Coral Reefs

, Volume 33, Issue 1, pp 207–219

The thermal tolerance of crown-of-thorns (Acanthaster planci) embryos and bipinnaria larvae: implications for spatial and temporal variation in adult populations

Authors

  • M. Lamare
    • Department of Marine ScienceUniversity of Otago
  • D. Pecorino
    • Department of Marine ScienceUniversity of Otago
    • Department for Earth, Environment and Life Sciences (DISTAV)University of Genoa
  • N. Hardy
    • Schools of Medical and Biological SciencesUniversity of Sydney
  • M. Liddy
    • Australian Institute of Marine Science
  • M. Byrne
    • Schools of Medical and Biological SciencesUniversity of Sydney
    • Australian Institute of Marine Science
Open AccessReport

DOI: 10.1007/s00338-013-1112-3

Cite this article as:
Lamare, M., Pecorino, D., Hardy, N. et al. Coral Reefs (2014) 33: 207. doi:10.1007/s00338-013-1112-3

Abstract

To understand the role of sea temperature on the population biology of the crown-of-thorns sea star Acanthaster planci, the thermal window for embryonic and larval development was investigated. In two experiments, the response of embryos and larvae across 12 temperatures from 19.4 to 36.5 °C was quantified as the percentage of individuals reaching cleavage stage embryos, blastula, gastrula, early-bipinnaria, late-bipinnaria larvae or abnormal. Measurements were made at 7 times up to 72 h post-fertilisation, with the morphometrics of larvae measured in the 72-h sample. Acanthaster planci developed at temperatures between 19.4 and 33.2 °C, with a thermal window for development to the late-bipinnaria stage between 25.6 and 31.6 °C. Development rate, normal development and larval size were optimal at 28.7 °C, with development rates remaining relatively constant up to 31.6 °C. Rates of abnormality increased steadily (early embryonic stages) above 28.7 °C and was 100 % at temperatures approaching 33 °C. These experiments provide a more detailed insight into the response of A. planci developmental stages to temperature. The present day distribution of the species in eastern Australia overlap with the optimal thermal window for development to the late-bipinnaria stage (≈25–32 °C), implying a role of temperature in controlling population distributions and abundances. Despite this, short- or long-term temperature increases may not be a major modulator of the crown-of-thorns recruitment success, population dynamics and distribution in the future as no significant change in development rates, larval survival and growth occurred within this thermal window. Therefore, moderate (1–2 °C) increases in sea temperatures caused by El Niño or near-future ocean warming may not drive an increase in developmental and settlement success. Indeed, without any acclimation to warmer temperatures expected under near-future warming (+2 to 4 °C), climate change could ultimately reduce larval survival due to elevated mortality above the optimal development temperature.

Keywords

Crown-of-thornsTemperatureEarly life stagesThermotoleranceThermal windowClimate change

Introduction

Changes in the abundance and distribution of marine species will be an important outcome of near-future increases in sea temperatures (Hoegh-Guldberg and Bruno 2010). For instance, coral reefs in Japan have shifted by as much as 14 km yr−1 towards the north as sea temperatures in the region warm (Yamano et al. 2011). Similarly, Barry et al. (1995) reported an increase in the abundance of southern marine invertebrate species and a decrease in northern species for a site along the Californian coastline. This coincided with an increase in the annual mean shoreline ocean temperature of 0.75 °C over the 60-yr period between observations.

For marine species with free-living embryos and larvae, changes in survival and growth rates of their developmental stages as a result of ocean warming can drive spatial and temporal population changes. One of the clearest examples of this process is the expansion of the sea urchin Centrostephanus rodgersii as a result of sea temperature warming off coastal south-eastern Australia and Tasmania (Ling et al. 2009). In this region, the southern expansion of the sea urchin is almost certainly the outcome of new regions entering the thermal window of larval development (12–22 °C) as winter sea temperatures increase (Ling et al. 2008).

These observations indicate the importance of quantifying the responses of embryos and larvae to temperature when considering regional warming of the ocean under various climate change scenarios. Developmental stages of marine invertebrates are directly influenced by temperature, and within thermal tolerance windows, developmental rate typically increases with warming due to the stimulating effects on physiological rates (Enquist et al. 2003; Brown et al. 2004; Allen et al. 2006). For echinoderm development, faster progression through embryonic and larval stages occurs with, with increased temperature (Hoegh-Guldberg and Pearse 1995; Hardy et al. 2013; Pecorino et al. 2013). For sea stars specifically, increases in developmental rate with increasing temperature has been described for one polar (Hoegh-Guldberg and Pearse 1995; Stanwell-Smith and Peck 1998), four temperate (Hoegh-Guldberg and Pearse 1995; Lee et al. 2004; Villalobos et al. 2006) and one tropical species (Hoegh-Guldberg and Pearse 1995).

Survival of developmental stages may also be temperature-dependent, with reduced survival outside the thermal window as a result of physiological stresses (Roccheri et al. 1986; Hofmann and Somero 1996; Somero 2010; Tomanek 2010). The number of larvae surviving to settlement may also be influenced by increased temperature, where faster developing larvae are exposed for less time to high predation mortality in the plankton (i.e. instantaneous mortality rates ≈0.10–0.20 d−1, Rumrill 1990; Lamare and Barker 1999). Shorter larval duration may also reduce dispersion and recruitment, which can enhance local recruitment rates, although this would reduce the capacity to colonise across wider geographical regions (Hedgecock 1986).

Tropical coral reef ecosystems have degraded in recent decades as a result of human over-exploitation, pollution, bleaching, storm damage and outbreaks of the crown-of-thorns sea star (COTS) Acanthaster planci (Pandolfi et al. 2003; Bruno and Selig 2007; De’ath et al. 2012). For example, the Australian Great Barrier Reef (GBR) may have experienced a 50 % reduction in coral cover between 1985 and 2012 (De’ath et al. 2012), with A. planci outbreaks of particular concern (De’ath et al. 2012). In the case of the GBR, a recent assessment of the impact of three stressors (storms, bleaching, A. planci) estimated that predation by A. planci accounted for 42 % of the observed loss (De’ath et al. 2012). Outbreaks of the species, characterised by sudden increases in the abundance of adult populations, have been recorded on most Indo-Pacific coral reefs, including the GBR (review Uthicke et al. 2009). The close link between A. planci outbreaks and coral cover loss is an outcome of specialised diet of A. planci, which is an exclusively corallivorous sea star that results in a very high predation pressure on coral when population densities increase (Fabricius 2013).

On the GBR, A. planci ossicles can be found in sediment core slices >2,000 yrs old, but there is no indication of population outbreaks prior to the 1960s (Fabricius and Fabricius 1992). The prevalence of outbreaks has, however, been well documented over the past half-century (Birkeland 1982; Moran 1986; Lourey et al. 2000; Bellwood et al. 2004; Fabricius et al. 2010), suggesting that it may be a relatively recent phenomena. Such increases in COTS population sizes have been attributed to a number of factors including reductions in predation pressure on juveniles and adults (McCallum 1987; review Fabricius 2013), reduced salinity (Lucas 1973) and increased phytoplankton productivity and biomass favouring larval development (review Uthicke et al. 2009; Fabricius et al. 2010). The link between A. planci outbreaks and enhanced larval survival to settlement has been established using evidence from laboratory, field and modelling studies (Fabricius et al. 2010). In this scenario, the eutrophication-driven increases in phytoplankton production release larvae from food-limited development and subsequently an increase in the number of larvae completing development (Fabricius et al. 2010).

In addition to food levels, temperature can also affect the pace of embryonic and larval development in A. planci (Hoegh-Guldberg and Pearse 1995) and could potentially contribute to increases in larval survival. In this regard, it was shown that larval development was fastest at temperatures of ≈28 °C (Henderson and Lucas 1971; Lucas 1973). A more comprehensive study of the response of A. planci larvae to temperature by Johnson and Babcock (1994) found similar results for the development pace and a narrowing of the temperature tolerance window for development of ≈1 °C between gastrula and bipinnaria. Confirming the suggestion of a thermal window for A. planci, Hoegh-Guldberg and Pearse (1995) examined the time required to reach hatching noting development rate increased between 20 and 32 °C, with a break at 25 °C.

The contribution of development thermal windows to the distribution of adult sea stars is an important consideration. Lucas (1973) and Johnson and Babcock (1994) discussed the relationship between temperature tolerance and the distribution of A. planci around Australia. Lucas (1973) suggested that the southern distribution of A. planci is limited by intolerance of the larval stages to temperatures less than 27 °C, although Johnson and Babcock (1994) noted A. planci occurs in regions (namely Lord Howe Island) where maximum summer temperatures at the time of spawning are ≈24 °C. Johnson and Babcock (1994) also pointed out that A. planci outbreaks initiate in the northern GBR, where sea temperature may be closer to the optimum for development, and fewer smaller outbreaks occur in the cooler southern part of the range.

In this study, we hypothesise that spatial and temporal variability in Acanthaster planci populations may be determined by the thermal tolerance of developmental stages and that warming sea temperatures may alter the population biology of the sea star through changes in early development rates and survival. To test this hypothesis, we determined the thermal window of A. planci developmental stages. This was achieved by examining the response of A. planci larvae to temperature across a 12-step thermal gradient ranging from 19 to 37 °C. Across this temperature gradient, we examined the pace of development, abnormal development rates and larval morphometrics after 72 h. Using these observations, we firstly re-examine the relationship between larval thermal windows and distributions of A. planci, and secondly, we contemplate the potential effects of increases in sea surface temperatures of 2–4 °C that are predicted to occur along eastern Australia over the coming century (Hobday and Lough 2011).

Methods

Specimen collection and spawning

Twenty Pacific (sensu Vogler et al. 2008) adult Acanthaster planci were collected by SCUBA divers in early November 2012 from Green Island (GBR, Australia, 16°46.5′S, 145°59.3′E, Fig. 1) at a depth of 6–12 m, placed in containers with flow-through seawater, and transported to the Australian Institute of Marine Science (Cape Ferguson, North Queensland). There, specimens were kept in seawater tanks provided with running unfiltered seawater at the ambient seawater temperature of 27–28 °C. Biopsies were performed for sex determination, and males and females separated until spawning.
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Fig. 1

Map or eastern Australia showing location of the collection site (Green Island), and other locations mentioned in the text (Davies Reef and Lord Howe Island). Site locations are overlaid on early-summer (November–December) sea surface temperature around eastern Australia (latitude from 5°48.3′S to 35°00′S, longitude from 138°48.5′E to 159°36.8′E) averaged across years from 2003 to 2013. Temperatures are recorded from the SST probe of the satellite Terra MODIS at a resolution of 4 km. Isotherms are at 1 °C intervals. The months examined coincide with the yearly period of maximum spawning activity of Acanthaster planci in the region

For each experiment, a small (≈1 cm) incision was made near the proximal end of one of the arms of three males and three females and three to four lobes from the gonads were removed from each individual. Testes were placed in Petri dishes and covered in Parafilm™ to prevent desiccation. Ovarian lobes were rinsed of loose eggs with filtered seawater and were then submerged in a 10−5 M 1-methyladenine in seawater solution to induce egg maturation and egg release. After 2 h, released eggs were pooled to make a stock egg suspension (concentration of 500 eggs mL−1). The eggs were transferred to 30 mL vials filled with filtered seawater to give a final egg density of 20 eggs mL−1. Fertilisation was achieved in the vials (see section ‘Experimental design’) by adding sperm at a sperm:egg ratio of 100:1 (i.e. 2,000 sperm mL−1). After fertilisation, excess sperm was removed by replacing one-third of the seawater from each experimental vial with water at the appropriate temperature.

Experimental design

Two thermal window experiments were performed using the same experimental setup. Two aluminium thermal blocks (length = 784 mm, height = 60 mm, width = 170 mm; Pecorino et al. 2013) with twelve holes (diameter = 31 mm, depth = 54 mm) in four rows were used. To achieve a thermal gradient in the aluminium blocks from ≈19 to 37 °C, heated or cooled water from temperature-controlled water baths was pumped through the opposite ends of the heat blocks. Each hole in the block held a 30-mL glass vial containing the egg suspension. The six central rows were used as experimental treatments, and the two outer rows were used as a reservoir of filtered seawater at the appropriate experimental temperatures. In total, there were twelve temperature treatments (19.4, 20.3, 22.2, 24.0, 25.6, 27.2, 28.7, 30.2, 31.6, 33.2, 34.8 and 36.5 °C), each replicated six times. Lids were placed on each vial during the experiment to prevent evaporation. Temperature was checked at the beginning and at the end of the experiments in the actual experimental vials, and, in both cases, fluctuations within each treatment group over time were minimal (<0.2 °C). Water was replaced in each vial after each sampling time with the same amount of seawater at the appropriate experimental temperature to prevent oxygen depletion. A previous experiment in the same setup (Hardy et al. 2013) indicated that oxygen depletion did not occur using frequency water changes as applied here. All seawater had previously been filtered to 0.5 μM to reduce organic and particular load.

At each sampling point, a 2 mL aliquot was sampled from each vial after gently mixing by inversion. For experiment 1, sampling times were 5, 10 and 24 h after fertilisation, and for experiment 2, sampling times were 16, 24, 48 and 72 h after fertilisation. Samples were placed in 2-mL Eppendorf™ tubes and fixed immediately with 2 drops of 7 % borax-buffered formalin. Samples were later checked under a dissection microscope and the number of embryos and larvae in each of six developmental stages, namely, cleavage stage embryos, hatched blastula, gastrula, early-bipinnaria and late-bipinnaria recorded. At least 50 embryos or larvae were scored for each sample. We also recorded the number of abnormal embryos, defined as individuals that displayed an asymmetrical shape, exogastrulation, the presence of a compact cell agglomerate in the coelom or the lack of any of the basic morphological feature of a bipinnaria (e.g. lobes, well-formed gut), depending on developmental stage.

The number in each developmental stage was reported as a percentage of the total number of embryos or larvae scored. For the second experiment, photomicrographs of 10 larvae from each experimental vial at the last sampling time (72 h) were taken and six body dimensions were measured (aboral hood, oral hood, body length, body width, stomach width, stomach length; Fig. 2), after appropriate calibration, using the software ImageJ (Schneider et al. 2012).
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Fig. 2

A 72-h-old bipinnarian Acanthaster planci larvae showing six body components measured in this study: body length (Length), body width (Width), gut width, gut length, oral hood width (Mouth Hood) and aboral hood width (Gut Hood). Scale bar 100 μm

Sea surface temperatures

November to December is the major period of spawning of Acanthaster planci (Babcock and Mundy 1992). Therefore, the average sea surface temperature (SST) measurements during both months over an 11-yr time frame (2003–2013) were collected from the SST probe of the satellite Terra MODIS (http://oceancolor.gsfc.nasa.gov/) from southern Papua New Guinea to just south of the Lord Howe Islands (latitude from 5°48.3′S to 35°00′S, longitude from 138°48.5′E to 159°36.8′E) at a resolution of 4 km. The area chosen roughly corresponds to the present day geographical range of A. planci in the West-Pacific Ocean. These data were then plotted as a coloured map with highlighted isotherms at 1 °C intervals (Fig. 1). Water temperature at the sampling date of the spawners (07/11/12) on Green Island was 27 °C (C. Collier, pers comm).

Statistical analyses

The percentages of each developmental stage and abnormal embryos at each given time were arcsine-square root transformed, and significance of the differences in the proportion of larvae at that stage among temperatures was tested using one-way ANOVA (one analysis for each developmental stage at each sampling time), after checking that the assumptions of normality and homoscedasticity were met. Differences between pairs of temperature treatments were then checked using Tukey’s HSD test. Morphological data were square root transformed and analysed using principal component analysis (PCA) to identify the body dimensions that most contribute to the difference in morphology of the larvae. A PERMANOVA was performed on the morphological data with the software PERMANOVA for Primer (Anderson et al. 2008) to test for a significant effect of temperature on the global morphology of larvae. Temperature was used as a fixed factor with 12 levels corresponding each to temperature treatment. There were six response variables corresponding to the six aforementioned morphological measurements taken on each larva.

Results

Experiment 1

The effect of temperature on the percentage of cleavage stage embryos, hatched blastulae, gastrulae and on the percentage of abnormal embryos was significant at all sampling times (Table 1), and most treatments were significantly different from each other (Electronic Supplementary Material, ESM Table 1). At 5 h, the highest percentage of cleavage stage embryos (Fig. 3a) was recorded between 24.0 and 33.2 °C (39–78.9 % cleavage across temperatures), with the maximum percentage of cleavage stage embryos (78.9 %) occurring at 28.7 °C. No developing embryos were recorded at temperatures >33.2 °C and <20 % at 19.4, 20.3 and 22.2 °C. At 10 h (Fig. 3a), most embryos in the 24.0 and 31.6 °C treatments had divided, while <20 % had cleaved at 22.2 and 33.2 °C. The embryos at lower or higher temperatures had not developed. After 24 h (Fig. 3a), cleavage stage embryos (always <20 %) were recorded between 22.2 and 31.6 °C, with the percentage decreasing with increasing temperature, and maximum number of cleavage stage embryos remaining (19.7 %) occurring at 22.2 °C. At 24 h, an opposite trend in the percentage of hatched embryos was found between 22.2 and 31.6 °C, with the percentage increasing with increasing temperature. The percentage of hatched embryos that had not yet undergone gastrulation was ≈15 % for all the temperature treatments, apart from 28.7 °C, where it was 21.6 %. The highest percentage of gastrulae staged embryos was recorded between 27.2 and 30.2 °C (33.4–41.7 % across this temperature range), with fewer present at 24.0 °C (9.8 %), 25.6 °C (19.4 %) and 31.6 °C (5.7 %). No gastrulae were found at other temperatures.
Table 1

ANOVA of the percentage of cleaved embryos, hatched blastulae, gastrulae, early-bipinnaria, late-bipinnaria and abnormal embryos of Acanthaster planci from Green Island (Great Barrier Reef, Australia) among 12 temperature treatments. Sampling times in experiment 1 are denoted by A, and sampling times in experiment 2 are denoted by B

Sampling time (h)

Developmental stage

F ratio

p value

5 A

Cleaved embryos

92.01

<0.001

 

Abnormal

77.63

<0.001

10 A

Cleaved embryos

523.48

<0.001

 

Abnormal

117.18

<0.001

16 B

Cleaved embryos

59.58

<0.001

 

Hatched blastulae

46.00

<0.001

 

Gastrulae

318.06

<0.001

 

Abnormal

124.92

<0.001

24 A

Cleaved embryos

49.57

<0.001

 

Hatched blastulae

29.39

<0.001

 

Gastrulae

29.24

<0.001

 

Abnormal

51.89

<0.001

24 B

Cleaved embryos

24.45

<0.001

 

Hatched blastulae

17.23

<0.001

 

Gastrulae

140.54

<0.001

 

Abnormal

85.01

<0.001

48 B

Gastrulae

48.75

<0.001

 

Early-bipinnaria

85.85

<0.001

 

Late-bipinnaria

141.28

<0.001

 

Abnormal

109.14

<0.001

72 B

Gastrulae

54.54

<0.001

 

Early-bipinnaria

30.78

<0.001

 

Late-bipinnaria

242.41

<0.001

 

Abnormal

140.67

<0.001

The factor analysed is ‘Temperature treatment’. Numerator df = 11, denominator df = 60 for all the analyses

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Fig. 3

Percentage of cleavage stage embryos, hatched blastulae, gastrulae, at 5, 10 and 24 h post-fertilisation for Acanthaster planci at 12 temperature treatments. Points represent mean values ± standard error (>240 embryos and larvae were scored across n = 6 replicate vials for each data point)

The percentage of abnormal embryos (Fig. 3b) after 5 h followed an opposite pattern to the percentage of hatching. Most abnormal embryos were found at temperatures ≤22.2 °C (>86.4 % of abnormal embryos) and ≥34.8 °C (100 % of abnormal embryos). At temperatures between this range, the percentage of abnormal embryos was between 23 and 64.2 %, with the minimum number of abnormal embryos at 28.7 °C (23.1 %). A similar pattern was found at 10 and 24 h after fertilisation, the only notable difference being an increase in the percentage of abnormal individuals at 31.6 °C (from 29.5 to 80.4 %) and at 33.2 °C (from 64.2 to 100 %).

Experiment 2

The influence of temperature on the percentage of cleavage stage embryos, hatched blastulae, gastrulae, early-bipinnaria, bipinnaria and abnormal embryos was significant at all sampling times (Table 1) and most treatments were significantly different from each other (ESM Table 2). At 16 h after fertilisation (Fig. 4a), cleavage stage embryos, hatched blastulae and gastrulae were recorded. The percentage of unhatched embryos was greatest at 24.0 °C (41.3 %). At temperatures lower than 20.3 °C or higher than 30.2 °C none of the embryos had hatched. The maximum percentage of hatched blastulae was found at 25.6 °C (38.1 %) and 27.2 °C (32.6 %) and this sharply decreased towards lower temperatures. No blastulae were found at <24.0 and >33.2 °C, while gastrulae were only recorded between 27.2 and 31.6 °C (35.9–61.2 % gastrulae). At 24 h after fertilisation (Fig. 4a) the proportion of each developmental stage was similar to that seen in Experiment 1 at the same time point. At 48 h after fertilisation (Fig. 4a) gastrulae, early bipinnariae and bipinnariae were present. At the cooler end of the temperature range most embryos had not developed past the gastrula stage (25.0 and 40.3 % at 22.2 and 24.0 °C, respectively). Between 25.6 and 31.6 °C most of the larvae were bipinnariae (from 31.3 to 64.3 %). By 72 h (Fig. 4a) the pattern was similar to 48 h in terms of developmental stages present and the percentages and temperatures at which they were recorded. One notable difference is that early bipinnariae were recorded at 22.2 and 24.0 °C (≈10 %) and that bipinnariae were found at 24.0 °C (40.4 %).
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Fig. 4

Percentage of cleavage stage embryos, hatched blastulae, gastrulae, early-bipinnaria larvae, and late-bipinnarian larvae at 16, 24, 48 and 72 h post-fertilisation for Acanthaster planci at 12 temperature treatments. Points represent mean values ± standard error (>240 embryos and larvae were scored across n = 6 replicate vials for each data point)

The percentage of abnormal embryos (Fig. 4b) followed a similar pattern over the 72 h period. It was 100 % at temperatures <20.3 and >33.2 °C, while at 48 and 72 h it was 100 % at 20.3 °C. Between 22.2 and 31.6 °C the percentage of abnormal embryos ranged from ≈15 to ≈80 % across the 72 h, with lower rates of abnormality recorded between 25.6 and 30.2 °C (15.7–37.8 %).

Larval morphology

The morphology of 72-h bipinnaria varied among temperature treatments, with individuals having a wider gut and a smaller aboral hood the higher the temperature (Fig. 5). Within the same temperature treatment the shape of the larvae was variable in terms of total larval width and length, gut length and oral hood width, although the effect of temperature on the global morphology of the larvae was significant (Table 2; PERMANOVA Pseudo-F = 7.1303, p (perm) < 0.001). A subsequent pairwise comparison showed that the difference between larvae at temperature treatments that were not contiguous was significant. In the PCA (Fig. 5), larvae were mostly dispersed along the PC1 axis, which explains 61.7 % or 62.2 % of the total explained variation (ESM Table 3) and is negatively correlated with the length and width of the larvae (ESM Table 4). Along this axis, however, there was no clear differentiation based on temperature with significant overlap among the treatments. While comparison of the length and width of larvae among temperatures (Fig. 6a, b) indicated a significant effect of temperature (Table 3; ANOVA on length F = 9.6, p < 0.001; ANOVA on width F = 5.5, p < 0.001), the average length and width between 24 and 30.2 °C were not significantly different (ESM Table 3). Significantly reduced (≈50 %) lengths and widths were only found at 31.6 °C compared to 30.2 °C (ESM Table 5).
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Fig. 5

Plot of the Principal Component Analysis of the morphometrics of 72-h-old Acanthaster planci larvae across 12 temperature treatments. n = 60 larvae for each temperature

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Fig. 6

Average (±SE) larval length and larval width in 72-h-old Acanthaster planci larvae across 12 temperature treatments. An asterisk indicates significant differences among temperature treatments. n = 60 larvae for each temperature

Table 2

PERMANOVA on morphological measurements of Acanthaster planci at 12 temperature treatments ranging from 19.4 to 36.5 °C

Source

df

SS

MS

Pseudo-F

p (perm)

Time

5

664.3

132.7

7.1

<0.001

Replicate(Time)

28

588.5

21

2.1

0.092

Residuals

404

3,961.5

9.8

  

Total

437

5,256.1

   
Table 3

ANOVA of the length and width of 72-h-old bipinnariae of Acanthaster planci from Green Island (Great Barrier Reef, Australia) among 12 temperature treatments

Dimension

SS

MS

F

p

Width

229,725

45,945

9.6

<0.001

Length

66,623

13,324.6

5.5

<0.001

The factor analysed is ‘Temperature treatment’. Numerator df = 5, denominator df = 60 for all the analyses

Sea surface temperature

Average sea surface temperature from November to December (Fig. 1), as derived from satellite data, ranged from ≈25 °C at Lord Howe Islands to ≈30 °C in the southern part of Papua New Guinea. Green Island, Northern Queensland (16°46.5′S, 145°59.3′E) is located where average sea surface temperature in November and December ≈29 °C.

Discussion

Response of Acanthaster planci development to temperature

In this study Acanthaster planci developed at temperatures >19.4 °C and <33.2 °C, with an optimal thermal window for development to the late-bipinnaria stage after 72 h between ≈25.6 and 31.6 °C. Johnson and Babcock (1994) proposed for Acanthaster planci, a thermal tolerance range of 18–31 °C during the gastrula and bipinnaria stages, and a much narrower window in brachiolaria and competent larvae of 27–31 °C. This later observation was based on earlier work by Lucas (1973) who further suggested that the distribution of the species would be limited to waters warmer than 27 °C.

A narrowing in the thermal window during development was also apparent in our experiments. We base this on the observations that at 5 h post-fertilisation, the optimal temperatures for early embryonic development were 25.6 and 31.6 °C (i.e. >50 % cleavage staged embryos, abnormality rate <50 %), but if development to gastrula, incorporating both the early and later-embryonic stages is considered, then the optimal temperature range is narrower. For example, at 16 h post-fertilisation, the greatest percentage (>50 %) of gastrula occurred between 28.7 and 31.6 °C, with minimum abnormality (<50 %) occurring between 25.6 and 31.6 °C. A similar optimal thermal window for early-bipinnaria stages was evident at 48 h, implying a constant thermal window through the gastrula and early-bipinnaria stages. Interestingly, at 72 h, there was a broadening of optimal thermal window to 25.6–31.6 °C for the presence of late-bipinnaria, which may indicate bipinnaria develop equally well across a wider temperature range. It could also reflect a general slowing of development during the bipinnaria stages allowing an accumulation of late-bipinnaria at 72 h.

Thermal windows in echinoderm larvae are most widely examined in echinoids and typically have a breadth of ≈6–7 °C (review by Byrne 2011; Pecorino et al. 2013). For asteroids, in addition to Acanthaster planci, the response of embryos and larvae to temperature has been quantified in two polar Odontaster species and a temperate species Asterias miniata (Hoegh-Guldberg and Pearse 1995; Stanwell-Smith and Peck 1998). In the present study, the thermal window is best described as a flat normal distribution of development rates, with an optimal temperature for development rate, normal development, and larval size in the 28.7 °C treatment. With decreasing temperatures, development rates slow, with no development occurring below ≈20 °C, following a pattern of slowing development rates with decreasing temperatures already reported in literature (Hoegh-Guldberg and Pearse 1995). This relationship between temperature and development (the slope of which appear to be the same within and among echinoderm species) has been interpreted as a lack of temperature compensation in echinoderm developmental processes (Hoegh-Guldberg and Pearse 1995). Hoegh-Guldberg and Pearse (1995) described an exponential reduction in hatching rates and development rate in A. planci and predicted a temperature at which develop would cease at 18.1 °C. In our experiments, development was negligible at 19.4 °C, while Johnson and Babcock (1994) noted cleavage was absent at 18 °C, suggesting that 18–19 °C represents the species lower thermal limit of the embryonic development.

At temperatures above the optimum, development rates in A. planci remained relatively constant, while rates of abnormality increased. The observation that embryonic and early-larval development rates were independent of temperature across an optimal range has been documented for echinoderm larvae (Stanwell-Smith and Peck 1998; Pecorino et al. 2013). In four sea star species, Hoegh-Guldberg and Pearse (1995) compared development rate and temperature using Arrhenius plots and noted a strong positive effect of temperature on the developmental rate up to a break point value, after which it exerts a small affect on development. In the case of A. planci, their calculated break point occurred at ≈25 °C, which is consistent with our observation that development to the late-bipinnaria stage at 72 h plateaued across temperatures between 25.6 and 31.6 °C. Similarly, our findings of no significant differences in total larval length and width between 24 and 30.2 °C would suggest development is similar across these temperatures. Johnson and Babcock (1994) also reported that A. planci larvae developed equally well at 31, 27 and 24 °C, but did not comment on the pace of development at cooler temperatures apart from noting normal larvae were produced.

Response of larvae to oxygen concentration

Dissolved oxygen concentration is a function of water temperature and therefore has the potential to confound our results. In the present experiments, 100 % O2 saturation would range from 7.48 mg L−1 at 19.4 °C to 5.64 mg L−1 at 36 °C, while the temperature at which we noted reduced survival (28.7 °C) would coincide with a calculated saturated oxygen concentration of 6.37 mg L−1 (Benson and Krause 1984). It is therefore possible that, in addition to the direct affects of temperature on larval development and survival, reduced larval fitness at warmer temperatures may also be a response to lower oxygen concentrations. Previous research has shown that larval development can be inhibited by hypoxia, although at concentrations distinctly lower than experienced in this study. For example, Crassostrea virginica larvae were inhibited at oxygen concentrations <0.07 mg L−1 for 24 h (Baker and Mann 1992), while oxygen concentrations of 0.6–1.3 mg L−1 over 60 h delayed Mytilus edulis embryonic and larval development (Wang and Widdows 1991). For the bivalve Mercenaria mercenaria, while survival was not affected, development stopped at <1.0 mg O2 L−1 (Morrison 1971). At similar oxygen concentrations (1 mg O2 L−1), polychaete larvae (Hydroides elegans) showed reduced feeding rates and delayed development (Shin et al. 2013). Eerkes-Medrano et al. (2013) examined the response of larvae to low oxygen concentrations in nine invertebrate species, noting sensitivity to hypoxic conditions varied among species and developmental stages. In all cases, however, there was no significance reduction in survival in treatments until oxygen concentrations were reduced below 1.8 mL O2 L−1.

Although not extensively studied in marine larvae, it has been suggested that reduced oxygen concentrations slow development through metabolic depression such as reduced ATP turnover (Hochachka 1997) and metabolic adjustment to survive hypoxic conditions (Wu 2002), while abnormal development has been attributed to disruption of histogenesis through altered apoptosis (Shang and Wu 2004).

Given that the oxygen levels in the present study were never lower than 5.64 mg O2 L−1 and remained >90 % saturation between water changes (Hardy et al. 2013), the effects of oxygen concentration may be less important than warming. Indeed, sea star larvae appear to have a high tolerance to hypoxia, with the bipinnaria and brachiolaria larvae of Pisaster ochraceus showing no decrease in survival, even after exposure to near-anoxia conditions (<0.5 mL O2 L−1) for up to 6 d (Eerkes-Medrano et al. 2013). For other marine invertebrate larvae, development was normal when oxygen concentrations remained greater than 3 mg O2 L−1 (which is lower than the minimum experienced in the present study). For example, Mercenaria mercenaria, eggs developed normally above 0.5 mg O2 mL−1, while larval growth was normal above 4.2 mg O2 L−1. For Hydroides elegans larvae, feeding and development was not significantly different between normal (6 mg O2 L−1) and reduced (3 mg O2 L−1) oxygen concentrations (Shin et al. 2013).

Thermal windows, temperature tolerances and Acanthaster planci distribution

Our observations give insight into the developmental responses of A. planci larvae to temperature, with development to the late-bipinnaria stages occurring in an optimal thermal window that spans ≈25–31 °C. Within this thermal window, development is largely independent of temperature. Our summary contrasts the Johnson and Babcock (1994) model of temperature tolerances in this species that spans from 19 to 31 °C for development to the late-bipinnaria stage. The distinction between thermal tolerance range (used by Johnson and Babcock 1994) and optimal thermal window (this study) is important; however, as the numbers of larvae reaching settlement is a function of both survival rate and development rate. As instantaneous mortality rates of echinoderm larvae in the plankton are high (i.e. M ≈ 0.1–0.2 d−1, Rumrill 1990; Lamare and Barker 1999) and generally associated with predation and not physiological stress, then in situ development rates is likely more important determinant of survival to settlement than temperature tolerance.

The distribution of A. planci around Australia occurs at locations where sea surface temperatures in November and December range from ≈25 to 31 °C (Fig. 1). For example, Benzie (1999) used data for A. planci from 23 localities, with the most southern occurring on Lord Howe Island (December SST ≈ 25 °C, Fig. 1) and the most northern in the Gulf of Carpentaria (December SST ≈ 30 °C, Fig. 1). The remaining populations are reported to occur within the GBR where SST in summer range from 26 to 30 °C (Fig. 1). The distribution of these populations occurs within the optimal thermal window for development to the late-bipinnarian stage that we propose and would be consistent with a suggestion that successful recruitment requires development within the optimal temperature range. Tolerance to cooler temperatures (i.e. 19 °C) documented by Johnson and Babcock (1994) does not appear to be a driver of distributions as there are no reports of A. planci populations in sea temperatures between 19 and 25 °C. Other factors, however, could influence the absence of A. planci from these cooler areas, such as the strict association of this sea star with coral, its only food source, and which are not found in these colder waters. The relationship between SST, larval thermal windows and adult distributions would not be unique to A. planci and occurs in other echinoderm species in the Australasia. For example, Centrostephanus rodgersii in eastern Australia has an optimal thermal window between ≈12 and 20 °C which has historically restricted the adult populations to waters where winter SST are warmer than 12 °C (Ling et al. 2009; Hardy et al. 2013; Pecorino et al. 2013). Furthermore, the same sea urchin species occurs in northern New Zealand where adults are restricted to waters where winter SST > 15 °C which is consistent with the well-defined minimum thermal window >16 °C for embryonic and plutei development.

While the distribution of A. planci overlaps with the optimal thermal window, we propose the patterns are not consistent with the Johnson and Babcock (1994) model of thermal tolerance that incorporates data from Lucas (1973) for later larval development (i.e. brachiolaria larvae) that restricts development to between 27 and 31 °C. The thermal window of late-staged larvae of A. planci may, in fact, be broader than that reported by Lucas (1973) if the apparent acclimation to temperature observed in this species is considered. For example, Johnson and Babcock (1994) found that larvae derived from individuals collected at two locations (Davies Reef and Gove Peninsula) varied in their response to temperature, with those from warmer locations appearing to have a warmer thermal window, thus supporting the hypothesis of scope for adaptation (see above). In addition, acclimation also appears to occur within populations as sea temperatures change seasonally. In this respect, Johnson and Babcock (1994) noted that larvae from animals collected earlier in the season were less tolerant of warmer temperatures compared with larvae derived from adults later in the season when sea temperatures were 1.5 °C higher. In the context of the thermal window of the later-staged brachiolaria larvae, those tested by Lucas (1973) were derived from individuals from the warmer part of the species range (GBR reefs around 146°51′E, 18°2′S, water temperatures ≈29 °C), and acclimation at these temperature may have meant they were less tolerant of cooler temperatures.

The questions of acclimation to temperature and the thermal window of the advanced larvae need to be quantified if the relationship between distributions and larval thermal tolerances is to be fully understood. Indeed, Johnson and Babcock (1994) commented that the thermal tolerances of later-staged larvae should be re-examined, especially for populations in the cooler regions of their distributions. Our experiments using heat blocks (where larvae were reared in small volumes, 30 mL) did not allow us to rear the larvae beyond the late-bipinnaria, although unpublished, experiments indicate that rapid development to metamorphosis (16 d) also occurred at 28 °C (Lucas 1973).

Responses of Acanthaster planci to ocean warming

Acanthaster planci population abundances undergo significant decadal-scale variation, and these outbreaks have been attributed to either natural fluctuations (Vine 1973), anthropogenic-related increasing in planktonic food supply that enhances larvae survival (Fabricius et al. 2010), or by the removal of juvenile predators (Bradbury and Seymour 1997). Some A. planci outbreaks have also been linked with El Niño events, as they both act as contemporary stressors on corals, causing higher mortality (Glynn 1990; Fong and Glynn 2001). Moreover, higher SST associated with El Niño events could favour A. planci larval survival at the cooler extreme of its distribution. It is interesting therefore to contemplate how increases in sea temperatures may affect A. planci abundances and future distributions.

Three observations from our experiments are relevant to this discussion. Firstly, A. planci larvae have a broad optimal thermal window (i.e. 25–31 °C), which encompasses the present day distribution of A. planci. Within this thermal window, there is no significant change in either development rates, larval survival or growth rates, and therefore, moderate increases in sea temperatures of 1–2 °C that occur during El Niño years, or longer-term warming under climate change (2–4 °C) may not directly enhance development rates in the plankton and hence survival to settlement. In fact, without any acclimation or adaptation to warmer temperatures, larval survival would decline if temperatures warm above 31 °C (the upper thermal limit). Presently, the entire GBR is at optimal temperature during spawning (Fig. 1), and such temperatures could be exceeded in the northern part including our source population, under near-future warming of +2 °C.

Secondly, if distributions of A. planci populations are, in part, related to the larval thermal window, then warming of sea temperatures in the southern range of the species would potentially extend its southern distribution around Australia. Coastal eastern Australia has experienced significant warming over the past half-century (Ridgway 2007) due to the well-documented increase in southerly flow by 350 km of the EAC (Ridgway 2007), and warm-water species ranges can expand as temperatures become favourable. Finally, it is possible that spawning seasons may shift to encompass optimal temperatures for larvae, as was observed in 5 populations along a latitudinal gradient in Japan (Yasuda et al. 2010).

Our experiments provide a more detailed (but not complete) insight into the response of A. planci developmental stages to temperature. We suggest that the present day distributions of the species in Australia broadly overlap with the optimal thermal window to late-bipinnarian development, which also coincides with the distribution of coral reefs. The broad thermal window would suggest that moderate (1–2 °C) increases in sea temperatures such as those during El Niño or near-future ocean warming would not drive an increase in the numbers of larvae surviving to settlement. Similarly, our findings also suggest that a potential poleward spread of coral reefs (Yamano et al. 2011) would also be accompanied by a spread of A. planci. Our observations would therefore support the hypothesis that in situ development and larval survival is principally controlled, not by temperature, but by other factors such as increases in food availability (Fabricius et al. 2010) or during El Niño events. To advance our conclusions, thermal windows for later-staged larvae and region differences in the thermal biology of larvae are required. In addition, other important changes in the region are underway, such as ocean acidification which can be detrimental to echinoderm larvae (Byrne 2011, Byrne et al. 2013a) including asteroid larvae (Gonzalez-Bernat et al. 2012; Byrne et al. 2013b) and several early life history stages in A. planci (Uthicke et al. 2013). The interaction of temperate and ocean pH needs to be considered in further experimental work.

Acknowledgments

We are very grateful to Steve Moon for organising Acanthaster planci collections. Funding was provided by the Australian Institute of Marine Science and the Australian Government’s National Environmental Research Program and an Australian Research Council Grant.

Supplementary material

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Supplementary material 1 (DOCX 43 kb)

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