shifts between autotrophy and heterotrophy in the reef ......(predação sobre zooplâncton). alguns...
TRANSCRIPT
ARTHUR DE ALBUQUERQUE TENÓRIO
Shifts between autotrophy and heterotrophy in the reef-building
coral Mussismilia hispida: an approach using fatty acid trophic
markers
Thesis presented at the Oceanographic Institute of the University of São Paulo, as part of the requirements for obtaining the title of Master in Sciences, Oceanography Program, concentration area of Biological Oceanography.
Supervisor: Prof. Dr. Paulo Y. G. Sumida.
São Paulo
2016
ARTHUR DE ALBUQUERQUE TENÓRIO
Shifts between autotrophy and heterotrophy in the reef-building
coral Mussismilia hispida: an approach using fatty acid trophic
markers
São Paulo
2016
Universidade de São Paulo
Instituto Oceanográfico
Shifts between autotrophy and heterotrophy in the reef-building coral Mussismilia
hispida: an approach using fatty acid trophic markers
Arthur de Albuquerque Tenório
Thesis presented at the Oceanographic Institute of the University of São Paulo, as part of the
requirements for obtaining the title of Master of Science, Oceanography Program,
concentration area Biological Oceanography.
Evaluated in: ___/___/____
Prof. Dr. Grade
Prof. Dr. Grade
Prof. Dr. Grade
i
SUMMARY
ACKNOWLEDGEMENTS ................................................................................................................. ii
RESUMO ....................................................................................................................................... iii
ABSTRACT ......................................................................................................................................iv
LIST OF FIGURES ............................................................................................................................ v
LIST OF TABLES ............................................................................................................................. vii
INTRODUCTION ............................................................................................................................. 1
MATERIALS & METHODS ............................................................................................................... 5
Study area and experimental design ......................................................................................... 5
Coral tissue sample processing ................................................................................................. 8
Symbiodinium cell count ........................................................................................................... 8
Fatty acid extraction .................................................................................................................. 9
Gas chromatography ............................................................................................................. 9
Fatty acid trophic markers reference samples ........................................................................ 10
Statistical analyses .................................................................................................................. 12
RESULTS ....................................................................................................................................... 14
Environmental data and Symbiodinium concentration .......................................................... 14
Fatty Acids Trophic Markers reference samples ..................................................................... 21
Fatty Acids Trophic Markers.................................................................................................... 24
Autotrophy vs. heterotrophy – Coral Trophic Index ............................................................... 28
DISCUSSION ................................................................................................................................. 30
LITERATURE CITED ....................................................................................................................... 34
ii
ACKNOWLEDGEMENTS
This work would never been possible to complete without the support of my family. I
will be forever thankful to my Aunt Ana Paula von Sothen and Uncle Otto von Sothen, which
received me in their house and made my stay in São Paulo conceivable. I thanks my parents
Virginia Maria Albuquerque de Araújo and José Ivon Tenório Uchoa for the support, love and
care.
I want to express here my gratitude for the opportunity given to me by my supervisor
Dr. Prof. Paulo Yukio Gomes Sumida. His trust, guidance and friendship were crucial to overcome
all difficulties found during the last two and a half years.
This project would never exist without the help of many friends. I give a special thanks
to PhD student Miguel Mies for the full support, late nights of work and all great time along. Our
lab technician Arthur Z. Güth made my life a lot less miserable, thanks for the support in the
most needed moments. Undergraduation student Jonas Mendes volunteered his time and
strengths during most part of my field trips, without you I would probably still be underwater.
To all other friends from the Instituto Oceanográfico, thanks for the good times, coffee brakes
and everything between.
Friendships completes our lives and makes it more fun. I came to know many amazing
people during this master and I thanks every single one of you that crossed my path. I would like
to thanks Adrian Gonzales and Eric Siciliano for all great times we went through and will go
through. To all friends from Boulder CEPEGE and C.A. da Bio, thank you.
I thanks to CAPES for the scholarship provided. The Oceanographic Institute for the
logistics and operational support and to all employees from Clarimundo de Jesus Research Base
in Ubatuba. It was great to work with all of you.
Lastly, I would like to thanks Clarisse C. L. Miguelote for the best present a person can
receive in life. Thank you for the life of my sun Rafael Miguelote Tenório, and thank you for been
the best mom in the world during my absence.
iii
RESUMO
Os recifes de coral estão entre os ambientes marinhos mais produtivos e ricos em
biodiversidade. Esta biodiversidade está em parte associada a complexas estruturas
formadas por corais escleractíneos. Apesar da importância ecológica, social e econômica
dos recifes de corais, eles são expostos a várias ameaças relacionadas às atividades
humanas. Dentre os impactos antrópicos em recifes, o branqueamento, ou perda de
zooxantelas, é o mais notável e é diretamente relacionado à mortalidade dos corais. Por
possuírem uma associação simbiótica com essas zooxantelas, alguns corais
escleractíneos são considerados mixotróficos, caracterizados por modos de alimentação
autotrófico (através de simbiose com o dinoflagelado Symbiodinium) e heterotrófico
(predação sobre zooplâncton). Alguns estudos comprovam que corais com maior
capacidade de alimentação heterotrófica são mais resistentes ao branqueamento e,
consequentemente, às alterações climáticas. A fim de analisar se o coral escleractíneo
Mussismilia hispida, é capaz de alternar seu modo nutricional entre predominante
autotrófico e predominante heterotróficos, dezoito colônias foram amostradas ao longo
de um ano. Marcadores Tróficos de Ácidos Graxos (FATM, na sigla em inglês) foram
utilizados para determinar a fonte nutricional de carbono em tecido de corais. A
concentração de células de Symbiodinium e a temperatura local também foram
avaliadas. Branqueamento foi observado nos meses mais quentes do ano, quando a
concentração de Symbiodinium diminuiu, voltando a aumentar nos meses mais frios. O
marcador para dieta heterotrófica CGA (C20: 1ω9) foi encontrado em amostras de
zooplâncton de toda a área de estudo. Em laboratório, colônias sem acesso a
zooplâncton apresentaram perda significativa deste marcador após 10 dias. Amostras
de colônias naturalmente branqueadas não apresentaram nenhum vestígio dos
marcadores de autotrofia SDA (18: 4ω3) e DPA (22: 5ω3), mas continham tanto CGA e
DHA (22: 6ω3). Isso confirmou que SDA e DPA são marcadores autotróficos viáveis e
CGA é um marcador de heterotrofia. FATM relacionados com autotrofia apresentaram
padrão semelhante ao observado para as concentrações de Symbiodinium e foram
positivamente correlacionados com a densidade numérica de simbiontes e
negativamente com a temperatura. Para explorar os dados de concentração dos FATM,
o Índice Trófico de Corais foi desenvolvido para exibir as alternâncias entre modos
nutricionais. Mussismilia hispida de fato alterna entre predominância de modo nutritivo
ao longo do ano, sendo mais heterotrófica em períodos mais quentes e em condições
climáticas adversas, porem na maior parte do ano é predominantemente autotrófica. A
validação dos ácidos graxos marcadores tróficos específicos como referência para
autotrofia e heterotrofia em corais abre perspectivas para novos estudos em ecologia
trófica bêntica em recifes de coral. Este trabalho também inclui o primeiro
monitoramento de um ano do comportamento alimentar em um coral hermatípico no
Atlântico Sul e o acompanhamento de um evento de branqueamento.
PALAVRAS-CHAVE: Autotrofia, Branqueamento, Coral, FATM, Heterotrofia, Mixotrofia,
Symbiodinium.
iv
ABSTRACT
Coral reefs are among the most productive and biodiverse marine environments. This
remarkable biodiversity is partly associated to the complex structures formed by
scleractinian corals. Despite the ecological, social and economic importance of coral
reefs, they are constantly exposed to several threats mainly related to human activities.
Climate changes are one of the most notable impacts of human activity related to coral
mortality, mainly due to coral bleaching. Some scleractinian corals are proved to be
mixotrophs, displaying both autotrophic (through Symbiodinium) and heterotrophic
(predation on zooplankton) nutrition modes. Many studies emphasize that corals with
greater capability of heterotrophic feeding are more resilient to bleaching and
consequently to climate change. In order to analyze whether the endemic scleractinian
coral Mussismilia hispida is capable of shifting from predominant autotrophic and
predominant heterotrophic in Ubatuba-SP, 18 colonies were sampled monthly for 12
months. The Fatty Acid Trophic Markers (FATM) approach was used to determine the
source of carbon on coral tissues. Symbiodinium cell density and local seawater
temperature were also assessed. A mild bleaching was observed showing a decrease in
Symbiodinium numerical density during warmer months, but increasing in colder
months. Reference samples validated the relation between all selected FATM and its
corresponding nutritional mode. The heterotrophic feeding marker CGA (C20:1ω9) was
found in zooplankton samples collected throughout the study area. Laboratory starved
colonies (no access to zooplankton) lost any trace of this marker after 10. Samples from
naturally bleached colonies presented no traces of the autotrophic feeding markers SDA
(18:4ω3) and DPA (22:5ω3), but contained both CGA (C20:1ω9) and DHA (22:6ω3).
These results confirmed that the FATM analyzed where reliable trophic markers.
Autotrophic FATM presented a pattern similar to that observed for Symbiodinium
concentration in M. hispida tissues and were positively correlated with the symbiont and
negatively with temperature. The Coral Trophic Index showed that M. hispida undergoes
shifts in nutritional modes along the year, being more heterotrophic in adverse
conditions. The validation of specific FATM as proxies for autotrophic and heterotrophic
feeding in corals opens new perspectives for further studies in benthic trophic ecology
in coral reefs. This work also presents the first yearlong monitoring of the feeding
behavior in a hermatypic coral in the South Atlantic and the monitoring of a mild
bleaching event.
KEYWORDS: Autotrophy, Bleaching, Coral, FATM, Heterotrophy, Mixotrophy,
Symbiodinium.
v
LIST OF FIGURES
Figure 1. Sampling locations of Mussismilia hispida colonies along the coast of Ubatuba.
1: Anchieta I 2: Anchieta II 3: Fortaleza I 4: Fortaleza II 5: Lázaro 6: Praia do
Flamengo. Mussismilia hispida colonies were tagged and tissues were sampled
monthly in each location. Samples were analyzed for Symbiodinium
concentration and fatty acids related to autotrophic and heterotrophic feeding.
Illustration by Romina V. Barbosa. ...................................................................... 6
Figure 2. Mussismilia hispida colonies found in Ubatuba. Three colonies were selected
at each location in similar conditions, including orientation in the substrate,
depth (3 m ± 0.75 m), and absence of fouling and competitors such as frondose
macroalgae. ......................................................................................................... 7
Figure 3. (A) HOBO data logger (Onset®, accuracy of ± 0.53°C; resolution of 0.14°C at
25°C) for the continuous recording of temperature; (B) Structure built to fix
loggers on the substrate next to Mussismilia hispida colonies; (C) Fouling on
data logger and structure after 35 days at sea. .................................................. 7
Figure 4. Symbiodinium cells (arrows) from the coral Mussismilia hispida in the Nageotte
counting chamber. (A) 10 x magnification; (B) 40 x magnification. .................... 9
Figure 5. Experimental set up to assess the decrease of heterotrophic FATM (CGA – cis
gondoic acid) contents in Mussismilia hispida tissue under starving conditions
(i.e., absence of zooplankton). Left: Recirculated aquaria built for keeping the
colonies. Right: Close up of the experimental colonies in the beginning of the
experiment. ....................................................................................................... 11
Figure 6. Bleached Mussismilia hispida colonies sampled in situ to assess the autotrophic
FATM (SDA, DPA and DHA) content and Symbiodinium cells concentration in
the coral tissue. ................................................................................................. 11
Figure 7. Seawater temperature from each Mussismilia hispida coral colony site in
Ubatuba along the sampling period. The horizontal line represents the local
mean temperature. ........................................................................................... 14
Figure 8. Average Symbiodinium cell concentration of Mussismilia hispida samples at
each site through a year cycle (standard deviation not shown for graphic
reasons – see Fig. 9). ......................................................................................... 16
Figure 9. Average Symbiodinium cells concentration in Mussismilia hispida colonies
collected monthly on the six sampling sites at Ubatuba. Vertical lines represent
the standard deviation. ..................................................................................... 17
vi
Figure 10. Average Symbiodinium cell concentration in Mussismilia hispida tissue for all
locations and average water temperature along year cycle in Ubatuba (n=18
colonies). Vertical lines with diamonds are the standard deviation of
Symbiodinium and the light grey lines are the standard deviation of the average
temperature. ..................................................................................................... 18
Figure 11. Symbiodinium cell concentration in Mussismilia hispida for each site and the
average monthly water temperature in Ubatuba. Vertical lines represent the
standard deviation. ........................................................................................... 19
Figure 12. Pearson correlation between Symbiodinium cell concentration from
Mussismilia hispida corals and seawater temperature at Ubatuba. ................ 19
Figure 13. Box Plot for Symbiodinium cell concentrations of bleached Mussismilia hispida
colonies found in Ubatuba (n=3). The horizontal line represents the median and
the diamond, the mean. .................................................................................... 20
Figure 14. Box Plot for Symbiodinium cell concentrations of all Mussismilia hispida
colonies from Ubatuba (n=189). The horizontal line represents the median and
the diamond, the mean. The red X are outliers and vertical lines are lower and
upper whiskers. ................................................................................................. 20
Figure 15. Monthly average concentration of the fatty acid trophic marker cis-gondoic
acid (CGA) for the zooplankton samples collected in the six experimental sites
in Ubatuba. Vertical lines represent the standard deviation. ........................... 21
Figure 16. Starving experiment on Mussismilia hispida colonies. Samples were taken
every two days for 10 days. (A) Docosahexaenoic acid - DHA; (B) Stearidonic
acid - SDA; (C) Docosapentaenoic acid - DPA; and (D) Cis-gondoic acid - CGA.
The gray line indicates the Symbiodinium cell concentration. Vertical lines
represent the standard deviation. .................................................................... 22
Figure 17. Fatty acid composition of bleached Mussismilia hispida colonies (BL 1-3)
performed with naturally bleached found in Ubatuba. The fatty acid C20:1ω9
(CGA) is the heterotrophy FATM while C18:4ω3 (SDA), C22:5ω3 (DPA) and
C22:6ω3 (DHA) are the autotrophy FATM. The value for SDA and DPA is zero for
all samples. DHA value is zero for BL3. ............................................................. 24
Figure 18. Monthly average of Symbiodinium concentration and average concentration
of (A) C18:4ω3 (SDA), (B) C22:5ω3 (DPA) and (C) C20:1ω9 (CGA) of Mussismilia
hispida in Ubatuba. Vertical lines (continuous and dashed) represent the
standard deviation. ........................................................................................... 25
Figure 19. Monthly average temperature and average concentration of (A) C18:4ω3
(SDA), (B) C22:5ω3 (DPA) and (C) C20:1ω9 (CGA), from Mussismilia hispida in
Ubatuba. Vertical lines represent the standard deviation. ............................... 26
vii
Figure 20. Pearson correlation between temperature and SDA (C18:4ω3) concentrations
from Mussismilia hispida corals at Ubatuba. .................................................... 27
Figure 21. Pearson correlation between temperature and DPA (C22:5ω3) concentrations
from Mussismilia hispida corals at Ubatuba. .................................................... 27
Figure 22. Mussismilia hispida Coral Trophic Index (CTI) representing the differences
between the ratios of autotrophy fatty acids trophic markers (SDA, C18:4ω3
and DPA, C22:5ω3) and heterotrophy fatty acid trophic marker (CGA, C20:1ω9).
Positive values indicate a predominance of autotrophic input to the corals’
whereas values below zero indicate the prevalence of heterotrophy. ............ 28
Figure 23. Coral Trophic Index with starved colonies experiment FATM data. The index
is representing the differences between the ratios of autotrophy fatty acids
trophic markers (SDA, C18:4ω3 and DPA, C22:5ω3) and heterotrophy fatty acid
trophic marker (CGA, C20:1ω9). Positive values indicate a predominance of
autotrophic input to the corals’ fatty acids content and values below zero
represent a prevalence of heterotrophy........................................................... 29
LIST OF TABLES
Table 1. Geographic coordinates for each site of Mussismilia hispida sampling. ............ 6
Table 2. Weekly and monthly wave height (m) and direction (WH/D). Weekly, monthly
and between sampling percentage of cloud cover (%CC) and weekly, monthly
and between sampling accumulated rain (AR) for Ubatuba-SP, Brazil (CC and
WH/D source CPETC/INPE, AR source NAP-Oceano Sustentável USP. ............. 15
Table 3. Starving experiment 01 ANOVA and Tukey’s post-hoc test results for the
concentration of Symbiodinium, stearidonic acid (SDA), docosapentaenoic acid
(DPA) and cis-gondoic acid (CGA) in the five (Day2 to Day 10) sampling periods
in the starved colonies. ..................................................................................... 23
1
INTRODUCTION
Coral reefs are among the most productive and biodiverse marine environments
(Connell, 1978; Schnell, 2004; Sheppard et al., 2009). Even though they are mostly found
under oligotrophic conditions, coral reefs are highly productive ecosystems because of
the photosynthesis performed by symbiotic dinoflagellates and macroalgae (Falter et
al., 2011). Despite occupying an area less than 300,000 km2 corresponding to 1% of the
ocean surface area (Sheppard et al., 2009), this ecosystem provides habitat for more
than 25% of the known marine species, including one third of marine fish species, 5,000
mollusk species, 800 hard corals, and a large number of echinoderms, polychaetes,
sponges and crustaceans (UNEP, 2003, Schnell, 2004; Lalli and Parsons, 2006 Sorokin,
2013). With the exception of Onychophora, all metazoan phyla are found in coral reefs
making this the most diverse environment on Earth at higher taxonomic levels (Glynn
and Enochs, 2011).
The high biodiversity of coral reefs is of relevant economical importance, since
approximately 10 million people depend directly on them (Salvat, 1992; Wilkinson,
2008). The main commercial activities related to coral reefs include tourism (diving
centers, hotels and restaurants – see Moberg and Folke, 1999), fisheries (fishes such as
parrotfishes and groupers are important examples of coral reef species harvested for
human consumption – see Bellwood and Wainwright, 2002), production of
pharmaceuticals and medication (Cinel et al., 2000; Alves de Lima et al., 2013) and the
marine aquarium trade (more than 1,000 ornamental fish species are commercially
targeted in an economic activity that is worth more than U$ 15 billion – see Wabnitz et
al., 2003; Olivotto et al., 2006). These activities generate roughly U$ 797 billion every
year (Cesar et al., 2003).
Despite the ecological, social and economic importance of corals reefs, they are
constantly exposed to several threats mainly related to human activities (Roberts et al.,
2002; Burke et al., 2011). These include marine pollution, overfishing, habitat
destruction and climate change associated with carbon dioxide emissions that alter
water temperature and carbonate chemistry (Calado, 2006; Hoegh-Guldberg et al.,
2007). These have destroyed approximately 20% of coral reefs worldwide, while another
2
35% are seriously threatened (Wilkinson, 2008). In some cases, anthropogenic impacts
to coral reefs have exceeded their regenerative capacity, causing dramatic shifts in
species composition and severe biodiversity reduction, which directly led to economic
loss (Bellwood et al., 2004).
The remarkable biodiversity found in coral reefs is partly associated to the complex
calcium carbonate structure formed by scleractinian corals (Cnidaria: Anthozoa). These
are the true reef-building organisms, also called hermatypic, which provide structural
habitat for numerous other species (Krueger et al., 2015). Surface irregularities, crevices
and tunnels in the reef limestone form a variety of microhabitats and the erosion of the
main reef structure creates areas of rubble and sand around it (Hallock, 1997). Most
hermatypic corals live in clear, oligotrophic and shallow tropical waters (Sheppard et al.,
2009). The rate at which hermatypic corals deposit calcium carbonate depends on the
species, but some of the branching species (e.g., Acropora spp.) can grow approximately
10 cm per year (Ruppert et al., 2004), thus making coral reef damage recovery a slow
and fragile process.
Some species of hermatypic corals live in a mutualistic association with unicellular
photosynthetic dinoflagellates of the genus Symbiodinium, also known as zooxanthellae
(Stat et al., 2006; Venn et al., 2008). The coral host provides shelter, nitrogen,
phosphorus and carbon dioxide to the symbiotic dinoflagellate, which in return
translocates up to 95% of its photosynthetically-fixed carbon to the host (Falkowski et
al., 1984; Muscatine and Weis, 2013). Symbiodinium dinoflagellates may contribute up
to 100% of the coral daily metabolic needs (Papina et al., 2003; Grottoli et al., 2006;
Hoegh-Guldberg et al., 2007). For many years reef-building corals were considered
mainly dependent on the photoautotrophy performed by Symbiodinium (Muscatine and
Porter, 1977). However, photosynthetic products may be deficient in nitrogen and
phosphorus (Crossland, 1987; Wild et al., 2004) and essential nutrients for growth and
reproduction may need to be acquired through a different feeding source (Ferrier-Pagès
et al., 2003).
Numerous studies have confirmed that most coral species can in fact be active
heterotrophs and prey on plankton organisms (Sebens et al., 1996; Grottoli, 2002;
Houlbrèque et al., 2004; Palardy et al., 2005, 2006; Houlbrèque and Ferrier-Pagès,
3
2009). Heterotrophic input is necessary for maximal coral growth and it can contribute
up to 66% of the fixed carbon found in both coral tissue and skeleton (Grottoli and
Wellington, 1999; Houlbrèque et al., 2003; Palardy et al., 2005). The ability to feed as
both autotrophs and heterotrophs renders corals the status of mixotrophs.
Mixotrophy supplies corals with different compounds, including a wide range of lipid
compounds (Crossland et al., 1980; Grottoli et al., 2006), which play an essential role in
coral nutrition and metabolism. Among these, fatty acids (FA) are important since they
may be used in ecological studies as trophic markers (i.e., fatty acid trophic makers -
FATM) (Sargent, et al., 1990; Volkman, 1999; Dalsgaard et al., 2003). Animals, differently
from many phototrophs, cannot produce FA with unsaturated bonds beyond a
determinate carbon position (position Δ9; Dewick, 1997). Moreover, animals are
incapable of synthesis de novo for most FA (Dalsgaard et al., 2003) and these are
produced through different cellular pathways. In animals, this occurs in the
phospholipids of the endoplasmic reticulum, whereas in most autotrophs FA are
synthesized in the thylakoid membranes of chloroplasts (Papina et al., 2003). The only
manner in which animals can obtain polyunsaturated fatty acids is by consuming
organisms that produce them (such as phytoplankton) or organisms that have consumed
a producer (Persson and Vrede, 2006). Specific FA obtained in such ways may then serve
as food-source markers (Sargent et al., 1990; Dalsgaard et al., 2003).
Many studies used the approach of FATM to evaluate carbon source in scleractinian
corals (Wilson et al., 2001; Treignier et al., 2008; Dodds et al., 2009; Figueiredo et al.,
2012). It is known that specific FATM in coral tissues may be traced back to the
photosynthetic contribution of Symbiodinium, such as 18:4ω3, 22:5ω3 and 22:6ω3
(Papina et al., 2003; Treignier et al., 2008). Other FA may be specific to heterotrophy,
such as those produced by crustacean zooplankton (e.g., C20:1ω9 and C22:1ω11;
Dalsgaard et al., 2003), which are relevant prey items for hard corals.
However, both autotrophy and heterotrophy may be regulated by abiotic factors.
Increased seawater temperature is associated with declines in photosynthetically-
driven carbon fixation rates (Clark and Jensen, 1982) and with decrease in calcification
rates, tissue biomass and FA reserves (Grottoli et al., 2006; Rodrigues and Grottoli, 2006,
2007; Cantin et al., 2010; Levas et al., 2013). High temperatures and excessive light
4
exposure are the main causes of coral bleaching, which is the paling or whitening of
corals as a result of the loss of Symbiodinium or a decrease in its pigment content
(Douglas, 2003). In addition, ex situ experiments show that corals upregulate
heterotrophic feeding when photosynthesis is suppressed either due to decreased
water clarity and deprivation of sun light (Anthony and Fabricius, 2000; Hoogenboom et
al., 2010) or when symbionts are lost from coral tissue due to bleaching (Grottoli et al.,
2006). The local zooplankton community composition may as well affect heterotrophic
intake because different species of coral prey on certain zooplankton size ranges
(Palardy et al., 2006). However, many studies have demonstrated that not all species
are capable of using heterotrophy to compensate for reduced photosynthesis (Anthony
and Fabricius, 2000; Grottolli et al., 2006). Despite all of this information, no study has
monitored in situ if hermatypic corals shift between feeding modes and what may
regulate these shifts.
The present work aimed to determine if the scleractinian coral Mussismilia hispida
is both autotrophic and heterotrophic and to investigate the influence of abiotic factors
on the relative intensity of those trophic modes. This work is based on the following
hypotheses: i) Mussismilia hispida shifts its feeding mode between predominantly
autotrophic and predominantly heterotrophic; and ii) Mussismilia hispida is
predominantly heterotrophic throughout the year. In order to answer these questions,
we monitored the concentration of specific FATM related to both autotrophy and
heterotrophy in M. hispida colonies for a year at Ubatuba (São Paulo state, Brazil), while
also taking continuous measurements of seawater temperature.
Mussismilia hispida is an endemic and hermatypic species of the Brazilian coast and
Ubatuba is almost at its distribution limit to the south being the only hermatypic coral
species found in the São Paulo state. Understanding how this species feeds and thrives
at such higher latitudes may be important not only for coral reef trophic ecology, but
also may contribute to the current knowledge of possible habitat expansion of more
resistant species and adaptation facing climate change.
5
MATERIALS & METHODS
Study area and experimental design
Sampling took place in the coastal region of the town of Ubatuba (São Paulo
state), Brazil (23°30'01.9"S 45°07'07.9"W). This area is under the influence of the
relatively warm and low salinity Coastal Water (CW) and seasonal summer intrusions of
the South Atlantic Central Water (SACW), with lower temperatures and higher salinity
(Castro Filho et al., 1987). Sea surface temperature in the area ranges from 14.6 to
27.9°C and salinity from 31.7 to 35.8 ppt (Castro, 1995). Low intensity waves come from
the East and stronger waves come from South and Southwest (Castro Filho et al., 1987).
Fine sand, silt and clay predominate, while coarser material is found in enclosed areas
(Mahiques, 1995)
Six experimental sites were selected in Flamengo and Fortaleza Bays and
Anchieta Island (Fig. 1). In each site, three colonies of the Brazilian endemic scleractinian
coral Mussismilia hispida (Fig. 2) were tagged and monthly sampled. In order to have
replicated individuals, colonies were chosen in areas with similar conditions, i.e., similar
position/orientation on the substrate, depth of 3 m ± 0.75 m, direct exposure to sunlight
and near absence of competing organisms such as turf and frondose algae and sessile
invertebrates like barnacles and mussels. All colonies were sampled nearly monthly for
a year (Feb/2015 – Jan/2016), with intervals varying from 20 – 40 days, depending on
climate and hydrodynamic conditions. Approximately one polyp from each colony was
collected monthly with hammer and chisel. Immediately after removal, polyps were
placed in tagged plastic bags with seawater and refrigerated on ice.
Seawater temperature was continuously recorded at each site using HOBO
Onset®data loggers (accuracy of ± 0.53°C; resolution of 0.14°C at 25°C) (Fig. 3). In every
sampling event data loggers were cleaned and the recorded information was retrieved.
All temperature data are presented as a continuous measurement for each site. The
local mean temperature was calculated individually for each site using the whole data
set, specific to each site. Temperature means used for comparisons with Symbiodinium
6
concentration and fatty acid trophic markers (FATM) were calculated using all of the
temperature data recorded in between each sampling period.
Figure 1. Sampling locations of Mussismilia hispida colonies along the coast of Ubatuba. 1: Anchieta I 2: Anchieta II 3:
Fortaleza I 4: Fortaleza II 5: Lázaro 6: Praia do Flamengo. Mussismilia hispida colonies were tagged and tissues were
sampled monthly in each location. Samples were analyzed for Symbiodinium concentration and fatty acids related to
autotrophic and heterotrophic feeding. Illustration by Romina V. Barbosa.
Table 1. Geographic coordinates for each site of Mussismilia hispida sampling.
Location Coordinates
1 Anchieta I S 23°32'02.5404"; W 45°04'40.8144"
2 Anchieta II S 23°32'39.2820"; W 45°04'46.3800"
3 Fortaleza I S 23°31'52.2372"; W 45°09'44.0748"
4 Fortaleza II S 23°31'46.4232"; W 45°09'31.4064"
5 Lázaro S 23°30'30.2364"; W 45°08'11.0904"
6 Praia do Flamengo S 23°30'37.6164"; W 45°06'29.5200"
7
Ocean and climate data were also obtained from CPTEC/INPE (Centro De
Previsão de Tempo e Estudos Climáticos/Instituto Nacional de Pesquisas Espaciais) and
monthly-accumulated rainfall was obtained from NAP-Oceano Sustentável (Núcleo de
apoio à pesquisa oceano sustentável). Percentage of cloud coverage data and mean
wave height and direction were compiled for each week and month of 2015 and for
January 2016. For the periods in between samplings, accumulated rain and percentage
cloud coverage were calculated as well.
Sampling was not performed in July due to rough weather, as waves were
frequently higher than 2.0 m and hindering sampling conditions. Tagged colonies from
Anchieta II were not sampled in July, September and October, as they were not found
due to poor water visibility and weather conditions.
Figure 2. Mussismilia hispida colonies found in Ubatuba. Three colonies were selected at each location in similar conditions, including orientation in the substrate, depth (3 m ± 0.75 m), and absence of fouling and competitors such as frondose macroalgae.
Figure 3. (A) HOBO data logger (Onset®, accuracy of ± 0.53°C; resolution of 0.14°C at 25°C) for the continuous recording of temperature; (B) Structure built to fix loggers on the substrate next to Mussismilia hispida colonies; (C) Fouling on data logger and structure after 35 days at sea.
8
Coral tissue sample processing
Major skeleton fragments were removed with pliers and tweezers. Each sample was
then divided in two aliquots of approximately 0.1 g each. The aliquots were used for (i)
Symbiodinium cell count and (ii) fatty acid extraction for gas chromatography analysis.
Symbiodinium cell count
Skeleton fragments were removed from soft tissue through sample homogenization
and decantation. Excess water from the tissues was removed by briefly stirring the
sample on a dry petri dish followed by weighing. Samples were then transferred to 2-mL
centrifuge tubes with 1 mL of distilled water. The contents were grinded with a pestle,
homogenized for 5 minutes and agitated for 3 minutes. The resulting solution was
filtered through a 100-µm mesh in order to remove unwanted debris, and then washed
with 4 ml of distilled water. The final filtered solution had a volume of 5 ml.
Symbiodinium cells were counted in a Nageotte counting chamber (Fig. 4). The number
of Symbiodinium cells per mg of coral soft tissue was obtained according to equation (1).
(1) 𝑆𝑦𝑚𝑏/𝑚𝑔𝑐𝑠𝑡 =(1,25𝐶𝐶×1000𝑁𝐿)×5
𝑆𝑊
Where:
𝑐𝑠𝑡 - Coral soft tissue;
CC - Counted Symbiodinium cells;
NL - Counted Nageotte chamber lines;
SW - Coral soft tissue weight.
9
Figure 4. Symbiodinium cells (arrows) from the coral Mussismilia hispida in the Nageotte counting chamber. (A) 10 x magnification; (B) 40 x magnification.
Fatty acid extraction
Lipids were extracted from samples using a method adapted from Bligh & Dyer
(1959). The soft tissue (skeleton-free) was weighed and added to a glass tube. One
milliliter of a solution of 100% methanol and 100% dichloromethane (1 : 1) was added
to each tube and agitated for one minute, followed by the addition of 100 µL of internal
standard (tricosanoic acid, C23:0). Samples were then esterified with 5 mL of a 1 : 0.02
solution of methanol and sulfuric acid. Subsequently, 2 mL of 100% hexane was added
and agitated. Condensers were attached to the tubes and placed in a 50°C bath for 30
minutes. The tubes were cooled to room temperature and phases separated with a 5
mL saturated solution of NaCl. The top phase was retrieved (2 mL) for GC analysis. When
samples weighed less than 50 mg, concentration to 1 mL was performed by evaporation
with pure (99.999%) Nitrogen gas.
Gas chromatography
Esterified samples were analyzed in a 6890 Agilent gas chromatograph coupled
with a flame ionization detector (GC-FID). The column used was the Agilent J & W (50 m
long, 0.35 mm internal diameter and 0.17 mm thick with a 5% phenylmethylsiloxane
film). Two microliters of the sample were injected and carried by ultra-pure hydrogen
and nitrogen gases. The oven ramp temperature started at 50 °C, and kept constant for
10
2 minutes, then it increased at the rate of 9°C min- 1, remaining constant until it reached
300°C and maintained for 10 minutes.
The concentrations of four fatty acids were investigated: stearidonic acid (SDA,
18:4ω3), docosapentaenoic acid (DPA, 22:5ω3), docosahexaenoic acid (DHA, 22:6ω3)
and cis-gondoic acid (CGA, C20:1ω9). The first three are markers for autotrophy
(translocated from Symbiodinium to the host – see Papina et al., 2003) whereas the last
one is for heterotrophy (CGA is found in copepods – see Dalsgaard et al., 2003). The
identification of methyl esters of fatty acids was done by comparison of the retention
times of the target fatty acids with a reference analytical standard (47033 PUFA No. 1
Marine Source - Sigma-Aldrich Co.®), based on the calibration curves fitted with at least
5 different concentrations.
Fatty acid trophic markers reference samples
Three different reference samples were produced in order to confirm if the
investigated FATM were adequate. The first group of reference samples was the
monthly night-time collection of zooplankton on each site to confirm the presence of
CGA in zooplankton organisms. This is a marker specific to crustaceans (Dalsgaard et al.,
2003) and was selected as a proxy for heterotrophic feeding. Zooplankton oblique tows
were made with a 300-µm mesh conical net for 5 minutes at 3 knots.
The second group of reference samples was produced through an experiment
that intended to verify if CGA found in the host tissue was indeed related to
heterotrophic feeding. For that purpose, four Mussismilia hispida colonies (Fig. 5) were
maintained for 10 days in a tank with filtered seawater and no zooplankton at a
temperature of 25°C ± 1.8, salinity of 34 and with indirect sunlight. Approximately 70%
of the water was changed daily and samples were taken every two days to monitor the
concentration of CGA in the host tissue and to observe the concentration of
Symbiodinium cells concentration. From hereafter we call these starving colonies. Day
0 were sampled prior to colonies removal from the environment and it was considered
11
as a stress period due to removal disturbances and adaptation to the experiment
system.
The last analysis had the purpose of verifying if the three autotrophy FATM, i.e.,
SDA, DPA and DHA, were specific to Symbiodinium as previously reported (Papina et al.,
2003). For that, we collected bleached colonies in which there would be little or no
Symbiodinium (Fig. 6) and most likely a very small or undetectable amount of these
FATM.
Figure 5. Experimental set up to assess the decrease of heterotrophic FATM (CGA – cis gondoic acid) contents in Mussismilia hispida tissue under starving conditions (i.e., absence of zooplankton). Left: Recirculated aquaria built for keeping the colonies. Right: Close up of the experimental colonies in the beginning of the experiment.
Figure 6. Bleached Mussismilia hispida colonies sampled in situ to assess the autotrophic FATM (SDA, DPA and DHA) content and Symbiodinium cells concentration in the coral tissue.
12
Statistical analyses
Mean temperature differences among sampled months were tested using a one-
way Analysis of Variance (ANOVA), using sites as replicates (one temperature sensor per
site, n=6). Mean temperature differences among sites was tested also with a one-way
ANOVA, using sampled months as replicates (n=11; in October 2015 at Lázaro, the
sensor was lost).
For the starving experiment, each FATM (DHA, SDA, DPA and CGA) was tested
for differences among sampling times using a one-way ANOVA. Differences between
individual sampling times for each FATM were tested for significance with a pairwise
post-hoc Tukey test.
Symbiodinium cell concentrations were tested for differences among sites and
sampling periods using a 2-way nested ANOVA, with the sampled months nested within
each site. If significant difference was found, each pair was compared for significant
differences with a post-hoc Tukey test.
Significant relationships between pairs of variables, such as Symbiodinium
concentration and mean temperature, FATM and mean temperature, and between the
specific FATM (DHA, SDA, DPA and CGA) to Symbiodinium concentration was assessed
using Pearson’s correlation test.
Statistical analyses were performed using the statistical packages JMP (version
8). Biological data (Symbiodinium cell concentration and FATM concentrations) were
log-transformed [log(x+1)] to guarantee homoscedasticity and normalization
requirements for parametric tests (ANOVA and Tukey). All the figures were produced
with Grapher 8 and Microsoft Excel software.
13
Coral Trophic Index
In order to answer the proposed hypotheses, three equations (2-4) were created
using the results of the concentrations of fatty acids for both autotrophy and
heterotrophy. Equations (2) and (3) determine if the intensity of each trophic mode
increased or decreased from one sampling month (t0) to another (t1). The difference
between equations (2) and (3) was calculated to determine which of the trophic modes
predominates in a colony at a specific moment. The resulting value was denominated
Coral Trophic Index (CTI). A positive value reflects a predominantly autotrophic feeding
behavior, whereas negative values indicate a predominantly heterotrophic behavior.
(2) heteroFATMRatio = [(𝑋𝑡1ℎ𝑒𝑡𝑒𝑟𝑜𝐹𝐴𝑇𝑀
𝑋𝑡0ℎ𝑒𝑡𝑒𝑟𝑜𝐹𝐴𝑇𝑀) − 1]
(3) autoFATMRatio = [(𝑋𝑡1𝑎𝑢𝑡𝑜𝐹𝐴𝑇𝑀
𝑋𝑡0𝑎𝑢𝑡𝑜𝐹𝐴𝑇𝑀) − 1]
(4) CTI = (autoFATMRatio − heteroFATMRatio)
Where:
Xt1heteroFATM = [µg g-1] of CGA of sample x at t1
Xt0heteroFATM = [µg g-1] of CGA of sample x at t0
Xt1autoFATM = [µg g-1] of autoFATM (SDA + DPA) of sample x at t1
Xt0autoFATM = [µg g-1] of autoFATM (SDA + DPA) of sample x at t0
14
RESULTS
Environmental data and Symbiodinium concentration
There were no differences in seawater temperature between sites, but there are
significant differences between months of samples (F(10,54) = 41.699, p = 0.001) (Fig. 7).
The lowest temperature was registered in July 2015 at Lázaro (18.6°C), and the highest
in January 2015 at Praia do Flamengo (33.7°C), with an overall year average of 25.5°C.
Figure 7. Seawater temperature from each Mussismilia hispida coral colony site in Ubatuba along the sampling period. The horizontal line represents the local mean temperature.
15
During 2015 a few unusual climatic events were observed. According to the
National Oceanic and Atmospheric Administration (NOAA), one of the biggest El Niño
formations was registered in 2015 in the Pacific Ocean. July/2015 was the warmest
month ever recorded for the globe and Brazil experienced the worst drought in 80 years.
All this reflected in the water conditions for the coast of Brazil. During summer, calm,
warm and clear waters were observed in Ubatuba. In March and April, heavy rains,
winds and rough water were expected, but this was not observed during the
experiment. The water maintained good conditions (calm waters with good visibility) all
the way to June, and rough weather started to hit the Ubatuba coast only after the
second half of June 2015 (Table 2). From the end of June to the beginning of August,
consecutive storms in the coast generated waves higher than two meters. Furthermore,
heavy cloud coverage of 68.3% in October and 82% in November marked the beginning
of the summer 2015/2016 (Table 2). In Brazil, the summer months are typically hot and
humid while winter months are cold and dry.
Table 2. Weekly and monthly wave height (m) and direction (WH/D). Weekly, monthly and between sampling percentage of cloud cover (%CC) and weekly, monthly and between sampling accumulated rain (AR) for Ubatuba-SP, Brazil (CC and WH/D source CPETC/INPE, AR source NAP-Oceano Sustentável USP.
%CC WH/D %CC WH/D %CC WH/D %CC WH/D %CC WH AR (mm) %CC AR (mm)
January/2015 74.6 1.0/S 67.3 1.1/E 71.7 0.9/SE 86.4 1/E 75.0 1.0 246.9 - -
February/2015 55.7 1.2/SSE 44.0 1/ESE 78.3 1.3/SE 53.9 1/E 57.5 1.1 345.6 67.2 512.5
March/2015 40.0 1.4/SSE 73.0 1/E 80.0 1/ESE 53.0 1.3/SSE 62.2 1.2 327 65.0 244.7
April/2015 37.4 1.2/SE 39.0 1/S 66.3 1.1/SSE 30.5 1.5/S 43.6 1.2 180.1 51.0 289.0
May/2015 43.0 1.4/SE 65.5 1.7/S 48.7 1.5/ESE 48.2 1.2/S 49.7 1.4 86.3 46.9 157.2
June/2015 25.8 1.0/E 19.5 1.4/S 34.0 1.7/S 40.0 1.6/E 27.2 1.4 214.6 35.6 21.3
July/2015 97.9 2.1/SSE 55.0 1.1/ESE 55.8 1.5/E 98.0 2.0/S 51.0 1.5 50.7 - -
August/2015 0.8 1.2/SE 5.0 2/E 19.4 1.6/ESE 37.4 1.5/SE 17.0 1.5 16.6 50.1 287.7
September/2015 59.2 1.5/S 73.3 1.3/E 7.7 1.4/SE 47.5 1.2/S 46.4 1.3 169.3 31.3 183.3
October/2015 59.1 1.3/S 62.3 1.4/ESE 73.3 1.4/SE 79.6 1.5/SE 68.3 1.4 217.6 64.4 159.6
November/2015 86.6 1.6/S 77.0 1.0/E 77.0 1.3/SE 86.2 1.3/SE 82.0 1.3 341.2 78.7 299.5
December/2015 90.6 1.3/S 72.2 1.0/S 66.7 1.1/SE 78.8 1.1/E 78.8 1.1 155.8 81.5 303.7
January/2016 89.4 1.5/SE 93.2 1.2/S 64.8 1.1/SE 73.4 1.1/SE 80.2 1.2 278.7 80.1 234.8
Months
Week AverageMonthly
Between
Sampling1 2 3 4
16
Symbiodinium cell concentrations in M. hispida tissue were significantly different
among sites (F(5,53) = 2.541, p = 0.0334), but with a similar variation over time (F(5,53) =
0.780, p = 0.8369) (Fig. 8). In the beginning of the experiment in February, all coral
colonies had a relatively low concentration of Symbiodinium. Overall, throughout the
year the major difference between sites was the absolute numbers while the variation
pattern of Symbiodinium cell concentration was similar for all sites.
Figure 8. Average Symbiodinium cell concentration of Mussismilia hispida samples at each site through a year cycle (standard deviation not shown for graphic reasons – see Fig. 9).
A high variability in Symbiodinium concentration was observed throughout the
experiment (Fig. 9). The average concentration was 8,244.4 ± 5,307.3 cells per mg-1 of
coral soft tissue. Maximum cell concentration was measured at Praia do Flamengo in
April (23,987.9 ± 1,636.5) and Fortaleza II in September (23,202.7 ± 2,072.0) (Fig. 9).
Minimum concentrations were found at Lázaro in February (157.4 ± 55.1) and Fortaleza
I in May (178.4 ± 43.0) (Fig. 9). Anchieta II was the location with higher concentration of
symbionts for the most part of the experiment.
0
5000
10000
15000
20000
[Cel
ls m
g-1]
Anchieta I Anchieta II Fortaleza I
Fortaleza II Lázaro P. Flamengo
17
Figure 9. Average Symbiodinium cells concentration in Mussismilia hispida colonies collected monthly on the six sampling sites at Ubatuba. Vertical lines represent the standard deviation.
Symbiodinium concentration decreased in periods of high seawater
temperatures (29-33°C) that occurred in summer months (November to April) (Figs. 10
and 11). During warmer months, there was a mild bleaching in M. hispida, as colonies
were found with a low Symbiodinium concentration (minimum average 4,563.0 ±
2,437.5), nearly three times less than the maximum average cell concentration 12,946.0
18
± 4132.6 (Fig.10 and 14). However, there were no clear visual signs of bleaching. Visually
confirmed bleached colonies (collected for the third group of reference samples) had an
average of 66.4 ± 9.2 Symbiodinium cells mg-1, which differed to the minimum (157.4 ±
55.1) by nearly two-and-a-half times (Fig. 13 and 14). The opposite trend was observed
in colder months (May to September), where temperature decreases were associated
with a rise in Symbiodinium concentration, as colonies slowly recovered (23,202.7 ±
2,072.0 cells mg-1 in September) (Fig. 10, 11, 13 and 14). An oscillation of 99.3% was
found between maximum and minimum symbiont concentration (Fig. 13 and 14).
Statistically, there was a significant negative correlation between temperature and
Symbiodinium concentration (r(198) = -0.318, p = 0.001 – Fig. 12).
The pattern of high symbiont concentration in winter months vs. low
concentration in summer months is clearer on Anchieta I, Anchieta II and Fortaleza II
(Fig. 11). Symbiodinium concentration observed from March to May in fig. 9 is an
exception to the pattern observed throughout the year. It is clear that an increase in
symbiont concentration in April followed by a decrease in May is found only at Anchieta
I and Praia do Flamengo (Fig. 11), and at this last site it is noticeable a sudden drop in
water temperature (below 20°C). A rapid increase in Symbiodinium concentration in
March was observed at Fortaleza I and Lázaro, but in April the symbiont concentrations
seemed to resume a steady increase through the winter.
Figure 10. Average Symbiodinium cell concentration in Mussismilia hispida tissue for all locations and average water temperature along year cycle in Ubatuba (n=18 colonies). Vertical lines with diamonds are the standard deviation of Symbiodinium and the light grey lines are the standard deviation of the average temperature.
15
20
25
30
0
5000
10000
15000
°C
[Cel
ls m
g-1]
Symbiodinium Average Temp.
19
Figure 11. Symbiodinium cell concentration in Mussismilia hispida for each site and the average monthly water temperature in Ubatuba. Vertical lines represent the standard deviation.
Figure 12. Pearson correlation between Symbiodinium cell concentration from Mussismilia hispida corals and seawater temperature at Ubatuba.
20
Figure 13. Box Plot for Symbiodinium cell concentrations of bleached Mussismilia hispida colonies found in Ubatuba (n=3). The horizontal line represents the median and the diamond, the mean.
Figure 14. Box Plot for Symbiodinium cell concentrations of all Mussismilia hispida colonies from Ubatuba (n=189). The horizontal line represents the median and the diamond, the mean. The red X are outliers and vertical lines are lower and upper whiskers.
21
Fatty Acids Trophic Markers reference samples
All zooplankton samples contained C20:1ω9 (CGA – cis-gondoic acid), averaging
0.3% of the total FA composition. Mean CGA total content was 4.99 ± 3.11 µg g-1 (Fig.
15). Higher CGA concentration was found during winter months and January 2016.
The experiment for the second group of reference samples monitored the
changes in FATM on Mussismilia hispida colonies in the absence of zooplankton
throughout ten days. The FATM profile for the four fatty acids and Symbiodinium cell
concentrations through the whole experiment period is shown in Fig. 16. After the stress
period (Day 0), Symbiodinium concentration stabilizes and there is no significant
difference in its concentration from day 2 to day 10 (F(4,10) = 0.034, p = 0.0526) (Table 3).
All three symbiont-specific fatty acids (18:4ω3 - SDA, 22:5ω3 - DPA and 22:6ω3 – DHA)
presented similar trends to the Symbiodinium concentration and there were no
significant differences on their oscillation (Fig. 16 and Table 3). However, the
concentration of the heterotrophy-specific fatty acid CGA was significantly different
(F(4,9) = 0.042, p = 0.033) (Table 3). The concentration of the heterotrophy specific marker
continuously dropped from D0 to D10 (Fig. 16 D).
0
5
10
15
20
[µg
g -1
]
Figure 15. Monthly average concentration of the fatty acid trophic marker cis-gondoic acid (CGA) for the zooplankton samples collected in the six experimental sites in Ubatuba. Vertical lines represent the standard deviation.
22
Figure 16. Starving experiment on Mussismilia hispida colonies. Samples were taken every two days for 10 days. (A) Docosahexaenoic acid - DHA; (B) Stearidonic acid - SDA; (C) Docosapentaenoic acid - DPA; and (D) Cis-gondoic acid - CGA. The gray line indicates the Symbiodinium cell concentration. Vertical lines represent the standard deviation.
23
Table 3. Starving experiment 01 ANOVA and Tukey’s post-hoc test results for the concentration of Symbiodinium, stearidonic acid (SDA), docosapentaenoic acid (DPA) and cis-gondoic acid (CGA) in the five (Day2 to Day 10) sampling periods in the starved colonies.
Test One-way ANOVA
Tukey’s post-hoc DF F p
Symbiodinium
Sample Time 4 3.410 0.052 D2 D4 D6 D10 D8
Error 10
SDA
Sample Time 4 0.411 0.769 D10 D4 D8 D2 D6
Error 9
DPA
Sample Time 4 0.505 0.733 D2 D4 D10 D8 D6
Error 9 CGA
Sample Time 4 4.236 0.033 D4 D2 D6 D8 D10
Error 9
24
For the last reference samples, the three bleached colonies had an average of
66.4 ± 9.2 Symbiodinium cells, which is more than two orders of magnitude than the
average (7,834.5 ± 5,447.2) found in the Ubatuba area (Figs. 13, 14 and 17). The FATM
composition of the bleached colonies was similar and none of them had detectable SDA
or DPA (Fig. 17). The DHA, however, was found in two of the colonies. From all the FATM,
CGA was the only FA found in all colonies and the most abundant.
Figure 17. Fatty acid composition of bleached Mussismilia hispida colonies (BL 1-3) performed with naturally bleached found in Ubatuba. The fatty acid C20:1ω9 (CGA) is the heterotrophy FATM while C18:4ω3 (SDA), C22:5ω3 (DPA) and C22:6ω3 (DHA) are the autotrophy FATM. The value for SDA and DPA is zero for all samples. DHA value is zero for BL3.
Fatty Acids Trophic Markers
The three markers for autotrophy varied similarly to the Symbiodinium
concentration (SDA - r(198) = 0.375, p = 0.0001; DHA - r(198) = 0.237, p = 0.0008; and DPA -
r(198) = 0.141, p = 0.0473). Their concentrations were low in the beginning of the year
and increased until May, despite the drop in Symbiodinium concentration in this month.
From May to August, the autotrophy FATM decreased, rising again from September
2015 to January 2016 (Fig. 18 A-C).
The concentration of CGA appeared to increase while the other FATM decrease.
The highest concentration of this FATM was found in December 2015 and January 2016
(Fig. 18 D), when symbiont concentration was decreasing. Overall, it had no significant
correlation with Symbiodinium concentration (r(198) = 0.065, p = 0.362).
6,190
3,353 3,1282,578 2,567
00 0 00 0 00
2
4
6
8
10
BL1 BL2 BL3
[µg
g-1]
CGA DHA SDA DPA
25
To better represent the autotrophic feeding behavior, combinations of the three
different markers were tested, and the stronger correlation with Symbiodinium was
found when SDA and DPA were pooled together (r(186) = 0.387, p = 0.001), discarding the
DHA (Fig. 20). The combination of SDA and DPA is from hereafter denominated as
autoFATM.
Figure 18. Monthly average of Symbiodinium concentration and average concentration of (A) C18:4ω3 (SDA), (B) C22:5ω3 (DPA) and (C) C20:1ω9 (CGA) of Mussismilia hispida in Ubatuba. Vertical lines (continuous and dashed) represent the standard deviation.
26
A significantly negative correlation was found between temperature and
autoFATM (SDA r(183) = -0.385, p = 0.0001, and DPA r(183) = -0.154, p = 0.0299) (Fig. 19-
21). CGA did not correlate with temperature (r(183) = -0.032, p = 0.649). A trend in the
concentration of the autoFATM markers with the variation of temperature was noticed.
CGA concentration oscillated differently, reaching higher concentrations in the
beginning of summer (Fig. 19 C).
Figure 19. Monthly average temperature and average concentration of (A) C18:4ω3 (SDA), (B) C22:5ω3 (DPA) and (C) C20:1ω9 (CGA), from Mussismilia hispida in Ubatuba. Vertical lines represent the standard deviation.
27
Figure 20. Pearson correlation between temperature and SDA (C18:4ω3) concentrations from Mussismilia hispida corals at Ubatuba.
Figure 21. Pearson correlation between temperature and DPA (C22:5ω3) concentrations from Mussismilia hispida corals at Ubatuba.
28
Autotrophy vs. heterotrophy – Coral Trophic Index
Ratios for the variation (from one time point to another) of both autotrophy and
heterotrophy FATMs (equations 2 and 3) were produced. Twelve months of sampling
only generated 10 comparison intervals (not 11 because of the missing data in July 2015)
on the coral trophic index. Mussismilia hispida corals were predominantly dependent
on autotrophy during most part of the experiment (6 out of 10 times) (Fig. 22).
Heterotrophy only appeared as the coral main nutrition source in 4 moments, May/Jun,
Ago/Sep, Nov/Dec and Dec/Jan (Fig. 22). There was a predominance of autotrophy in
Feb/Mar, which followed the trend observed for Symbiodinium concentration (Figs. 10-
11). In Apr/May and May/Jun values were close to zero, indicating a balance of both
nutrition modes.
Figure 22. Mussismilia hispida Coral Trophic Index (CTI) representing the differences between the ratios of autotrophy fatty acids trophic markers (SDA, C18:4ω3 and DPA, C22:5ω3) and heterotrophy fatty acid trophic marker (CGA, C20:1ω9). Positive values indicate a predominance of autotrophic input to the corals’ whereas values below zero indicate the prevalence of heterotrophy.
To further explore and validate the CTI, FATM data from the starving experiment
(Fig. 16) was applied to the index and it is displayed on Figure 23. As described for the
experiment, the corals started with a slight predominance of heterotrophy on
Day0/Day2. The deprivation of zooplankton reflected on a loss of CGA and consequently
-1,5
-1
-0,5
0
0,5
1
1,5
CTI
29
on the increase of autotrophy prevalence. By the end of the test, autotrophy increased
by 62% in relation to heterotrophy.
Figure 23. Coral Trophic Index with starved colonies experiment FATM data. The index is representing the differences between the ratios of autotrophy fatty acids trophic markers (SDA, C18:4ω3 and DPA, C22:5ω3) and heterotrophy fatty acid trophic marker (CGA, C20:1ω9). Positive values indicate a predominance of autotrophic input to the corals’ fatty acids content and values below zero represent a prevalence of heterotrophy.
30
DISCUSSION
The present work aimed to determine whether the Brazilian endemic
scleractinian coral Mussismilia hispida is capable of shifting between nutritional modes
and to investigate if heterotrophy is the most predominant mode throughout the year.
To answer the proposed hypotheses, specific fatty acid trophic markers (FATM) were
used to identify the source of fatty acids (FA) present in M. hispida tissues at Ubatuba.
The FATM approach is based on the premise that the selected markers cannot be
selectively processed through food uptake or incorporation and are not synthetized by
the targeted animal, instead they should be transferred from one trophic level to the
next by incorporation or ingestion from the animal nutritional source (Napolitano et al.,
1997; Dalsgaard et al., 2003; Iverson et al., 2004). Despite strong evidence that SDA, DPA
and DHA are translocated from Symbiodinium to its coral host (Papina et al., 2003) and
that CGA is a specific marker for crustacean zooplankton (Dalsgaard et al., 2003), we
produced three reference samples in order to confirm that these markers were
adequate indicators of autotrophic and heterotrophic carbon input for M. hispida.
Scleractinian corals of many different species have been observed to prey on
zooplankton (Ferrier-Pagès et al., 2003; Sebens et al., 2003; Palardy et al., 2005). There
is evidence that within the zooplankton, copepods are the dominant food source for
corals (Dodds et al., 2009) and CGA has been reported as a FATM produced by calanoid
copepods (Dalsgaard et al., 2003). These are the most abundant organisms found in
zooplankton communities at Ubatuba (Lopes, 2003). The first group of reference
samples demonstrated that CGA was found in all zooplankton samples collected at all
locations throughout the year, thus showing that this marker is representative of the
local community.
Under controlled laboratory conditions, M. hispida colonies were placed in
closed and recirculated aquaria without the presence of zooplankton (i.e., in starving
conditions), but with free access to sunlight. The concentration of CGA significantly
decreased during this period and the FATM for autotrophy (SDA, DPA and DHA) did not;
in fact, after the sixth day they increased. Therefore, coupled with the zooplankton
31
samples, these results confirm that CGA can be regarded as an effective trophic marker
for heterotrophic feeding in M. hispida, reassuring the findings in Dalsgaard et al. (2003).
The last reference samples consisted of three highly-bleached colonies that were
found and collected at Ubatuba. Both FATM SDA and DPA were absent and the
heterotrophy marker (CGA) was found at much higher concentrations. This confirms
that that SDA and DPA found in M. hispida are specific to Symbiodinium. The corals were
likely compensating symbiont loss with prey capture (Grottoli et al., 2006). However,
DHA was found in these bleached colonies. This is most likely related to the fact that
DHA is not specific to dinoflagellates, but is also abundantly produced by many
phytoplankton species (Volkman, 1999), and may have been present in zooplankton that
had consumed diatoms and microalgae. Therefore, despite being produced by
Symbiodinium, DHA is an ambiguous marker and was excluded from most of the
analyses. Thus, the combination of SDA and DPA (defined as the autoFATM) is an
adequate FATM for the autotrophic contribution from Symbiodinium to the coral host.
It is important to note that the concentration of SDA and DPA is not a proxy for
the concentration of Symbiodinium in the coral tissue. Production rates of these fatty
acids vary considerably (Titlyanov et al., 2001; Zhukova and Titlyanov, 2002), especially
due to cell size, shape, strain and associated host (Bishop and Kenrick, 1980; Titlyanov
et al., 2001). For instance, Symbiodinium undergoing photoacclimation typically produce
higher concentrations of photosynthates (Anthony and Hoegh-Guldberg, 2003a, 2003b;
Hoogenboom et al., 2006). Furthermore, a very weak correlation was found between
Symbiodinium concentration and the combined content of SDA and DPA (r(186) = 0.387).
Therefore, we consider an increase in SDA and DPA as an increase in their production by
the Symbiodinium population inside the coral tissue.
Our first hypothesis was confirmed as the Coral Trophic Index (CTI) constantly
oscillated between positive and negative values, showing that indeed there are shifts
between predominantly autotrophic and predominantly heterotrophic feeding modes
(Fig. 22). It is generally accepted that most of these shifts are related to turbid waters
(Anthony, 2000; Fabricius and Dommisse, 2000), temperature changes, reduced
photosynthesis and Symbiodinium concentration, as a compensatory strategy (Ferrier-
Pagès et al., 2003; Palardy et al., 2005; Grottoli et al., 2006; Houlbréque and Ferrier-
32
Pagés, 2009). While we expected that temperature would be the major factor driving
theses shifts, as reported in (Rodrigues and Grottoli, 2007; Palardy et al., 2007; Connolly
et al., 2012; Ezzat et al., 2016), we found no correlation between the CTI and
temperature or temperature variations. However, these shifts do coincide with the
sporadic adverse weather conditions reported. These conditions include strong rainfall
from February to March, turbulent hydrodynamics and sediment resuspension from July
to August and increased temperature and cloud cover from October to November (Table
2 and Fig. 7). All these events coincided with shifts from autotrophy to heterotrophy
(Fig. 22). Intense weather has been linked with coral damaging (Crabbe et al., 2008),
while increased rainfall, severe terrestrial runoff and high wave energy have been
reported to cause severe damage, bleaching and/or mortality of coral colonies (Connell,
1997; Connell et al., 1997; Mallela and Crabbe, 2009).
Our second hypothesis was rejected, as the CTI indicates that M. hispida was
predominantly autotrophic, for 6 periods out of 10, which represent the greater part of
the experiment. Heterotrophy was expected to predominate due to the environmental
conditions found at Ubatuba, which is near the limit of the species distribution (e.g., low
seawater temperature in the winter and autumn and high turbidity throughout the
year). These are the main factors that lead the corals to upregulate heterotrophy and
suppress photosynthesis (Anthony and Fabricius, 2000; Grottolli et al., 2006;
Hoogenboom et al., 2010; Levas et al., 2013). Our results show that this species resorts
to heterotrophy when adverse climate conditions seem to hinder photosynthetic
production by Symbiodinium.
Interestingly, our data has shown that M. hispida colonies in Ubatuba go through
a mild seasonal bleaching during the warmer months in the summer and recover during
the remainder of the year when temperatures are lower (Fig. 10 and 11). The
phenomenon of coral bleaching is defined by the loss of Symbiodinium cells, resulting in
accessory pigment breakdown and subsequent tissue loss, leaving only the white
skeleton (Iglesias-Prieto et al., 1992; Hoegh-Guldberg, 1999; Fitt et al., 2001). The main
cause of bleaching is elevated seawater temperature (Fitt et al., 2001) and data collected
at Ubatuba revealed a yearly oscillation of 15°C, which is significantly high for
hermatypic corals. Another experiment did monitor seasonal variation in Symbiodinium
33
concentrations in M. hispida and other two species of endemic corals at Picãozinho
(Paraíba State, Northeast Brazil), but no bleaching was detected (Costa et al., 2005).
Several parameters such as temperature, salinity, nutrients, light availability and
hydrodynamics define the geographical limits for the occurrence of scleractinian corals
(Smith and Buddmeiro 1992; Kleypas 1997; Kleypas et al., 1999). The distribution limit
of Mussismilia hispida is the state of São Paulo (approx. 24° S) (Francini et al., 2002), and
at Ubatuba (S 23º 26' 02"; W 45º 04' 16") they are considered to be marginal to their
distribution (Leão et al., 2003). M. hispida is the only reef-building representative of the
order Scleractinia in the region, and it has been reported as capable of spawning in this
area (Francini et al., 2002). The heterotrophic feeding by M. hispida may be an important
adaptation to less than optimal conditions, as they may resort to this nutritional mode
when photosynthesis is suppressed. It has been reported that, after prolonged bleaching
events, corals without significant input of heterotrophic carbon such as Porites are
expected to be more susceptible to mortality than corals such as Montipora capitata,
which presents high rates of heterotrophic feeding (Grottoli et al., 2006). This fact
suggests that Mussismilia hispida has an ecological advantage over other species due to
its ability to feed on zooplankton and survive during prolonged periods of bleaching
(Grottoli et al., 2006). Furthermore, it is feasible that due to its heterotrophic capacity,
M. hispida has evolved and adapted to survive and reproduce under suboptimal
conditions, expanding its distribution. These adaptations may prove crucial in view of
current climate change projections, since this species may expand its distribution to
areas previously occupied by less tolerant species. In the future, the disproportional
presence of M. hispida could maybe used as a proxy for coral habitat degradation.
Our major findings show that M. hispida is able to frequently shift between
predominantly autotrophic and predominantly heterotrophic, especially when adverse
climate events occur. Furthermore, we have validated the use of specific fatty acid
trophic markers as proxies for these feeding modes in corals. This opens perspectives
for further studies of benthic trophic ecology in coral reefs. The contribution of this work
also includes the first yearlong monitoring of the feeding behavior in a hermatypic coral
in the South Atlantic, with the occurrence and monitoring of a mild bleaching event.
34
LITERATURE CITED
ALVES DE LIMA, L., MIGLIOLO, L., BARREIRO E CASTRO, C., DE OLIVEIRA PIRES, D., LÓPEZ
ABARRATEGUI, C., FERREIRA GONCALVES, E., MARIA VASCONCELOS, I., JOSE, C. T. A.
O., OTERO-GONZALEZ, A. J., OCTAVIO, L. F., AND CAMPOS DIAS, S. (2013).
Identification of a novel antimicrobial peptide from Brazilian coast coral Phyllogorgia
ilatata. Protein and peptide letters, 20(10), 1153-1158.
ANTHONY, K. R. N., AND FABRICIUS, K. E. (2000). Shifting roles of heterotrophy and
autotrophy in coral energetics under varying turbidity. Journal of experimental
marine biology and ecology, 252(2), 221-253.
ANTHONY, K. R. N., AND HOEGH‐GULDBERG, O. (2003a). Variation in coral
photosynthesis, respiration and growth characteristics in contrasting light
microhabitats: an analogue to plants in forest gaps and understoreys? Functional
Ecology, 17(2), 246-259.
ANTHONY, K. R. N., AND HOEGH-GULDBERG, O. (2003b). Kinetics of photoacclimation in
corals. Oecologia, 134(1), 23-31.
BACHOK, Z., MFILINGE, P., AND TSUCHIYA, M. (2006). Characterization of fatty acid
composition in healthy and bleached corals from Okinawa, Japan. Coral Reefs, 25(4),
545-554.
BELLWOOD, D. R., AND WAINWRIGHT, P. C. (2002). The history and biogeography of
fishes on coral reefs. Coral reef fishes: dynamics and diversity in a complex
ecosystem, 5-32.
BELLWOOD, D. R., HUGHES, T. P., FOLKE, C., AND NYSTRÖM, M. (2004). Confronting the
coral reef crisis. Nature, 429(6994), 827-833.
BISHOP, D. G., AND KENRICK, J. R. (1980). Fatty acid composition of symbiotic
zooxanthellae in relation to their hosts. Lipids, 15(10), 799-804.
BLIGH, E. G., AND DYER, W. J. (1959). A rapid method of total lipid extraction and
purification. Canadian journal of biochemistry and physiology, 37(8), 911-917.
BURKE, L., REYTAR, K., SPALDING, M., AND PERRY, A. (2011). Reefs at risk revisited.
World Resouces Institue: Washington DC. ISBN 98-1-56973-762.0 115 pp. Available
at: https://goo.gl/Vu8t3N. Accessed in: 16/09/2016.
CALADO, L. (2006). Dinâmica da interação da atividade de meso-escala da Corrente do
Brasil com o fenômeno da ressurgência costeira ao largo de Cabo Frio e Cabo de Sao
Tome, RJ (Doctoral dissertation, Universidade de São Paulo).
35
CANTIN, N. E., COHEN, A. L., KARNAUSKAS, K. B., TARRANT, A. M., AND MCCORKLE, D.
C. (2010). Ocean warming slows coral growth in the central Red Sea.
Science, 329(5989), 322-325.
CASTRO FILHO, B. M., MIRANDA, L.B. AND MYAO, S.Y. (1987). Considerações
hidrográficas na plataforma continental ao largo de Ubatuba: variações sazonais e
em média escala. Boletim do Instituto Oceanográfico, 35: 135-151.
CESAR, H., BURKE, L., AND PET-SOEDE, L. (2003). The economics of worldwide coral reef
degradation. Cesar Environmental Economics Consulting. Technical Report.
CINEL, B., ROBERGE, M., BEHRISCH, H., VAN OFWEGEN, L., CASTRO, C. B., AND
ANDERSEN, R. J. (2000). Antimitotic Diterpenes from Erythropodium c aribaeorum
Test pharmacophore Models for Microtubule Stabilization. Organic letters, 2(3), 257-
260.
CLARK, K. B., AND JENSEN, K. R. (1982). Effects of temperature on carbon fixation and
carbon budget partitioning in the zooxanthellal symbiosis of Aiptasia pallida
(Verrill). Journal of Experimental Marine Biology and Ecology, 64(3), 215-230.
CONNELL, J. H. (1978). Diversity in tropical rain forests and coral reefs.
Science, 199(4335), 1302-1310.
CONNELL, J.H., 1997. Disturbance and recovery of coral assemblages. Coral Reefs 16,
s101–s113.
CONNELL, J.H., HUGHES, T.P., AND WALLACE, C.C. (1997). A 30 year study of coral
abundance, recruitment, and disturbance at several scales in space and time.
Ecological Monographs, 67, 461–488.
CONNOLLY, S. R., LOPEZ-YGLESIAS, M. A., AND ANTHONY, K. R. N. (2012). Food
availability promotes rapid recovery from thermal stress in a scleractinian coral. Coral
Reefs, 31(4), 951-960.
COSTA, C. F., SASSI, R., AND AMARAL, F. D. (2005). Annual cycle of symbiotic
dinoflagellates from three species of scleractinian corals from coastal reefs of
northeastern Brazil. Coral Reefs, 24(2), 191-193.
COSTANZA, R., D'ARGE, R., DE GROOT, R., FABER, S., GRASSO, M., HANNON, B., AND
RASKIN, R. G. (1997). The value of the world's ecosystem services and natural capital.
The Globalization and Environment Reader, 117.
CRABBE, M.J.C., MENDES, J.M., AND WARNER, G.F. (2002). Lack of recruitment of
nonbranching corals in Discovery Bay is linked to severe storms. Bulletin of Marine
Science, 70, 939–945.
36
CRABBE, M.J.C., WALKER, E.L.L., AND STEPHENSON, D.B. (2008). The impact of weather
and climate extremes on coral growth. In: Diaz, H., Murnane, R. (Eds.), Climate
Extremes and Society. Cambridge University Press, Cambridge, UK, 165– 188.
CROSSLAND, C. J. (1987). In situ release of mucus and DOC-lipid from the corals Acropora
variabilis and Stylophora pistillata in different light regimes. Coral reefs, 6(1), 35-42.
CROSSLAND, C. J., BARNES, D. J., AND BOROWITZKA, M. A. (1980). Diurnal lipid and
mucus production in the staghorn coral Acropora acuminata. Marine Biology,60(2-3),
81-90.
DALSGAARD, J., JOHN, M. S., KATTNER, G., MÜLLER-NAVARRA, D., AND HAGEN, W.
(2003). Fatty acid trophic markers in the pelagic marine environment. Advances in
marine biology, 46, 225-340.
DEWICK, P. M. (1997). The biosynthesis of C 5–C 25 terpenoid compounds. Natural
Product Reports, 14(2), 111-144.
DODDS, L. A., BLACK, K. D., ORR, H., AND ROBERTS, J. M. (2009). Lipid biomarkers reveal
geographical differences in food supply to the cold-water coral Lophelia pertusa
(Scleractinia). Marine Ecology Progress Series, 397, 113-124.
DOUGLAS, A. E. (2003). Coral bleaching––how and why? Marine Pollution Bulletin, 46(4),
385-392.
DUBINSKY, Z., AND FALKOWSKI, P. (2011). Light as a source of information and energy
in zooxanthellate corals. Springer Netherlands, (pp. 107-118).
EZZAT, L., TOWLE, E., IRISSON, J. O., LANGDON, C., AND FERRIER‐PAGÈS, C. (2016). The
relationship between heterotrophic feeding and inorganic nutrient availability in the
scleractinian coral T. reniformis under a short‐term temperature increase. Limnology
and Oceanography, 61(1), 89-102.
FABRICIUS, K. (1999). Tissue loss and mortality in soft corals following mass-
bleaching. Coral Reefs,18(1), 54-54.
FABRICIUS, K. E., AND DOMMISSE, M. (2000). Depletion of suspended particulate matter
over coastal reef communities dominated by zooxanthellate soft corals. Marine
Ecology Progress Series, 196, 157-167.
FALKOWSKI, P. G., DUBINSKY, Z., MUSCATINE, L., AND PORTER, J. W. (1984). Light and
the bioenergetics of a symbiotic coral. Bioscience, 34(11), 705-709.
FALTER, J. L., ATKINSON, M. J., SCHAR, D. W., LOWE, R. J., AND MONISMITH, S. G. (2011).
Short-term coherency between gross primary production and community respiration
in an algal-dominated reef flat. Coral Reefs, 30(1), 53-58.
37
FERRIER-PAGES, C., WITTING, J., TAMBUTTÉ, E., AND SEBENS, K. P. (2003). Effect of
natural zooplankton feeding on the tissue and skeletal growth of the scleractinian
coral Stylophora pistillata. Coral Reefs, 22(3), 229-240.
FIGUEIREDO, J., BAIRD, A. H., COHEN, M. F., FLOT, J. F., KAMIKI, T., MEZIANE, T., AND
YAMASAKI, H. (2012). Ontogenetic change in the lipid and fatty acid composition of
scleractinian coral larvae. Coral Reefs, 31(2), 613-619.
FITT, W. K., BROWN, B. E., WARNER, M. E., AND DUNNE, R. P. (2001). Coral bleaching:
interpretation of thermal tolerance limits and thermal thresholds in tropical
corals. Coral Reefs, 20(1), 51-65.
FRANCINI, C. L. B., CASTRO, C. B., AND PIRES, D. O. (2002). First record of a reef coral
spawning event in the western South Atlantic. Invertebrate reproduction and
development, 42(1), 17-19.
GILMOUR, J. P., SMITH, L. D., HEYWARD, A. J., BAIRD, A. H., AND PRATCHETT, M. S.
(2013). Recovery of an isolated coral reef system following severe
disturbance. Science, 340(6128), 69-71.
GLYNN, P. W., AND ENOCHS, I. C. (2011). Invertebrates and their roles in coral reef
ecosystems. In Coral reefs: an ecosystem in transition. Springer Netherlands, 273-325
GROTTOLI, A. G. (2002). Effect of light and brine shrimp on skeletal δ 13 C in the
Hawaiian coral Porites compressa: a tank experiment. Geochimica et Cosmochimica
Acta, 66(11), 1955-1967.
GROTTOLI, A. G., AND WELLINGTON, G. M. (1999). Effect of light and zooplankton on
skeletal δ13C values in the eastern Pacific corals Pavona clavus and Pavona
gigantea. Coral Reefs, 18(1), 29-41.
GROTTOLI, A. G., RODRIGUES, L. J., AND PALARDY, J. E. (2006). Heterotrophic plasticity
and resilience in bleached corals. Nature, 440(7088), 1186-1189.
HALFAR, J., GODINEZ-ORTA, L., RIEGL, B., VALDEZ-HOLGUIN, J. E., AND BORGES, J. M.
(2005). Living on the edge: high-latitude Porites carbonate production under
temperate eutrophic conditions. Coral Reefs, 24(4), 582-592.
HALLOCK, P. (1997). Reefs and reef limestones in Earth history. In: Birkeland, C (Ed.), Life
and Death of Coral Reefs. Chapman and Hall, New York, 13-42.
HODGSON, G. (1999). A global assessment of human effects on coral reefs. Marine
Pollution Bulletin, 38, 2–8.
HOEGH-GULDBERG, O. (1999). Climate change, coral bleaching and the future of the
world's coral reefs. Marine and freshwater research, 50(8), 839-866.
38
HOEGH-GULDBERG, O., MUMBY, P. J., HOOTEN, A. J., STENECK, R. S., GREENFIELD, P.,
GOMEZ, E., AND KNOWLTON, N. (2007). Coral reefs under rapid climate change and
ocean acidification. Science, 318(5857), 1737-1742.
HOOGENBOOM, M., E. BERAUD, AND C. FERRIER-PAGÈS. (2010). Relationship between
symbiont density and photosynthetic carbon acquisition in the temperate coral
Cladocora caespitosa. Coral Reefs 29: 21–29. DOI: 10.1007/s00338-009-0558-9
HOOGENBOOM, M., RODOLFO-METALPA, R., AND FERRIER-PAGÈS, C. (2010). Co-
variation between autotrophy and heterotrophy in the Mediterranean coral
Cladocora caespitosa. Journal of Experimental Biology, 213(14), 2399-2409.
HOULBREQUE, F., AND C. FERRIER-PAGES. (2009). Heterotrophy in tropical scleractinian
corals. Biological Reviews. 84: 1–17. DOI: 10.1111/j.1469-185X.2008.00058.x
HOULBRÈQUE, F., TAMBUTTÉ, E., ALLEMAND, D., AND FERRIER-PAGÈS, C. (2004).
Interactions between zooplankton feeding, photosynthesis and skeletal growth in the
scleractinian coral Stylophora pistillata. Journal of Experimental Biology, 207(9),
1461-1469.
HOULBRÈQUE, F., TAMBUTTÉ, E., AND FERRIER-PAGÈS, C. (2003). Effect of zooplankton
availability on the rates of photosynthesis, and tissue and skeletal growth in the
scleractinian coral Stylophora pistillata. Journal of Experimental Biology, 296, 145–
166.
Hughes, T. P., Baird, A. H., Bellwood, D. R., Card, M., Connolly, S. R., Folke, C., Grosberg
R., Hoegh-Guldberg, O., Jackson, J. B. C., Kleypas, J., Lough, J. M., Marshall, P.,
Nyström, M., Palumbi, S. R., Pandolfi, M., Rosen, M., AND Lough, J. M. (2003). Climate
change, human impacts, and the resilience of coral reefs. Science, 301(5635), 929-
933.
IGLESIAS-PRIETO, R., MATTA, J. L., ROBINS, W. A., AND TRENCH, R. K. (1992).
Photosynthetic response to elevated temperature in the symbiotic dinoflagellate
Symbiodinium microadriaticum in culture. Proceedings of the national Academy of
Sciences, 89(21), 10302-10305.
IVERSON, S. J., FIELD, C., DON BOWEN, W., AND BLANCHARD, W. (2004). Quantitative
fatty acid signature analysis: a new method of estimating predator diets. Ecological
Monographs, 74(2), 211-235.
JOHANNES, R. E., COLES, S. L., AND KUENZEL, N. T. (1970). The role of zooplankton in the
nutrition of some scleractinian corals. Limnology and oceanography, 15(4), 579-586.
KLEYPAS, J. A. (1997). Modeled estimates of global reef habitat and carbonate
production since the last glacial maximum. Paleoceanography, 12(4), 533-545.
39
KLEYPAS, J. A., MCMANUS, J. W., AND MEÑEZ, L. A. (1999). Environmental limits to coral
reef development: where do we draw the line? American Zoologist, 39(1), 146-159.
KRUEGER, T., HAWKINS, T. D., BECKER, S., PONTASCH, S., DOVE, S., HOEGH-GULDBERG,
O., AND DAVY, S. K. (2015). Differential coral bleaching—Contrasting the activity and
response of enzymatic antioxidants in symbiotic partners under thermal
stress. Comparative Biochemistry and Physiology Part A: Molecular AND Integrative
Physiology, 190, 15-25.
LALLI, C. M. AND PARSONS, T. R. 2004. Biological oceanography. An introduction. 2nd
edition. Elsevier Butterworth–Heinemann, 314.
Leãoa, Z. M., Kikuchi, R. K., AND Testa, V. (2003). Corals and coral reefs of Brazil. In: Latin
American Coral Reefs. Elsevier Science B.V. 9-52.
LEVAS, S. J., GROTTOLI, A. G., HUGHES, A., OSBURN, C. L., AND MATSUI, Y. (2013).
Physiological and biogeochemical traits of bleaching and recovery in the mounding
species of coral Porites lobata: implications for resilience in mounding corals. PloS
one, 8(5), e63267.
LOPES, R. M. (2013). Variação temporal e crescimento do zooplâncton no litoral norte
de São Paulo, com ênfase em estágios imaturos de copépodes(Doctoral dissertation,
Universidade de São Paulo).
MAHIQUES, M. D. (1995). Dinâmica sedimentar atual nas enseadas da região de
Ubatuba, Estado de São Paulo. Boletim do Instituto Oceanográfico, 43(2), 111-122.
MALLELA, J. AND CRABBE, M. J. C. (2009). Hurricanes and coral bleaching linked to
changes in coral recruitment in Tobago. Marine Environmental Research, 68(4), 158-
162.
CRABBE, M.J.C., MENDES, J.M., WARNER, G.F., (2002). Lack of recruitment of
nonbranching corals in Discovery Bay is linked to severe storms. Bulletin of Marine
Science, 70, 939–945.
MALLELA, J. (2007). Coral reef encruster communities and carbonate production in
cryptic and exposed coral reef habitats along a gradient of terrestrial disturbance.
Coral Reefs 26, 775–785.
MCCLANAHAN, T. R., MUTHIGA, N. A., KAMUKURU, A. T., MACHANO, H., AND KIAMBO,
R. W. (1999). The effects of marine parks and fishing on coral reefs of northern
Tanzania. Biological Conservation, 89(2), 161-182.
MILLER, M. W. (1995). Growth of a temperate coral: effects of temperature, light, depth,
and heterotrophy. Marine Ecology Progress Series, 122, 217-225.
40
MOBERG, F., AND FOLKE, C. (1999). Ecological goods and services of coral reef
ecosystems. Ecological economics, 29(2), 215-233.
MUSCATINE, L., AND PORTER, J. W. (1977). Reef corals: mutualistic symbioses adapted
to nutrient-poor environments. Bioscience, 27(7), 454-460.
MUSCATINE, L., AND WEIS, V. (2013). Productivity of zooxanthellae and
biogeochemical. Primary Productivity and Biogeochemical Cycles in the Sea, 43, 257.
NAPOLITANO, G. E., POLLERO, R. J., GAYOSO, A. M., MACDONALD, B. A., AND
THOMPSON, R. J. (1997). Fatty acids as trophic markers of phytoplankton blooms in
the Bahia Blanca estuary (Buenos Aires, Argentina) and in Trinity Bay (Newfoundland,
Canada). Biochemical Systematics and Ecology, 25(8), 739-755.
SCHNELL, R. C. (2004). Climate Monitoring and Diagnostics Laboratory summary. Report,
2002–2003. In: National Oceanic Atmospheric Administration, 27, 174.
OLIVOTTO I., ROLLO A., SULPIZIO R., AVELLA M., TOSTI L., CARNEVALI O. (2006) Breeding
and rearing the Sunrise Dotty back Pseudo chromis flavivertex: the importance of live
prey enrichment during larval development. Aquaculture, 255, 480–487.
OSINGA, R., SCHUTTER, M., GRIFFIOEN, B., WIJFFELS, R. H., VERRETH, J. A., SHAFIR, S.,
AND LAVORANO, S. (2011). The biology and economics of coral growth. Marine
Biotechnology, 13(4), 658-671.
PALARDY, J. E., GROTTOLI, A. G., AND MATTHEWS, K. A. (2005). Effects of upwelling,
depth, morphology and polyp size on feeding in three species of Panamanian
corals. Marine Ecology Progress Series, 300, 79-89.
PALARDY, J. E., GROTTOLI, A. G., AND MATTHEWS, K. A. (2006). Effect of naturally
changing zooplankton concentrations on feeding rates of two coral species in the
Eastern Pacific. Journal of Experimental Marine Biology and Ecology, 331(1), 99-107.
PAPINA, M., MEZIANE, T., AND VAN WOESIK, R. (2003). Symbiotic zooxanthellae provide
the host-coral Montipora digitata with polyunsaturated fatty acids. Comparative
Biochemistry and Physiology Part B: Biochemistry and Molecular Biology, 135(3), 533-
537.
PAPINA, M., MEZIANE, T., AND VAN WOESIK, R. (2007). Acclimation effect on fatty acids
of the coral Montipora digitata and its symbiotic algae. Comparative Biochemistry
and Physiology Part B: Biochemistry and Molecular Biology, 147(4), 583-589.
PERSSON, J., AND VREDE, T. (2006). Polyunsaturated fatty acids in zooplankton:
variation due to taxonomy and trophic position. Freshwater Biology, 51(5), 887-900.
ROBERTS, C.M., MCCLEAN, C.J., VERON, J.E.N., HAWKINS, J.P., ALLEN, G.R., MCALLISTER,
D.E., MITTERMEIER, C.G., SCHUELER, F.W., SPALDING, M., WELLS, F., VYNNE, C., AND
41
WERNER, T.B. (2002). Marine biodiversity hotspots and conservation priorities for
tropical reefs. Science, 295, 1280–1284.
RODRIGUES, L. J., AND GROTTOLI, A. G. (2006). Calcification rate and the stable carbon,
oxygen, and nitrogen isotopes in the skeleton, host tissue, and zooxanthellae of
bleached and recovering Hawaiian corals. Geochimica et Cosmochimica Acta, 70(11),
2781-2789.
RODRIGUES, L. J., AND GROTTOLI, A. G. (2007). Energy reserves and metabolism as
indicators of coral recovery from bleaching. Limnology and oceanography, 52(5),
1874-1882.
RUPPERT, E. E., FOX, R. S. BARNES, R. D. (2004). Invertebrate Zoology, 7th edition.
Cengage Learning. 132–137. ISBN 978-81-315-0104-7.
SALVAT, B. (1992). Coral reefs: a challenging ecosystem for human societies. Global
Environmental Change, 2(1), 12-18.
SARGENT, J.R., BELL MV, HENDERSEN, R.J., AND TOCHER, D.R. (1990) Polyunsaturated
fatty acids in marine and terrestrial food webs. In: Mellinger, J. (eds) Animal nutrition
and transport processes, 1, Nutrition in wild and domestic animals. Comparative
physiology. Karger, Basel, 11–23.
SEBENS, K. P., HELMUTH, B., CARRINGTON, E., AND AGIUS, B. (2003). Effects of water
flow on growth and energetics of the scleractinian coral Agaricia tenuifolia in
Belize. Coral Reefs, 22(1), 35-47.
SEBENS, K. P., VANDERSALL, K. S., SAVINA, L. A., AND GRAHAM, K. R. (1996). Zooplankton
capture by two scleractinian corals, Madracis mirabilis andMontastrea cavernosa, in
a field enclosure. Marine Biology, 127(2), 303-317.
SHEPPARD, C. R., DAVY, S. K., AND PILLING, G. M. (2009). The biology of coral reefs. OUP
Oxford.
SMITH, S. V., AND BUDDEMEIER, R. W. (1992). Global change and coral reef
ecosystems. Annual Review of Ecology and Systematics, 23, 89-118.
SOROKIN, Y. I. (2013). Coral reef ecology. Springer Science AND Business Media, (102).
STAT, M., CARTER, D., AND HOEGH-GULDBERG, O. (2006). The evolutionary history of
Symbiodinium and scleractinian hosts: symbiosis, diversity, and the effect of climate
change. Perspectives in Plant Ecology, Evolution and Systematics, 8(1), 23-43.
TITLYANOV, E. A., TITLYANOVA, T. V., YAMAZATO, K., AND VAN WOESIK, R. (2001).
Photo-acclimation dynamics of the coral Stylophora pistillata to low and extremely
low light. Journal of Experimental Marine Biology and Ecology, 263(2), 211-225.
42
TREIGNIER, C., GROVER, R., FERRIER-PAGES, C., AND TOLOSA, I. (2008). Effect of light
and feeding on the fatty acid and sterol composition of zooxanthellae and host tissue
isolated from the scleractinian coral Turbinaria reniformis. Limnology and
Oceanography, 53(6), 2702-2710.
UNEP - UNITED NATIONS ENVIRONMENT PROGRAM (2003): Conventions and Coral
Reef, Fourteen Multilateral Environment Agreements, Programmes, Partnerships
and Networks Relevant to the Protection and Conservation of Coral Reef, and the
World Summit on Sustainable Development Plan of Implementation. Produced by the
UNEP Coral Reef Unit in collaboration with the WWF Coral Reef Advocacy Initiative.
Available at - http://www.unep.org/annualreport/2013/landing.asp (Last accessed
in: 06/21/2016).
VENN, A. A., TAMBUTTÉ, E., HOLCOMB, M., LAURENT, J., ALLEMAND, D., AND
TAMBUTTÉ, S. (2013). Impact of seawater acidification on pH at the tissue–skeleton
interface and calcification in reef corals. Proceedings of the National Academy of
Sciences, 110(5), 1634-1639.
VOLKMAN, J. K., BARRETT, S. M., AND BLACKBURN, S. I. (1999). Eustigmatophyte
microalgae are potential sources of C 29 sterols, C 22–C 28 n-alcohols and C 28–C 32
n-alkyl diols in freshwater environments. Organic Geochemistry, 30(5), 307-318.
WABNITZ C., TAYLOR M., GREEN E., RAZAK T. (2003) From Ocean to Aquarium.
Cambridge: UNEP–WCMC.
WILD, C., HUETTEL, M., KLUETER, A., KREMB, S. G., RASHEED, M. Y., AND JØRGENSEN, B.
B. (2004). Coral mucus functions as an energy carrier and particle trap in the reef
ecosystem. Nature, 428(6978), 66-70.
WILKINSON, C. (2008). Status of coral reefs of the world: 2008. Global Coral Reef
Monitoring Network and Reef and Rainforest Research Centre, Townsville, Australia.
WILSON, S. K., BURNS, K., AND CODI, S. (2001). Sources of dietary lipids in the coral reef
blenny Salarias patzneri. Marine Ecology Progress Series, 222, 291-296.
WPACFIN (Western Pacific Fishery Information Network). NOAA-National Marine
Fisheries Service, Pacific Islands Fisheries Science Center, 2570 Dole Street, Honolulu,
96822–2396. Available at: http://www.pifsc.noaa.gov/wpacfin (Last accessed
07/30/2016).
ZHUKOVA, N. V., AND TITLYANOV, E. A. (2003). Fatty acid variations in symbiotic
dinoflagellates from Okinawan corals. Phytochemistry, 62(2), 191-195.