Bei den globalen Veränderungen und deren Mitigation durch Umstellung auf erneuerbare Energiequellen (z. B. Offshore-Wind- und Solarparks) müssen nachteilige Auswirkungen auf die Lebensräume im Meer besser erkannt und vermieden werden. So hat die internationale Fischereipolitik in letzter Zeit der marinen Aquakultur Vorrang eingeräumt, um die globale Nahrungsmittel- und Ernährungssicherheit vieler Staaten zu gewährleisten, ohne deren tatsächliche Auswirkungen auf die Meeresumwelt zu kennen. Das Verständnis der räumlichen Ökologie freilebender Tiere, einschließlich ihrer Verbreitung, Bewegungen und Wanderungen, ihrer Phänologie und ihrer Ernährung, führt zu einer besseren Bewirtschaftung und Erhaltung. So können beispielsweise Bemühungen zur Erhaltung wandernder Populationen, die sich ausschließlich auf Brutgebiete konzentrieren, diese Populationen nicht vor Bedrohungen entlang der Wanderrouten oder in Nicht-Brutgebieten schützen. Tierbewegungen und Wanderungen sind auch deshalb wichtig, weil sie das Verhalten, die Lebensweise und sogar die Anatomie vieler Arten beeinflussen. Darüber hinaus kann sich das Wander- und Ernährungsverhalten innerhalb und zwischen den Arten und Populationen unterscheiden. Daher ist es von entscheidender Bedeutung, die auf jeder dieser Ebenen genutzten Routen und Nichtbrutgebiete zu ermitteln, zumal sie auch mit unterschiedlichen Bedrohungen verbunden sein können. Darüber hinaus kann die Untersuchung verschiedener Populationen auch dazu beitragen, zu verstehen, ob die räumliche Ökologie der Art durch genetischen und/oder Umweltvariablen bestimmt wird. Eine Möglichkeit, die Bewegungen und die Verteilung außerhalb der Fortpflanzungszeit bei wandernden Arten zu bestimmen, und zwar neuerdings auch bei den kleinsten Arten, ist der Einsatz von Geolokatoren auf Lichtniveau. Darüber hinaus können feinräumige Bewegungen mit dem kleinsten GPS-Gerät von nur 0,95 g verfolgt werden. Sturmschwalben (Familien Hydrobatidae und Oceanitidae) sind die kleinsten Seevögel und für die Forscher normalerweise nur zugänglich, wenn sie während der Brutzeit in den Kolonien an Land sind. Daher ist es besonders schwierig, sie außerhalb dieses Zeitraums zu untersuchen, wenn sie sich irgendwo auf dem Meer aufhalten und während dieser Zeit wandern und normalerweise ihr Gefieder mausern. Von den meisten Arten ist bekannt, dass sie sich während der Brutzeit bevorzugt von Ichthyoplankton und Zooplankton ernähren, und oft wird diese Beute zusammen mit einem relevanten Anteil an Mikroplastik verzehrt. Obwohl die Interaktion von Sturmschwalben mit anthropogenen Offshore-Aktivitäten teilweise untersucht wurde, zielt der vorliegende Vorschlag darauf ab, wichtige Erkenntnisse über die globale räumliche Ökologie dieser wenig erforschten Taxa zu sammeln und dazu beizutragen, Wissenslücken in Bezug auf die biologische Vielfalt der Meere und die anthropogenen Einflüsse auf sie entlang der europäischen Meere zu bewerten.
Dieser Dienst stellt Layer zu folgenden Themen bereit: - Kabel- und Leitungsbau (beeinflusste Flächen) - Offshore Windenergie (Lage, Ausdehnung, Anzahl, Größe, Fundament-Typ) - Küstenschutzmaßnahmen (Lage, Ausdehnung, beeinflusste Flächen) - Sonstige Flächeninanspruchnahmen (Lage, Ausdehnung, Art und Zeitpunkt der Herstellung), z. B. Plattformen - Baggerungen, Sandentnahmen (Volumen m³/a, betroffene Flächen) - Verklappungen (Volumen m³/a, betroffene Flächen) - Wellen- bzw. strömungsinduzierte Sedimentumlagerung (shear stress) - Schifffahrt - Fischereidruck - Marikulturen (Lage, Ausdehnung, Menge pro Fläche und Art) - Muschelfang und Muschelkulturflächen (Zeit/Fläche pro Jahr, Menge pro Fläche und Art)
We assessed the heat tolerance of microscopic, juvenile and adult sporophytes under heat stress and in response to gametophyte or sporophyte priming in five experiments. Experiment 1: we primed Saccharina latissima gametophytes (Lofoten 2023; 15°C clonal culture; n = 7) for 3 weeks at 0°C, 10°C, and 20°C and induced gametogenesis at 10°C for 2 weeks. Resulting microscopic sporophytes were subjected to a 14-day heat stress treatment at 20°C, 21.5°C, and 23°C, where we counted the number of alive and dead sporophytes and calculated the survival rates. Experiment 2: sporophytes were cultivated after gametogenesis for an additional 4 weeks before we subjected them to a 14-day simulated heat wave (13°C for 3 days, 16°C for 2 days, 18°C for 2 days, 20°C, 21°C and 22°C for 1 day each, 23°C and 24°C for 4 days each, and recovery at 20°C for 7 days), during which we assessed the photosynthetic performance by measuring quantum yield (Fv/Fm). Sporophytes that survived the heat wave were cultivated at 15°C for 64 days to recover, after which we measured their size (length and blade area). Experiment 3: primed (0°C, 10°C, 20°C; 3 weeks) gametophytes (Lofoten 2023; 10°C mixed culture; n = 5) were sown on ropes and reared in a mariculture experiment (2 months hatchery, 4 months mariculture). Adult sporophytes were sampled and exposed to the same 14-day heat stress treatment at 20°C, 21.5°C, 23°C with a 10°C control group. We measured growth (length and blade area), Fv/Fm, and the percentage of healthy area (as % blade area with Fv/Fm > 0.6). Experiment 4: sporophytes from the 0°C gametophyte priming treatment of the same mariculture experiment recovered at 10°C for 24 days. Meristematic discs were exposed to a 1-day sporophyte priming trigger (T). A control group (C) remained at 10°C. After 3 days recovery at 10°C both groups were subjected to a 7-day heat stress treatment at 20°C, 21.5°C, 23°C, and 25°C, where we measured growth (disc area) and Fv/Fm. Experiment 5: gametogenesis of gametophytes (Spitsbergen 2011, 2015; 5°C clonal culture, n = 5) was induced at 5°C and sporophytes reared for 6 months. Sporophytes were distributed to three treatment groups. A 17-day heat wave (from 5°C to 20°C and back) followed by a 1-day priming trigger at 21.5°C (HWT); 17 days at 10°C and a 1-day priming trigger (T); a control remaining at 10°C throughout (C). All groups were subjected to a 7-day heat stress treatment at 20°C, 21.5°C, 23°C, and 25°C, where we measured Fv/Fm, percentage of healthy area and survival. All laboratory experiments were carried out at the Alfred Wegener Institute in Bremerhaven, from January to July 2024. The mariculture experiment took place at the hatchery of Polaralge AS (Sandhornøy, Norway; December - February 2024) and the deployment site of Lofoten Blue Harvest (Lilje Engla, Lofoten, Norway; 68°16'02.8N 15°06'14.8E; February – June 2024).
We assessed the heat tolerance of microscopic, juvenile and adult sporophytes under heat stress and in response to gametophyte or sporophyte priming in five experiments. Experiment 1: we primed Saccharina latissima gametophytes (Lofoten 2023; 15°C clonal culture; n = 7) for 3 weeks at 0°C, 10°C, and 20°C and induced gametogenesis at 10°C for 2 weeks. Resulting microscopic sporophytes were subjected to a 14-day heat stress treatment at 20°C, 21.5°C, and 23°C, where we counted the number of alive and dead sporophytes and calculated the survival rates. Experiment 2: sporophytes were cultivated after gametogenesis for an additional 4 weeks before we subjected them to a 14-day simulated heat wave (13°C for 3 days, 16°C for 2 days, 18°C for 2 days, 20°C, 21°C and 22°C for 1 day each, 23°C and 24°C for 4 days each, and recovery at 20°C for 7 days), during which we assessed the photosynthetic performance by measuring quantum yield (Fv/Fm). Sporophytes that survived the heat wave were cultivated at 15°C for 64 days to recover, after which we measured their size (length and blade area). Experiment 3: primed (0°C, 10°C, 20°C; 3 weeks) gametophytes (Lofoten 2023; 10°C mixed culture; n = 5) were sown on ropes and reared in a mariculture experiment (2 months hatchery, 4 months mariculture). Adult sporophytes were sampled and exposed to the same 14-day heat stress treatment at 20°C, 21.5°C, 23°C with a 10°C control group. We measured growth (length and blade area), Fv/Fm, and the percentage of healthy area (as % blade area with Fv/Fm > 0.6). Experiment 4: sporophytes from the 0°C gametophyte priming treatment of the same mariculture experiment recovered at 10°C for 24 days. Meristematic discs were exposed to a 1-day sporophyte priming trigger (T). A control group (C) remained at 10°C. After 3 days recovery at 10°C both groups were subjected to a 7-day heat stress treatment at 20°C, 21.5°C, 23°C, and 25°C, where we measured growth (disc area) and Fv/Fm. Experiment 5: gametogenesis of gametophytes (Spitsbergen 2011, 2015; 5°C clonal culture, n = 5) was induced at 5°C and sporophytes reared for 6 months. Sporophytes were distributed to three treatment groups. A 17-day heat wave (from 5°C to 20°C and back) followed by a 1-day priming trigger at 21.5°C (HWT); 17 days at 10°C and a 1-day priming trigger (T); a control remaining at 10°C throughout (C). All groups were subjected to a 7-day heat stress treatment at 20°C, 21.5°C, 23°C, and 25°C, where we measured Fv/Fm, percentage of healthy area and survival. All laboratory experiments were carried out at the Alfred Wegener Institute in Bremerhaven, from January to July 2024. The mariculture experiment took place at the hatchery of Polaralge AS (Sandhornøy, Norway; December - February 2024) and the deployment site of Lofoten Blue Harvest (Lilje Engla, Lofoten, Norway; 68°16'02.8N 15°06'14.8E; February – June 2024).
We assessed the heat tolerance of microscopic, juvenile and adult sporophytes under heat stress and in response to gametophyte or sporophyte priming in five experiments. Experiment 1: we primed Saccharina latissima gametophytes (Lofoten 2023; 15°C clonal culture; n = 7) for 3 weeks at 0°C, 10°C, and 20°C and induced gametogenesis at 10°C for 2 weeks. Resulting microscopic sporophytes were subjected to a 14-day heat stress treatment at 20°C, 21.5°C, and 23°C, where we counted the number of alive and dead sporophytes and calculated the survival rates. Experiment 2: sporophytes were cultivated after gametogenesis for an additional 4 weeks before we subjected them to a 14-day simulated heat wave (13°C for 3 days, 16°C for 2 days, 18°C for 2 days, 20°C, 21°C and 22°C for 1 day each, 23°C and 24°C for 4 days each, and recovery at 20°C for 7 days), during which we assessed the photosynthetic performance by measuring quantum yield (Fv/Fm). Sporophytes that survived the heat wave were cultivated at 15°C for 64 days to recover, after which we measured their size (length and blade area). Experiment 3: primed (0°C, 10°C, 20°C; 3 weeks) gametophytes (Lofoten 2023; 10°C mixed culture; n = 5) were sown on ropes and reared in a mariculture experiment (2 months hatchery, 4 months mariculture). Adult sporophytes were sampled and exposed to the same 14-day heat stress treatment at 20°C, 21.5°C, 23°C with a 10°C control group. We measured growth (length and blade area), Fv/Fm, and the percentage of healthy area (as % blade area with Fv/Fm > 0.6). Experiment 4: sporophytes from the 0°C gametophyte priming treatment of the same mariculture experiment recovered at 10°C for 24 days. Meristematic discs were exposed to a 1-day sporophyte priming trigger (T). A control group (C) remained at 10°C. After 3 days recovery at 10°C both groups were subjected to a 7-day heat stress treatment at 20°C, 21.5°C, 23°C, and 25°C, where we measured growth (disc area) and Fv/Fm. Experiment 5: gametogenesis of gametophytes (Spitsbergen 2011, 2015; 5°C clonal culture, n = 5) was induced at 5°C and sporophytes reared for 6 months. Sporophytes were distributed to three treatment groups. A 17-day heat wave (from 5°C to 20°C and back) followed by a 1-day priming trigger at 21.5°C (HWT); 17 days at 10°C and a 1-day priming trigger (T); a control remaining at 10°C throughout (C). All groups were subjected to a 7-day heat stress treatment at 20°C, 21.5°C, 23°C, and 25°C, where we measured Fv/Fm, percentage of healthy area and survival. All laboratory experiments were carried out at the Alfred Wegener Institute in Bremerhaven, from January to July 2024. The mariculture experiment took place at the hatchery of Polaralge AS (Sandhornøy, Norway; December - February 2024) and the deployment site of Lofoten Blue Harvest (Lilje Engla, Lofoten, Norway; 68°16'02.8N 15°06'14.8E; February – June 2024).
We examined the effect of gametophyte priming on early life stages of Saccharina latissima (gametophyte growth, sporophyte recruitment, juvenile sporophyte growth) and adult sporophytes harvested after growing for six months in mariculture (size and biomass, biochemical composition) in two experiments. Experiment 1: we primed S. latissima gametophytes (Lofoten 2023; 15°C clonal culture; n = 7) for 3 weeks at 0°C, 10°C, and 20°C and induced gametogenesis at 10°C for 2 weeks, during which we assessed relative gametophyte growth rates (from day 0 – 5), progression of gametogenesis, and sporophyte recruitment. Resulting sporophytes reared at 10°C were subjected to a 14-day temperature gradient treatment spanning 7 temperatures (0, 5, 10, 15, 20, 21.5, 23°C). We measured sporophyte growth (length and relative growth rates) after 7 and 14 days. Experiment 2: primed (0°C, 10°C, 20°C; 3 weeks) gametophytes (Lofoten 2023; 10°C mixed culture; n = 5) were sown on ropes and reared in a mariculture experiment (2 months hatchery, 4 months mariculture). Adult sporophytes were sampled and we measured growth (sporophyte length and width), total biomass (in fresh weight per m rope) and biochemical composition (C, N, mannitol, laminarin, and mineral composition). During the mariculture experiment, seawater temperature and nutrient composition was recorded at different time points. The mariculture field experiment took place at the hatchery of Polaralge AS (Sandhornøy, Norway; December - February 2024) and the deployment site of Lofoten Blue Harvest (Lilje Engla, Lofoten, Norway; 68°16'02.8N 15°06'14.8E; February – June 2024). The laboratory experiments of experiment 1 and the CN-analysis were carried out at the Alfred Wegener Institute in Bremerhaven, Germany; the mannitol analysis at the University of Rostock, Germany; the laminarin analysis at the MPI Bremen, Germany; and the mineral analysis at NIBIO Bodø, Norway.
This dataset contains measurements of seawater pH and total alkalinity from a short-term factorial feeding experiment conducted independently of the main chronic alkalinity-enhancement exposure. The experiment tested whether the shellfish diet used to feed the oysters in the main experiment (Reed Mariculture SD1800, a concentrated microalgae feed) contributes to seawater total alkalinity, and whether this contribution depends on the presence of oysters. Four treatment combinations were run in parallel over a 9-day period (12 to 21 November 2024): unamended seawater without oysters or feed (control), seawater with food but without oysters (SD 1800), seawater with oysters but without feed (oysters) and seawater with both oysters and feed (oysters + SD 1800). Oysters in the unfed treatments were left entirely without feed for the full 9 days. Each treatment was sampled on six days (day 0, 1, 3, 5, 7 and 9) in triplicate. Seawater pH was measured with a pH electrode and total alkalinity by open-cell potentiometric titration, both on a Metrohm 855 Robotic Titrosampler.
Adult European flat oysters (Ostrea edulis) were exposed in indoor mesocosms to two contrasting approaches for ocean alkalinity enhancement (OAE): dissolved alkalinity addition using NaOH and CaCl2, and olivine-based coastal enhanced silicate weathering, each targeting a total alkalinity increase of +250 or +500 µmol/kg over unamended seawater. An alkalinization phase (17 April to 19 June 2024) established the target total alkalinity in each treatment tank before oysters were introduced for a subsequent chronic exposure phase (8 May to 10 July 2024). Seawater pH and total alkalinity, salinity, temperature, dissolved oxygen, chlorophyll a, suspended particulate matter and ammonia were monitored throughout both phases, alongside oyster mortality. Full carbonate system parameters (CO2, HCO3-, CO32-, dissolved inorganic carbon, pCO2 and the aragonite and calcite saturation states) were calculated from the measured pH, total alkalinity, salinity and temperature using the seacarb package in R. At the end of the chronic exposure, oyster gill, mantle and hepatopancreas tissue was sampled for trace metal accumulation (nickel, chromium and cobalt) by ICP-OES, gill and mantle tissue for untargeted polar metabolite profiling by ¹H-NMR spectroscopy, and labial palps tissue for glycogen quantification. A separate short-term feeding experiment (12 to 21 November 2024) tested whether the shellfish diet used to feed the oysters (Reed Mariculture SD1800) contributes to the total alkalinity increase observed in the treatment tanks, independent of the OAE treatments. This submission bundles nine related data tables from this study; an individual, table-specific abstract accompanies each file in the file description.
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