On October 10 2011 an underwater eruption gave rise to a novel shallow submarine volcano south of the island of El Hierro, Canary Islands, Spain. During the eruption large quantities of mantle-derived gases, solutes and heat were released into the surrounding waters. In order to monitor the impact of the eruption on the marine ecosystem, periodic multidisciplinary cruises were carried out. Here, we present an initial report of the extreme physical-chemical perturbations caused by this event, comprising thermal changes, water acidification, deoxygenation and metal-enrichment, which resulted in significant alterations to the activity and composition of local plankton communities. Our findings highlight the potential role of this eruptive process as a natural ecosystem-scale experiment for the study of extreme effects of global change stressors on marine environments.
Active submarine volcanoes constitute a significant source of mantle-derived gases, solutes and heat to the ocean. Their emissions react with seawater leading to important physical-chemical anomalies that may strongly impact the marine ecosystem1,2. However, the impacts of short-term submarine volcanic activity on the surrounding biota, especially planktonic communities, are still poorly understood. Here, we provide evidence that one of the richest and most sensitive marine ecosystems of the subtropical northeast Atlantic Ocean has been dramatically affected by the recent submarine eruption at the island of El Hierro (Canary Islands).
After three months of volcanic unrest, characterized by more than 10,000 earthquakes (M≤4.3) and 5 cm of ground deformation, on October 10 2011 the national seismic network recorded a substantial decrease of seismicity together with continuous volcanic tremor, indicating the beginning of an eruptive phase. Since then, regular multidisciplinary monitoring has been carried out in order to quantify environmental impacts caused by the submarine eruption (Figure 1).
Periodic bathymetric measurements located the main vent 1.8 km offshore of the southern coast of El Hierro and indicated a major uplift of the volcano, raising it from 300 m depth to just 88 m below the surface. Conductivity-Temperature-Depth measurements of the waters affected by the volcanic emissions revealed temperature and salinity anomalies of +3°C and −0.3, respectively, at 80 m depth and 290 m from the volcano. Maximum temperature anomalies of +18.8°C were observed over the crater at 210 m depth using expendable bathythermograph probes (Figure 2). The release of CO2 produced total inorganic carbon concentrations ranging from 4,000 to 7,500 µmol kg−1 causing water acidification of up to 2.8 units within the first 100 m depth and 2 km from the volcano. These high CO2levels generated high pCO2 (partial pressure of CO2) waters with values ranging from 12,000 to 150,000 µatm at the surface. The most affected part of the water column was the layer from 75 to 125 m depth which experienced oxygen depletion near to anoxic levels, enhanced light attenuation (transmittance decrease), negative redox potential, pH decrease, maximum concentrations of reduced sulfur and total Fe(II) species (200 and 50 µmol kg−1, respectively) and higher concentrations of dissolved Cu, Cd, Pb and Al with maximum values of 6.1, 6.7, 5.8 and 2,122 nM, respectively.
These physical-chemical anomalies had a major impact on local pelagic communities. No fish schools were acoustically detected within the volcano affected area and many dead fish were observed floating at the surface. Due to low light penetration, the upper limit of the deep scattering layer (produced by plankton and nekton echoes) was around 100 m shallower than usual in waters affected by the volcano. There, diel vertical migration was rather weak or absent as a consequence of anoxic levels in shallow layers (Figure 3). Small picoplankton communities showed a variable response to the volcanic emissions. Picophytoplankton at surface layers were not affected. However, at 75 m depth, Prochlorococcus showed a three-fold and Synechococcus a two-fold significant decline of abundance (t-test, p<0.06 and p = 0.1, respectively), compared to far-field stations. Conversely, heterotrophic bacterial abundances (particularly large cells with high green fluorescence) increased dramatically with depth at stations affected by the volcanic emissions. The distinct response of the picophytoplankton groups to the volcano's influence is suggestive of ecotype selection under the rapidly changing conditions. Indeed, preliminary phylogenetic analyses of 16S rDNA from surface waters revealed Prochlorococcus ecotypes characterized by lower chlorophyll b/a ratios and higher cupric ion tolerance (High Light-adapted3, HLI and HLII) (Figure 4). The lack of HLI ecotypes in waters affected by the volcanic emissions may indicate a volcano-induced selection towards higher growth-temperature optima, an attribute associated with the HLII ecotypes.
Five months after the beginning of the eruptive process, monitoring of the physical-chemical properties around the volcano continues to show significant variations within the different fields being measured (Figure 5). Surface temperature and salinity above the crater show small but notable differences of +0.02°C and −0.018, respectively. Although CO2 values have decreased considerably since the eruption, they continue to be highly variable. pCO2 ranges between 16,000 and 19,000 µatm (compared with 150,000 µatm at the time of the eruption) and surface pH values show a decrease of 1.8 points below normal levels to 6.2.
During the eruption of a submarine volcano at the island of El Hierro, volcanic emissions resulted in major physical-chemical alteration of the surrounding waters, such as warming, acidification and deoxygenation. These three processes are also the main stressors of global climate change, driven primarily by elevated anthropogenic release of carbon dioxide into the atmosphere4. Global climate models predict for the next century a rise of 0.6°C in ocean surface temperature5, a decrease of 0.3 – 0.4 pH units in surface waters6 and a decline of 1 – 7% in the global ocean oxygen inventory7. Marine organisms have already responded to these changes through variations in their distribution and survival8, decreased calcification rates6 and alteration of diurnal and ontogenetic vertical migrations of pelagic communities9,10. These effects directly impact the structure and functioning of marine ecosystem.
The volcano affected area has exhibited responses that are occurring globally, making El Hierro into a unique natural laboratory where the principal climate change stressors are acting simultaneously. The results emerging from this volcanic eruption will help to improve our understanding of how future climate change may impact marine biota.
Vertical profiles of conductivity, temperature, pressure, oxygen and transmittance were collected using a SeaBird 9/11-plus CTD equipped with dual conductivity and temperature sensors. CTD sensors were calibrated at the SeaBird laboratory before the cruise. Water samples were obtained using a rosette of 24 10-liter Niskin bottles.
Vessel-mounted Simrad EK60 (38 and 70 kHz) split-beam echosounders were used to collect acoustic data. During the acoustic tracks, average navigation speed, temporal resolution (ping rate) and pulse length were 3 kn, 1 s−1 and 1.024 ms, respectively, for both frequencies. Acoustic raw data were post-processed with LSSS software.
pH was measured on the total scale at a constant temperature of 25°C (pHT,25) using two different techniques. The UV-Vis spectrophotometric technique11 that used the m-cresol purple as an indicator12 removes the dye effect for each pH reading. The standard deviation for the measurements was ± 0.002. The potentiometric technique was used in the stations that were more affected by the submarine volcanic emissions. A ROSSTM combined glass pH electrode was used. The electrode was calibrated using a Tris/HCl buffer in synthetic seawater13. The standard deviation for the potentiometric pH measurements was ± 0.005.
Total dissolved inorganic carbon and total alkalinity
The VINDTA 3C (Marianda, Germany) was used for the determination of both total dissolved inorganic carbon and total alkalinity. The VINDTA 3C was connected to a coulometer to determine the total dissolved inorganic carbon14. Total alkalinity was determined15 on the VINDTA 3C using differential potentiometry. The certified reference material for oceanic CO2, CRMs batch #105, was used to test the performance of both total inorganic carbon and total alkalinity, resulting in a precision of ±1.0 µmol kg−1 for both parameters.
The concentration of Fe(II) was determined by UV-Vis spectrophotometry using a 5-m-long waveguide capillary flow cell (LWCFC) from World Precision Instruments. A modified version of the Ferrozine method was used18,19. The standard deviation of the method was ± 1 nM of Fe(II). Samples were diluted when necessary in order to achieve a nanomolar range of concentrations.
Reduced S species
The term reduced S species is defined as the sum of both hydrogen sulfide dissolved in water (H2S) together with the products of its dissociation (HS−, S2−) and the reduced compounds of sulfur (colloid sulfur, S0), sulfites (SO32−), polysulfides (Sx2−) and polythionates (S2O32−, S4O62−). These species were determined by the iodometric method20,21 using an automatic potentiometry titrator equipped with a platinum electrode (Metrohm). The method presented a standard deviation of ± 1 µM kgsw−1.
Samples from the Niskin bottles were stored in 250 ml Nalgene bottles and immediately frozen (−20°C) until analysis at a land-based laboratory. To prevent contamination, all containers were previously cleaned using 3 M HNO3 (1 week) and 0.1 M HCl (1 week) and rinsed thoroughly with ultra high purity water after each step. Samples were cleaned-filtered through 0.2 μm acid washed Nucleopore filter in a Class-100 laminar flow clean bench. Analysis of trace metal concentrations was carried out by High Speed Scan Cathodic Stripping Voltammetry (HSACSV) using a polarographic system22 and a mercury drop electrode (EG&G, 303A) with a Ag-AgCl reference and platinum counter electrode. The standard addition method was used for quantifying trace metals in the samples. The procedure for the determination of dissolved aluminium23 in seawater is based on the complexation of Al by 1,2-dihydroxyanthroquinone-3-sulphonic acid (DASA). Samples were prepared in Teflon cups of polarographic cells, containing 10 ml of water, 2·10−6 M DASA and 0.01 M BES (7.1 pH). The DASA-Al peak appears at ca. −1.25 V. Oxygen was removed by purging the solution with nitrogen for 5 minutes. Metal analysis was performed in a diluted solution to avoid drop saturation. The voltammetric procedure for Cu, Pb and Cd was carried out in unpurged seawater using a background scan correction. pH was adjusted to 7.6 by addition of 100 μl of 1 M HEPES and 20 μl of 4 10−3 M oxine (8-quinolinol). Copper, lead and cadmium peaks appear at −0.52 V, −0.62 V and −0.87 V, respectively.
Flow Cytometric analysis
Heterotrophic bacteria (HB), small photosynthetic eukaryotic cells (picoeukaryotes, PE) and Prochlorococcus (Pro) and Synechococcus (Syn) type cyanobacteria were counted by flow cytometry using a FACScalibur. To count HB, samples (4 ml) were fixed with 2% final concentration of paraformaldehyde, incubated for 15–30 min at 4°C and then stored frozen in liquid nitrogen until analyzed. Then, 200 µl were stained with a DMSO-diluted SYTO-13 (Molecular Probes Inc.) stock (10:1) at 2.5 µM final concentration. The identification of small phytoplankton groups (Pro, Syn and PE) was based on interactive analysis of multiple bivariate scatter plots of side scatter, red and orange fluorescence without staining. Samples were run at low speed for HB and at medium or high speed for phytoplankton until at least 10,000 events were acquired. A suspension of yellow–green 1 µm latex beads (∼105 beads ml−1 for phytoplankton and ∼106 beads ml−1 for HB) was added as an internal standard (Polysciences, Inc.). Cell abundances were calculated from bead concentrations. The bead solution was checked daily by epifluorescence microscopy counting.
Samples (50 ml) were filtered through 50 µm polycarbonate filters and 0.2 µm pore size cellulose acetate syringe filters. The cellulose acetate filters were stored in liquid nitrogen. For DNA extraction, the filter membranes were extracted using sterile scissors and forceps and processed using the NucleoSpin® Plant II kit (Macherey-Nagel, Germany) with a Proteinase K (Takara, Japan) digestion step (0.2 mg/ml) at 55°C for 1 h. DNA concentration and purity was determined by spectrophotometry and DNA was stored at −20°C.
rDNA clone libraries and sequencing
Partial rDNA operons (>4,400 nt from 16S rDNA-Helix 4 [H39] to 23S rDNA-Helix H4 [H2735]) were amplified using universal SSU rRNA (SSU-4-forw, 5′-GATCCTKGCTCAGGATKAACGCTGGC-3′) and cyanobacterial- specific ptLSU (CD-rev, 5′-GCCGGCTCATTCTTCAAC-3′)24 primers. PCR reactions (25 µl) contained 75 ng DNA, primers (0.4 µM), dNTPs (200 µM), 1X KAPATaq buffer and 0.5 U/µl KAPATaq DNA polymerase (KAPA Biosystems, USA) and was subjected to the following program: 95°C for 3 min, 30 cycles of 95°C for 1 min, 55°C for 2 min and 72°C for 3 min and 72°C for 5 min. Clone libraries were constructed using the TOPO TA Cloning® Kit (Invitrogen, USA) following manufacturer's instructions (pCR®2.1-TOPO® vector, TOP10 Escherichia coli cells). Positive clones were used as template for an additional PCR reaction. PCR products were purified using the NucleoSpin® Extract II kit (Macherey-Nagel GmbH & Co. KG, Germany) and sequencing was performed at a commercial sequencing service (Macrogen Inc., Korea) using the primers: Seq_16S_H4_forw (5′-TKGCTCAGGATKAACGCTGGC-3′), Seq_16S_pos874_forw (5′-ACTCAAAGGAATTGACG-3′), Seq_16S_39_rev (5′-ACTTAACCCRACATCTCACGACACG-3′) and Seq_16S_49_rev (5′-TACGGCTACCTTGTTACGACTTC-3′)25.
Alignment and phylogenetic analyses
Six Prochlorococcus sequences were identified by BLAST26 and deposited on GenBank [JQ670967-JQ670972]. These sequences were combined with 16S rDNA database sequences of Prochlorococcus strains (MED4: BX548174, MIT9515: CP000552, MIT9312: CP000111, MIT9202: AF115269, MIT9301: CP000576, MIT9215: CP000825, AS9601: CP000551, NATL1A: CP000553, NATL2A: CP000095, SS120: AE017126, MIT9211: CP000878, MIT9313: NC_005071, MIT9303: CP000554) and Synechococcus (outgroup) strains (CC9902: CP000097, CC9311: CP000435, CC9605: CP000110) and manually aligned using SEAVIEW427 considering the 16S rDNA secondary structure of Synechococcus sp. PCC6301. Alignments are available upon request. A total of 1,397 unambiguously aligned positions were used for analyses with maximum likelihood (ML), Bayesian inference (BI), distance methods (NJ) and maximum parsimony (MP). ML was performed using RAxML v7.2.828 for 10 runs and 1,000 (thorough) bootstrap (BS) replicates under the GTR+I+Γ model. BI was carried out through MrBayes v3.1.229 with two independent MCMC runs of four Metropolis-coupled chains under the GTR+I+Γ model, assuming default priors. Chains were sampled every 1.000 generations for 5x106 generations. Convergence of chains was assessed using Tracer 1.5 (http://tree.bio.ed.ac.uk/software/tracer/) and the first 500 trees were discarded as burn-in. NJ was carried out using SEAVIEW427 performing 1,000 BS replicates under the HKY model and using LogDet distances. MP was carried out using PHYLIP v3.52 (http://evolution.genetics.washington.edu/phylip.html) with 10 random starts, 1,000 BS replicates and retaining the best 10,000 trees.
Hall-Spencer, J. M. et al. Volcanic carbon dioxide vents show ecosystem effects of ocean acidification. Nature 454, 96 (2008).
Resing, J. A. et al. Chemistry of hydrothermal plumes above submarine volcanoes of the Mariana. Arc. Geochem. Geophys. Geosyst. 10, Q02009, 10.1029/2008GC002141. (2009).
Johnson, Z. I. et al. Niche partitioning among Prochlorococcus ecotypes along ocean-scale environmental gradients. Science 311, 1737 (2006).
Gruber, N. Warming up, turning sour, losing breath: ocean biogeochemistry under global change. Phil. Trans. R. Soc. A 369, 1980, doi:10.1098/rsta.2011.0003 (2011).
Intergovernmental Panel on Climate Change. Summary for Policymakers. In Climate Change 2007: The Physical Science Basis. Working Group I Contribution to the Fourth Assessment Report of the IPCC (eds Solomon S., et al.), Cambridge Univ. Press, Cambridge (2007).
Orr, J. C. et al. Anthropogenic ocean acidification over the twenty-first century and its impact on calcifying organisms. Nature 437, 681–686 (2005).
Keeling, R. F., Körtzinger, A. & Gruber, N. Ocean deoxygenation in a warming world. Annu. Rev. Mar. Sci. 2, 199–229 (2010).
Burrows, M. T. et al. The pace of shifting climate in marine and terrestrial ecosystems. Science 334, 652–655 (2011).
Ekau, W., Auel, H., Poertner, H.-O. Gilbert, D. Impacts of hypoxia on the structure and processes in pelagic communities (zooplankton, macroinvertebrates and fish). Biogeosciences 7, 1669–1699 (2010).
Stramma, L., Schmidtko, S., Levin, L. A. & Johnson, G. C. Ocean oxygen minima expansions and their biological impacts. Deep-Sea Res. I 57, 587–595 (2010).
Clayton, T. D. & Byrne, R. H. Spectrophotometric seawater pH measurements: total hydrogen ion concentration scale calibration of m-cresol purple and at-sea results. Deep-Sea Res. I 40, 2115–2129 (1993).
González-Dávila, M., Santana-Casiano, J. M., Rueda, M. J., Llinás, O. & González-Dávila, E. F. Seasonal and interannual variability of sea surface carbon dioxide species at the European Station for Time Series in the Ocean at the Canary Islands (ESTOC) between 1996 and 2000. Global Biogeochem. Cycles 17, 1076 (2003).
Millero, F. J. The pH of estuarine seawater. Limnol. Oceanogr. 31, 839–847 (1986).
Dickson A. G., Sabine C. L., & Christian J. R. (Eds.) Guide to best practices for ocean CO2 measurements. PICES Special Publication 3, IOCCP report No. 8 (2007).
Mintrop, L. Versatile instruments for the determination of titration alkalinity. Manual for versions 3S and 3C (2008).
Mehrbach, C., Culberson, C. H., Hawlay, J. E., & Pytkowicz, R. M. Measurement of the apparent dissociation constants of carbonic acid in seawater at atmospheric pressure. Limnol. Oceanogr. 18, 897–907 (1973).
Dickson, A. G. & Millero, F. J. A comparison of the equilibrium constants for the dissociation of carbonic acid in seawater media. Deep-Sea Res. 34, 1733–1743 (1987).
Santana-Casiano, J. M., González-Dávila, M. & Millero, F. J. Oxidation of nanomolar level of Fe(II) with oxygen in natural waters. Environ. Sci. Technol. 39, 2073–2079 (2005).
González-Dávila, M., Santana-Casiano, J. M. & Millero, F. J. Oxidation of iron(II) nanomolar with H2O2 in seawater. Geochim. Cosmochim. Acta 69, 83–93 (2005).
Konovalov, S. K. et al. Intercalibration of CoMSBlack-93a chemical data; unification methods for dissolved oxygen and hydrogen sulfide analyses and sampling strategies of CoMSBlack-94a cruise. Rep. Inst. Mar. Sci. Edermil, Turkey. (1994).
Konovalov, S. K. & Romanov, A. S. Spectrophotometric and iodometric methods for the detection of hydrogen sulfide in the Black Sea: comparison of the results of analysis. Phys. Oceanogr. 10, 365–377 (1999).
Hernández-Brito, J. J., Cardona-Castellano, P., Siruela-Matos, V. & Pérez-Peña, J. A. High-speed computerized polarographic system for cathodic stripping voltammetry in seawater. Electroanalysis 6, 1141 (1994).
Hernández-Brito, J. J., Gelado-Caballero, M. D., Pérez-Peña, J. & Herrera-Melián, J. A. Fast determination of Aluminum reactive to 1,2-Dihydroxyanthra-quinone-3-sulfonic Acid in Sea-Water. Analyst 119, 1593–1597 (1994).
Marin, B., Nowack, E. C. M. & Melkonian, M. A plastid in the making: Evidence for a second primary endosymbiosis. Protist 156, 425–432 (2005).
Marin, B. & Melkonian, M. Molecular Phylogeny and Classification of the Mamiellophyceae class. nov. (Chlorophyta) based on Sequence Comparisons of the Nuclear- and Plastid-encoded rRNA Operons. Protist 161, 304–336 (2010).
Altschul, S. F., Gish, W., Miller, W., Myers, E. W. & Lipman, D. J. Basic Local Alignment Search Tool. Journal of Molecular Biology 215, 403–410 (1990).
Gouy, M., Guindon, S. & Gascuel, O. SeaView version 4: a multiplatform graphical user interface for sequence alignment and phylogenetic tree building. Molecular Biology and Evolution 27, 221-224 (2010).
Stamatakis, A. RAxML-VI-HPC: Maximum Likelihood-based Phylogenetic Analyses with Thousands of Taxa and Mixed Models. Bioinformatics 22, 2688–2690 (2006).
Huelsenbeck, J. P. & Ronquist, F. MRBAYES: Bayesian inference of phylogeny. Bioinformatics 17, 754–755 (2001).
This study has been supported by the Instituto Español de Oceanografía (I.E.O). The European project CARBOCHANGE-264879 has supported the analyses of carbon dioxide, reduced S species and Fe. We thank the Captain of the R/V Ramón Margalef, Luis Gago and its crew for the help during this research.
The authors declare no competing financial interests.
About this article
Cite this article
Fraile-Nuez, E., González-Dávila, M., Santana-Casiano, J. et al. The submarine volcano eruption at the island of El Hierro: physical-chemical perturbation and biological response. Sci Rep 2, 486 (2012). https://doi.org/10.1038/srep00486
Nature Ecology & Evolution (2017)
Significant discharge of CO2 from hydrothermalism associated with the submarine volcano of El Hierro Island
Scientific Reports (2016)
Influence of hydrothermal venting on water column properties in the crater of the Kolumbo submarine volcano, Santorini volcanic field (Greece)
Geo-Marine Letters (2016)
Comment on “Evidence from acoustic imaging for submarine volcanic activity in 2012 off the west coast of El Hierro (Canary Islands, Spain)” by Pérez NM, Somoza L, Hernández PA, González de Vallejo L, León R, Sagiya T, Biain A, González FJ, Medialdea T, Barrancos J, Ibáñez J, Sumino H, Nogami K and Romero C [Bull Volcanol (2014) 76:882-896]
Bulletin of Volcanology (2015)