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1 Bacterial community composition of the sea grape Caulerpa lentillifera: a comparison
2 between healthy and diseased states
3 Germán A. Kopprioa*, Nguyen Dinh Luyenb,c, Le Huu Cuongb,c, Anna Fricked, Andreas
4 Kunzmanne, Le Mai Huongb,c, Astrid Gärdesf,g
5 a Leibniz Institute of Freshwater Ecology and Inland Fisheries, Berlin, Germany
6 b Institute of Natural Product Chemistry, Vietnam Academy of Science and Technology, Hanoi,
7 Vietnam
8 c Graduate University of Science and Technology, Vietnam Academy of Science and
9 Technology, Hanoi, Vietnam
10 d Leibniz Institute of Vegetable and Ornamental Crops, Großbeeren, Germany
11 e Leibniz Centre for Tropical Marine Research, Bremen, Germany
12 f University of Applied Sciences, Bremerhaven, Germany
13 g Alfred Wegener Institute, Helmholtz Centre for Polar and Marine Research, Bremerhaven,
14 Germany
15 * Corresponding author at: Chemical Analytics and Biogeochemistry, Leibniz Institute of
16 Freshwater Ecology and Inland Fisheries, Müggelseedamm 301, 12587 Berlin, Germany. E-
17 mail: [email protected]
18 Key words: Vietnam, seaweed, aquaculture, green caviar, 16S rRNA diversity
19
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20 Summary
21 The bacterial communities of the sea grape Caulerpa lentillifera were studied during a disease
22 outbreak in Vietnam. The Rhodobacteraceae and Rhodovulum dominated the composition of
23 healthy C. lentillifera. Clear differences between healthy and diseased cases were observed at
24 order, genus and Operational Taxonomic Unit (OTU) level. Bacterial diversity was lower in
25 healthy C. lentillifera, probably because of antimicrobial compounds from the macroalgae and/or
26 from Clostridium, Cutibacterium or Micrococcus bacteria. The likely beneficial role of
27 Bradyrhizobium, Paracoccus and Brevundimonas strains on nutrient cycling and phytohormone
28 production was discussed. The white coloration of diseased C. lentillifera may not only be
29 associated with pathogens but also with an oxidative response. Aquibacter, Winogradskyella
30 and other OTUs of the family Flavobacteriaceae were hypothesized as detrimental bacteria, this
31 family comprises some well-known seaweed pathogens. Moreover, Thalassobius OTU 2935
32 and 1635 may represent detrimental Rhodobacteraceae. Phycisphaera together with other
33 Planctomycetes and Woeseia were probably saprophytes of C. lentillifera. This study offers
34 pioneering insights on the co-occurrence of C. lentillifera-attached bacteria, potential detrimental
35 or beneficial microbes, and a baseline for understanding the C. lentillifera holobiont. Further
36 metagenomic and biotechnological approaches are needed to confirm functions of some
37 microbes on this macroalgae to enhance food security in the tropics.
38 Introduction
39 The sea grape or green caviar Caulerpa lentillifera is a green macroalgae widely cultivated in
40 tropical countries of the Indo-Pacific region, and its market as seafood delicacy has been
41 expanded drastically in the last decades. Not only C. lentillifera flavor, vesicular ramuli and
42 succulent texture which resembles caviar, but also elevated contents of polyunsaturated fatty
bioRxiv preprint doi: https://doi.org/10.1101/2021.06.30.450479; this version posted June 30, 2021. The copyright holder for this preprint (which was not certified by peer review) is the author/funder, who has granted bioRxiv a license to display the preprint in perpetuity. It is made available under aCC-BY-NC-ND 4.0 International license.
43 acids, antioxidants, vitamins and trace elements (Saito et al., 2010; Paul et al., 2014; de
44 Gaillande et al., 2017; Yap et al., 2019), together with its marketing as functional food increased
45 exponentially its demand. Moreover, the combination of the high nutritional quality of C.
46 lentillifera with its simple and low-cost cultivation transforms this macroalgae in a promising
47 candidate to enhance food security of tropical countries (de Gaillande et al., 2017; Stuthmann et
48 al., 2021). However, one of the major factor contributing to the worldwide decline of macroalgal
49 populations are microbial diseases (Egan et al., 2014) and C. lentillifera aquaculture is currently
50 endangered by outbreaks.
51 Macroalgae provide a nutrient-rich niche for microbes and some bacteria are capable to invade
52 algal tissue degrading complex polymers causing disease. Agarases, carrageenases, alginases,
53 fucoidanases, fucanases, mannanases, cellulases and pectinases are depolymerizing enzymes
54 detected in several marine bacteria for the breakdown of algal cell walls (Goecke et al., 2010).
55 Moreover, the low genetic diversity of cultured algae and their tight distribution in aquaculture
56 settings facilitate the rapid spread of detrimental microbes. Several bacterial diseases have
57 been reported in commercial macroalgae such as the rote spot and hole-rotten diseases caused
58 by Pseudomonas spp. in Saccharina japonica, rotten thallus syndrome by Vibrio sp. in
59 Gracilaria verrucosa, or Anaaki by Flavobacterium spp. in Pyropia yezoensis (Goecke et al.,
60 2010b; Egan et al., 2014; Ward et al., 2020). Nevertheless, the role of microbes is not only
61 detrimental but can also be beneficial.
62 Some bacteria are essential for algal health, growth and development. Beneficial bacteria
63 attached to macroalgae induce morphogenesis, fix nitrogen, produce phytohormones, release
64 antifouling and antimicrobial compounds, transport metabolites and nutrients, detoxify
65 pollutants, contribute to algal reproduction and are key for their adaptation to new environments
66 (Aires et al., 2013; Hollants et al., 2013; Singh and Reddy, 2014). The relation between
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67 macroalgae and bacteria is generally mutualistic, and bacteria are mainly benefited with organic
68 substrates for their metabolism and a stable micro-environment protected from predators and
69 changing environmental conditions. The relations between macroalgae and bacterial
70 communities are so tight and reciprocal that the whole entity is considered a holobiont (Egan et
71 al., 2013; Arnaud-Haond et al., 2017; Califano et al., 2020). Furthermore, the bioactive
72 compounds produced by microbes in the holobiont have an enormous potential for drug
73 discovery and biotechnological applications (Friedrich, 2012; Luyen et al., 2019).
74 Despite the commercial importance of C. lentillifera and its relevance for human nutrition under
75 future climate-driven and overpopulation scenarios, studies about their microbiome are very
76 limited. Liang et al., (2019) described a disease in C. lentillifera in Chinese aquaculture systems
77 characterized by a dark-green biofouling, pink-colorated and missing ramuli. In this particular
78 case, Bacteroidetes and Cyanobacteria dominated the bacterial communities of diseased C.
79 lentillifera. Although recent advances in the study of the macroalgal microbiome using next
80 generation techniques, the information is still limited and mostly derived from culture methods
81 with their intrinsic limitations. The 16S rRNA gene approach offers broader insights on the
82 natural composition of bacterial communities attached to algae and plays an important role in
83 understanding algal diseases (Egan et al., 2014; Kopprio et al., 2021). Aims of this work were:
84 1) to characterize the bacterial communities of C. lentillifera in Vietnamese aquaculture, and 2)
85 to assess the effect of an unknown disease on its bacterial community composition. We
86 hypothesize strong differences in bacterial communities of C. lentillifera between healthy and
87 diseased cases.
88 Results
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89 The order Rhodobacterales (class Alphaproteobacteria) and the genus Rhodovulum of the
90 mentioned order presented the highest relative sequence abundance in C. lentillifera at each
91 respective taxonomic level (Fig. 1). The Rhodobacteraceae was the only family detected within
92 the order Rhodobacterales. According to the Mann-Whitney test, the mean relative abundance
93 of Clostridiales (phylum Firmicutes) was significantly higher in healthy C. lentillifera, whereas the
94 abundances of Flavobacteriales (phylum Bacteroidetes), Phycisphaerales (phylum
95 Planctomycetes) and Steroidobacterales (class Gammaproteobacteria) characterized diseased
96 C. lentillifera thalli. The 99.7 % of the OTUs for the order Flavobacteriales corresponded to the
97 family Flavobacteriaceae. The trend observed at order level was similar at genus level: the
98 relative sequence abundance of Clostridium sensu stricto 7 (Clostridiales) was significantly
99 higher in healthy cases, while Aquibacter and Flavobacteriaceae unclassified (Flavobacteriales),
100 Phycisphaera (Phycisphaerales) and Woeseia (Steroidobacterales) were typical of diseased
101 cases. Without significant differences, other abundant genera were Rhodovulum, Cutibacterium
102 and Paracocccus for healthy C. lentillifera, while Thalassobius, Tropicibacter and Blastopirellula
103 for diseased C. lentillifera.
104
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105 Fig 1 Mean relative sequence abundance (± standard deviation) of the main orders and genera in healthy and
106 diseased individuals of the sea grape Caulerpa lentillifera. (*) indicates significant differences at p < 0.05 according to
107 Mann-Whitney test. Caption superscript: shows correspondence between order and genus (e.g., Rho =
108 Rhodobacterales). uncl.: unclassified, Aphaproteobact.: Alphaproteobacteria, Clostr.: Clostridium, Cand. Kaiserbact.:
109 Candidatus Kaiserbacteria, Flavobact.: Flavobacteriaceae, mar. gr.: marine group, Methyloligel.: Methyloligellaceae
110 PERMANOVA revealed significant differences between the healthy and diseased cases at order
111 level (Pseudo-F = 3.89, p = 0.016). According to SIMPER analyses, the total dissimilarity
112 between healthy and diseased cases was 41.3%. The orders which presented significant
113 differences in the Mann-Whitney test were also important contributors to the dissimilarities and
114 evidenced the same trend in healthy or diseased C. lentillifera (Table I). Other relevant orders
115 with higher percentages of dissimilarities but without significant differences were
116 Propionibacteriales and Betaproteobacteriales for the healthy cases, while Saccharimonadales
117 and Verrucomicrobiales for the diseased cases. Furthermore, PERMANOVA detected
118 significant differences at OTU level between healthy and diseased C. lentillifera (Pseudo-F =
119 3.12, p = 0.015). According to SIMPER analysis, the total dissimilarity at OTU level was 71.3%
120 and the main OTUs contributing to this value are detailed in Table I.
121 Table I Main orders and operational taxonomic units (OTUs) of the sea grape Caulerpa lentillifera contributing to the
122 dissimilarity (41 and 71 % in total, respectively) according to SIMPER analyses. Taxa are grouped based on their
123 dominance in healthy or diseased cases.
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124
125 The OTUs of order Clostridiales, typical of healthy C. lentillifera, were Clostridium sensu stricto
126 7 4975 and 1787 (Table I). Other OTUs dominating with elevated percentages of dissimilarity in
127 the healthy cases were those of the genera: Paracoccus, Spongiimonas, Cutibacterium,
128 Aliihoeflea, Pelomonas, Brevundimonas and Bradyrhizobium. In the case of diseased cases, the
129 major OTUs were those of Flavobacteriaceae unidentified, Aquibacter, Winogradskyella,
130 Aureicoccus and Ulvibacter for the order Flavobacteriales (all belonging to the family
131 Flavobacteriaceae), Phycisphaera for the order Phycisphaerales and Woeseia for the order
132 Steroidobacterales. Other OTUs with elevated percentages of dissimilarity in the diseased
133 cases were Methyloligellaceae unclassified 0867, Thalassobius 2935, Pir4 lineage 0189 and
134 JGI 069-P22 unclassified 0837. A list with other relevant OTUs according to their dissimilarity is
135 presented in table I. Moreover, the NMDS ordination of C. lentillifera samples at OTU level (Fig
136 2) suggested contrasting bacterial communities between healthy and diseased cases .
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137
138 Fig 2 Non-metric Multi-Dimensional Scaling (NMDS) ordination of healthy and diseased individuals of the sea grape
139 Caulerpa lentillifera at Operational Taxonomic Unit (OTU) level
140
141 Fig 3. Heatmap of the main Operational Taxonomic Units (OTUs) on healthy (H) and diseased (D) individuals of the
142 sea grape Caulerpa lentillifera. (*) unclassified (**) sensu stricto 7
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143 The heat map (Fig. 3) showed a similar cluster of 4 diseased C. lentillifera, while a variable
144 ordination of the other cases. OTUs associated exclusively to diseased status were Aquibacter
145 3662, Flavobacteriaceae unclassified 2304, Woeseia 0634, Phycisphaera 3117 and Muricauda
146 2354; while those exclusively detected in the healthy status were Bradyrhizobium 1899,
147 Paracoccus 4667 and Paracoccus 2980. OTUs of the genera JGI 069-P22 unclassified,
148 Thalassobius, Saccharimonadales unclassified, Flavobacteriaceae unclassified,
149 Winogradskyella, Aureicoccus, Pir4 lineage, Tropicibacter, Algisphaera, Cellvibrionaceae
150 unclassified and Aquibacter dominated mainly in the diseased cases. Other OTUs which
151 dominated but not exclusively in the healthy cases are displayed in the heat map. The inverse
152 Simpson indexes at the bottom of the heat map indicated mainly a higher diversity in diseased
153 C. lentillifera.
154 Discussion
155 Main composition and potential beneficial bacteria
156 The bacterial communities of C. lentillifera presented a similar composition than other green
157 algae at higher taxonomic levels. The dominance of Alphaproteobacteria and Bacteroidetes has
158 been reported in green macroalgae and some Caulerpa species (Friedrich, 2012; Aires et al.,
159 2013; Singh and Reddy, 2014). The order Rhodobacterales and family Rhodobacteraceae
160 dominated the bacterial communities of C. lentillifera in this particular case from the Vietnamese
161 aquaculture. Bacteria within the order Rhodobacterales are generally surface colonizers and
162 facilitate the settlement of microbial communities with the production of extracellular polymeric
163 substances (Kopprio et al., 2020). According to Simon et al. (2017), marine Rhodobacteraceae
164 are characterized by genes for the degradation of sulfated polysaccharides from algae,
165 production of phytohormones, metabolism of osmolytes, transport of metals and detoxification.
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166 The bacterial communities at lower taxonomic levels are generally highly variable in seaweeds
167 and their composition may be associated with a particular function within the holobiont. The
168 microbiome composition depends generally on the geographic location, environmental factors,
169 seaweed tissues, developmental stage and even among local individuals (reviewed by
170 Friedrich, 2012). Burke et al., (2011) explain the pattern of bacterial colonization on a green
171 macroalgae with the competitive lottery model, according to this model different species with
172 similar functional traits can occupy the same niche depending on a stochastic probability. The
173 highest relative abundance of Rhodobacterales coincided with the results obtained in C.
174 lentillifera from China (Liang et al., 2019); nevertheless, one of the differences was in the
175 dominant genus within this order: Leisingera in contrast to Rhodovulum in our study. Moreover,
176 the last authors reported a higher abundance Planctomycetales and Oceanospirillales in healthy
177 C. lentillifera and not the elevated values of Clostridiales observed in this study.
178 Rhodovulum and particularly Paracoccus are Rhodobacteraceae with potential beneficial roles
179 for C. lentillifera. Rhodovulum species have a high metabolic versatility with the capability to
180 degrade organic pollutants, to produce polymers and to contribute with photosynthetic functions
181 (Khandavalli et al., 2018; Foong et al., 2019; Baker et al., 2021). Paracoccus is a common
182 genus among seaweed-associated bacteria with a key role in the cycle of nitrogen and in the
183 production of siderophores (Mei et al., 2019). Paracoccus strains promote the growth and the
184 morphogenesis in Ulva species (Ghaderiardakani et al., 2017) and were described as auxin
185 producers (Kurepin et al., 2014). Plant hormone production seems to be widespread in various
186 genera of marine bacteria (Goecke et al., 2010). Furthermore, Paracoccus sp. presented
187 algicidal activity (Zhang et al., 2018) and some members of this genus might contribute with
188 antifouling activities. The macroalgal surfaces constitute a highly competitive niche for nutrient
189 and space.
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190 The likely production of antimicrobial compound of C. lentillifera may explain partially the low
191 diversity in healthy C. lentillifera. The same diversity trend was reported comparing healthy and
192 diseased C. lentillifera from the Chinese aquaculture (Liang et al., 2019). Some Caulerpa
193 species contain antibacterial compounds such as alkaloids, terpenoids, phenols and flavonoids
194 (Goecke et al., 2010; Yap et al., 2019; Zainuddin et al., 2019). Moreover, strains of Clostridium
195 sensu stricto 7 and Cutibacterium may reduce diversity with the production of antimicrobial
196 metabolites in healthy C. lentillifera. Some green algae provide a habitat for Clostridium species
197 and even for potential pathogens (Chun et al., 2013). Clostridium spp. can catabolize several
198 algal polymers (Song et al., 2011), have a likely function of copper detoxification in Codium
199 tormentosum (Le Pennec and Gall, 2019), and are sources of novel antimicrobial compounds
200 (Schieferdecker et al., 2019; Pahalagedara et al., 2020). A new thiopeptide antibiotic as
201 microflora modulator was detected on Cutibacterium sp. (Claesen et al., 2020) and some
202 species of this genus might produce antibiotics on Kappaphycus striatus (Kopprio et al., 2021).
203 A similar role on algal defense is suspected in the other Actinobacteria Micrococcus spp. (e.g.,
204 Hollants et al., 2013). In addition, this genus together with Bradyrhizobium were reported as
205 beneficial endophytic bacteria in many terrestrial plants with agronomic value (Afzal et al.,
206 2019).
207 Bradyrhizobium and Allihoeflea of the order Rhizobiales may participate in the cycle of nitrogen
208 and the production of phytohormones. “Rhizobacteria” were extensively studied in terrestrial
209 plants because of their ability to fix nitrogen and to modify genetically their host. Some
210 organisms of the family Rhizobiaceae presented growth-enhancing and probiotic properties on
211 green microalgae (Rivas et al., 2010). Furthermore, an endosymbiotic bacterium of this taxa
212 was responsible for the nitrogen supply in Caulerpa taxifolia (Chisholm et al., 1996).
213 Bradyrhizobium japonicum increases the biomass and starch content of the green microalgae
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214 Chlamydomonas reinhardtii (Xu et al., 2016) and some strains of B. japonicum are producers of
215 the several phytohormones such as indole-3-acetic acid, gibberellic acid, zeatin, abscisic acid
216 and ethylene (Boiero et al., 2007).
217 A key role for C. lentillifera growth and health is supposed on strains of Brevundimonas spp.
218 Member of this genus establish a symbiotic relationship with green microalgae promoting their
219 growth, producing indole-3-acetic acid and enhancing nutrient uptake (Tate et al., 2013; Sforza
220 et al., 2018; Zhang et al., 2021). Some of their strains have a potential antifouling activity
221 against cyanobacteria (Lin et al., 2014) and in some terrestrial plants: alleviate toxicity, fix
222 nitrogen and promote growth (Singh et al., 2016; Naqqash et al., 2020). Pelomonas OTU 1964
223 sustains presumably a healthy status on C. lentillifera. This genus is common in the rhizosphere
224 of some plants with a nitrogen fixation function (Terakado-Tonooka et al., 2008) and some of
225 their aquatic strains produce the antibacterial compounds such as pelopuradazole (He et al.,
226 2014). Surprisingly, potential human pathogens like Escherichia-Shigella and Staphylococcus
227 were related to the healthy state of C. lentillifera according to SIMPER analysis. Hollants et al.,
228 (2013) reported these bacteria with the beneficial functions of defense and morphogenesis in
229 seaweeds, respectively.
230 Potential detrimental bacteria
231 The lack of production of antibacterial compounds by diseased C. lentillifera or the absence of
232 of some defense microorganisms may increase bacterial diversity. As mentioned in the above
233 section, this pattern was also observed in China, where the orders Flavobacteriales,
234 Phycisphaerales and Cellvibrionales dominated the diseased and decayed thalli of C. lentillifera
235 (Liang et al., 2019). With different disease symptoms, a similar pattern was observed in our
236 study: Flavobacteriales, Phycisphaerales and an unidentified genus of the family
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237 Cellvibrionaceae were typical of diseased C. lentillifera. The bleaching and white coloration
238 symptom in C. lentillifera may not only be linked to a pathogen invasion, but also to an oxidative
239 burst response as a defense mechanism. Some Caulerpa species produce reactive oxygen
240 species like hydrogen peroxide against invasive organisms (Box et al., 2008).
241 The copiotrophic nature and ability to catabolize algal polymers of the Flavobacteriaceae gives
242 to this family, the potential to breakdown algal walls, to invade tissues and to cause disease
243 under certain conditions. Bacteroidetes and particularly Flavobacteriaceae are degraders of
244 complex biopolymers like sulfated polysaccharides from algal tissues (Yilmaz et al., 2016; Jain
245 et al., 2019). Many members of the Flavobacteriaceae have been confirmed or suspected as
246 causative agents of seaweed diseases (Goecke et al., 2010; Kumar et al., 2016; Ward et al.,
247 2020). In our particular case, we hypothesize as potential pathogens: strains of Aquibacter,
248 Winogradskyella, Aureicoccus, Ulvibacter and Muricauda. Aquibacter spp. characterized the
249 senescent state and decayed phase of the diatom Skeletonema dohrnii (Liu et al., 2021). In the
250 case of Winogradskyella spp., higher abundances have been observed on Pyropia yezoensis
251 with yellow spot disease (Liu et al., 2020) and on Delisea pulchra with a bleaching disease
252 (Kumar et al., 2016). On the other hand, Flavobacteriales are a common order among green
253 algae (Hollants et al., 2013) and Spongiimonas was linked to healthy C. lentillifera.
254 We hypothesize that Phycisphaera and Algisphaera spp. of the order Phycisphaerales were
255 opportunistic pathogens or saprophytes of C. lentillifera. As mentioned before, the order
256 Phycisphaerales was typical of the disease cases from the Chinese aquaculture and strains of
257 these genera were isolated from marine macroalgae presenting agarolitic activity (Fukunaga et
258 al., 2009; Yoon et al., 2014). Nevertheless, Planctomycetes are widespread in the epiphytic
259 microbial community of macroalgae, possess potential beneficial effects for their host like the
260 production of bioactive compounds, and are rarely identified as seaweed pathogens (Lage and
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261 Bondoso, 2014). Some strains of Phycisphaera, Algisphaera, Pir 4 lineage and Blastopirellula
262 may be using their higher number of sulfatases for the degradation of algal polysaccharides
263 (Bondoso et al., 2017) from the dead or senescent tissue of C. lentillifera, which could be injured
264 by other pathogen or degraded because of an oxidative defense response. Other probable
265 saprophyte was Woeseia, species of this genus can utilize a broad range of energy-yielding
266 metabolisms and substrates (Mußmann et al., 2017). Some bacteria may be specialized on
267 small molecules derived from the breakdown of algal polymers and benefited from the
268 degradation of algal tissue. Members of the family Methyloligellaceae oxidize generally one
269 carbon atom molecules (Walker et al., 2021) and Patescibacteria (JGI 069-P22 and some
270 Saccharimonadales in this study) may be using monosaccharides because they have reduced
271 genes for polysaccharide catabolism in their simple genomes (Tian et al., 2020).
272 The classification of potential beneficial or detrimental bacteria at higher taxonomic levels in C.
273 lentillifera is not clear. The orders Verrucomicrobiales is well-known as active polysaccharide
274 degraders (Martinez-Garcia et al., 2012) but only a few genera were linked to algal disease. For
275 example, several OTUs of Rubritalea within this order were typical of Saccharina japonica with
276 symptoms of rotten hole disease (Zhang et al., 2020). Furthermore, the ability to metabolize
277 algal compounds of Rhodobacteraceae in a mutualistic relationship with seaweeds, may
278 became detrimental with some members of this family such as Thalassobius and Tropicibacter.
279 Thalassobius spp. characterized diseased Delisea pulchra (Kumar et al., 2016) and were
280 responsible of the direct lysis of a red-tide microalgae (Wang et al., 2010). Tropicibacter
281 multivorans has been detected in the microbiome of Caulerpa cylindraceae but little information
282 is available about its function (Rizzo et al., 2016). In this study case, Tropicibacter spp. may
283 contribute with the degradation of algal polymers.
284 Conclusions
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285 Despite of different symptoms comparing cases from Vietnamese and Chinese C. lentillifera
286 cultures, a common bacterial pattern was observed on diseased organisms. A disease on C.
287 lentillifera may be caused by a community of detrimental bacteria together with changes on
288 algal response, and not only by a particular pathogen. Moreover, with this 16S rRNA approach
289 is not possible to identify clearly pathogens from saprophytes. A mutualistic relationship with a
290 particular bacteria may change and became detrimental under certain conditions; nevertheless,
291 clear differences between the healthy and diseased states were observed at several taxonomic
292 levels. This work explores changes in the bacterial community composition of C. lentillifera
293 under two conditions, detects co-occurrence but not causality, we cannot discard other
294 etiological agent not covered by the selected amplicon. Common patterns and roles were
295 inferred on this pioneer work from the Vietnamese aquaculture, which contribute to the
296 understanding of potential key players in the holobiont. A further metagenomic approach will
297 confirm the presence of functional genes for a particular microorganisms and their potential
298 biotechnological applications.
299 Experimental Procedures
300 Culture conditions, sampling and disease symptoms
301 Caulerpa lentillifera thalli were sampled in the culture facilities of the company VIJA at Van
302 Phong bay (N 12° 35' 17.67", E 109°13' 39.76") in the central eastern coastline of Vietnam. The
303 ponds for C. lentillifera culture were used previously for shrimp farming and contained
304 apparently a considerable load of organic matter. Water temperature in the ponds reached
305 ~31°C in May, with pH values of ~ 8.1, conductivity ~53 mS cm-1 and dissolved oxygen ~5.6 mg
306 L-1. The sea grape ponds were covered from direct sunlight radiance with shade cloths. Six
307 healthy and seven diseased thalli of C. lentillifera were collected during an outbreak of an
bioRxiv preprint doi: https://doi.org/10.1101/2021.06.30.450479; this version posted June 30, 2021. The copyright holder for this preprint (which was not certified by peer review) is the author/funder, who has granted bioRxiv a license to display the preprint in perpetuity. It is made available under aCC-BY-NC-ND 4.0 International license.
308 unknown disease. In contrast to the bright green color of healthy individuals (Fig. 1A), the
309 diseased C. lentillifera showed a marked tissue discoloration and a white biofilm on the external
310 circumference of the vesicular ramuli (Fig. 1B). After the described symptoms, the diseased
311 algae lost their turgid appearance and decayed with the consequent loss of their commercial
312 value.
313 314 Fig 4. A) Healthy thalli of Caulerpa lentillifera and aquaculture facilities in Vietnam. B) A comparison between healthy
315 (up) and diseased (down) individuals, the diseased individuals showed bleaching of thalli and a white biofilm on the
316 external circumference of the ramuli.
317 DNA extraction and amplification
318 Caulerpa lentillifera individuals were collected in sterile vials and preserved at -20°C until further
319 analysis. Under laboratory conditions, DNA was extracted basically according to Griffiths et al.,
320 (2000). Fragments of the thalli were immersed in 600 µL of hexadecyltrimethylammonium
321 bromide (CTAB) with 60 µL of 10 % SDS and 60 µL of 10 % N-lauroylsarcosin. Glass beads
bioRxiv preprint doi: https://doi.org/10.1101/2021.06.30.450479; this version posted June 30, 2021. The copyright holder for this preprint (which was not certified by peer review) is the author/funder, who has granted bioRxiv a license to display the preprint in perpetuity. It is made available under aCC-BY-NC-ND 4.0 International license.
322 were added and the tissue was homogenized in a FastPrep at 5 m s-1. Homogenates were
323 rinsed with 600 µL of phenol-chloroform-isoamylalcohol (25:24:1) and centrifuged at 16,000 g
324 and 4°C for 10 min. The upper aqueous layer was transferred to a clean reaction tube, mixed
325 with 2 volumes of 30 % polyethylene glycol (PEG) 6000 and 1.6 M NaCl and incubated at 4°C
326 for 120 min. Subsequently, the sample was centrifuged at 17,000 g and 4°C for 90 min, the
327 supernatant was carefully removed and the pellet was washed with ice-cold 70% ethanol. The
328 pellet was air-dry at 37°C for a few minutes, dissolved in PCR grade water and stored at -20°C.
329 The hypervariable region V3-V4 of the 16S rRNA gene was amplified with the set of primers
330 according to Klindworth et al., (2013): Bact-341F (5´-3´: CCT ACG GGN GGC WGC AG) and
331 Bact-785R (GAC TAC HVG GGT ATC TAA KCC)
332 Sequencing, bioinformatics and statistical analysis
333 The amplicon V3-V4 of the 16S rRNA gene was sequenced with a 2 x 300-bp paired-end run on
334 an Illumina MiSeq platform. Sequencing, removal of primer sequences and demultiplexing were
335 conducted by the company LGC genomics. Sequences were trimmed and merged using
336 Trimmomatic v0.36 (Bolger et al., 2014) and PEAR v0.9.8 (Zhang et al., 2014), respectively.
337 Operational Taxonomic Units (OTUs) were clustered by Minimum Entropy Decomposition MED
338 v2.1 (Eren et al., 2015) and their representatives were submitted to SilvaNGS (v132,
339 https://ngs.arb-silva.de/silvangs/) using a sequence similarity of one for clustering and the
340 remaining variables as default. Singleton, doubleton and sequences from mitochondria,
341 chloroplasts and archaea were removed from the analysis. A total of ~222,000 reads remained
342 after data curation and the mean OTU number per sample was ~17,100 ± 14,500 (± standard
343 deviation). Demultiplexed and primer-clipped sequences were deposited at the European
344 Nucleotide Archive (ENA) using the data brokerage service of the German Federation for
bioRxiv preprint doi: https://doi.org/10.1101/2021.06.30.450479; this version posted June 30, 2021. The copyright holder for this preprint (which was not certified by peer review) is the author/funder, who has granted bioRxiv a license to display the preprint in perpetuity. It is made available under aCC-BY-NC-ND 4.0 International license.
345 Biological Data (Diepenbroek et al., 2014) with the number PRJEB42826, in compliance with
346 the Minimal Information about any (x) Sequence (MIxS) standard (Yilmaz et al., 2011).
347 Pooling of taxa, removal of OTUs with poor alignment quality and relative sequence abundance
348 and diversity calculations were conducted in R v4.0.5 (R Core Team, 2021) and additional
349 packages. The relative sequence abundances of the main orders between the diseased and
350 healthy cases were compared with a Mann-Whitney test. Data were transformed, a Bray Curtis
351 similarity matrix was calculated, and differences between the states at order and OTU level
352 were evaluated using permutational multivariate analysis of variance (PERMANOVA). In case of
353 significance differences, similarity percentage analysis (SIMPER) was performed to detect the
354 main taxa contributing to dissimilarities. Samples at OTU level were ordinated by Non-metric
355 Multi-Dimensional Scaling (NMDS). A heat map based on the 60 most abundant OTUs,
356 covering the 64 ± 11 % of the total relative sequence abundance, was displayed to compare
357 healthy and diseased cases. Graphics and statistics were performed with R 4.0.5, Xact 7.21,
358 PRIMER v6 + PERMANOVA, and XLSTAT-Ecology
359 Acknowledgment
360 We are grateful with T. M. Duc for logistical support.
361 Data availability
362 16S sequencing data are available at ENA (https://www.ebi.ac.uk/ena/data/view/PRJEB42826).
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