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Journal Pre-proof Sea urchin recruitment: Effect of diatom based biofilms on Paracentrotus lividus
competent larvae
Marta Castilla-Gavilán, Meshi Reznicov, Vincent Turpin, Priscilla Decottignies, Bruno Cognie
To cite this version:
Marta Castilla-Gavilán, Meshi Reznicov, Vincent Turpin, Priscilla Decottignies, Bruno Cognie. Jour- nal Pre-proof Sea urchin recruitment: Effect of diatom based biofilms on Paracentrotus lividus com- petent larvae. Aquaculture, Elsevier, 2020, 515, pp.734559. �10.1016/j.aquaculture.2019.734559�.
�hal-02378591�
Journal Pre-proof
Sea urchin recruitment: Effect of diatom based biofilms on Paracentrotus lividus competent larvae
Marta Castilla-Gavilán, Meshi Reznicov, Vincent Turpin, Priscilla Decottignies, Bruno Cognie
PII: S0044-8486(19)31658-8
DOI:
https://doi.org/10.1016/j.aquaculture.2019.734559Reference: AQUA 734559
To appear in:
AquacultureReceived Date: 5 July 2019
Revised Date: 13 September 2019 Accepted Date: 1 October 2019
Please cite this article as: Castilla-Gavilán, M., Reznicov, M., Turpin, V., Decottignies, P., Cognie, B., Sea urchin recruitment: Effect of diatom based biofilms on Paracentrotus lividus competent larvae,
Aquaculture (2019), doi: https://doi.org/10.1016/j.aquaculture.2019.734559.This is a PDF file of an article that has undergone enhancements after acceptance, such as the addition of a cover page and metadata, and formatting for readability, but it is not yet the definitive version of record. This version will undergo additional copyediting, typesetting and review before it is published in its final form, but we are providing this version to give early visibility of the article. Please note that, during the production process, errors may be discovered which could affect the content, and all legal disclaimers that apply to the journal pertain.
© 2019 Published by Elsevier B.V.
-1-
Sea urchin recruitment: effect of diatom based biofilms on Paracentrotus lividus 1
competent larvae 2
Marta Castilla-Gavilán*
┼, Meshi Reznicov
┼, Vincent Turpin, Priscilla Decottignies, 3
Bruno Cognie 4
Université de Nantes, Institut Universitaire Mer et Littoral, EA 2160 Mer Molécules 5
Santé, 2 rue de la Houssinière BP 92208, 44322 Nantes cedex 3 (France) 6
┼
These authors contributed equally 7
*Corresponding author: mcasgavilan@gmail.com 8
Abstract 9
Eight different experimental substrates were tested on Paracentrotus lividus competent 10
larvae in order to evaluate their potential for inducing metamorphosis and enhance 11
survival after recruitment. Two benthic diatoms species, Nitzschia laevis (NL) and 12
Halamphora coffeaeformis (HC), were selected according to their capacity to adhere 13
and to form strong biofilms. They were tested in monocultures and in a mixed biofilm 14
(MIX) that was also tried in combination with Gamma-Aminobutyric Acid, involved in 15
triggering some invertebrate metamorphosis (MIX+GABA). Histamine (HIS) was also 16
used as a treatment according to the high metamorphosis rates that have been recorded 17
for this compound on other sea urchin species. Finally, a natural microphytobenthic 18
biofilm (NATURAL) and oyster shells particles colonized by epiphytic diatoms 19
(SHELL) were sampled from the mud of a refining oyster pond. Batches of 21 days-old 20
larvae were placed on each experimental substrate and their effect was compared to a 21
negative control of filtered sea water (without any treatment; FSW). Metamorphosis rate 22
was daily recorded in each treatment. The sea urchin larvae on substrates NL, 23
NATURAL, GABA+MIX and SHELL showed significantly higher metamorphosis 24
rates than larvae on the other treatments (P < 0.001), reaching more than 90% in 72h.
25
-2-
Survival rate was assessed at 10 days post-metamorphosis in these four treatments. No 26
difference was observed between them in terms of metamorphosis rate or survival rate 27
(more than 60% for the four experimental substrates). Results demonstrate that the 28
transition from planktonic larvae to benthic juvenile could be promoted through diatom- 29
based biofilms. These substrates represent efficient metamorphosis inducers for P.
30
lividus larviculture but we suggest to use preferably N. laevis biofilms in order to 31
promote practical and safe solutions for farmers.
32
Keywords: aquaculture diversification; echinoculture; Nitzschia laevis; metamorphosis 33
rate; post-settlement survival rate 34
Introduction 35
Sea urchin roes are considered as a delicacy and they are among the most valued sea 36
food products. Sea urchin become highly trendy due to their unique taste and the spread 37
of Japanese food around the globe. The leading country in consumption of sea urchins is 38
Japan followed by France, the first market in Europe (Stefánsson et al., 2017). To fulfil 39
this demand, wild populations have been overexploited worldwide leading to a decline 40
since the 90’s (Ceccherelli et al., 2011; Couvray et al., 2015; McBride, 2005). Beyond 41
the economic impact, this depletion has ecological implications as sea urchins have a 42
key role in the infra-littoral rocky shore areas (Giakoumi et al., 2012; Kitching and 43
Thain, 1983; Privitera et al., 2011; Scheibling, 1986).
44
To deal with overexploitation, echinoculture of several species has been developed 45
worldwide (Andrew et al., 2002): for exemple Paracentrotus lividus in Europe, 46
Loxechinus albus in Chile, Strongylocentrotus spp. in China or S. depressus, S.
47
intermedius and S. nudus in Japan. In Europe, certain constraints remain to be solved for
48
-3-
a sustainable and cost-effective industry, notably in the phase of transition between 49
planktonic larvae to a benthic juvenile (Grosjean et al., 1998). Settlement, 50
metamorphosis and post-metamorphosis survival rates are still not high enough to 51
produce juveniles in hatcheries at an industrial-scale (Carbonara et al., 2018; Hannon et 52
al., 2017; Zupo et al., 2018). Researches have been conducted on several sea urchin 53
species to find reliable metamorphosis-inducing-factors for this crucial development 54
stage. Various levels of success have been shown with different species of algae 55
(Carbonara et al., 2018; Castilla-Gavilán et al., 2018b; De la Uz et al., 2013), diatoms 56
and bacterial biofilms (Ab Rahim et al., 2004; Brundu et al., 2016; Dworjanyn and 57
Pirozzi, 2008; Rial et al., 2018; Xing et al., 2007; Zupo et al., 2018), conspecifics 58
(Dworjanyn and Pirozzi, 2008; Gosselin and Jangoux, 1996), and chemical compounds 59
(Carbonara et al., 2018; Pearce and Scheibling, 1990; Swanson et al., 2012). It seems 60
that the most successful metamorphosis-inducing signals are microbial biofilms, 61
whether or not they are linked to the surface of seaweed thalli or inorganic surfaces such 62
as rocks or shells (Hadfield and Paul, 2001). Recent studies have shown the 63
metamorphosis induction effect of benthic diatoms on the culture of P. lividus, 64
obtaining high settlement and survival rates (Rial et al., 2018; Zupo et al., 2018). This 65
zootechnics are also largely used in Japan, China and Chile for sea urchin production in 66
plates covered by natural benthic diatoms biofilms (Ab Rahim et al., 2004; Hagen, 67
1996; McBride, 2005; Rahman et al., 2014; Takahashi et al., 2002; Xing et al., 2007).
68
Moreover, neurotransmitters have been shown to regulate developmental transition in 69
sea urchins, as histamine (Sutherby et al., 2012; Swanson et al., 2012, 2004) and 70
Gamma-Aminobutyric Acid (GABA) (Pearce and Scheibling, 1990; Rahman and 71
Uehara, 2001).
72
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The main objective of the present study was to compare the effect of different inducing 73
cues on the metamorphosis of Paracentrotus lividus and to identify those that could be 74
of easy and cheap application. We tested histamine and GABA, two benthic diatoms 75
(Halamphora coffeaeformis and Nitzschia laevis), a natural benthic biofilm and oyster 76
shells colonized by epiphytic diatoms.
77
Materials and Methods 78
Hatchery of sea urchin larvae 79
Larvae of P. lividus were raised in the Benth’Ostrea Prod aquaculture farm (Bouin, 80
Vendée, France). They were fed on a combined diet consisting of three microalgae 81
species: Isochrysis aff. galbana (clone T-ISO), Rhodomonas sp. and Dunaliella 82
tertiolecta (Castilla-Gavilán et al., 2018a). Larvae were reared in continuous dark at a 83
density of 1 per ml, in 2-m
3conical PVC tanks filled with aerated seawater. A complete 84
water exchange and a thorough cleaning of the tanks were carried out every day. Prior 85
to the experiment, pre-competent larvae were transferred to the laboratory and kept at 86
the same density in an aerated 5 L glass reactor balloon, until competence was achieved.
87
Competence was considered when 75% of larvae had a developed rudiment that was 88
equal or larger than the stomach, as proposed by Kelly et al. (2000).
89
Experimental treatments 90
The chosen treatments for P. lividus competent larvae recruitment assay (see next 91
section) were:
92
- Nitzschia laevis biofilm (NL) 93
- Halamphora coffeaeformis biofilm (HC) 94
- Mix biofilm of both N. laevis and H. coffeaeformis (MIX)
95
-5-
- Natural biofilm sampled from refining oyster ponds (NATURAL) 96
- Broken oyster shells 10 g (SHELL) 97
- Histamine 10
-6M (HIS) 98
- GABA 10
-3M (GABA) 99
- GABA 10
-3M + Mix biofilm of both N. laevis and H. coffeaeformis 100
(GABA+MIX) 101
- Control of filtered seawater (FSW) 102
The diatoms N. laevis and H. coffeaeformis were obtained from the Nantes Culture 103
Collection (UTCC58 and NCC39 from the Mer-Molécules-Santé Laboratory, Nantes, 104
France). These species were chosen for their ability to adhere and to form strong 105
biofilms. Prior to experimental assays, growth kinetics of the two diatoms species 106
selected were assessed (lag time, maximal biomass and maximal specific growth rate).
107
They were grown in 80 mm diameter Pyrex
®Crystallizing Dishes filled with 100 ml of 108
F/2 media. Each dish was inoculated with 50 000 cells/ml. The diatom biofilms were 109
grown in triplicates under conditions of 15°C, 14h:10h L/D cycle at 120 µmol. photons 110
m
-2s
-1. Growth curves were assessed by daily cell counting using a haemocytometer.
111
All experimental treatments were carried out in four replicates in filtered seawater (5 112
µm filtered and UV treated). For NL and HC treatments, biofilms were cultured as 113
explained above. For the MIX treatment, biofilms were cultured by inoculating 25 000 114
cells/ml of each species. Seven days old biofilms were used. One day prior to the 115
recruitment assay, the F/2 media was gently removed and replaced with 100 ml of 116
filtered seawater. For the NATURAL treatment, 3 kg of sediment from an oyster pond 117
of the Benth’Ostrea Prod farm was collected two days prior to the recruitment assay.
118
The natural biofilm was sampled following the protocol described by Eaton and Moss
119
-6-
(1966) and homogenized in 400 ml of filtered seawater. Finally, 100 ml were inoculated 120
in four Crystallizing Dishes for 24 h under natural photoperiod at 20 °C. Oyster shells 121
(SHELL treatment) were collected in an oyster pond from the Benth’Ostrea Prod farm.
122
They were broken into small pieces (1.5-5 cm) placed in four Crystallizing Dishes (10 g 123
in each dish) filled with 100 ml filtered seawater. Prior to the recruitment assay, the 124
presence of an active photosynthetic biofilm on the broken shells was checked using a 125
chlorophyll fluorescence imaging system (Imaging-PAM M-Series, Maxi version, 126
Waltz GmbH; Fig.1). HIS and GABA treatments were prepared in 100 ml of filtered 127
seawater at a concentration of 10
-6M and 10
-3M respectively. Concentrations were 128
chosen according to previous works that have been done with other sea urchins species 129
(Rahman and Uehara, 2001; Swanson et al., 2012). For GABA+MIX treatment, a single 130
MIX treatment was reproduced and 10
-3M of GABA was added. A negative control of 131
100 ml filtered seawater (FSW treatment) was realised in order to estimate the 132
percentage of larvae undergoing spontaneous metamorphosis.
133
Recruitment assay 134
Twenty-one days after fertilisation, when most larvae were competent, 30 larvae were 135
transferred into each experimental treatments. They were kept in the dark at 20°C 136
(Carbonara et al., 2018). Every 24h the metamorphosis was recorded under a 137
stereoscope for all treatments and assessed as follows:
138
metamorphosis % = metamorphosed juveniles
larvae initially dispensed into the dishes x 100
The first four treatments providing a metamorphosis rate of more than 90% were 139
transferred into little tanks (25 x 15 x 10 cm). Each dish was placed on the bottom of a 140
tank filled with aerated filtered seawater changed every 2 days in a 50%. They were
141
-7-
kept at 20°C under a natural photoperiod in order to assess survival of early juveniles.
142
At 10 days post-metamorphosis (DPM), survival was assessed by counting living 143
juveniles on each treatment under a stereoscope as:
144
post − settlement survival % = living juveniles in the dishes
post − larvae initially dispensed into the dishes x 100 Data analysis
145
Growth curves for the diatoms species were established. The collected data from the cell 146
counting was analysed in MATLAB
®R2018a software for fitting to the Gompertz 147
model. This model is known to fit well to diatoms growth kinetic analysis (Lépinay et 148
al., 2018; Zwietering et al., 1990):
149
150
where f(x) is expressed in ln (cell ml
-1); t is time in days to attain maximum biomass of 151
the culture; µ max stands for maximum specific growth rate per day (ln cell ml
-1d
-1); A 152
(ln cell ml
-1) represents maximum biomass and λ is the lag time in days. For both 153
diatom species, these three parameters were compared using a t-test.
154
For metamorphosis and survival data, statistical analyses were performed using the 155
SigmaStat
®9.0 software. Differences were tested using a one-way ANOVA test. When 156
normality test failed, a Kruskal-Wallis one-way analysis of variance on ranks was used.
157
Student-Newman-Keuls a posteriori multiple comparisons tests were carried out when 158
significant differences (P < 0.05) were observed.
159
( ) = exp −exp μ max " #(1) (λ − t) + 1&'
-8- Results
160
For diatom biofilms, A and µ max were significantly higher for N. laevis than H.
161
coffeaeformis (P < 0.01; Table 1). Similar λ were obtained for both species.
162
Growth curves represented by the Gompertz model indicated that both species were in 163
the exponential phase when the experiment was carried out (i.e. 7 days old biofilms).
164
Nevertheless, at this moment of the cultures, biomass was significantly higher in N.
165
laevis biofilms than in H. coffeaeformis (P < 0.001; Fig. 2).
166
After 72h of the experiment, larvae on treatments NL and HC reached more than 91%
167
and 33% of metamorphosis rate respectively (Fig. 3). Both species, on treatment MIX, 168
reached a lower rate (19%). However, when the MIX treatment was associated to the 169
GABA, more than 92% of metamorphosis was observed.
170
The separate treatment of GABA showed a low metamorphosis rate (21%) and no 171
metamorphosed larvae were observed with the HIS treatment. Metamorphosis in the 172
FSW control was less than 1%.
173
With the SHELL and the NATURAL treatment, which were originated from the same 174
environment, metamorphosis reached more than 97%. It is important to note that with 175
the SHELL treatment, larvae did not settled on the shells themselves but on the plates.
176
For easier comparison, we can divide treatments in three groups by their metamorphosis 177
rate results (Fig. 3): group A - NL, NATURAL, GABA+MIX and SHELL, group B - 178
HC, GABA and MIX, and group C - HIS and FSW. Treatments in group A showed 179
significantly higher metamorphosis rates than the treatments in group B and C (P <
180
0.001). Significant differences were also found between treatments in groups B and C 181
(P < 0.05). Between treatments in the same group there was no statistical difference.
182
-9-
Larvae with the treatments of the group A were those transferred to the tanks for 183
survival assessment.
184
Survival 10 DPM was higher than 60% for the four treatments. No difference was found 185
between them (Fig. 4).
186
Discussion 187
In this study we demonstrated that the transition from planktonic larvae to benthic 188
juvenile could be promoted through diatom-based biofilms.
189
The higher metamorphosis rate observed in larvae on N. laevis biofilm compared with 190
larvae on H. coffeaeformis biofilm are in agreement with the results obtained by Xing et 191
al. (2007). This study on Strongylocentrotus intermedius showed that, from a variety of 192
eight species of benthic diatoms, Nitzschia sp. induced the highest metamorphosis rate 193
compare to H. coffeaeformis that induced the lowest. Xing et al. (2007) suggested that 194
the observed differences could be explained by the variability in some characteristics of 195
the biofilms, notably the amount of extracellular polymeric substances (EPS). Nitzschia 196
laevis secrets relatively high amount of EPS that allow it to attach strongly to the 197
substrate and create a robust film. On the opposite, H. coffeaeformis secrets moderate 198
amount of EPS making the adhesive strength of the biofilm poorer. Another 199
characteristic that may vary between diatoms species is their ability to produce toxins 200
and repellent metabolites, sometimes as a protection measurement from grazers 201
(Maibam et al., 2014). Therefore, we can also hypothesize that H. coffeaeformis could 202
produce a repellent substance perturbing the cascade of events that induce settlement 203
and metamorphosis.
204
These substances could also explain the significantly lower metamorphosis rate 205
obtained with both N. laevis and H. coffeaeformis (MIX treatment). As in our
206
-10-
experiment, Xing et al. (2007) obtained higher metamorphosis rates using monospecific 207
diatom biofilms compare to multispecific ones. Further investigation could be done in 208
order to check if H. coffeaeformis produce antifouling compounds or if a significant 209
chemical compound modification appear when co-cultivated with N. laevis (Paul et al., 210
2009).
211
Encrusting algae extracts are known to have an inducing metamorphosis effect on 212
invertebrate larvae. This inducer is an oligopeptide that mimics the action of GABA, an 213
inhibitory neurotransmitter (Morse and Morse, 1984; Rowley, 1989). The 214
metamorphosis effect of GABA has been demonstrated on the sea urchin 215
Strongylocentrotus droebachiensis (Pearce and Scheibling, 1990). In the present study 216
this molecule induced a low metamorphosis rate on P. lividus. However, a different 217
behaviour was observed in the larvae exposed to our GABA treatment: they were all 218
found on the bottom of the plate. In the other treatments the metamorphosed larvae were 219
spread in the water column, which is the normal behaviour in P. lividus, metamorphosis 220
occurring before settlement (Fenaux and Pedrotti, 1988). The behaviour pattern 221
observed with GABA could indicate that this neurotransmitter may function in P.
222
lividus as a separate settlement cue and not as a metamorphosis one. Moreover, as we 223
found similar result in the GABA+MIX and NL treatments, we can hypothesize that 224
GABA could also counteract the negative effect that we observed for H. coffeaeformis 225
on N. laevis.
226
Histamine (HIS treatment) did not induced settlement or metamorphosis in any case.
227
This result agree with the study of Carbonara et al. (2018) that tested five different 228
concentrations of histamine on metamorphosis induction of P. lividus and obtained no 229
metamorphosed larvae.
230
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A similarity was found on the influence of the SHELL treatment and the sediment from 231
the oyster pond (NATURAL treatment) on the larvae. It can be hypothesized that 232
epibionts population on the oyster shell is similar or very close to the one that colonizes 233
the sediment. The metamorphosis rates obtained with these two treatments were similar 234
to the one obtained with NL treatment. This can be explained by the high relative 235
abundance of Nitzschia spp. on oyster shells and mudflats of this region (Barillé et al., 236
2017; Méléder et al., 2007).
237
The four treatments (1) N. laevis biofilms, (2) natural biofilms, (3) oyster shells and (4) 238
a combination of GABA+N. laevis+H. coffeaeformis displayed no statistically different 239
survival rates. They represent metamorphosis inducers of high and similar efficiency for 240
P. lividus larviculture. Biofilms coming from oyster ponds (i.e. natural biofilms and 241
oyster shells) could represent a low cost and sustainable source of metamorphosis 242
inducing cue for oyster farmers. However, these substrates can be a contamination 243
vector and their success could be limited by the spatiotemporal variations in the benthic 244
diatoms communities. To overcome these risks and to promote practical and safe 245
solutions for farmers, this study suggests using preferably N. laevis. Its culture can be 246
conducted by farmers all around the year controlling the quality in terms of growth rates 247
and nutritional profile in an industrial production cycle. This can, on the long term, help 248
oyster farmers to diversify through “echinoculture”.
249
Acknowledgements 250
This study was supported by the Erasmus Mundus Joint Master Degree program ACES 251
(Aquaculture, Environment and Society) and by two European projects: TAPAS “Tools 252
for Assessment and Planning of Aquaculture Sustainability” (Horizon 2020 Grant 253
Agreement No 678396) and BIO-Tide “The role of microbial biodiversity in the
254
-12-
functioning of marine tidal flat sediments” (H 2020 ERA-NET Biodiversia, ANR-16- 255
EBI13-0008-02). The authors wish to thank Benth’Ostrea Prod for providing the living 256
resources. They are also grateful to V. Méléder and E. Cointet for their assistance 257
during diatom-based biofilms culture.
258
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Fig. 1 Imaging of variable chlorophyll fluorescence on oyster shells. Scale bar 403
represents intensity in false colour. Outlines of the oyster shells are indicated as a white 404
line.
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Fig. 2 Growth curves of (A) N. laevis and (B) H. coffeaeformis (mean ± sd).
406
Fig. 3 Metamorphosis rate (%) of P. lividus larvae after 72h exposure to the different 407
treatments. NL = N. laevis, NATURAL = natural biofilm, GABA+MIX = GABA+N.
408
laevis+H. coffeaeformis, SHELL = broken oyster shells, HC = H. coffeaeformis, MIX = 409
N. laevis+H. coffeaeformis, HIS = histamine, FSW = filtered seawater. Data are 410
expressed as mean ± confidence interval 95% (n=4).
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Fig. 4 Survival rate (%) of P. lividus 10 days post-metamorphosis (DPM). NL = N.
412
laevis, NATURAL = natural biofilm, SHELL = broken oyster shells, GABA+MIX = 413
GABA+N. laevis+H. coffeaeformis. Data are expressed as mean ± confidence interval 414
95% (n=4).
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Table 1 Maximum biomass (A in ln cell ml-1), maximum specific growth rate per day (µMax in ln cell ml-1 d-1) and
417
lag time (λ in days) of the two diatoms based biofilms. Data are expressed as mean ± confidence interval.
418
N. laevis H. coffeaeformis A 1.3 x 10
6± 0.3 x 10
60.9 x 10
6± 0.09 x 10
6µMax 0.71 ± 0.14 0.39 ± 0.14
λ 0.04 ± 0.19 0.4 ± 1.69
419
Fig. 1
Fig. 2
Fig. 3
Fig. 4