditions. The responses in life history parameters of aquatic organisms may be related to variation in food availability being indicative of the status of the ecosystem.

As a follow up of our previous studies, we aimed to evaluate the adequacy of a single R. rubra diet and a mixed diet (R. rubra plus R. subcapitata) in two different bacterial concentrations in the D. magnaperformance along a chronic exposure (21 days). This assessment was based on the analysis of life-history parameters, and several physiological parameters: energetic reserves-protein and glycogen content; pigments-carotenoids and haemoglobin content; oxidative stress-antioxidant catalase (CAT) activity, detoxification glutathione S-transferase (GST) activity and lipid peroxidation (thiobarbituric acid assay-TBARS levels), and also on carbon, nitrogen, and carotenoids contents of the diets Furthermore, the effect of diets with the low amount of bacterium in D. magna longevity was also evaluated, regarding the life-history parameters.

2. Materials and Methods
2.1 Cultures of Organisms

The planctomycete R. rubra LF2 was isolated from the biofilm community of the marine macroalga Laminaria sp. from the north coast of Portugal [38]. R. rubra strain LF2 was first grown on solid modified M13 medium [38] at 26 °C and then transferred into liquid modified M13 medium with continuous stirring at 200 rpm. The culture was upscaled each three days, in exponential growth phase, starting with a culture volume of 50 mL, passed to 250 mL and finally to 1.5 L using always a 1:10 volume of inoculum. Cells in exponential growth phase (3 days of growth) were collected by centrifugation at 4000 rpm for 10 min. The cell pellets were resuspended in distilled water and the optical density adjusted at λ = 600 nm to 0.2 or 0.4 arbitrary units (AU). The cell suspensions were divided into aliquots of 50 mL and stored at –20 °C for later use in the feeding assays. Before being used in the feeding assays and due to the formation of cell clusters, the bacteria cell suspension was defrosted and subsequently sonicated for 1 to 2 min in a Misonix Microson Ultrasonic Cell Disruptor XL at 10 watts intensity. After this procedure, the cell suspension was again adjusted to 0.2 AU or 0.4 AU at λ = 600 nm, before being provided as food for D. magna in the feeding assays.

D. magna monoclonal cultures were maintained over several generations of pure parthenogenetic cultures under controlled conditions of temperature (20 ± 2 °C) and photoperiod (16 hL:8 hD). Cultures with 30 organisms were maintained in 500 mL of the synthetic medium, ASTM hard water according to standard procedures [39]. To provide essential elements to Daphnia, an organic additive (suspension extracted from brown algae Ascophyllum nodosum) [40] was added to the cultures. The culture medium was renewed every two days and D. magna was fed with the microalgae R. subcapitata with a ratio of 3.0 × 105 cellsmL-1day-1. Neonates born between the 3rd and the 5th brood, with less than 24 h old, were used to establish a new culture or to initiate the feeding assays. The microalga R. subcapitata Korshikov (Hindak) (formerly known as Selenastrum capricornutum and Pseudokirchneriella subcapitata) was kept in cultures with Woods Hole MBL medium [41], under controlled conditions of temperature (20 ± 2 °C) and continuous light (~6000 lux). The microalga culture was cyclically renewed in the exponential growth phase (5–7 days old) and inoculated in fresh Woods Hole MBL medium [42, 43]. Algal cell concentration was calculated based on the correlation of absorbance measured at λ = 440 nm and cell concentration previously determined [44].

Carbon, nitrogen, and carotenoids content were quantified in the five food regimens tested (Table 1). To quantify carbon in R. rubra, 2.5 mL of the sample at 0.2 AU and 0.4 AU, was centrifuged at 13,000 rpm for 60 seconds. The supernatant was discarded, and the pellets were lyophilized for subsequent quantification For R. subcapitata 3 × 105 cellsmL-1 suspension was centrifuged at 13,000 rpm for 60 seconds. The supernatant was discarded, and the pellet was lyophilized for subsequent carbon and nitrogen quantifications. For C quantification each sample was carefully wrapped in tin foil, making sure there was no remaining atmospheric air inside. Before the analysis, blank experiments were run, and three measurements with D-phenylalanine (used as CHN standard) were made to obtain an average daily factor, to properly correct the measured results. The analyses were performed in a CHNS analyzer from Elementar® (model Vario MACRO Cube), equipped with a combustion tube set at 1050 °C, a reduction tube set at 850 °C and three adsorption columns, each one with a specific filling and set at a specific temperature to adsorb CO2, H2O and SO2. These columns were then heated up sequentially to release the adsorbed gas to be detected by a Thermal Conductivity Detector (TCD). The gases were always detected in the following order: N2 followed by CO2, H2O and finally SO2. The analyses were performed and registered in VarioMACRO software version 4.0.8.

Table 1.Composition of the diets provided in the feeding assay of D. magna, and diets characterization of carbon, nitrogen and carotenoids contents.
A 0.2 0.4 0.2+A 0.2+A
R. subcapitata (cells·mL-1·day-1) 3.0 × 105 3.0 × 105 3.0 × 105
R. rubra (AU·day-1) 2500 μL at 0.2 2500 μL at 0.4 2500 μL at 0.2 2500 μL at 0.4
Carbon (mgC·sample diet-1) 0.198 0.165 0.344 0.329 0.536
Nitrogen (mgC·sample diet-1) 0.0240 0.0423 0.0922 0.0688 0.118
Carotenoids (mg·L-1) 1.20 ± 0.10 0.038 ± 0.007 0.063 ± 0.012 1.68 ± 0.29 2.15 ± 0.34

Carotenoids content was quantified by the method described by Zhang and Hu [45], where 10 mL of acetone (99.5%; V1) was added to the cell pellet from culture cell suspension (V2) and sonicated for 3 min in a Misonix Microson Ultrasonic Cell Disruptor XL, at 20 watts. Then, the tubes were kept in a water bath at 20 °C for 10 min. After centrifugation at 3000 rpm for 10 min, the total carotenoids were determined by reading the absorbance at 480 nm (A) and applying the following equation [45]:

(1) Carotenoids yield ( mg L - 1 ) = AV1 / 0.16 V2

2.2 Feeding Assays

To evaluate the potential of R. rubra as a nutritional and supplementary food source for D. magna, feeding assays were performed according to standard protocols for assessing chronic toxicity [46, 47]. The feeding assays had a duration of 21 days and were conducted under the same conditions as described for cultures maintenance. The experimental setup comprised 5 food regimens as describe in Table 1.

For each food regimen, twenty individual replicates were placed in a single glass vial filled with 50 mL of the synthetic ASTM hard water medium [39]. Daily, the daphniids were fed with corresponding food regimen (Table 1), and the medium renewed was conducted every two days. Mortality and the reproductive state were checked daily, and the neonates born during the assay were counted and discarded. At the end of the assay, the following endpoints were quantified: age at first reproduction (days), reproductive output (mean of offspring produced by all the mothers), fecundity (mean of offspring produced by the survivor mother at the end of the assay), number of broods, fecundity of the first brood, somatic growth rate (day-1) and rate of population increase (r, day-1).

Somatic growth rate was determined regarding the difference between the initial and final body size of the organisms, measured from the top of the head to the base of the caudal spine, in a binocular stereoscope. At the beginning of the assay, average of initial body length was calculated in a sub-sample of 20 neonates from the same brood of the organisms used in the assay. At the end of the feeding assay all the survivor organisms were measured. The somatic growth rate was calculated, according to the following expression:

(2) Somatic growth rate = ( Ln ( L f ) - ( Ln ( L i ) Δ t

where Lf stands for body size (mm) of the organism at the end of the assay, Li is the average body size (mm) of a subsample (n = 20) of neonates, and Δt is the duration of the assay (in days).

Survival and fecundity related data were used for the estimation of the per capita intrinsic rate of population increase (r), which was iterated from the Euler–Lotka equation:

(3) 1 = x = 0 n e - r x l x m x

where r is the intrinsic rate of increase (day-1), x is the age class in days (0 … n), lx is the probability of surviving to age x, and mx is the fecundity at age x. Standard errors for r were estimated using the jack-knifing technique described by Meyer et al. [48].

At the end of the feeding assay, after body length and weight measurements, 3 daphnids were collected for carotenoids quantification. Firstly, the organisms were placed in a vessel containing ASTM medium for 2 hours to promote gut cleaning, and afterward were storage in Eppendorf microtubes for carotenoids quantification. For each food regimen, the remaining organisms were storage in 5 individual groups at –20 °C for the next day quantifications (protein, glycogen, haemoglobin, carotenoid contents and the activity of catalase (CAT) and of glutathione S-transferase (GST), and levels of lipid peroxidation).

2.3 Longevity Assay

Regarding the results obtained in the feeding assay and to assess the potential effects of different food regimens on the longevity of D. magna, a new assay was performed with 20 individualized neonates exposed to the feeding regimens: A (standard food), 0.2 and 0.2+A (Table 1). The food regimens selected to assess the D. magna longevity were chosen according to the results obtained in the life-history parameters of the previous feeding assays. The assay was performed in vessels with 30 mL of ASTM medium and the organisms were kept under the same conditions as described for the culture’s maintenance and the feeding assay. Culture medium were completely renewed three times a week and daphniids feed at the same time (fed three days a week, as described in OECD guidelines [47] — “the food provided to organisms should preferably be done daily, or at least three times a week when the medium is changed”). The organisms were checked daily for mortality, and if there were neonates, these were counted and discarded. The endpoints measured at the end of the assay were: survival, age at first reproduction (days), reproductive output, fecundity of the first brood, and rate of population increase (r, day-1). The assay finished when the death of all organisms was observed at least in one of the feed treatments.

2.4 Biochemical Determinations

At the end of the feeding assay a set of biomarkers were measured in the organisms exposed to the different food regimens: energetic reserves-protein and glycogen content; pigments-carotenoid and haemoglobin content; oxidative stress-antioxidant catalase (CAT) activity, detoxification glutathione S-transferase (GST) activity and lipid peroxidation (thiobarbituric acid assay-TBARS levels). Organisms’ homogenization was performed in 1.2 mL of cold phosphate buffer (50 mM, pH = 7.0 with 0.1% Triton X-100), and the homogenates were centrifuged at 13,400 rpm for 6 min at 4 °C. The supernatants were recovered for the biochemical analysis. The supernatant was divided into aliquots for subsequent determination of biochemical biomarkers, and all endpoints were determined in triplicate. The absorbances (except for haemoglobin determination) were performed in a microplate reader Thermo Scientific Multiskan GO spectrophotometer, version 1.00.40, with SkanIt Software 3.2.

Haemoglobin was determined by reading the absorbance of 1 mL of supernatant from each homogenized sample in a UV-1600 PC Spectrophotometer from 350 to 500 nm at 1 nm interval [49]. The specific absorbance of haemoglobin at 414 nm was normalized according to the technique described by Williams et al. [49]. The slope of the absorption spectrum within the wavelength intervals of 370–470 nm was determined by linear regression, from which the peak of haemoglobin specific absorbance (394–434 nm) was omitted. As for the 370–395 nm and 430–470 nm intervals, the corresponding values belong to non-haemoglobin materials that are present in Daphnia tissues. The observed absorbance value at the haemoglobin peak (414 nm) was subtracted by the expected absorbance value (calculated by linear regression calculated in the omitted interval of absorbance).

The glycogen quantification was conducted according to Lo et al. [50], where 100 μL of 30% KOH, saturated with Na2SO4, was added to 150 μL of homogenized supernatant. The suspension was boiled in a water bath (100 °C) for 10 min, and afterward placed on ice for 5 min. After cooling, 250 μL of ethanol (96%) were added and incubated for 10 min on ice (separation of glycogen from other saccharides-alkaline digestion). After this time, the sample was centrifuged at 1,550 rpm for 10 min at 4 °C and the pellet was resuspended in 125 μL of distilled water and homogenized. To each sample such as for glycogen standards (0, 3.125, 6.25, 12.5, 25, 50, and 100 μgmL-1), 125 μL of 5% phenol and 625 μL of H2SO4 were added and kept in ice for 10 min. The absorbance of the samples and the glycogen standards were read in quadruplicate in a spectrophotometer at λ = 490 nm. A standard curve was built regarding the values of the absorbance of glycogen standard concentrations and the results were calculated following the equation:

(4) Y ( abs ) = 0.00324 x + 0.07010

where Y is the absorbance values in the sample and x is the glycogen content (μgmL-1).

Catalase activity was determined following the procedure by Aebi [51], where the degradation of H2O2 to H2O and O2 decreases absorbance at a wavelength of 240 nm. The results were expressed by considering equivalent one unit of CAT activity to the number of moles of H2O2 consumed per minute per milligram of protein.

Glutathione S-transferase activity was measured according to the method by Habig et al. [52]. GST catalysis the conjugation of glutathione with the substrate 1-chloro-2,4-dinitrobenzene (CDNB), forming a thioether that increases absorbance at 340 nm. The results were expressed considering the equivalent one unit of GST activity to the number of moles of thioether produced per minute per milligram of protein.

Lipid peroxidation was measured by the quantification of the concentration of thiobarbituric acid reactive substances (TBARS), according to Buege and Aust et al. [53]. The main by-products of oxidative damage to lipids membranes caused by reactive oxygen species (ROS) are malondialdehyde (MDA) and MDA-like compounds. This methodology is based on the reaction of compounds, such as MDA, formed by degradation of initial products from lipid membranes by free radical attack, with 2-thiobarbituric acid (TBA). Absorbance readings of each sample were measured at a wavelength of 535 nm and expressed as MDA equivalents per milligram of protein.

Protein was determined according to the methodology described by Bradford [54], adapted to microplates. This involves the binding of a dye (Bradford reagent) to the total protein, giving rise to a stable and colored complex that can be quantified at 595 nm. The γ-globulin (1 mgmL-1) was used as standard.

For the quantification of the carotenoid content 0.5 mL of 100% ethanol was added to the samples. The microtubes were wrapped in aluminum foil for protection from light and placed in the refrigerator overnight at –4 °C, according to Moeller et al. [55]. The day after, the total carotenoid absorption of the supernatant was measured in the spectrophotometer at λ = 450 nm. The extraction solution was used as blank. The wavelength of 450 nm is very close to the maximum absorption of β-carotene; therefore, the total carotenoid content was quantified according to the following equation Moeller et al. [55]:

(5) Total carotenoids ( μ g mg - 1 ) = 1 × 10 4 x ( OD 450 / 2620 ) × ( V / W )

where V is the extract volume (mL), W is total dry weight (mg) of organisms and OD = optical density (λ).

2.5 Statistical Analysis

One-way Analysis of Variance (ANOVA) was applied at all the endpoints measured in the feeding and longevity assays: age at first reproduction, fecundity, reproductive output, number of broods, number of N1 offspring, somatic growth rate and rate of population increase (these endpoints were log (x + 1) transformed prior to the ANOVA, to comply with ANOVA requirements), glycogen, protein, TBARS, GST and CAT. When ANOVA results showed significant differences a post-hoc Tukey test was conducted to assess statistical differences between the different food regimens. For all analyses, the level of significance (α) used was 0.05.

3. Results and Discussion
3.1 Feeding Assays, Life-History Parameters

One of the main questions addressed in this work was if an increase in the amount of R. rubra provided to D. magna as food would enhance its growth. As previously observed by Marinho et al. [34, 35], R. rubra at a concentration of 0.2 AU proved not to be sufficient to provide the nutritional requirements needed by D. magna. In fact, a significant delay of the age at first reproduction, a decrease of broods, and an increase of somatic growth rate, fecundity, reproductive output, and the rate of population increase were observed (Fig. 1). The obtained results suggest that 0.2 R. rubra concentration, when provided as exclusively food source, is below the “incipient limiting level” (ILL—the external level above which there is no limiting effect of food supply, terminology described by Fry et al. [56], when the daphnids filter at a maximum rate [1, 57]. Regarding the double R. rubra concentration (0.4), D. magna performance was not improved, and the parameters of the life history even aggravated (Fig. 1). The cell aggregate formation typical of R. rubra may justify this result, as the feeding structures of D. magna may be inadequate to efficiently filter the bacteria. In fact, and as already demonstrated by Gliwicz et al. [58], filtration rate and particle size affect the amount of food collected and ingested by Daphnia as well as in other organisms (e.g., rotifers [59]). On the other hand, the higher amount of food in diet 0.4 may reduce the ability of Daphnia to ingest the bacteria due to occlusion of the filter apparatus, fact already observed by Martínez-Jerónimo et al. [60]. Both food regimens (0.2 and 0.4) presented to be poor diets compared to the mixed diets (0.2+A and 0.2+A) and the diet with only alga (A).

Fig. 1.

Life-history parameters; (A) age at first reproduction; (B) offspring of first brood; (C) number of broods; (D) somatic growth rate; (E) fecundity and reproductive output; and (F) rate of population increase, results of D. magna after exposure for 21 days to several food regimens (see Table 1). Error bars represent standard error (n = 20) and different letters (a,b,c,d) represent significant differences between food regimens (Tukey test, p < 0.05).

On the other hand, when D. magna was fed with the mixed diet 0.2+A, a significant reduction of the age at first reproduction, and a significant increase of somatic growth rate, fecundity, reproductive output and rate of population increase were recorded (Fig. 1), corroborating the data from Marinho et al. [34, 35]. Moreover, when comparing the two mixed diets (0.2+A and 0.2+A), no differences were observed (a similar D. magna behavior was obtained; Fig. 1). This implies that, under the same laboratorial conditions, D. magna did not need an additional quantity of bacteria to achieve the same levels of reproduction and growth. The elemental analyses of the levels of C and N in the five diets showed an increase from the single to the mixed diets (Table 1). This carbon increase in the diets, from A to 0.4 or from 0.2+A to 0.2+A, showed to be insufficient to improve D. magna life-history parameters. On the other hand, the quality of the food provided by the alga (although comparatively lower) is essential to D. magna rearing. Curiously, the levels of N present in the bacterium are higher in all diets than in the algal diet. The level of this element may explain the important role of this bacterium in the N availability to D. magna in the mixed diets. Taipale et al. [28] and Freese et al. [29], also recorded that when bacteria [Micrococcus luteus, Methylomonas methanica, Methylosinus trichosporium (2.5 mgCL-1 of bacteria in 5 mgCL-1 of total food concentration), Escherichia coli (4.4 × 106 cellmL-1) and Flavobacterium sp. (4 × 106 cellmL-1)] were used as supplement to algae diets, an increase of somatic growth rate and reproduction of Daphnia was observed, when compared to an exclusive algal diet. Indeed, two different carbon sources provided in the diet (from bacteria and from alga—Table 1) improved the nutritional diversity of the diet, which implies a greater availability of carbon for the growth of primary consumers such as Daphnia [61].

3.2 Feeding Assays, Biochemical Parameters

The effects of the different diets on D. magna physiological parameters were also evaluated and are presented in Figs. 2,3. The protein levels recorded in 0.2 and 0.2+A were similar to the A diet, while in 0.4 and 0.2+A a significant decrease (0.7 ×) and increase (1.6 ×), respectively, were observed (Fig. 2A). The nutritional value of a diet is determined by the level of essential elements, such as nitrogen, phosphorus, and carbon, which are important for zooplankton growth and reproduction and for the competitive abilities of various zooplankton species [62, 63]. Furthermore, proteins, lipids and carbohydrates are also important since these nutrients are essential molecules and reserves necessary for the enhancement and the effectiveness of growth and reproduction [35, 64, 65]. Although daphnids can accumulate large amounts of proteins, this content can be influenced by the age of organisms, the diet provided and the number of eggs produced [66, 67]. Protein content reflects the entire physiological state of the organism and a measure of its energy balance [68]. Our results showed the highest protein content in organisms fed with the mixed diet 0.2+A, demonstrating that this diet is the more suitable for protein production and that 0.4 diet is the less adequate to fed D. magna. Indeed, the diets characterization (Table 1) showed an increase of C, N, and carotenoids content in the mixed diets, demonstrated higher diversity and nutritional food provided to D. magna with essential elements to the Daphnia development (Fig. 1).

Fig. 2.

Variation in protein (A) glycogen, (B) haemoglobin and carotenoids in D. magna after exposure for 21 days to several feeding regimes (see Table 1). Error bars represent standard error (n = 20), different letters (a,b,c,d) represent significant differences between food levels (Tukey test, p < 0.05).

Fig. 3.

Results of oxidative stress biomarkers (A) CAT; and (B) GST activities; (C) TBARS concentrations, in D. magna after exposure for 21 days to several feeding regimens (see Table 1). Error bars represent standard error (n = 20) and different letters (a,b,c,d,e) represent significant differences between food levels (Tukey test, p < 0.05).

Glycogen represents the main form of glucose storage in animal organisms, which fuels glycolysis as a first response in the case of a lack of food [69, 70]. In the 0.2 and 0.4 diets, D. magna had no difference in the glycogen levels comparatively to A diet (Fig. 2B). Indeed, a significant lower somatic growth rate and reproduction values (see Fig. 1D–F) were observed in the single bacterial diets, showing that the organisms allocated the energy available for self-maintenance instead of supporting growth and reproduction. Several studies already demonstrated that under conditions of low feeding, daphnids increase the allocation of energy for self-maintenance [71, 72]. Regarding the glycogen contents in the mixed diets, a significant decrease was observed relatively to the bacterial single diets (Fig. 2B). As a significant increase of somatic growth rate and reproductive parameters was observed in the mixed diets (Fig. 1D, E), D. magna was not able to accumulate glycogen due to consumption for reproductive needs. This indicates that D. magna energy allocation strategy was directed for growth and reproduction having not the possibility for reserve storage. When glycogen is used for energy production it is rapidly catabolized, leading to large losses of this energy reserve [68].

Haemoglobin in Daphnia is a respiratory pigment, which is part of the oxygen transport system [73]. In invertebrates, haemoglobin is involved in adaptive response to changes in environmental conditions, such as oxygen availability, pH, salinity, CO2, sulfides, carbon monoxide and temperature [74]. Haemoglobin as to be synthetized by Daphnia with intake of matter and energy [75]. Fox [76] verified that Daphnia does not synthetize this pigment under insufficient food conditions as well-fed organisms do. Our results showed that haemoglobin levels increased in all diets provided, with the highest values recorded for the two mixed diets (Fig. 2C). Even though the increase in haemoglobin concentration recorded in the mixed diets (Fig. 2), no effects were observed in the life-history parameters on D. magna (Fig. 1). Schwerin et al. [77] reported that, under laboratory conditions with ideal feeding regimens, D. galeata-hyalina showed higher haemoglobin concentrations.

Several different types of carotenoids are present in algae and bacteria. R. subcapitata belongs to the phylum Chlorophyta which contains, among others, β-carotene, violaxanthin, 9’-cis neoxanthine and lutein, as well as chlorophyll a and b [78]. The Planctomycetota R. rubra possesses three saproxanthin-type carotenoids, including a rare C45 carotenoid [79]. Animals do not synthesize carotenoids de novo and they obtain them from food or through modified metabolic reactions [80]. In addition, carotenoids are important for immunity, non-enzymatic antioxidant defense, photoprotection against photodegradation and contribute to the increase of reproduction [80]. The quantification of carotenoids in the different food regimens is shown in Table 1 and Fig. 2 shows the carotenoids content for D. magna feed with the different food regimens. Our results showed that the levels of carotenoids quantified in D. magna were highly increased in the diet 0.4 (2.0 ×) while in the mixed diets a decrease (0.7 ×) was observed (Fig. 2C). Therefore, these last results are somehow unexpected due to the high levels of pigments provided by the two mixed diets, specially the 0.2+A (Table 1). This suggests that the highest levels of carotenoids provided by the mixed diets (Table 1) were used for reproductive purposes of the daphniids, evidenced by the increase of the reproductive output (Fig. 1E). Similarly, Schneider et al. [81] also observed a depletion of carotenoids in the copepod Leptodiaptomus minutus during the increase of offspring production. On the other hand, the two bacterial diets showed low and similar levels of carotenoids (Table 1). As these diets showed a significant decrease in the reproductive output, higher levels of these pigments were observed in D. magna fed with the two single bacterium diets (Fig. 1E). Comparing in between the two single diets, carotenoids levels in the diet 0.2 were lower than in diet 0.4, which may be due to pigment transfer to a greater number of neonates. This suggests that the mothers in the 0.4 diet accumulated the pigment, as there was a decrease in fertility despite the increased concentration of the bacterium. Hairston Jr [82] collected, at regular intervals, zooplankton samples from two central Washington lakes and observed that adult females of two copepod Diaptomus species (Diaptomus sicilis and Diaptomus neuadensis) accumulated carotenoids and transferred them to the eggs and nauplii. Indeed, Marinho et al. [35] already demonstrated that D. magna can absorb R. rubra carotenoids and transferred them to the next generation.

It is known that food deprivation or lack of nutritional factors, such as vitamins, causes changes in the activities of tissue antioxidant enzymes [83]. The effect of diet on free radicals’ formation varies in function of the type of organism, age, physiological status, and ingested food [84]. For example, a study of fed and fasted mammalian species (male Wistar rats) showed that malnutrition accelerated the production of free radicals with the consequent depletion of the liver antioxidant stores [85]. If vitamins C and E were added to mice erythrocytes previously incubated with hydrogen peroxide (H2O2), a decrease in the plasma concentration of malondialdehyde, a product of lipid peroxidation, was observed [86]. Sharma et al. [87] observed an improvement in the antioxidant defense system (lower lipid peroxidation and higher activity of antioxidant enzymes (glutathione [GSH], GST, CAT and superoxide dismutase [SOD]) in muscle tissue of juvenile fish Clarias gariepinu fed with the microalgae Ascochloris spp. comparatively to organisms fed with a commercial diet. CAT is a protective enzyme responsible for the degradation of hydrogen peroxide and is present in almost all animal cells [88]. GSTs are present in all aerobic organisms, belong to the family of multifunctional cytosolic enzymes and are detoxifying enzymes [89]. Lipid peroxidation occurs when free radicals react with lipids containing carbon-carbon double bond(s), especially polyunsaturated fatty acids (PUFAs) [90]. As noted by Harris [91], organisms always maintain basal levels of antioxidant enzymes activity. As it is known, oxygen is a highly reactive molecule, which can form free radicals or reactive oxygen species (ROS). When this happens, the cell’s antioxidant systems kick in, and regulate the balance between ROS production. If this balance is disrupted, oxidative stress results, with alterations in cellular functions leading to various pathological conditions [88].

Results from the evaluation of oxidative stress in D. magna under the different feeding regimens are provided in Fig. 3. The levels of CAT activity in the mixed diets were similar to A diet, showing a non-oxidative stress response. CAT activity was significantly increased in D. magna fed with the two bacterial diets (Fig. 3A). This result may be justified by a potential increase in hydrogen peroxide levels and consequent oxidative stress due to D. magna undernutrition status (Fig. 3A —0.2 and 0.4). Im et al. [92] also demonstrated that under low food concentration and high temperatures D. magna showed increased activity of antioxidant enzymes (SOD and CAT) and reduced adult somatic growth rate. Regarding the GST activity, a significant increase in D. magna fed with the diets 0.2 (1.8 ×), 0.2+A (2.6 ×) and 0.2+A (2.5 ×) was observed (Fig. 3B). Under 0.2 diet the increase in GST values may be due to insufficient levels of food. On the other hand, Metcalfe et al. [93] described that reproduction increases oxidative stress and that this stress may tend to increase with the effort in the quantity and quality of offspring. This may explain the increase of GSTs values due to the high reproductive output recorded (Fig. 1E) in the mixed diets. A significant reduction of the lipid peroxidation was recorded in the bacterial diets and the mixed ones (Fig. 3C). The low levels observed in the four diets may be due to the high activities values of the antioxidant enzymes CAT and GST (Fig. 3A,B) and consequent improvement of D. magna antioxidant defense system [87]. In the algal diet A, the levels of peroxidation are within the values already observed for D. magna by Rodrigues et al. [17]. In fact, in this study a slightly higher values of lipid peroxidation were observed in the A diet (3.8 mmolmg prot-1), than the ones recorded in our study (2.1 mmolmg prot-1). Several studies also described that, between other functions, the GST prevents lipid peroxidation by reducing lipid hydroperoxides [94, 95]. Among other functions, the antioxidant capacity of carotenoids, such as singlet oxygen (1O2) suppression, protects cells against free radicals and inhibits lipid peroxidation [96]. Furthermore, R. rubra possesses the carotenoid saproxanthin [79] that was already referred as leading to the reinforcement and stabilization of biological membranes and enhancing protection against radical-induced peroxidation [97]. The existence of this kind of carotenoids suggests that they may have been used by D. magna for detoxification, with a significant decrease in TBARS.

3.3 Longevity Assay

A longevity study (from birth to natural death) was also performed with D. magna fed with 3 feeding regimens (A, 0.2 and 0.2+A; Figs. 4,5). No death occurred in the first 25 days of the assay for any of the feeding regimens (Fig. 4A). After this period, survival felt abruptly from day 30 to day 60 in the A diet (with a slope of –1.039) with 50% death recorded at day 50 (Fig. 4A). In the 0.2 feeding regimen, death occurred from day 40 to day 90 (with a slope of –1.243) with 50% mortality around day 70, with complete organisms’ death recorded at day 107 (Fig. 4A). In the 0.2+A feeding regimen, the decrease survival was from day 30 to day 100 (with a slope of –0.831) with 50% death occurring at day 70. No significant differences were recorded in D. magna survival (days) regarding the three feeding regimens tested (Fig. 4A). The reproductive output along the 110 days of experiment is shown in Fig. 4B. A significant decrease of reproductive output was recorded for the 0.2 diet (with a slope of 1.479), while a significant increase was observed for 0.2+A diet (with a much higher slope of 6.671) and for A diet (a slope of 3.405) (Fig. 4B). Although this assay was performed for 110 days instead of 21 days, comparable results were obtained (for comparison see Fig. 1). A significant delay in the age at first reproduction (Fig. 5A), and a significant decrease of N1 fecundity (Fig. 5B) were observed in 0.2 feeding regimen. The rate of population increase showed similar results obtained in the 21-day assay (Fig. 1F) where a significant decrease was observed for 0.2 while for 0.2+A a significant increase was recorded (Fig. 5C).

Fig. 4.

Survival curves (A) and reproductive output (B) for D. magna fed with the green microalgae R. subcapitata (A), the planctomycete R. rubra suspension at 0.2 AU (0.2) and a mixed diet of R. rubra suspension at 0.2 AU plus R. subcapitata (0.2+A). Different letters (a,b,c) stands for significant differences between the food regimens (Tukey test, p 0.05).

Fig. 5.

Life history parameters (A) age at first reproduction; (B) offspring of first brood; and (C) rate of population increase in longevity assay of D. magna fed on the green microalgae R. subcapitata (A), the planctomycete R. rubra suspension at 0.2 AU (0.2) and a mixed diet of R. rubra suspension at 0.2 AU plus R. subcapitata (0.2+A). Error bars represent standard error (n = 20), and letters (a,b,c) stands significant differences between the food regimens (Tukey test, p 0.05).

Vijverberg [98] observed that well fed D. hyalina lived for 43.4 days while poorly fed organisms lived for 64.4 days. Ingle [99] reported that well fed D. longispina organisms had an average life duration time of 29.9 days while malnourished organisms lived longer, for 41.4 days. Indeed, previous studies with D. magna also reported that survival increased under limiting food conditions [60]. D. magna fed with 0.05, 0.15, 0.5, 1.5, and 4.5 mgCL-1 of Scenedesmus obliquus lived longer at the lowest C concentration (0.15 mgCL-1, 114 days) than at the highest concentration (4.5 mgCL-1, 65 days) [18]. The here-obtained results are not in agreement with these results because survival did not increase in the lower food condition. Pietrzak et al. [18] also observed that when organisms live longer, the fecundity was significantly reduced. In our study, the bacteria feeding regimen 0.2 induced a decrease of D. magna rate of population increase, due to investment of the energy in maintenance and survival at the expense of reproduction. This was already showed by a study performed by Antunes et al. [100] where different Daphnia longispina clones under starvation conditions for 21 days, registered a significant decreased in the reproductive output. Martínez-Jerónimo et al. [60] observed similar results in D. magna fed with low food concentration of the microalgae Ankistrodesmus falcatus and Scenedesmus incrassatulus, while, in the highest food densities a shorter life span, higher fecundity, and larger clutch sizes were observed. The here-obtained results also showed that the diet provided to D. magna influences longevity and reproduction performance. When the 0.2+A diet was supplied, individuals had similar longevity comparatively to the A diet when considering the 110 days, but obtained higher reproductive output, rate of population increase, and the offspring increased significantly. Although several studies demonstrated that longevity increases with lower food concentration [58, 98, 99], our results showed that the quality of food also affected the longevity. Furthermore, they also showed that in the feeding regimen with the highest diverse food sources (0.2+A), a higher Daphnia performance was recorded compared to the single diets (A and 0.2).

4. Conclusions

The elemental analyses of the levels of C, N, and carotenoids in the five diets showed overall an increase from single diets to the mixed diets. These results demonstrated that different diets (algae and bacterium) provided a diversified and different nutritional food to the daphnids that represent differences in the performance of D. magna, even in laboratory conditions.

The bacterium (R. rubra) proved to be a good supplement food for growing D. magna since the mixed feeding regimens 0.2+A and 0.2+A (bacteria + algae) significantly improved its performance, reinforcing the previous results obtained by our group. We also showed that a food regimen with higher R. rubra levels (from 0.2 to 0.4) is not enough to fill D. magna nutritional needs. Moreover, these results are supported by the longevity assay. The high protein content observed showed that the mixed diet tested (0.2+A diet) is, in fact, the best diet for D. magna. Low levels of lipid peroxidation were registered in all bacterial diets which may be due to the levels of activity of the antioxidant enzymes (CAT and GST) observed, and the intake of carotenoids (non-enzymatic antioxidant defense) provided by the bacterium. Thus, our results evidenced that biological, biochemical, and physiological processes are affected by the food conditions to which organisms are subjected.

Thus, and reinforcing our previous studies, we can conclude that R. rubra is a good diet supplement for D. magna that improve the growth, fecundity and survival of D. magna under laboratorial conditions enhancing this daphnid’ performance. Although different food sources are already used in the maintenance of Daphnia spp, a diversified diet, that includes the bacterium R. rubra, can be adopted to improve D. magna performance in laboratory maintenance.

Author Contributions

MM, GJ, OML and SCA contributed to the study conception and design. MM, GJ, JC, LS and SCA performed all material preparation, data collection and analysis. MM and GJ have written the first draft of the manuscript and all authors commented on the various versions of the manuscript. All authors read and approved the final manuscript.

Ethics Approval and Consent to Participate

All applicable international, national, and/or institutional guidelines for the care and use of animals were followed.

Acknowledgment

Not applicable.

Funding

Conceição Marinho received a PhD fellowship (SFRH/BD//146190/2019) from Foundation for Science and Technology (FCT - Government of Portugal). This work was supported by National Funds (through the FCT - Foundation for Science and Technology) and by the European Regional Development Fund (through COMPETE2020 and PT2020) through the strategic program UIDB/04423/2020 and UIDP/04423/2020. Sara Antunes is hired through the Regulamento do Emprego Científico e Tecnológico – RJEC from the Portuguese Foundation for Science and Technology program (CEEC-IND/01756/2017).

Conflict of Interest

The authors declare no conflict of interest.

References
[1]
Ebert D. Ecology, epidemiology, and evolution of parasitism in Daphnia. National Library of Medicine (US), National Center for Biotechnology Information. Bethesda. 2005.
[2]
Lampert W. Daphnia: model herbivore, predator and prey. Polish Journal of Ecology. 2006; 54: 607–620.
[3]
Shaw JR, Pfrender ME, Eads BD, Klaper R, Callaghan A, Colbourne JK, et al. Daphnia as an emerging model for toxicological genomics. Advances in Experimental Biology. 2008; 2: 165–328.
[4]
Watanabe H, Kobayashi K, Kato Y, Oda S, Abe R, Tatarazako N, et al. Transcriptome profiling in crustaceans as a tool for ecotoxicogenomics. Cell Biology and Toxicology. 2008; 24: 641–647.
[5]
Janssen R, Le Gouar M, Pechmann M, Poulin F, Bolognesi R, Schwager EE, et al. Conservation, loss, and redeployment of Wnt ligands in protostomes: implications for understanding the evolution of segment formation. BMC Evolutionary Biology. 2010; 10: 374.
[6]
Altshuler I, Demiri B, Xu S, Constantin A, Yan ND, Cristescu ME. An integrated multi-disciplinary approach for studying multiple stressors in freshwater ecosystems: Daphnia as a model organism. Integrative and Comparative Biology. 2011; 51: 623–633.
[7]
Harris KDM, Bartlett NJ, Lloyd VK. Daphnia as an Emerging Epigenetic Model Organism. Genetics Research International. 2012; 2012: 1–8.
[8]
Castro BT, De Lara AR, Castro MG, Castro MJ, Malpica SA. Alimento vivo en la acuicultura. Contactos. 2003; 48: 27–33.
[9]
Sánchez-Estudillo L. Alimento nutritivo, colorido y en movimiento: Los cultivos de apoyo en Acuicultura. Ciencia y Mar. 2011; 43: 55–60.
[10]
Fereidouni AE, Fathi N, Khalesi MK. Enrichment of Daphnia magna with canola oil and its effects on the growth, survival and stress resistance of the Caspian kutum (Rutilus frisii kutum) larvae. Turkish Journal of Fisheries and Aquatic Sciences. 2013; 13:119–126.
[11]
Warren E. On the reaction of Daphnia magna to certain changes in its environment. Journal of Cell Science. 1900; 43: 199–224.
[12]
Jansen M, Coors A, Stoks R, De Meester L. Evolutionary ecotoxicology of pesticide resistance: a case study in Daphnia. Ecotoxicology. 2011; 20: 543–551.
[13]
Lee J, Bang SH, Kim Y, Min J. Toxicities of Four Parabens and their Mixtures to Daphnia magna and Aliivibrio fischeri. Environmental Health and Toxicology. 2018; 33: e2018018.
[14]
Nunes B, Leal C, Rodrigues S, Antunes SC. Assessment of ecotoxicological effects of ciprofloxacin in Daphnia magna: life-history traits, biochemical and genotoxic effects. Water Science and Technology. 2018; 2017: 835–844.
[15]
Tkaczyk A, Bownik A, Dudka J, Kowal K, Ślaska B. Daphnia magna model in the toxicity assessment of pharmaceuticals: a review. Science of the Total Environment. 2020; 763: 143038.
[16]
Rodrigues S, Pinto I, Martins F, Formigo N, Antunes SC. Can biochemical endpoints improve the sensitivity of the biomonitoring strategy using bioassays with standard species, for water quality evaluation? Ecotoxicology and Environmental Safety. 2021; 215: 112151.
[17]
Rodrigues S, Silva AM, Antunes SC. Assessment of 17a-ethinylestradiol effects in Daphnia magna: life-history traits, biochemical and genotoxic parameters. Environmental Science and Pollution Research. 2021; 28: 23160–23173.
[18]
Pietrzak B, Grzesiuk M, Bednarska A. Food quantity shapes life history and survival strategies in Daphnia magna (Cladocera). Hydrobiologia. 2010; 643: 51–54.
[19]
Bukovinszky T, Verschoor AM, Helmsing NR, Bezemer TM, Bakker ES, Vos M, et al. The good, the bad and the plenty: interactive effects of food quality and quantity on the growth of different Daphnia species. PLoS ONE. 2012; 7: e42966.
[20]
Antunes SC, Castro BB, Gonçalves F. Effect of food level on the acute and chronic responses of daphnids to lindane. Environmental Pollution. 2004; 127: 367–375.
[21]
Pereira JL, Gonçalves F. Effects of food availability on the acute and chronic toxicity of the insecticide methomyl to Daphnia spp. The Science of the Total Environment. 2007; 386: 9–20.
[22]
Shahid N, Rolle-Kampczyk U, Siddique A, von Bergen M, Liess M. Pesticide-induced metabolic changes are amplified by food stress. Science of the Total Environment. 2021; 792: 148350.
[23]
Baird DJ, Barber I, Bradley M, Calow P, Soares AMVM. The Daphnia bioassay: a critique. Hydrobiologia. 1989; 188: 403–406.
[24]
Beatrici AC, Arenzon A, Coimbra NJ, Raya-Rodriguez MT. Fertilidade e Sensibilidade de Daphnia similis e Daphnia magna Submetidas a Diferentes Cultivos. Journal of the Brazilian Society of Ecotoxicology. 2006; 1: 123–126.
[25]
Choi J, Kim S, Chang K, Kim M, La G, Joo G, et al. Population growth of the Cladoceran, Daphnia magna: a quantitative analysis of the effects of different algal food. PLoS ONE. 2014; 9: e95591.
[26]
Choi J, Kim S, La G, Chang K, Kim D, Jeong K, et al. Effects of algal food quality on sexual reproduction of Daphnia magna. Ecology and Evolution. 2016; 6: 2817–2832.
[27]
Jonczyk E, Gilron G. Acute and Chronic Toxicity Testing with Daphnia Sp. In Blaise C, Férard JF, editors. Small-scale Freshwater Toxicity Investigations (pp. 337–393). Springer: Dordrecht. 2005.
[28]
Taipale SJ, Brett MT, Pulkkinen K, Kainz MJ. The influence of bacteria-dominated diets on Daphnia magna somatic growth, reproduction, and lipid composition. FEMS Microbiology Ecology. 2012; 82: 50–62.
[29]
Freese HM, Martin-Creuzburg D. Food quality of mixed bacteria–algae diets for Daphnia magna. Hydrobiologia. 2013; 715: 63–76.
[30]
Wenzel A, Vrede T, Jansson M, Bergström AK. Daphnia performance on diets containing different combinations of high‐quality algae, heterotrophic bacteria, and allochthonous particulate organic matter. Freshwater Biology. 2021; 66: 157–168.
[31]
Mona MH, El-Gamal MM, Abdel Razek FA, Elgiar EA, Nour Eldeen MF. Effect of different feeding regimes on the performance of Daphnia longispina. Sci-Afric Journal of Scientific Issues, Research and Essays. 2014; 2: 173–179.
[32]
Castro-Mejía J, Ocampo-Cervantes JA, Castro-Mejía G, Cruz-Cruz I, Monroy-Dosta MDC, Becerril-Cortes D. Laboratory production of Daphnia magna (Straus, 1820) fed with microalgae and active dry yeast. Journal of Entomology and Zoology Studies. 2016; 4: 548–553.
[33]
Antunes SC, Almeida RA, Carvalho T, Lage OM. Feasibility of planctomycetes as a nutritional or supplementary food source for Daphnia spp. Annales De Limnologie - International Journal of Limnology. 2016; 52: 317–325.
[34]
Marinho MC, Lage OM, Catita J, Antunes SC. Adequacy of planctomycetes as supplementary food source for Daphnia magna. Antonie Van Leeuwenhoek. 2018; 111: 825–840.
[35]
da Conceição Marinho M, Lage OM, Sousa CD, Catita J, Antunes SC. Assessment of Rhodopirellula rubra as a supplementary and nutritional food source to the microcrustacean Daphnia magna. Antonie Van Leeuwenhoek. 2019; 112: 1231–1243.
[36]
Hessen DO, Færøvig PJ, Andersen T. Light, nutrients, and P:C ratios in algae: grazer performance related to food quality and quantity. Ecology. 2002; 83: 1886–1898.
[37]
Betini GS, Wang X, Avgar T, Guzzo MM, Fryxell JM. Food availability modulates temperature‐dependent effects on growth, reproduction, and survival in Daphnia magna. Ecology and Evolution. 2020; 10: 756–762.
[38]
Lage OM, Bondoso J. Planctomycetes diversity associated with macroalgae. FEMS Microbiology Ecology. 2011; 78: 366–375.
[39]
ASTM. Standard practice for conducting acute toxicity tests with fishes, macroinvertebrates and amphibians. (Report No.: E 729–780). American Society for Testing and Materials: Philadelphia, USA. 1980.
[40]
Baird DJ, Soares AMVM, Girling A, Barber I, Bradley MC, Calow P. The long-term maintenance of Daphnia magna Straus for use in ecotoxicity tests: problems and prospects. In Proceedings of the first European conference on ecotoxicology (pp. 144–148). Lyngby: Denmark. 1989.
[41]
Stein JR. Handbook of Phycological Methods - Culture Methods and Growth Measurements. Cambridge University Press: UK. 1973.
[42]
Environment Canada. Biological Test Method: growth inhibition test using the freshwater alga Selenastrum capricornutum. (Report No.: EPS1/RM/25). Environment Canada, Ottawa, Ont., Canada. 1992.
[43]
OECD. Algal Growth Inhibition Test. Guidelines for Testing of Chemicals, Test Guideline Nº 201. OECD (Organisation for Economic Cooperation and Development): Paris, France. 2006.
[44]
Carvalho F, Guilhermino L, Ribeiro R, Gonçalves F, Soares AMVM. METIER (modular ecotoxicity tests incorporating ecological relevance). II. Ecotoxicity of poorly water-soluble compounds: Concentration versus dose. Archives of Environmental Contamination and Toxicology. 1995; 29.
[45]
Zhang H, Hu QP. Isolation, identification and physiological characteristics of high carotenoids yield Rhodopseudomonas faecalis PSB-B. International Journal of Recent Scientific Research. 2015; 6: 3893–3899.
[46]
ASTM. Standard Guide for Conducting Daphnia magna Life-cycle Toxicity Tests. (Report No.: E 1193–1197). American Society for Testing and Materials: Philadelphia, USA. 1997.
[47]
OECD. Daphnia magna Reproduction Test, Test Guideline Nº 211, OECD (Organisation for Economic Cooperation and Development): Paris, France. 2012.
[48]
Meyer JS, Ingersoll CG, McDonald LL, Boyce MS. Estimating uncertainty in population growth rates: jackknife versus bootstrap techniques. Ecology. 1986; 67: 1156–1166.
[49]
Williams PJ, Dick KB, Yampolsky LY. Heat tolerance, temperature acclimation, acute oxidative damage and canalization of haemoglobin expression in Daphnia. Evolutionary Ecology. 2012; 26: 591–609.
[50]
Lo S, Russell JC, Taylor AW. Determination of glycogen in small tissue samples. Journal of Applied Physiology. 1970; 28: 234–236.
[51]
Aebi H. Catalase in vitro. Methods Enzymol. 1984; 6: 114–121.
[52]
Habig WH, Pabst MJ, Jakoby WB. Glutathione S-transferases. The first enzymatic step in mercapturic acid formation. The Journal of Biological Chemistry. 1974; 249: 7130–7139.
[53]
Buege JA, Aust SD. Microsomal lipid peroxidation. Methods in Enzymology. 1978; 52: 302–310.
[54]
Bradford MM. A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Analytical Biochemistry. 1976; 72: 248–254.
[55]
Moeller RE, Gilroy S, Williamson CE, Grad G, Sommaruga R. Dietary acquisition of photoprotective compounds (mycosporine-like amino acids, carotenoids) and acclimation to ultraviolet radiation in a freshwater copepod. Limnology and Oceanography. 2005; 50: 427–439.
[56]
Fry FEJ. Effects of the environment on animal activity. Ontario Fisheries Research Laboratory Publication, University of Toronto Studies, Biological Series Nº 55. 1947; 55: 1–62.
[57]
Lampert W. Response of the respiratory rate of Daphnia magna to changing food conditions. Oecologia. 1986; 70: 495–501.
[58]
Gliwicz ZM, Siedlar E. Food size limitation and algae interfering with food collection in Daphnia. Archiv für Hydrobiologie. 1980; 88: 155–177.
[59]
Starkweather PL, Gilbert JJ, Frost TM. Bacterial feeding by the rotifer Brachionus calyciflorus: Clearance and ingestion rates, behavior and population dynamics. Oecologia. 1979; 44: 26–30.
[60]
Martínez-Jerónimo F, Villaseñor R, Rios G, Espinosa F. Effect of food type and concentration on the survival, longevity, and reproduction of Daphnia magna. Hydrobiologia. 1994; 287: 207–214.
[61]
Persson J, Brett MT, Vrede T, Ravet JL. Food quantity and quality regulation of trophic transfer between primary producers and a keystone grazer (Daphnia) in pelagic freshwater food webs. Oikos. 2007; 116: 1152–1163.
[62]
Hessen DO, Andersen T. Bacteria as a source of phosphorus for zooplankton. Hydrobiologia. 1990; 206: 217–223.
[63]
Taipale SJ, Brett MT, Hahn MW, Martin-Creuzburg D, Yeung S, Hiltunen M, et al. Differing Daphnia magna assimilation efficiencies for terrestrial, bacterial, and algal carbon and fatty acids. Ecology. 2014; 95: 563–576.
[64]
Harmelin-Vivien M, Bӑnaru D, Dromard CR, Ourgaud M, Carlotti F. Biochemical composition and energy content of size-fractionated zooplankton east of the Kerguelen Islands. Polar Biology. 2019; 42: 603–617.
[65]
Dararat W, Lomthaisong K, Sanoamuang LO. Biochemical composition of three species of fairy shrimp (Branchiopoda: Anostraca) from Thailand. Journal of Crustacean biology. 2012; 32: 81–87.
[66]
Bogut I, Adamek Z, Puskadija Z, Galovic D. Nutritional value of planktonic cladoceran Daphnia magna for common carp (Cyprinus carpio) fry feeding. Croatian Journal of Fisheries: Ribarstvo. 2010; 68: 1–10.
[67]
Cheban L, Grynko O, Marchenko M. Nutritional value of Daphnia magna (Straus, 1820) under conditions of co-cultivation with fodder microalgae. Biolohichni Systemy. 2017; 9: 166–170.
[68]
Villarroel MJ, Sancho E, Andreu-Moliner E, Ferrando MD. Biochemical stress response in tetradifon exposed Daphnia magna and its relationship to individual growth and reproduction. Science of the Total Environment. 2009; 407: 5537–5542.
[69]
Chang JC, Wu S, Tseng Y, Lee Y, Baba O, Hwang P. Regulation of glycogen metabolism in gills and liver of the euryhaline tilapia (Oreochromis mossambicus) during acclimation to seawater. The Journal of Experimental Biology. 2007; 210: 3494–3504.
[70]
Klumpen E, Hoffschröer N, Schwalb A, Gigengack U, Koch M, Paul RJ, et al. Metabolic adjustments during starvation in Daphnia pulex. Comparative Biochemistry and Physiology Part B: Biochemistry and Molecular Biology. 2021; 255: 110591.
[71]
Smolders R, Baillieul M, Blust R. Relationship between the energy status of Daphnia magna and its sensitivity to environmental stress. Aquatic Toxicology. 2005; 73: 155–170.
[72]
Pérez-Fuentetaja A, Goodberry F. Daphnia’s challenge: survival and reproduction when calcium and food are limiting. Journal of Plankton Research. 2016; 38: 1379–1388.
[73]
Ha M, Choi J. Effects of Environmental Contaminants on Hemoglobin Gene Expression in Daphnia magna: a Potential Biomarker for Freshwater Quality Monitoring. Archives of Environmental Contamination and Toxicology. 2009; 57: 330–337.
[74]
Weber RE, Vinogradov SN. Nonvertebrate hemoglobins: functions and molecular adaptations. Physiological Reviews. 2001; 81: 569–628.
[75]
Pirow R, Bäumer C, Paul RJ. Benefits of haemoglobin in the cladoceran crustacean Daphnia magna. The Journal of Experimental Biology. 2001; 204: 3425–3441.
[76]
Fox HM. The haemoglobin of Daphnia. Proceedings of the Royal Society of London. Series B-Biological Sciences. 1948; 135: 195–212.
[77]
Schwerin S, Zeis B, Horn W, Horn H, Paul RJ. Hemoglobin concentration in Daphnia (D. galeata‐hyalina) from the epilimnion is related to the state of nutrition and the degree of protein homeostasis. Limnol Oceanogr. 2010; 55: 639–652.
[78]
Takaichi S. Carotenoids in algae: distributions, biosyntheses and functions. Marine Drugs. 2012; 9: 1101–1118.
[79]
Kallscheuer N, Moreira C, Airs R, Llewellyn CA, Wiegand S, Lage OM, et al. Pink‐and orange‐pigmented Planctomycetes produce saproxanthin‐type carotenoids including a rare C45 carotenoid. Environmental Microbiology Reports. 2019; 11: 741–748.
[80]
Maoka T. Carotenoids as natural functional pigments. Journal of Natural Medicines. 2020; 74: 1–16.
[81]
Schneider T, Grosbois G, Vincent WF, Rautio M. Carotenoid accumulation in copepods is related to lipid metabolism and reproduction rather than to UV-protection. Limnology and Oceanography. 2016; 61: 1201–1213.
[82]
Hairston Jr NG. The relationship between pigmentation and reproduction in two species of Diaptomus (Copepoda). Limnol Oceanogr. 1979; 24: 38–44.
[83]
Gaál T, Mézes M, Miskucza O, Ribiczey-Szabó P. Effect of fasting on blood lipid peroxidation parameters of sheep. Research in Veterinary Science. 1993; 55: 104–107.
[84]
Vannucchi H, Moreira EA, da Cunha DF, Junqueira-Franco MV, Bernardes MM, Jordão-Jr AA. Papel dos nutrientes na peroxidação lipídica e no sistema de defesa antioxidante. Medicina. 1998; 31: 31–44.
[85]
Robinson MK, Rustum RR, Chambers EA, Rounds JD, Wilmore DW, Jacobs DO. Starvation enhances hepatic free radical release following endotoxemia. The Journal of Surgical Research. 1997; 69: 325–330.
[86]
Shiva Shankar Reddy CS, Subramanyam MVV, Vani R, Asha Devi S. In vitro models of oxidative stress in rat erythrocytes: effect of antioxidant supplements. Toxicology in Vitro. 2007; 21: 1355–1364.
[87]
Sharma S, Shah E, Davla D, Dixit G, Patel A, Kumar AK. Effect of microalga-based diet on oxidative stress enzymes of African catfish, Clarias gariepinus. International Aquatic Research. 2019; 11: 377–387.
[88]
Krishnamurthy P, Wadhwani A. Antioxidant enzymes and human health. Antioxidant Enzyme. 2012; 3: 1–17.
[89]
Balseiro E, Souza MS, Modenutti B, Reissig M. Living in transparent lakes: Low food P:C ratio decreases antioxidant response to ultraviolet radiation in Daphnia. Limnology and Oceanography. 2008; 53: 2383–2390.
[90]
Ayala A, Muñoz MF, Argüelles S. Lipid peroxidation: production, metabolism, and signaling mechanisms of malondialdehyde and 4-hydroxy-2-nonenal. Oxidative Medicine and Cellular Longevity. 2014; 2014: 1–31.
[91]
Harris ED. Regulation of antioxidant enzymes. FASEB Journal. 1992; 6: 2675–2683.
[92]
Im H, Na J, Jung J. The effect of food availability on thermal stress in Daphnia magna: trade-offs among oxidative stress, somatic growth, and reproduction. Aquatic Ecology. 2020; 54: 1201–1210.
[93]
Metcalfe NB, Alonso-Alvarez C. Oxidative stress as a life-history constraint: the role of reactive oxygen species in shaping phenotypes from conception to death. Functional Ecology. 2010; 24: 984–996.
[94]
Bartling D, Radzio R, Steiner U, Weiler EW. A glutathione S-transferase with glutathione-peroxidase activity from Arabidopsis thaliana: Molecular cloning and functional characterization. European Journal of Biochemistry. 1993; 216: 579–586.
[95]
Jackson MJ, Papa S, Bolaños J, Bruckdorfer R, Carlsen H, Elliott RM, et al. Antioxidants, reactive oxygen and nitrogen species, gene induction and mitochondrial function. Molecular Aspects of Medicine. 2002; 23: 209–285.
[96]
Zhang Y, He D, Chang F, Dang C, Fu J. Combined effects of sulfamethoxazole and erythromycin on a freshwater microalga, Raphidocelis subcapitata: Toxicity and oxidative stress. Antibiotics. 2021; 10: 1–11.
[97]
Shindo K, Kikuta K, Suzuki A, Katsuta A, Kasai H, Yasumoto-Hirose M, et al. Rare carotenoids, (3R)-saproxanthin and (3R,2′S)-myxol, isolated from novel marine bacteria (Flavobacteriaceae) and their antioxidative activities. Applied Microbiology and Biotechnology. 2007; 74: 1350–1357.
[98]
Vijverberg J. The effect of food quantity and quality on the growth, birth-rate and longevity of Daphnia hyalina Leydig. Hydrobiologia. 1976; 51: 99–108.
[99]
Ingle L, Wood TR, Banta AM. A study of longevity, growth, reproduction and heart rate in Daphnia longispina as influenced by limitations in quantity of food. Journal of Experimental Zoology. 1937; 76: 325–352.
[100]
Antunes SC, Castro BB, Gonçalves F. Chronic responses of different clones of Daphnia longispina (field and ephippia) to different food levels. Acta Oecologica. 2003; 24: S325–S332.
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