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Long-term exposure to acidification disrupts reproduction in a marine invertebrate

  • Christian Pansch ,

    Roles Conceptualization, Data curation, Formal analysis, Funding acquisition, Investigation, Methodology, Project administration, Resources, Software, Supervision, Validation, Visualization, Writing – original draft, Writing – review & editing

    ch.pansch@gmail.com

    Current address: Department of Marine Ecology, GEOMAR Helmholtz Centre for Ocean Research Kiel, Kiel, Germany

    Affiliation Department of Marine Sciences – Tjärnö, University of Gothenburg, Tjärnö, Strömstad, Sweden

  • Giannina S. I. Hattich,

    Roles Data curation, Formal analysis, Methodology, Visualization, Writing – original draft, Writing – review & editing

    Current address: Department of Marine Ecology, GEOMAR Helmholtz Centre for Ocean Research Kiel, Kiel, Germany

    Affiliation Department of Marine Sciences – Tjärnö, University of Gothenburg, Tjärnö, Strömstad, Sweden

  • Mara E. Heinrichs,

    Roles Data curation, Formal analysis, Investigation, Writing – original draft

    Current address: Institute for Chemistry and Biology of the Marine Environment (ICBM), University of Oldenburg, Oldenburg, Germany

    Affiliation Department of Marine Sciences – Tjärnö, University of Gothenburg, Tjärnö, Strömstad, Sweden

  • Andreas Pansch,

    Roles Data curation, Formal analysis, Investigation, Methodology, Writing – original draft

    Affiliation Alfred-Wegener-Institut, Helmholtz-Zentrum für Polar- und Meeresforschung, Wattenmeerstation Sylt, List, Germany

  • Zuzanna Zagrodzka,

    Roles Data curation, Formal analysis, Investigation, Methodology, Writing – original draft

    Current address: Department of Animal and Plant Sciences, University of Sheffield, Sheffield, United Kingdom

    Affiliation Department of Marine Sciences – Tjärnö, University of Gothenburg, Tjärnö, Strömstad, Sweden

  • Jonathan N. Havenhand

    Roles Conceptualization, Formal analysis, Funding acquisition, Investigation, Methodology, Project administration, Resources, Software, Supervision, Validation, Visualization, Writing – original draft, Writing – review & editing

    Affiliation Department of Marine Sciences – Tjärnö, University of Gothenburg, Tjärnö, Strömstad, Sweden

Long-term exposure to acidification disrupts reproduction in a marine invertebrate

  • Christian Pansch, 
  • Giannina S. I. Hattich, 
  • Mara E. Heinrichs, 
  • Andreas Pansch, 
  • Zuzanna Zagrodzka, 
  • Jonathan N. Havenhand
PLOS
x

Abstract

Climate change research is advancing to more complex and more comprehensive studies that include long-term experiments, multiple life-history stages, multi-population, and multi-trait approaches. We used a population of the barnacle Balanus improvisus known to be sensitive to short-term acidification to determine its potential for long-term acclimation to acidification. We reared laboratory-bred individuals (as singles or pairs), and field-collected assemblages of barnacles, at pH 8.1 and 7.5 (≈ 400 and 1600 μatm pCO2 respectively) for up to 16 months. Acidification caused strong mortality and reduced growth rates. Acidification suppressed respiration rates and induced a higher feeding activity of barnacles after 6 months, but this suppression of respiration rate was absent after 15 months. Laboratory-bred barnacles developed mature gonads only when they were held in pairs, but nonetheless failed to produce fertilized embryos. Field-collected barnacles reared in the laboratory for 8 months at the same pH’s developed mature gonads, but only those in pH 8.1 produced viable embryos and larvae. Because survivors of long-term acidification were not capable of reproducing, this demonstrates that B. improvisus can only partially acclimate to long-term acidification. This represents a clear and significant bottleneck in the ontogeny of this barnacle population that may limit its potential to persist in a future ocean.

Introduction

Globally, rising atmospheric CO2 concentrations are causing acidification of the oceans [1]. The effects of ocean acidification as a single driver have been investigated in numerous manipulative and field experiments on (usually) single species [24]. These experiments have shown that ocean acidification can impair physiology [5, 6], survival, calcification, development and growth [3, 7] as well as behavioural processes [8] in a wide variety marine species.

Climate change research has now advanced towards more complex and comprehensive studies, testing multiple simultaneous drivers such as ocean warming, freshening, or eutrophication, in combination with ocean acidification in multiple species [3, 6, 911]. These studies have demonstrated synergistic, additive and antagonistic effects of multiple drivers [3, 12]. Despite these advances, recent reviews illustrate the limits of our current knowledge with respect to expected shifts from climate change impacts [1315]. Thus, an up-scaling from single species to ecosystems, and from short-term incubations to long-term acclimated and adapted species, is urgently needed [14]. Implicit in this concept are investigations of multiple life-history stages of species and comparisons among multiple populations [15].

Acclimation is a reversible short-term change in the performance of an individual within its phenotypic plasticity [16]. Particularly in the light of a strong variability in drivers, such as diurnal and seasonal fluctuations in pH [1719], acclimation represents an important process that allows organisms to cope with environmental variability [12]. Species with better regulatory capabilities—and the energy reserves to fuel them—should be more tolerant of acidification-induced stress [5, 2022]. Experimental studies that have investigated acclimatory capacity to acidification in e.g. sea urchins [2326] and corals [27], have found this capacity to be considerable, with much reduced effects of acidification after an acclimation period of several months. Similarly, an in situ transplant experiment in a CO2 vent system with pH-sensitive and pH-tolerant polychaete species demonstrated that acclimation (as well as adaptation) can be a viable strategy for the successful colonization of low-pH habitats [28]. Nevertheless, there are very few studies of long-term acclimation of marine species to acidification, and almost none on barnacles (but see [20, 29]).

Intertidal barnacles are ecologically and economically important and widely studied ecosystem engineers [30, 31]. Their larval stages can reach abundances of up to 20,000 individuals per m3 seawater [32] at which times they provide a substantial source of food for higher trophic levels. Several studies have investigated barnacle responses to acidification [29, 3339], finding inter alia that larval stages are less sensitive to reduced pH than juveniles and adults ([20, 29, 3740], but see [29]). Interestingly, acidification tolerance in barnacles from habitats with strong natural fluctuations in pH has been shown to be greater than that in barnacles from less variable habitats [20], and diurnal fluctuations in pH elicit strong phenotypic variance in susceptibility [41]. These findings suggest that acclimatory capacity in barnacles may be considerable.

With regard to reproduction, life-long exposure of barnacles to ocean acidification has been found to have no significant impact on egg production (Amphibalanus amphitrite; [29]), or larval output (Balanus improvisus population from the Western Baltic Sea, Kiel Germany; [20]), although one other study found slower embryonic development at lower pH (Semibalanus balanoides; [36]). More generally, the effects of ocean acidification on reproduction in barnacles have received little attention, which is surprising given that this vital life-cycle event influences all subsequent population dynamics, and barnacles are very widely studied.

Barnacles are cross-fertilising simultaneous hermaphrodites: by random penis movements, functional males search for functional females to deposit sperm into their mantle cavity [42]. After this pseudo-copulation, eggs are released into the mantle cavity, where fertilisation and development take place [4244]. After a period of development, free-swimming Stage-I nauplius larvae hatch, and are released into the water column, where they pass through six developmental stages before they metamorphose into the non-feeding cypris larva [45], which finds a suitable location in which to settle and metamorphose into a juvenile. The presence of fertilised eggs in reproductively isolated individuals has led some authors to suggest that self-fertilisation may be possible in some barnacle species [43, 46], although there is no direct evidence of this. Sperm-casting [47] has been reported in stalked barnacles (not in acorn barnacles) that typically inhabit surge channels on exposed rocky coasts [48, 49]. While it is possible that sperm-casting could also occur in acorn barnacles such as B. improvisus, habitat, wave-action, and lifestyle, all argue against this way of reproduction.

In the present study, we tested the long-term (≤ 16 months) potential for acclimation to ocean acidification in a population of the bay barnacle B. improvisus that previous work has shown to be sensitive to ocean acidification [20]. Specifically, we hypothesized that long-term acclimation will allow this particular population to better cope with ocean acidification stress. We used both field-collected, and laboratory-bred, barnacles to investigate survival, growth, respiration rate, activity, and condition index across this experimental period, but focussed on assessing whether the reproductive capacity might be a bottleneck for the species’ capacity to acclimate to future ocean acidification.

Materials and methods

Study species

Balanus improvisus [50, 51] can be found worldwide in oceanic and brackish waters and is by far the most common barnacle species in the Baltic Sea [52]. Natural recruitment takes place mainly during summer and early autumn [53] but can also be observed all-year round in some populations [37]. In laboratory culture, high reproductive rates can be seen year-round, with generation times of ~ 4 months, and this has been achieved routinely in our laboratory [39, 41, 53, 54].

Experimental treatments

All experiments were conducted at the Tjärnö Marine Research Station, Sweden between January 2013 and June 2014. In two experiments, laboratory-bred or field-collected and settled, juveniles of the barnacle B. improvisus were grown to maturity under two different pH regimes for 16 and 8 months, respectively (S1 Fig). All experiments were terminated in June 2014.

For all experiments, through-flowing deep-seawater (salinity of ~32) was pumped from the field into a conditioning tank in a constant temperature room at 20°C. The salinity in this tank was adjusted to a salinity of 25 (mean surface conditions in this region [55]) with the aid of tap water and an automatic salinity-control unit (LF Controller, Aqua Medic, Germany). This conditioned water was then pumped into the header tanks of three independent partially-recirculating seawater systems of approximately 350 l each, as described in [56]. The flow rate of conditioned water into each system was set to maintain a replacement rate of approximately once every second day (~ 8 l h-1). In each system, all recirculating water was filtered (90 μm mesh on the outlet of each experimental unit) and UV-sterilized (HW Wiegandt GmbH, Germany) to maintain water quality and kill any waterborne sperm, (respectively). In order to prevent location- or system-specific effects within the constant temperature room, experimental treatments were moved to a recently cleaned system within the room every second week, such that all treatments were rotated among the available partly-recirculating systems (3 systems in all, of which only 2 were in use at any one time). Each system held laboratory-bred and field-collected barnacles (see below) simultaneously. All experiments were run under a 12:12 hours light:dark cycle.

Two acidification levels were chosen to reflect natural ambient pCO2 in the coastal system from which the population was taken, and a future scenario [15, 18, 57, 58]: an ambient pCO2 of 400 μatm (equivalent to pH ≈ 8.1) and a future projected pCO2 of 1560 μatm (pH ≈ 7.5, thereby maintaining a Δ pH of 0.6 units; see S1 Table). Acidification was achieved by aeration of the experimental systems with either ambient air (‘ambient’, ~400 ppm pCO2) or air enriched with CO2 (‘acidified’) controlled by computerized pH controllers (NBS calibrated, resolution: 0.01 pH units; Aqua Medic, Germany).

Temperature, salinity and pHNBS were maintained (see above) but were additionally measured once per week in three random replicates using either a WTW 330i pH meter equipped with a SenTix81 pH electrode and a WTW Cond 340i equipped with a TetraCon (WTW, Germany) 325 salinity electrode, or with a YSI 30 multiprobe (YSI, Brannum Lane, USA). Seawater total pH (pHT) was determined within 10 minutes after sampling using a pH electrode calibrated with Tris/HCl seawater buffers [59]. The voltage recorded by the pH sensor in the sample was converted into pHT after Dickson et al. (2007) [59]. Total alkalinity (TA) was estimated from salinity using a long-term salinity:alkalinity relationship for this region (r = 0.94; [41]). Uncertainties arising from estimating alkalinity using this relationship were equivalent to ±0.01 pHT and ±0.08 ΩAr (data for 99% CI around mean salinity:alkalinity relationship; see [41] for more details). All other carbonate system parameters were calculated using the CO2Calc program [60] with dissociation constants (K1 and K2) according to Hansson (1973) [61] refitted by Dickson and Millero (1987) [62] and KHSO4 dissociation constant after Dickson (1990) [63].

The same procedure as described above was followed for weekly water samples from the field taken at 50 cm depth from July 2013 to July 2014, at the Tjärnö Marine Research Station pier (58°52'32.94"N, 11°8'42.90"E) as well as from a close-by floating pontoon (58°52'55.03"N, 11°8'1.64"E). The floating pontoon was the collection point for the newly settled "field-collected" barnacles, and (6 months earlier) for the broodstock used in the in-house breeding cultures to produce "laboratory-bred" barnacles.

Laboratory-bred single barnacles

Multiple batches of nauplius larvae of B. improvisus were collected from in-house breeding cultures in January 2013 (11th to 29th) and grown to the cypris stage following established laboratory protocols [54, 64, 65]. The in-house broodstock comprised several hundred field-collected barnacles, renewed once per year during summer season (June to August). Survival and performance of laboratory-cultured barnacles can strongly depend on the specific larval batch investigated [39, 41], and therefore we used a mix of individuals from multiple different batches to reduce random effects. Barnacle cyprids were settled onto transparent 2 x 4 cm PMMA (Poly-Methyl MethAcrylate; Plexiglas) settlement plates and grown on a mixed diet of microalgae (Chaetoceros calcitrans, Skeletonema marinoi, and Thalassiosira pseodonana; first two weeks) and Artemia salina (thereafter) until the start of the experiment at ad libitum concentrations. Initial barnacle density was standardized to 5 individuals (< 1 mm diameter) per settlement plate by gently removing surplus barnacles. One plate was placed into each of 96 1 l Kautex bottles and distributed evenly to one of the two different pH treatments (February 2nd 2013) yielding 48 replicates per treatment. A flow of 2 l per minute was supplied to each bottle from the partly-recirculating flow-through system. In each bottle, a 90 μm mesh upstream of the outflow retained Artemia nauplii as food. Before reproductive maturation (about three months of age, June 4th 2013), surplus barnacles were culled to reduce density to one barnacle per plate.

Laboratory-bred pairs

Barnacles settled and grown as outlined above (in control and acidified conditions), were permanently paired by gluing (Reef Construct, Aqua Medic, Germany) two PMMA panels together, such that the two barnacles were close enough to copulate. Eight replicate pairs per treatment (one pair per bottle) were placed into 1 l Kautex bottles (August 20th 2013) and maintained as described above.

Field-collected barnacle assemblages

Juvenile B. improvisus were collected on transparent 2 x 4 cm PMMA settlement plates from the subtidal zone during the peak settlement season in the Tjärnö archipelago (58°52.5’N, 11°08.1’E; the same location from which the broodstock adults were sourced). Plates were submerged vertically at 1.5 m depth for four weeks (July 19th to August 16th 2013). After retrieval from the field, barnacle density was standardized (as above) to five individuals per plate, and dispersion maximized by gently removing surplus barnacles. Barnacles were grown in the laboratory on mixed diatom and Artemia diets as outlined above. After ~3 months (November 22nd 2013), 9 plates, each holding 5 barnacles, were placed into each of ten 6 l aquaria, and exposed to one of the two different pH treatments described above (9 plates per aquarium = 45 individuals per replicate, 5 replicate aquaria per treatment). Aquaria received filtered seawater at a flow rate of 2 l per minute.

Survival and growth

Barnacle survival was monitored weekly in laboratory-bred single barnacles. Dead individuals were replaced by stock barnacles from the same batches of larvae in order to maintain the same number of individuals in each system (no data were collected from re-stocked barnacles). For field-collected barnacle assemblages, survival was assessed at the end of the experiment only. Barnacle growth was assessed from digital images (Olympus E-3 DSLR with Zuiko Digital ED 50 mm macro lens) of the back of each transparent settlement panel. This was done monthly (month 1 to 10) and bi-monthly (months 10 to 16) for laboratory-bred single barnacles, or at the end of the experiment (only) for field-collected barnacle assemblages. The maximum basal diameter of each barnacle was determined using image analysis software (ImageJ 1.43u). No survival and growth data were collected for the laboratory-bred pairs.

Weight and condition index

For determination of dry weight, ash weight, and condition index, barnacles were frozen at –20°C, and stored. For dry weight, barnacles were subsequently dried at 80°C for 48 hours and weighed to the nearest 0.0001 g. Samples were then burned at 500°C for 12 hours and the remaining ash weight determined. Ash-free dry weight, as a measure of organic material, was calculated as dry weight—ash weight and condition index as ash-free dry weight / ash weight [20, 38, 40, 56].

Respiration

Respiration rates were only assessed in laboratory-bred single barnacles in closed glass respirometers (100 ml DURAN bottles) at treatment pH conditions. In order to reduce microbial background respiration, bottles were sterilized with boiling water and filled with filtered (0.2 μm) seawater equilibrated to the respective treatment pH. One single barnacle specimen was added per bottle. Bottles were closed under water (in 0.2 μm-filtered seawater at treatment pH) in order to avoid air bubbles in the system. A magnetic stirrer was used to gently homogenise the water body within each bottle, which were kept at a constant temperature of 20°C. Oxygen concentration of the water was recorded using O2-sensitive dye spots glued onto the inner side of the bottles and an optic fibre connected to an Oxy-4-mini instrument (PRESENS, Regensburg, Germany). Two-point calibration was performed with air-saturated water for 100% saturation and 1% (w/v) Na2SO3 for the 0% calibration, according to the manufacturer’s instructions. Measurements lasted for four hours and avoided oxygen tensions below 80% air saturation. Following measurements, barnacles were removed from the respirometers, and the respirometers were closed again (under water in 0.2 μm-filtered seawater at treatment pH) to measure bacterial background respiration for a period of ~12 hours. Oxygen consumption was calculated as oxygen depletion from 30 minutes to four hours, minus the proportional bacterial respiration, per unit time. Respiration rates were measured in randomly chosen individuals of similar size after 6 months of incubation (7.8–10.7 mm; N = 5; ANOVA of size comparisons between ambient and acidified: F1 = 3.307, p = 0.106), and in the same individuals after 15 months of incubation (10.3–12.7 mm; N = 5; ANOVA of size comparisons between ambient and acidified: F1 = 0.235, p = 0.641). A log:log regression of size (mm) and AFDW (g) (r2 = 0.97; S2 Fig) was used to calculate respiration rates of each individual barnacle biomass (μmol O2 g AFDW-1 h-1). Data for the log:log correlation were collected over an entire experimental cycle in barnacles of the same species (2–4 mm length; [20]), and at the end of the present study in barnacles 8–17 mm (S2 Fig).

Barnacle activity

Barnacle cirral activity was determined in parallel to respiration rate measurements after 6 months in laboratory-bred single barnacles only. Digital photographs were taken through the glass walls of the respirometers (Canon EOS 500 D with EFS 18-55mm lens, Canon EOS 600 D with Sigma 70mm Macro lens). Images were taken every 30 s for the duration of the respiration rate measurements (~4 hours). In order to leave sufficient time for barnacles to acclimatize to the conditions in the glass bottles, images were evaluated from 30 minutes post-start for two hours. For each bottle, cirral activity of single barnacles was recorded by manual inspection of the images and categorized into “active” or “closed”. The data were transformed into percentages of the images during the two hours in which the barnacles were active.

Reproduction

Rates of larval release were determined in all experiments by placing filters (90 μm mesh) at the outflow of a newly cleaned experimental unit. Before the assay, barnacles were gently stressed by cleaning them with a smooth brush and by exposing them to air for two hours. No Artemia were fed during the assay period. Larvae were collected overnight every second day for eight days post-stress, and the numbers of larvae released were counted under a stereomicroscope. When necessary, larvae were diluted for counting. For laboratory-bred single barnacles, two individuals of the same pH treatment were placed in close proximity for one week to allow copulation prior to the larval collection assay. Following this, barnacles were separated and larval collection was performed as described above. Larval collection assays were run repeatedly (4 times) for single barnacles and once each for pairs and field-collected barnacle assemblages (S1 Fig).

To assess the reproductive maturity of barnacles, ovary development status was determined at the end of the experiments (in June 2014: after 16 months for laboratory-bred single barnacles and eight months for field-collected barnacles). Haphazardly selected (sensu [66]) barnacle specimens from each aquarium were anaesthetised with isotonic MgCl2 (73.2g MgCl2.6H2O per l freshwater) for one hour and then dissected. Ovaries were categorized into three distinct groups: (1) no, or small and early-stage, gonads; (2) mature well developed gonads but not fertilized; and (3) fertilized eggs (classification modified from [67], see also [56]). For laboratory-bred single barnacles, 7 individuals were sampled per treatment (N = 7), for laboratory-bred pairs 6 individuals (3 pairs; N = 3) were sampled per treatment, and for field-collected barnacles 45 individuals were sampled per treatment (9 individuals per replicate, N = 5). For the 9 barnacle individuals per replicate unit in the field-collected barnacles, data are expressed as the percentage of those barnacles that developed mature gonads (category 2) or that carried fertilized eggs (category 2 and 3).

Statistical analysis

Data were analysed using a fixed one-factorial design (pH) with 2 levels (ambient and acidified), or—for responses, which were measured more than once—using a repeated-measures design. Normality was assured by inspections of box-plots (no transformations were necessary). Percentage data were square-root arcsine transformed before statistical analyses. Respiration rates of laboratory-bred single barnacles as well as their growth rates over time were analysed using repeated measures ANOVA. For growth in laboratory-bred single barnacles, the data did not meet the assumption of sphericity (Mauchly’s test for sphericity), and therefore p-values were corrected using the Greenhouse-Geisser correction. All other data were analysed using one-way ANOVA. Post-hoc comparisons were done using Fisher's least significant difference (LSD) test. All statistics were generated using the software STATISTICA 8.0 (Stat-Soft, Inc., USA).

Results

Laboratory-bred single barnacles

Survival of laboratory-bred single individuals of B. improvisus was significantly reduced under acidified conditions. Only 50% (of an initial 48 individuals) survived to the end of the experiment (16 months) compared to 79% in ambient conditions (z-test, P = 0.0015). This resulted in mean mortality rates of 0.57 and 1.38 barnacles per month in ambient and acidified conditions, respectively. Mortality rates in the acidified treatment were highest throughout the first two months of the experiment (Fig 1A).

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Fig 1. Survival (A) and growth (B; size over time) of laboratory-bred single barnacles.

B. improvisus was incubated at two different pH treatments (Δ of 0.6 pH units) for 16 months. Deviations denote 95% CIs from the mean. Treatment differences following posthoc comparisons are indicated by *p < 0.05, **p < 0.01, ***p < 0.001 (survival: N = 48; final size: Nambient = 38, Nacidified = 23).

https://doi.org/10.1371/journal.pone.0192036.g001

Growth (shell diameter) over time was similar in the two treatments until about 6 months, after which growth rates in acidified conditions were slower. This resulted in significant differences in barnacle size between pH treatments after month 10 (interaction, pH * acclimation; F11 = 14.8, p < 0.001; S2 Table; Fig 1B).

Barnacles in acidified conditions had a lower final mean dry weight as well as lower condition index than barnacles in the ambient treatment (Fig 2A and 2B). However, both dry weight and condition index varied markedly among individuals within treatments after 16 months of incubation, and consequently the difference between treatments was not statistically significant (dry weight, F1 = 1.80, p = 0.188; condition index, F1 = 0.63, p = 0.433; S2 Table).

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Fig 2. Dry weight (A), condition index (B), cirral activity (C) and respiration rates (D) of laboratory-bred single barnacles.

B. improvisus was incubated at two different pH treatments (Δ of 0.6 pH units) for 16 months. Deviations denote 95% CIs from the mean. Treatment differences following posthoc comparisons are indicated by *p < 0.05, **p < 0.01, ***p < 0.00 (dry weight and condition index: Nambient = 20, Nacidified = 18; cirral activity and respiration rates: N = 5).

https://doi.org/10.1371/journal.pone.0192036.g002

Feeding activity of barnacles after 6 months in the treatments was greater in acidified conditions (F1 = 9.81, P = 0.014; S2 Table; Fig 2C).

Respiration rates after 6 months in the treatments were not significantly influenced by acidification, but tended to be lower in acidified conditions (reflected in a marginally significant interaction between pH and acclimation: F1 = 4.513, p = 0.066; S2 Table; Fig 2D). This trend was entirely absent after 15 months (Fig 2D).

Laboratory-bred single barnacles had neither mature gonads nor fertilised eggs (no positive case found in 14 specimens, 7 per pH treatment).

Laboratory-bred pairs

Laboratory-bred barnacles kept together in pairs grew mature gonads: 3 individuals (from 3 pairs) at ambient and 4 individuals (from 3 pairs) in acidified conditions had mature gonads. None of these barnacles, however, had fertilised eggs and none were observed to release larvae.

Field-collected barnacle assemblages

Survival of field-collected barnacle assemblages was significantly reduced under acidified conditions (F1 = 5.76, p = 0.043; S2 Table; Fig 3A), resulting in mean mortality rates of 0.72 ± 0.29 and 1.38 ± 0.58 per month in ambient and acidified conditions, respectively.

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Fig 3. Survival (A), size (B), dry weight (C) and condition index (D) of field-collected barnacle assemblages.

B. improvisus was incubated at two different pH treatments (Δ of 0.6 pH units) for 8 months. Deviations denote 95% CIs from the mean. Main ANOVA effects are indicated by *p < 0.05, **p < 0.01, ***p < 0.001 (N = 5).

https://doi.org/10.1371/journal.pone.0192036.g003

pH treatment also significantly affected the final size of barnacles: individuals in ambient conditions were 8% larger (basal length, mm) than those in acidified conditions (F1 = 15.49, p = 0.004; S2 Table; Fig 3B).

Barnacles held under acidified conditions had a significantly lower final dry weight than those at ambient pH (F1 = 23.52, p < 0.001; S2 Table; Fig 3C). The condition index of field-collected barnacle assemblages, however, was significantly greater in acidified conditions (F1 = 5.65, p = 0.045; Fig 3D).

Field-collected barnacle assemblages (≤ 5 individuals in close proximity), developed mature gonads regardless of pH (F1 = 0.14, p < 0.717; S2 Table; Fig 4A). 28% of individuals under ambient conditions were brooding fertilised eggs/embryos, whereas no fertilised eggs were found in barnacles from acidified conditions (Fig 4B). These findings were reflected in larval output: field-collected barnacle assemblages in ambient conditions released on average 720 larvae per week per individual, whereas no larvae were released by individuals in acidified conditions (Fig 4B).

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Fig 4. Reproductive maturity (A) and larval release rates (B) of field-collected barnacle assemblages.

B. improvisus was incubated at two different pH treatments (Δ of 0.6 pH units) for 8 months. Reproductive maturity was assessed after 8 months (A); the sum of larvae released per individual barnacle over one week was assessed after 7 months (B). Presented are proportions of barnacles, which developed either mature gonads or fertilized eggs. Deviations denote 95% CIs from the mean (N = 5).

https://doi.org/10.1371/journal.pone.0192036.g004

Discussion

Long-term (8–16 month) acidification led to an overall reduction in survival, size and dry weight of both laboratory-bred and field-settled barnacles (Figs 13). The effect of acidification on the condition index of barnacles depended on their reproductive status: acidification either reduced the condition index in (non-reproducing) laboratory-bred single barnacles (Fig 2B); or significantly increased the condition index in (reproductively active) field-collected barnacle assemblages (Fig 3D).

The strong acidification-induced mortality observed at the beginning of the experiments likely led to strong selection for pH-resistant phenotypes. About 50% of the isolated laboratory-bred single individuals in the acidified treatments died during the 16-month experiment (37.5% died within the first two months), whereas in ambient conditions only 21% died (0% within the first two months). Differences in response of laboratory-bred and field-settled barnacles to the acidification treatments could have resulted from environmental effects experienced prior to the beginning of the experiments, however, the most severe responses we observed were towards the end of the experiment, indicating that if there were carry-over effects from the parents, these were small and long-lived. Reduced survival rates of barnacles under acidification have been reported in Semibalanus balanoides [36] but not in Amphibalanus (Balanus) amphitrite [29] or previously for B. improvisus ([41], using the same laboratory culture as the present experiments). These findings contrast with observations from long-term incubation studies on other invertebrate species, which found no strong mortality effects of acidification in sea urchins [23, 24] or cold-water corals [27]. Local variation in environmental drivers creates locally different selection pressures, which can lead to local adaptation and the creation of different “ecotypes” within species [68]. This highlights the importance of understanding population-specific differences in the stress-tolerance of an organism [69, 70]. Pansch et al. (2014) showed that the sensitivity of B. improvisus to acidification is population-specific, and that these population-specific differences may be explained by periods of naturally low pH during early barnacle development [20]. Thus, reoccurring low pH might select for genotypes that are more tolerant to low pH (as seen in the Kiel Fjord habitat for barnacles [20] and mussels [18]).

Reduced growth (size) under acidification can arise through one—or several—processes that involve increased metabolic costs, such as osmoregulation and calcification, both of which are energetically costly [22, 71, 72]. Although 50% of laboratory-bred individuals survived the acidification treatment to the end of the experiment (16 months), their growth rates after month 10, and hence their final size and dry weight, were reduced in this treatment. Previous observations have found no strong impacts of acidification on shell growth of barnacles [20, 29, 36], however, those studies were only run for ≤ 5-months post-settlement albeit at higher levels of acidification than those used here. In this context, our observation that cirral activity—a proxy for feeding rate—was greater in acidified treatments is of interest: this implies that growth was lower in acidified treatments despite greater feeding activity, thus, suggesting that feeding demand may be greater. It is possible that barnacles in our acidified treatments suffered from reduced digestive efficiency [73], although we have no data supporting this. More likely, increased energetic demands for homeostasis led to these long-term effects of barnacle growth [6].

Acidification tended to suppress respiration rates in the early phase of our experiment (after 6 months). Metabolic depression is a widely observed, and controversially discussed, response of organisms to acidified conditions [6]. Acidification-induced acidosis can develop in both, the extra- and intracellular fluid compartments of marine invertebrates. Specifically, extracellular acid-base imbalance, if not compensated, can mediate metabolic depression, leading to a reduction in physiological performance and possibly reduced growth [74]. Suckling et al. (2015) found increased metabolic activity in sea urchins in low pH in the first month of incubation but this effect disappeared over the remaining incubation time (months 4–24; [24]). Similarly, we found that after 15 months metabolic depression in B. improvisus had disappeared (even slightly reversed), indicating that individuals may have acclimated to long-term exposure to acidification, possibly due to shifts in metabolic pathways [71]. Despite this apparent potential for metabolic (or at least, respiratory) acclimation, growth rates in the acidified treatment were low during the last months of the experiment.

As in other animals, maturing barnacles can be expected to divert resources from growth into reproduction [42, 44]. We found clear evidence that investment in gonad maturation depended strongly on the availability of a potential mating partner. Isolated individuals failed to develop mature gonads, whereas a subset of these same barnacles grown in the same conditions but with a mating partner for 6 months, did develop mature gonads. This is clear evidence that gonad development in B. improvisus is contingent on the proximity of a potential mate. Cessation of ovogenesis has also been shown in reproductively isolated bryozoans and ascidians [75]. Our finding that gonad maturation was not impaired by acidification corresponds to data for A. amphitrite [29]. Following these observations, we suggest that acidification is not likely to impose a strong bottleneck on sexual maturation of barnacles.

To our knowledge, these are the first published experimental data on the (lack of) sexual maturation of isolated barnacles. As noted earlier, observations by Barnes and Crisp (1956) [43] and Furman and Yule (1990) [46], suggested that isolated barnacles may be capable of self-fertilization. Barnes and Crisp (1956) [43] noted that isolated B. crenatus (isolated by a distance greater than the maximum extension of penis) seldom had fertilised eggs, however, as with all field observations it is difficult to know the prior history of individuals—particularly any absent past-neighbours. In our experiment, we found no evidence for self-fertilization, or indeed the capacity to do so: none of the 16-month old isolated barnacles dissected contained mature gonads (N = 14). Thus, we suggest it is unlikely that isolated B. improvisus would be capable of self-fertilising, although we accept that multiple experiments must be conducted in different populations of this species before stronger conclusions can be drawn.

Unlike gonad maturation, fertilisation and larval release were both entirely inhibited by acidification. This finding is in marked contrast to previous studies with the same species—but a different population from Kiel, Germany [20]. In the closely related species, S. balanoides, embryonic development was slower under acidified conditions [36], and it therefore seems possible that inter-population differences in responses to acidification may be at least as great—or even greater—than inter-specific differences. Other researchers have found no significant effect of acidification on egg production in other barnacles (e.g. Amphibalanus amphitrite; [29]).

From the present data, it remains unclear whether it was energetic provisioning to gonads, copulation, fertilisation, early embryonic development, or a combination of these that was negatively affected by acidification. In copepods and sea urchins, acidification has been reported to reduce fecundity and egg production [23, 76], whereas another study on copepods showed no changes in egg production rates in response to acidification, but a reduction in larval hatching success [77]. Other studies on sea urchins indicate that paternal success (sperm swimming) rather than maternal provisioning was the stronger factor influencing fertilisation [78]. With regard to fertilisation, little is known about the impacts of acidification in barnacles. Most investigations of the effects of ocean acidification on fertilisation are undertaken with broadcast spawning species [79]. Reduced sperm performance observed under acidified seawater conditions in several marine invertebrates might be a key driver for reduced fertilisation success [80, 81]. The effects of acidification on barnacle sperm are, however, completely unknown, not least because the extent to which conditions in the mantle cavity—into which barnacle sperm are released—differ from the conditions in the surrounding waters is not known. Clearly, multiple factors will influence this chain of events, and are likely to do so differently in different taxa responding to acidification. It seems likely, however, that in our study the reduced size and metabolic depression of adults held under acidified conditions led to reduced maternal provisioning, which could have impacted reproductive success.

Conclusions

Our results show the potential of a population of the barnacle B. improvisus to withstand, and partially acclimate to, long-term acidification. Most strikingly, barnacles under acidification did not reproduce successfully. It remains to be investigated whether egg development, copulation, fertilisation, or multiple processes, were influenced by acidification stress. Yet, it is clear from the present data that acidification represents a significant bottleneck to reproduction in this population of B. improvisus and, hence, will likely influence their potential to persist in a future ocean.

Supporting information

S1 Table. Measured means of salinity, temperature, and pHT (total scale) from weekly measurements throughout the experiments as well as at the institute jetty (pier) and the site of barnacle spat collection (raft).

Mean total alkalinity (TA) was estimated from observed mean salinity using a long-term salinity:alkalinity relationship for this location, r = 0.94, see [41]). pCO2 and saturation states of calcite and aragonite were estimated using CO2Calc with constants from with dissociation constants (K1 and K2) according to [61] refitted by [62] and KHSO4 dissociation constant after [63]. The pH between the treatments within the experimental systems showed a delta of 0.55 ± 0.06. Salinity, temperature and pHT were monitored from March 2013 to June 2014. Field measurements were conducted between July 2013 and July 2014. Measured data are presented as means and standard deviations, calculated data as means only.

https://doi.org/10.1371/journal.pone.0192036.s001

(DOCX)

S2 Table. Results from one-way ANOVA and repeated measures ANOVA from both experiments.

Significant effects are highlighted in bold, marginally significant underlined.

https://doi.org/10.1371/journal.pone.0192036.s002

(DOCX)

S1 Fig. Timeline of the conducted experiments with laboratory-bred single barnacles, laboratory-bred pairs and field-collected barnacle assemblages.

The * indicate times when activity and respiration were measured.

https://doi.org/10.1371/journal.pone.0192036.s003

(PDF)

S2 Fig. Correlations of size and body weight (AFDW) were transferred into log:log ratios.

Data explain 97% of the variation and are merged from Pansch et al. (2014) [20]; Pangaea dataset: doi:10.1111/gcb.12478) and from the present study.

https://doi.org/10.1371/journal.pone.0192036.s004

(PDF)

Acknowledgments

We would like to thank Martin Ogemark for excellent support in the laboratory, and Heike Link, Peter Thor and Sam Dupont for the loan of PRESENS equipment. We would also like to thank Anna-Lisa Wrange for her introduction to barnacle dissections and Shula Cowley for her support in this long-term study.

References

  1. 1. Doney SC, Fabry VJ, Feely RA, Kleypas JA. Ocean acidification: The other CO2 problem. Annual Review of Marine Science. 1. Palo Alto: Annual Reviews; 2009. p. 1:169–92. https://doi.org/10.1146/annurev.marine.010908.163834 pmid:21141034
  2. 2. Koch M, Bowes G, Ross C, Zhang XH. Climate change and ocean acidification effects on seagrasses and marine macroalgae. Global Change Biol. 2013;19(1):103–32.
  3. 3. Kroeker KJ, Kordas RL, Crim R, Hendriks IE, Ramajo L, Singh GS, et al. Impacts of ocean acidification on marine organisms: quantifying sensitivities and interaction with warming. Glob Chang Biol. 2013;19(6):1884–96. pmid:23505245
  4. 4. Hall-Spencer JM, Rodolfo-Metalpa R, Martin S, Ransome E, Fine M, Turner SM, et al. Volcanic carbon dioxide vents show ecosystem effects of ocean acidification. Nature. 2008;454(7200):96–9. pmid:18536730
  5. 5. Melzner F, Gutowska MA, Langenbuch M, Dupont S, Lucassen M, Thorndyke MC, et al. Physiological basis for high CO2 tolerance in marine ectothermic animals: pre-adaptation through lifestyle and ontogeny? Biogeosciences. 2009;6(10):2313–31.
  6. 6. Pörtner HO. Ecosystem effects of ocean acidification in times of ocean warming: a physiologist's view. Mar Ecol Prog Ser. 2008;373:203–17.
  7. 7. Kroeker KJ, Kordas RL, Crim RN, Singh GG. Meta-analysis reveals negative yet variable effects of ocean acidification on marine organisms. Ecol Lett. 2010;13(11):1419–34. pmid:20958904
  8. 8. Munday PL, Cheal AJ, Dixson DL, Rummer JL, Fabricius KE. Behavioural impairment in reef fishes caused by ocean acidification at CO2 seeps. Nat Clim Change,. 2014;4(6):487–92.
  9. 9. Harvey BP, Gwynn-Jones D, Moore PJ. Meta-analysis reveals complex marine biological responses to the interactive effects of ocean acidification and warming. Ecology and Evolution. 2013;3(4):1016–30. pmid:23610641
  10. 10. Alsterberg C, Eklof JS, Gamfeldt L, Havenhand J, Sundback K. Consumers Mediate the Effects of Experimental Ocean Acidification and Warming on Primary Producers. Phycologia. 2013;52(4):2-.
  11. 11. Werner FJ, Graiff A, Matthiessen B. Temperature effects on seaweed-sustaining top-down control vary with season. Oecologia. 2016;180(3):889–901. pmid:26566809
  12. 12. Gunderson AR, Armstrong EJ, Stillman JH. Multiple Stressors in a Changing World: The Need for an Improved Perspective on Physiological Responses to the Dynamic Marine Environment. Annu Rev Mar Sci. 2016; 8:1:357–378.
  13. 13. Andersson AJ, Kline DI, Edmunds PJ, Archer SD, Bednaršek N, Carpenter RC, et al. Understanding Ocean Acidification Impacts on Organismal to Ecological Scales. Oceanography. 2015; 28(2):16–27.
  14. 14. Riebesell U, Gattuso J-P. Lessons learned from ocean acidi cation research. Nat Clim Change,. 2015; 5:12–14.
  15. 15. Wahl M, Saderne V, Sawall Y. How good are we at assessing the impact of ocean acidification in coastal systems? Limitations, omissions and strengths of commonly used experimental approaches with special emphasis on the neglected role of fluctuations. Mar Freshw Res. 2015;67(1):25–36.
  16. 16. Boyd PW, Hutchins DA. Understanding the responses of ocean biota to a complex matrix of cumulative anthropogenic change. Mar Ecol Prog Ser. 2012;470:125–35.
  17. 17. Hofmann GE, Smith JE, Johnson KS, Send U, Levin LA, Micheli F, et al. High-frequency dynamics of ocean ph: a multi-ecosystem comparison. PLoS One. 2011;6(12):e28983. pmid:22205986
  18. 18. Thomsen J, Casties I, Pansch C, Kortzinger A, Melzner F. Food availability outweighs ocean acidification effects in juvenile Mytilus edulis: laboratory and field experiments. Global Change Biol. 2013;19(4):1017–27.
  19. 19. Saderne V, Fietzek P, Herman PMJ. Extreme Variations of pCO(2) and pH in a Macrophyte Meadow of the Baltic Sea in Summer: Evidence of the Effect of Photosynthesis and Local Upwelling. PLoS One. 2013;8(4): e62689. pmid:23626849
  20. 20. Pansch C, Schaub I, Havenhand J, Wahl M. Habitat traits and food availability determine the response of marine invertebrates to ocean acidification. Global Change Biol. 2014;20(3):765–77.
  21. 21. Pörtner HO, Langenbuch M, Reipschläger A. Biological impact of elevated ocean CO2 concentrations: Lessons from animal physiology and earth history. J Oceanogr. 2004;60(4):705–18.
  22. 22. Whiteley NM. Physiological and ecological responses of crustaceans to ocean acidification. Mar Ecol Prog Ser. 2011;430:257–71.
  23. 23. Dupont S, Dorey N, Stumpp M, Melzner F, Thorndyke M. Long-term and trans-life-cycle effects of exposure to ocean acidification in the green sea urchin Strongylocentrotus droebachiensis. Mar Biol. 2012:1–9.
  24. 24. Suckling CC, Clark MS, Richard J, Morley SA, Thorne MAS, Harper EM, et al. Adult acclimation to combined temperature and pH stressors significantly enhances reproductive outcomes compared to short-term exposures. J Anim Ecol. 2015;84(3):773–84. pmid:25491898
  25. 25. Morley SA, Suckling CC, Clark MS, Cross EL, Peck LS. Long-term effects of altered pH and temperature on the feeding energetics of the Antarctic sea urchin, Sterechinus neumayeri. Biodiversity. 2016;17(1–2):34–45
  26. 26. Carey N, Harianto J, Byrne M. Sea urchins in a high-CO2 world: partitioned effects of body size, ocean warming and acidification on metabolic rate. J Exp Biol. 2016;219(8):1178–86.
  27. 27. Form AU, Riebesell U. Acclimation to ocean acidification during long-term CO2 exposure in the cold-water coral Lophelia pertusa. Global Change Biol. 2012;18(3):843–53.
  28. 28. Calosi P, Rastrick SPS, Lombardi C, de Guzman H, Davidson L, Jahnke M, et al. Adaptation and acclimatization to ocean acidification in marine ectotherms: an in situ transplant experiment with polychaetes at a shallow CO2 vent system. Philosophical Transactions Of The Royal Society B-Biological Sciences. 2013;368(1627):20120444.
  29. 29. McDonald MR, McClintock JB, Amsler CD, Rittschof D, Angus RA, Orihuela B, et al. Effects of ocean acidification over the life history of the barnacle Amphibalanus amphitrite. Mar Ecol Prog Ser. 2009;385:179–87.
  30. 30. Gosselin LA, Qian PY. Juvenile mortality in benthic marine invertebrates. Mar Ecol Prog Ser. 1997;146(1–3):265–82.
  31. 31. Gaonkar CA, Anil AC. What do barnacle larvae feed on? Implications in biofouling ecology. J Mar Biol Assoc UK. 2010;90(6):1241–7.
  32. 32. Niehoff B, Schmithusen T, Knuppel N, Daase M, Czerny J, Boxhammer T. Mesozooplankton community development at elevated CO2 concentrations: results from a mesocosm experiment in an Arctic fjord. Biogeosciences. 2013;10(3):1391–406.
  33. 33. Findlay HS, Burrows MT, Kendall MA, Spicer JI, Widdicombe S. Can ocean acidification affect population dynamics of the barnacle Semibalanus balanoides at its southern range edge? Ecology. 2010c;91(10):2931–40.
  34. 34. Findlay HS, Kendall MA, Spicer JI, Widdicombe S. Post-larval development of two intertidal barnacles at elevated CO2 and temperature. Mar Biol. 2010a;157(4):725–35.
  35. 35. Findlay HS, Kendall MA, Spicer JI, Widdicombe S. Relative influences of ocean acidification and temperature on intertidal barnacle post-larvae at the northern edge of their geographic distribution. Estuar Coast Shelf Sci. 2010b;86(4):675–82.
  36. 36. Findlay HS, Kendall MA, Spicer JI, Widdicombe S. Future high CO2 in the intertidal may compromise adult barnacle Semibalanus balanoides survival and embryonic development rate. Mar Ecol Prog Ser. 2009;389:193–202.
  37. 37. Pansch C, Nasrolahi A, Appelhans YS, Wahl M. Impacts of ocean warming and acidification on the larval development of the barnacle Amphibalanus improvisus. J Exp Mar Biol Ecol. 2012;420-421(0):48–55.
  38. 38. Pansch C, Nasrolahi A, Appelhans YS, Wahl M. Tolerance of juvenile barnacles (Amphibalanus improvisus) to warming and elevated pCO2. Mar Biol. 2012; 160(8):2023–2035.
  39. 39. Pansch C, Schlegel P, Havenhand J. Larval development of the barnacle Amphibalanus improvisus responds variably but robustly to near-future ocean acidification. ICES J Mar Sci. 2013;70(4):805–11.
  40. 40. Nasrolahi A, Pansch C, Lenz M, Wahl M. Temperature and salinity interactively impact early juvenile development: a bottleneck in barnacle ontogeny. Mar Biol. 2013;160(5):1109–17.
  41. 41. Eriander L, Wrange AL, Havenhand JN. Simulated diurnal pH fluctuations radically increase variance in-but not the mean of-growth in the barnacle Balanus improvisus. ICES J Mar Sci. 2015;73(3):596–603.
  42. 42. Anderson DT. Barnacles: Structure, Function, Development and Evolution. Chapman & Hall, London, UK. 1994.
  43. 43. Barnes H, Crisp DJ. Evidence of self-fertilization in certain species of barnacles. J mar biol Ass UK. 1956;35(03):631–639.
  44. 44. Barnes H, Barnes M. Studies on Reproduction of Cirripedes. 2. Setting of lamellae—action of protease and disintegration of oviducal sac. J Exp Mar Biol Ecol. 1977;27(3):219–31.
  45. 45. Jones LWG, Crisp DJ. The larval stages of the barnacle Balanus improvisus Darwin. Proc Zool Soc Lond. 1954;123(4):765–80.
  46. 46. Furman ER, Yule AB. Self-fertilization in Balanus improvisus Darwin. J Exp Mar Biol Ecol. 1990;144(2–3):235–9.
  47. 47. Bishop JDD, Pemberton AJ. The third way: spermcast mating in sessile marine invertebrates. Integr Comp Biol. 2006;46(4):398–406. pmid:21672752
  48. 48. Barazandeh M, Davis CS, Neufeld CJ, Coltman DW, Palmer AR. Something Darwin didn't know about barnacles: spermcast mating in a common stalked species. Proc R Soc Lond, Ser B: Biol Sci. 2013;280(1754).
  49. 49. Kelly MW, Grosberg RK, Sanford E. Love the one you're with: proximity determines paternity success in the barnacle Tetraclita rubescens. Mol Ecol. 2012;21(20):5088–97. pmid:22967221
  50. 50. Darwin C. A Monograph on the Subclass Cirripedia, with Figures of All the Species. Royal Society, London, 684 pp. 1854.
  51. 51. Perez-Losada M, Hoeg JT, Simon-Blecher N, Achituv Y, Jones D, Crandall KA. Molecular phylogeny, systematics and morphological evolution of the acorn barnacles (Thoracica: Sessilia: Balanomorpha). Mol Phylogen Evol. 2014;81:147–58.
  52. 52. Leppäkoski E, Olenin S. Non-native Species and Rates of Spread: Lessons from the brackish Baltic Sea. Biol Invasions. 2000;2(2):151–63.
  53. 53. Berntsson KM, Jonsson PR. Temporal and spatial patterns in recruitment and succession of a temperate marine fouling assemblage: A comparison of static panels and boat hulls during the boating season. Biofouling. 2003;19(3):187–95. pmid:14619287
  54. 54. Pansch C, Jonsson PR, Berglin M, Pinori E, Wrange A-L. A new flow-through bioassay for testing low-emission antifouling coatings. Biofouling. 2017;33(7): 613–623.
  55. 55. Nasrolahi A, Havenhand J, Wrange A-L, Pansch C. Population and life-stage specific sensitivities to temperature and salinity stress in barnacles. Sci Rep-Uk. 2016;6:32263.
  56. 56. Wrange AL, Andre C, Lundh T, Lind U, Blomberg A, Jonsson PJ, et al. Importance of plasticity and local adaptation for coping with changing salinity in coastal areas: a test case with barnacles in the Baltic Sea. BMC Evol Biol. 2014; 14:156. pmid:25038588
  57. 57. Melzner F, Thomsen J, Koeve W, Oschlies A, Gutowska MA, Bange HW, et al. Future ocean acidification will be amplified by hypoxia in coastal habitats. Mar Biol. 2013;160(8):1875–88.
  58. 58. Waldbusser GG, Salisbury JE. Ocean acidification in the coastal zone from an organism's perspective: multiple system parameters, frequency domains, and habitats. Annual Review of Marine Science. 2014;6(1):221–47.
  59. 59. Dickson AG, Sabine CL, Christian JR. Guide to best practices for ocean CO2 measurements. PICES Special Publication 3, IOCCP Report No. 8. 2007.
  60. 60. Robbins LL, Hansen ME, Kleypas JA, Meylan SC. CO2Calc: A user-friendly seawater carbon calculator for Windows, Mac OS X, and iOS (iPhone). Report 2010–1280, Reston, VA. 2010.
  61. 61. Hansson I. A new set of acidity constants for carbonic acid and boric acid in sea water. Deep Sea Research and Oceanographic Abstracts. 1973;20(5):461–78.
  62. 62. Dickson AG, Millero FJ. A comparison of the equilibrium-constants for the dissociation of carbonic-acid in seawater media. Deep-Sea Research Part a-Oceanographic Research Papers. 1987;34(10):1733–43.
  63. 63. Dickson AG. Standard potential of the reaction -AgCls+1/2H-2g = Ags+HClaq and the standard acidity constant of the ion HSO4- in synthetic sea-water from 273.15-K to 318.15-K. J Chem Thermodyn. 1990;22(2):113–27.
  64. 64. Thiyagarajan V. A review on the role of chemical cues in habitat selection by barnacles: New insights from larval proteomics. J Exp Mar Biol Ecol. 2010;392(1–2):22–36.
  65. 65. Berntsson KM, Jonsson PR, Lejhall M, Gatenholm P. Analysis of behavioural rejection of micro-textured surfaces and implications for recruitment by the barnacle Balanus improvisus. J Exp Mar Biol Ecol. 2000;251(1):59–83. pmid:10958901
  66. 66. Quinn GP, Keough MJ. Experimental Design and Data Analysis for Biologists. 2002.
  67. 67. Crisp DJ. Factors influencing the time of breeding of Balanus balanoides. Oikos. 1959;10:275–289.
  68. 68. Sunday JM, Calosi P, Dupont S, Munday PL, Stillman JH, Reusch TBH. Evolution in an acidifying ocean. Trends Ecol Evol. 2014;29(2):117–25. pmid:24355315
  69. 69. Oney B, Reineking B, O'Neill G, Kreyling J. Intraspecific variation buffers projected climate change impacts on Pinus contorta. Ecology and Evolution. 2013;3(2):437–49. pmid:23467191
  70. 70. Valladares F, Matesanz S, Guilhaumon F, Araujo MB, Balaguer L, Benito-Garzon M, et al. The effects of phenotypic plasticity and local adaptation on forecasts of species range shifts under climate change. Ecol Lett. 2014;17(11):1351–64. pmid:25205436
  71. 71. Lannig G, Eilers S, Portner HO, Sokolova IM, Bock C. Impact of ocean acidification on energy metabolism of oyster, Crassostrea gigas—changes in metabolic pathways and thermal response. Mar Drugs. 2010;8(8):2318–39. pmid:20948910
  72. 72. Zittier ZMC, Bock C, Lannig G, Portner HO. Impact of ocean acidification on thermal tolerance and acid-base regulation of Mytilus edulis (L.) from the North Sea. J Exp Mar Biol Ecol. 2015;473:16–25.
  73. 73. Stumpp M, Hu M, Casties I, Saborowski R, Bleich M, Melzner F, et al. Digestion in sea urchin larvae impaired under ocean acidification. Nat Clim Change,. 2013;3(12):1044–9.
  74. 74. Michaelidis B, Ouzounis C, Paleras A, Pörtner HO. Effects of long-term moderate hypercapnia on acid-base balance and growth rate in marine mussels Mytilus galloprovincialis. Mar Ecol Prog Ser. 2005;293:109–18.
  75. 75. Bishop JDD, Manriquez PH, Hughes RN. Water-borne sperm trigger vitellogenic egg growth in two sessile marine invertebrates. Proc R Soc Lond, Ser B: Biol Sci. 2000;267(1449):1165–9.
  76. 76. Kurihara H, Shimode S, Shirayama Y. Effects of raised CO2 concentration on the egg production rate and early development of two marine copepods (Acartia steueri and Acartia erythraea). Mar Pollut Bull. 2004;49(9–10):721–7. pmid:15530515
  77. 77. Mayor DJ, Matthews C, Cook K, Zuur AF, Hay S. CO2-induced acidification affects hatching success in Calanus finmarchicus. Mar Ecol Prog Ser. 2007;350:91–7.
  78. 78. Foo SA, Dworjanyn SA, Poore AGB, Byrne M. Adaptive capacity of the habitat modifying sea urchin Centrostephanus rodgersii to ocean warming and ocean acidification: performance of early embryos. PLoS One. 2012;7(8).
  79. 79. Byrne M, Ho M, Selvakumaraswamy P, Nguyen HD, Dworjanyn SA, Davis AR. Temperature, but not pH, compromises sea urchin fertilization and early development under near-future climate change scenarios. Proc R Soc Lond, Ser B: Biol Sci. 2009;276(1663):1883–8.
  80. 80. Nakamura M, Morita M. Sperm motility of the scleractinian coral Acropora digitifera under preindustrial, current, and predicted ocean acidification regimes. Aquat Biol. 2012;15(3):299–302.
  81. 81. Schlegel P, Binet MT, Havenhand JN, Doyle CJ, Williamson JE. Ocean acidification impacts on sperm mitochondrial membrane potential bring sperm swimming behaviour near its tipping point. J Exp Biol. 2015;218(7):1084–90.