Unraveling the importance of solid and adsorbed phase mercury speciation for methylmercury formation, evasion and bioaccumulation Sofi Jonsson Department of Chemistry Umeå 2013 © Sofi Jonsson, Umeå 2013 This work is protected by the Swedish Copyright Legislation (Act 1960:729) ISBN: 978-91-7459-546-8 Cover: Sofi Jonsson (Fron cover: perch from Hennan, Ramsjö. Back cover: red (αHgS(s)) and black (β-HgS(s)) cinnbar, Mesocosms, Umeå Marine Sciences Centre) Electronic version available at http://umu.diva-portal.org/ Printed by: the service centre in KBC, Umeå University, January 2013 Umeå, Sweden 2013 Till Mathias ‒ min älskade och saknade Table of Contents List of publications ii Abstract iii Abbreviations v Sammanfattning (Summary in Swedish) vi 1. Introduction 1 2. Experimental systems and approaches 8 2.1 Hg speciation and fractionation analysis in environmental samples 1.1 Application of Hg stable isotope experimental approaches 10 1.1.1 Determination of gaseous Hg0, HgII, MeHg and DMHg 12 1.1.2 Methylation and demethylation rates and rate constants 14 1.1.3 Determination of methylation rate constants using solid or adsorbed chemical forms of HgII (paper II) 18 1.2 Scale of experiment – from micro- to mesocosms 19 Mercury methylation, evasion and bioaccumulation 21 3. 4. 8 3.1 Methylation of HgII 22 3.2 Demethylation of MeHg 26 3.3 Evasion of Hg 27 3.4 Bioaccumulation of mercury 28 Implication and final remarks 35 Acknowledgements 41 References 44 i List of publications Publications included in this thesis: I. Sofi Jonsson, Ulf Skyllberg, Erik Björn (2010), Substantial Emission of Gaseous Monomethylmercury from Contaminated Water-Sediment Microcosms, Environmental Science and Technology, 44, 278-283 II. Sofi Jonsson, Ulf Skyllberg, Mats B. Nilsson, Per-Olof Westlund, Andrey Shchukarev, Erik Lundberg, Erik Björn (2012), Mercury Methylation Rates for Geochemically Relevant HgII Species in Sediments, Environmental Science and Technology, 46, 11653-11659 III. Sofi Jonsson, Ulf Skyllberg, Mats B. Nilsson, Agneta Andersson, Erik Lundberg, Erik Björn, Differentiated reactivity of geochemical mercury pools control methylmercury levels in sediment and biota, Manuscript IV. Sofi Jonsson, Agneta Andersson, Mats B. Nilsson, Ulf Skyllberg, Erik Lundberg, Jeffra K. Schaefer, Staffan Åkerblom, Erik Björn, Impact of Nutrient and Humic Matter Loadings on Methylmercury Formation and Bioaccumulation in Estuarine Ecosystems, Manuscript Paper I and II is reprinted with permission from publisher. Copyright © 2010 and 2012, American Chemical Society. ii Abstract Monomethylmercury, MeHg, is formed under anoxic conditions in waters, sediments and soils and then bioaccumulated and biomagnified in aquatic food webs, negatively effecting both human and wildlife health. It is generally accepted that precipitation of mercury, Hg, and adsorption of Hg to e.g. organic matter and mineral surfaces are important processes limiting the reactivity of Hg mobilized in the environment by natural and anthropogenic activities. However, knowledge concerning the role of different solid and adsorbed chemical forms of Hg for MeHg formation, evasion and bioaccumulation is missing. Such information is vital for the understanding of environmental processes controlling MeHg formation and bioaccumulation, as well as for predicting how changes in e.g. loading rates of atmospheric Hg and the outcome of climate change scenarios and anthropogenic land use could alter Hg concentrations in biota. In this thesis, a novel experimental approach, using isotopically enriched solid and adsorbed phases of inorganic Hg, HgII, as tracers, was developed. Using this approach, we successfully determined rates of MeHg formation from solid and adsorbed Hg species in sediment slurries and in mesocosm systems under conditions closely resembling those in field. We conclude that the solid/adsorbed phase speciation of HgII is a major controlling factor for MeHg net formation rates. Microcosm experiments revealed that newly formed MeHg was a major contributor to the evasion of MeHg from the water‒sediment system, emphasizing the importance of MeHg formation rate, rather than MeHg concentration, in the sediment for this process. From mesocosm systems, we provide experimental evidence, as well as quantitate data, for that terrestrial and atmospheric sources of HgII and MeHg are more available for methylation and bioaccumulation processes than HgII and MeHg stored and formed in sediments. This suggests that the contribution from terrestrial and atmospheric sources to the accumulation of Hg in fish may have been underestimated. As a consequence, in regions where climate change is expected to further increase land runoff, terrestrial MeHg sources may have even higher negative effects on biota than previously thought. Data and concepts presented in this thesis lay the basis for unprecedented indepth modeling of processes in the Hg biogeochemical cycle that will iii improve our understanding and the predicting power on how aquatic ecosystems may respond to environmental changes or differences in loading rates for atmospheric Hg. iv Abbreviations BAF BSAF DMeHg DOM d.w. EXAFS GC GEM HPLC HgII ICPMS IDA IUPAC KD kd km LOD MeHg METALLICUS NOM rd RGM rm Sed UNEP US EPA Wt XAS XANES Biota Accumulation Factor Biota-Sediment Accumulation Factor Dimethylmercury Dissolved Organic Matter Dry Weight Extended X-ray Absorption Fine Structure Gas Chromatography Gaseous Elemental Mercury High Performance Liquid Chromatography Inorganic divalent mercury Inductively Coupled Plasma Mass Spectrometry Isotope Dilution Analysis International Union of Pure and Applied Chemistry Solid-liquid partition coefficient Demethylation rate constant Methylation rate constant Limit of Detection Monomethylmercury Mercury Experiment to Assess Atmospheric Loading in Canada and the United States Natural Organic Matter Rate of demethylation Reactive Gaseous Mercury Rate of methylation Sediment United Nations Environmental Program United States Environmental Protection Agency Water X-ray Absorption Spectroscopy X-ray Absorption near-edge Structure v Sammanfattning (Summary in Swedish) Monometylkvicksilver, MeHg, bildas under anoxiska förhållanden i naturliga vatten, sediment och jordar och bioackumuleras och magnifieras därefter i den akvatiska näringskedjan med negativa effekter på djur och människor som följd. Det är generellt vedertaget att utfällning av Hg och adsorption av Hg till exempelvis organiskt material och mineralytor begränsar tillgängligheten för biogeokemiska reaktioner av Hg som mobiliserats i miljön via naturliga och antropogena processer. Kunskap om betydelsen av speciationen av Hg i fasta och adsorberade faser för bildning, avgång och bioackumulering av MeHg är dock bristfällig. Denna information är kritisk för att förstå vilka processer som kontrollerar bildning och bioackumulering av MeHg samt för att kunna prediktera hur olika ekosystem kan förväntas svara på exempelvis ändrad deposition av atmosfäriskt Hg eller hur klimatförändringar kan påverka koncentrationerna av Hg i fisk. I denna avhandling har en experimentell metod utvecklades, där isotopanrikade fasta och adsorberade kemiska former av oorganiska tvåvärt Hg, HgII används som s.k. ”tracers”. Denna metod användes för att bestämma MeHg bildningshasigheter i homogeniserade sediment prover samt i mesokosmsystem där förhållandena efterliknar de som förväntas i naturliga ekosystem. Från dessa drar vi slutsatsen att speciationen av HgII i fast/adsorberad fas är en viktig kontrollerande faktor som begränsar nettobildningen av MeHg. Mikrokosmexperiment visade att i första hand nyligt bildad MeHg avgick till gasfas vilket understryker betydelsen av MeHg bildningshastighet, snarare än koncentration, i sedimentet för denna process. Från mesokosmexperimenten visar vi, med kvantitativa data, att terrestra och atmosfäriska källor av HgII och MeHg är mer tillgängliga för bildning och bioackumulering av MeHg än HgII och MeHg lagrat eller bildat i sedimenten. Orsaken till detta är framförallt skillnad i speciationen av Hg i fasta/adsorberade faser. Detta innebär att bidraget från MeHg från terrestra och atmosfäriska källor till koncentrationen av Hg i fisk kan ha underskattats, samt att de negativa effekterna på MeHg exponering i områden där exempelvis klimat-förändringar förväntas leda till ökad terrest avrinning kan bli mer allvarliga än vad som tidigare predikterats. Data som vi presenteras i denna avhandling möjliggör modellering av Hg’s biogeokemiska cykel på en ny detaljnivå samt möjliggör säkrare prediktioner av hur olika ekosystem kan förväntas svara mot miljöförändringar eller ändrad deposition av atmosfäriskt Hg. vii viii 1. Introduction Anthropogenic activities, such as combustion of fossil fuels and gold mining, have significantly increased the pool of mercury (Hg) mobilized in the environment.1-2 This has resulted in an increased chronic exposure of Hg for marine and terrestrial organisms.3-4 Figure 1 illustrates the principal transportation and biogeochemical processes in focus for a large community of politicians, policy makers and scientists.5 Mercury is emitted, primary to the atmosphere,6-8 by both natural and anthropogenic sources. A fraction of this Hg is methylated in sediment,9 soils10 and waters11 by sulfate12-13 and/or iron14-15 reducing bacteria to monomethylmercury (MeHg) and then bioaccumulated and biomagnified in aquatic food webs.16-18 Consumption of fish is the main exposure rout of Hg for humans in most regions.19 Acute poising of Hg causes severe damage to the nervous system and in worst case death,19 such events are however nowadays rare.20 For people with a varied diet (including fish but limited intake of certain fish species), the exposure is typically at levels considered being without any associated health risks. Still, 7 % of women in child-bearing age in the USA Figure 1. Illustration of the principal biogeochemical processes of Hg, from antropogenic emission to accumulation in fish. 1 are estimated by the United States Environmental Protection Agency (US EPA) to have a diet with Hg concentrations exceeding this level.19 MeHg is able to cross the blood-to-brain and placenta barriers.21 Fetuses are thus particularly vulnerable and low exposure levels of Hg have been suggested to result in decreased birth weight and negatively affect fine motor, memory and language skills.22 However, at present, unanimous evidence of negative effects from low Hg dose exposure exists only for neurocognitive effects at exposure levels typical in population groups with an unusually high intake of fish, marine mammals or highly Hg contaminated fish from areas with local Hg pollution sources. In Sweden alone, tenths of thousands of lakes have Hg concentrations in piscivorous fish exceeding the levels considered safe for human consumption.23-24 In addition to the concerns for human and wildlife health, Hg in fish results in financial losses (primary for commercial and sport fisheries) and forces to changes in way of life for populations traditionally depending on local fish sources.8,25-26 The bioaccumulated Hg primary originates from atmospherically deposited Hg and it has been suggested, and in some studies experimentally supported, that newly deposited Hg at a higher extent contribute to fish Hg than past depositions do.24-25,27-28 The atmospheric pool of Hg has increased 3-5 times since preindustrial time.29 It has however been difficult to establish an unambiguous relationship between recent changes in the atmospheric load and fish concentration of Hg.25,30-31 In Sweden and in the USA a general decrease in fish Hg was observed from the beginning of the 1980s to the end of the 1990s which was linked to decreased atmospheric deposition rates of Hg.4,32-34 Recent studies have however revealed a shift in this trend and increasing concentrations of Hg in fish has been reported during the last decade.31,33-34 In Sweden, Åkerblom31 et al. reported increased concentration of Hg in pike for 36 % of lakes (n = 25), between 1994 and 2006. The increase was positively related to total organic carbon in the lake water. It has been suggested that variations in hydrological conditions to (at least on a shorter time scale of decades to centuries) possibly can counteract the positive effects expected from further reduced atmospheric Hg load.33-34 2 Global emission inventories, although containing large uncertainties, reveals that the anthropogenic emissions of Hg to the atmosphere have decreased during the last decades due to implementation of emission controls and restricted use of Hg in high income countries (mainly Europe and North America).35 However, emissions are increasing in low income countries with a growing economy, industrialization and an increasing demand of energy and heat production. Pacyna et al.35-36 have predicted (for main atmospheric emission sources of Hg in an illustrative model) that the anthropogenic emissions could i) increase by 25% from year 2000 to 2020 if current control practices remain unchanged and with the expected global economic growth, ii) be reduced by 40% if currently implemented and planned emission controls for Europe and North America are implemented worldwide; and iii) be reduced by 55% if the technologically best available emission controls would be implemented worldwide. United Nations Environmental Program (UNEP) is currently leading international negotiations for a “global legally binding instrument on Hg” (negotiations are planned to result in an agreement open for signature in the beginning of 2013).37 The severeness of Hg as a global pollutant is to a large extent controlled by different environmental processes resulting in MeHg formation from fresh Hg deposits (from natural and anthropogenic emissions sources) and from Hg stored in the environmental compartments, and the subsequent bioaccumulation of MeHg in aquatic food webs.25,38-39 The largest fraction of Hg emitted is accumulated and stored in deep ocean waters, or in sediment and soils as solid and adsorbed phases of inorganic divalent Hg. Because fresh Hg deposits and Hg stored in the environmental compartments at the same time are contributing to the formation of MeHg formation and its bioaccumulation, the link between current anthropogenic Hg emissions and MeHg in fish is neither direct nor simple. It is currently uncertain to what extent and within what timeframe a reduction of anthropogenic emissions of Hg will result in reduced concentrations of Hg in fish. There is a consensus among scientist, as well as environmental organizations, that an improved understanding of Hg biogeochemistry is required to develop effective strategies for decreasing the anthropogenic contribution of Hg in fish.19,25,31,38,40 Unraveling the biogeochemical processes for MeHg formation, transportation and bioaccumulation is a key objective in this aspect. The biogeochemistry of Hg is obviously far more complex than 3 illustrated in Figure 1, involving multiple chemical forms of Hg (Table 1) that undergo photo-, biological-, and chemical reactions and that are readily cycled among the atmosphere, soils, wetlands, waters and sediments.38 A chemical specie is defined by IUPAC as “specific form of an element defined as to isotopic composition, electronic or oxidation state, and/or complex or molecular structure” and speciation is defined as “distribution of an element amongst defined chemical species in a system”.41 Throughout this thesis, the sum of all possible species of inorganic divalent mercury and monomethylmercury is referred to as HgII and MeHg, respectively. I will refer to geochemical pools of HgII and MeHg as differing with respect to their i) spatial distribution (e.g. buried in sediment or localized at the sediment surface), and/or with respect to their ii) chemical speciation. In the latter case, chemical species includes well-defined solid phases like α-HgS, β-HgS and HgII and MeHg adsorbed to more complex components such as natural organic matter (NOM) and iron sulphide minerals (Mackinawite, FeS(s)). Geochemical pools of Hg have been assumed to differ with respect to their availability for methylation, bioaccumulation and transportation.42-45 At what extent the different geochemical pools control Hg geo- and biogeochemistry is however to a large extent unknown. Current insights have been derived from experiment using quite simple model system44-46 but establishment of the importance of the processes in complex system at conditions realistic for natural environments are missing. This can partly be addressed to a previous lack of suitable experimental approaches. Understanding the importance of different geochemical HgII and MeHg pools is further complicated by the fact that analytical methods for determination of individual Hg species in most cases have a limit of detection (LOD) far above the concentrations found in environmental matrices.20 We thus rely on chemical speciation modelling,47-49 sequential extraction procedures isolating operationally defined phases50-51 or measurement techniques requiring addition of Hg in the lab.50,52-53 These uncertainties and lack of knowledge contributes to MeHg and HgII often being viewed as uniform pools in sediment and soils and the chemical speciation of solid-phase Hg is often neglected.30 Obviously, new analytical methods and experimental approaches are needed 4 5 (g, aq) -(OH/Cl/Br)nn-2(aq), −DOM(aq), −NOM, −(O/N/S)≡ -(OH/Cl/Br)(aq),−DOM(aq),, −(O/N/S)≡, (g, aq) Hg0 HgII MeHg DMeHg 0.2-15 ng L-1 DMeHg Hg MeHg 10-1300 ng g-1 d.w. Fish −S-biomolecules >95 <5 (g, aq) MeHg −S-biomolecules 0.06-4 −NOM, DOM(aq), SH(g), S- (aq), −(O/N/S)≡ HgII ng g-1 d.w /Soil II >96 -(OH/Cl/Br)nn-2(aq), (SH)2(aq), S2H-(aq), S22-(aq), DOM(aq), α and βHgS(s), -NOM, -(O/N/S)≡ Hg 30-90 10-54 <3 2-2200 (g, aq, l) <1.7 (g, aq) DMeHg 0 <1-30 (OH/Cl/Br)(aq), SH(g),−NOM, −(O/N/S)≡ MeHg <2 (OH/Cl/Br)nn-2(aq), −NOM, −(O/N/S)≡ HgII >95 % of Hg ng m-3 (g) 56-58 Hg0 Hg Species 1-170 19,50 Sediment Water Air [ total Hg ] 19,39,54-55 Table 1. Summary of concentrations and speciation of Hg in air, water, sediment/soils and fish (≡ denotes mineral surfaces). in order to improve our understanding of the role played by different geochemical pools of HgII and MeHg in the biogeochemical cycle of mercury. This thesis involves work with a recently developed analytical method for speciation analysis of gaseous MeHg, dimethylmercury (DMeHg), HgII and elemental Hg (Hg0) (paper I), and a new experimental approach for determination of Hg methylation of solid/adsorbed phase isotope tracers (paper II-IV). Both of these methods provide great opportunities to expand our understanding on Hg biogeochemistry and will be described and discussed in the following chapter. Using these methods, we have studied formation, transportation and bioaccumulation of Hg chemical forms originating from different geochemical pools as indicated with colored arrows (assigned paper I-IV) in Figure 2. Figure 2. Illustration of the biogeochemical processes studied in paper IIV (referred to by roman numerals and highlighted as colored arrows). 6 In summary, we (i) have showed a substantial emission of newly methylated Hg from a contaminated water-sediment system (paper I), (ii) have quantified the rates of methylation and bioaccumulation originating from different geochemical pools of HgII (paper II-IV) in sediment slurries as well as in larger-scale sediment-water systems with intact sediment cores, (iii) showed that newly deposited HgII and MeHg is significantly more available for MeHg formation and bioaccumulation than HgII and MeHg accumulated or formed in the sediment, and (iv) showed that, in the estuarine system, formation of MeHg from sediment pools of Hg increases with pelagic primary production whereas enhanced loading of terrestrial NOM results in higher formation of MeHg, as well as higher bioaccumulation, from newly deposited Hg (paper IV). 7 2. Experimental systems and approaches This chapter describes the possibilities and limitations of current methods when it comes to the determination of Hg speciation in environmental matrices. Thereafter I describe and discuss the new methods and approaches used in papers I-IV, as well as the experimental scale (from microcosm (papers I-II) to mesocosm (papers III-IV)). 2.1 Hg speciation and fractionation analysis in environmental samples Analytical methods available for quantifying concentrations of total Hg and concentrations of specific chemical forms of Hg present at trace levels (i.e. <100 parts per million atoms (ppma) or <100 µg g-1) in sediment, soil, water and air (Table 1) have provided the basis from which our current understanding of environmental Hg processes has evolved. These methods typically include procedures for i) extraction, purification and preconcentration of the analyte from the matrix, ii) separation of chemical species and iii) element specific detection.20 The most commonly used method is the determination of total Hg in solid, aqueous or gaseous samples.50 Methods for determination of individual Hg species (e.g. the dissolved HgII complexes Hg-(OH)2, -Cl2, and specific (-SR)2) generally requires softer extraction procedures and/or separation techniques e.g. high performance liquid chromatography (HPLC), which results in relatively high LOD (typical LOD for HPLC-ICPMS of 0.0001-1 µg L-1).20 In most cases, such as for the determination of specific HgII-thiols,56 LOD for suitable methodologies are far above the concentrations expected in e.g. natural water or sediment pore waters.20,56 As an alternative, fractionation, defined by IUPAC as “process of classification of an analyte or a group of analytes from a certain sample according to physical (e.g., size, solubility) or chemical (e.g., bonding, reactivity) properties”, are commonly used.20,41,50 The analytical methods and modelling approaches used for Hg fractionation and speciation in Papers I-IV are listed in Table 2. 8 Table 2. Analytical methods and model approaches used for total Hg, Hg fractionation and Hg speciation in Papers I-IV. Matrix Analyte Method Paper Ref Air Hg , MeHg, DMeHg On-line ethylation of MeHg (NaBEt4), purge and trap GC-ICPMS analysis I 59-60 Water total Hg Sample digestion (BrCl), Hg reduction (SnCl2), purge and trap ICPMS analysis I, II 61 total Hg Sample digestion (BrCl), on-line Hg reduction (SnCl2), ICPMS analysis III, IV 61 HgII speciation Chemical equilibrium modeling I MeHg Ethylation of MeHg (NaBEt4), purge and trap GC-ICPMS analysis I-IV 62 MeHg speciation Chemical equilibrium modeling I 47,63 total Hg Microwave assisted acid digestion (HNO3, HCl) and ICPMS analysis I-IV 64 HgII speciation Chemical equilibrium modeling II Hg speciation Hg LIII-edge EXAFS II 65-66 MeHg Double extraction of MeHg (CuSO4/KBr/H2SO4 followed by CH2Cl2) into MQ water, ethylation of MeHg (NaBEt4), purge and trap GC-ICPMS analysis I-IV 67 total Hg Sample digestion (80°C, HNO3 and H2SO4) ICPMS analysis III-IV 68 MeHg Alkaline digestion (tetraethylammonium hydroxide), ethylation of MeHg (NaBEt4), purge and trap GC-ICPMS analysis III-IV 69 Sediment 0 II Biota Mercury in air is commonly fractionated into gaseous elemental Hg (GEM, i.e. total gaseous Hg passing 0.45 µm filter, presumably Hg0), reactive gaseous Hg (RGM; i.e. gaseous Hg collected in mist chambers or denuders, presumably HgII(aq)) and particulate Hg (HgII(s), i.e. Hg collected using filter based techniques or denuder methods).54,70-71 Elemental Hg constitutes approximately 95 % of the atmospheric pool of Hg but RGM and particulate HgII(s) are the primary forms of Hg deposited to land and water and hence in many cases desirable to quantify.20 9 In water (including pore waters of sediment and soil), total Hg is often fractionated by a separate determination of MeHg, Hg0 and HgII (as total Hg - MeHg).61-62 The apparently dissolved fraction of MeHg and total Hg are determined after removal of particles, most commonly larger than 0.45 µm, by filtration.61 However, HgII and MeHg both have a strong affinity for binding sites on solid particles and the fraction defined as “dissolved” can be assumed to contain a significant part (12-93%)72-74 of HgII and MeHg adsorbed to particles with a size less than 0.45 µm. Analytical methods that enable quantification of specific MeHg and HgII species at natural concentration levels in waters are at present not available. Chemical equilibrium modeling approaches (thermodynamic calculations) thus play an important role since the speciation of dissolved MeHg and HgII control the mobility and bioavailability of Hg (paper I).47-49 As discussed by Skyllberg49, these models still involve large uncertainties and we are far from fully understanding Hg speciation in natural matrices. Further research is needed to determine accurate thermodynamic stability constants and understanding the adsorption properties of HgII and MeHg on e.g. metal sulfide surfaces. Total Hg in the solid phase (sediment and soils) is typically fractionated by a separate determination of MeHg and HgII.20,67,75 In samples contaminated by mining or chloro−alkali industry, the solid phase speciation of HgII (e.g. cinnbar, metacinnbar, HgSO4, HgO and HgCl2) can be determined using synchrotron radiation based X-ray Absorption Spectroscopy (XAS) techniques, e.g. X-ray Absorption Near-Edge Structure (XANES) and Extended X-ray Absorption Fine Structure (EXAFS) Spectroscopy.76-78 For less contaminated sediments or soils, the concentrations of Hg are however too low and additions of Hg are needed for XAS analysis.66,79 Such addition have however been proven useful in establishing the main adsorbed and solid phases of HgII, as well as adsorbed phases of MeHg in sediments and soils.49,53,66 1.1 Application of Hg stable isotope experimental approaches For elements such as carbon and nitrogen, the occurrence of two stable isotopes (12C, 13C and 14N, 15N, respectively) is widely used i) for quantification purposes by isotope dilution analysis, IDA, ii) to study reactions and processes in natural samples by addition of an isotope enriched 10 reactant or iii) to trace environmental processes in the field from natural isotope fractionation.80-82 Mercury has as many as seven naturally occurring stable isotopes (average natural abundance in %); 196Hg (0.14 %), 198Hg (10.0 %), 199Hg (16.8 %), 200Hg (23.1 %), 201Hg (13.2 %), 202Hg (29.8 %) and 204 Hg (6.9 %). Multiple isotope enriched Hg tracers can thus be added to a single system and be quantified using mass specific detection and signal deconvolution of the detected Hg isotopic composition.25,50,60,69 This allow us to simultaneously study several individual environmental processes in complex experimental systems containing a “background” of ambient Hg. Commercially available isotopically enriched Hg (often as Hg0, HgO or HgCl2) are typically enriched in the given isotope from 30 to >99 %.50,83 In most studies, isotopically enriched aqueous HgII or MeHg complexes are used, however isotopically enriched DMeHg and Hg0 has also been synthesized and used for quantification purposes.50 In this thesis also the isotopically enriched solid phases cinnabar (α-HgS(s)) and metacinnabar (βHgS(s)) and, HgII reacted with Makinawite (≡FeS-HgII), and HgII and MeHg adsorbed to natural organic matter (HgII-NOM, MeHg-NOM) have been synthesized and used (paper II-IV). In IDA, a known amount of an isotopically enriched Hg standard is added as internal standard to the experimental sample before sample workup is initiated.50 In contrast to external calibration methods, losses or incomplete extraction of the analyte during the analytical procedures can be accounted for (under the assumptions that added internal standard is properly equilibrated with the sample matrix and exhibits the same (or very similar) chemical and physical properties as the analyte). Larsson and co-workers5960,84 recently developed a method, applied in paper I, for determination of Hg species/fractions in gaseous samples. By using an isotope dilution approach, Larsson and co-workers successfully addressed several critical issues (most importantly incomplete recoveries and species transformation) associated with other methods. In paper II-IV, up to 5 different isotopically enriched tracers were used to study the reactivity and/or transportation of Hg (the 6th and 7th isotope are reserved for detection of ambient Hg and for internal standard). The use of isotopically enriched Hg as tracers is most commonly used to study 11 methylation and demethylation processes in sediment, soils and water.50 Typically, HgII(aq) and MeHg(aq) tracers are added to experimental samples and incubated for up to 48 h. Thereafter the rate constants for HgII methylation and MeHg demethylation can be calculated. The main concern with this approach is if tracers (added as labile aqueous HgII or MeHg complexes) will react differently than ambient Hg and MeHg, which under relevant environmental conditions can be assumed to bind to thiol groups in NOM, at FeS surfaces or precipitate as β-HgS(s). To address this issue we developed an approach, discussed below, where we synthesized and added isotopically enriched tracers as solid or adsorbed forms (paper II). Isotope fractionation of C, N and H have been studied since the 1950’s and is today widely used to study natural processes of these elements.85 Given the much lower natural isotope fractionation of the Hg atoms, and a previous lack of analytical techniques with sufficient accuracy of isotope ratio measurements, isotope fractionation of Hg have only during the last decade been recognized as a powerful tool to study biogeochemical processes of Hg.86 At present a number of environmental processes have been shown to fractionate Hg isotopes. Different anthropogenic sources of Hg are also known to differ in isotopic signature, but to what extent isotope fractionation could be used to e.g. track sources of Hg in the environment remains uncertain.86-87 The approach will however most likely contribute to future advances in our understanding of the environmental processes of Hg and gain a wide interest among Hg scientist. Although such techniques were not used in this thesis they are worth highlighting as emerging experimental tools based on stable Hg isotope measurement techniques. 1.1.1 Determination of gaseous Hg0, HgII, MeHg and DMHg The low concentrations of HgII, MeHg and DMeHg, in air makes preconcentration of the analytes (typical ambient concentrations around 2-100 pg m-3 and instrumental absolute LOD about 2 pg) the main challenge in the quantification of these chemical Hg forms.84 Available approaches, such as liquid absorbers, cryogenic trapping and solid adsorbents suffer from incomplete recoveries and potentially high blank levels and/or species transformation. The use of external calibration is thus neither reliable nor practical. By administrating isotopically enriched HgII(g), MeHg(g), 12 DMeHg(g) and Hg0(g) as internal standards to the gaseous sample, followed by ethylation of ionic Hg species (HgII(g) and MeHg(g)) and preconcentration on a solid sorbent (Carbotrap or Tenax), Larsson et al., could demonstrate reliable quantification of Hg0, MeHg, DMeHg and HgII.5960,84 The gaseous standards are generated from temperature controlled cells with permeation tubes and a constant transport gas flow. The permeation tubes contain the isotopically enriched standard as a solution or salt, and for Hg0 as a liquid. The permeation rates will depend on temperature, the concentration of standard, and material and dimension of the permeation tubes. Larsson et al. could quantify species transformation during the sampling and fairly extensive species transformations was observed.60 For transformation during sampling of ambient air as much as 24 % of the DMeHg(g) standard added was detected as MeHg(g) and 40 % as Hg0. During collection of only the internal standard in inert atmosphere (N2), less than 5 % of the DMeHg(g) standard was transformed to other chemical forms of Hg. This emphasizes the large variances that can be expected in Hg transformation reactions depending on the composition of the gaseous sample. Larsson recognized traceability as a challenge for the proposed methodology, since no closely defined standard methods or certified reference materials exist to assure traceability of the analytical results gained.84 Further, the amount of internal standard added in IDA should be matched to the expected ambient analyte concentration in the sample to minimize the uncertainty of the quantification.88-89 Adjusting the isotope standard additions close to the sampling occasion might however be challenging for gaseous samples due to the time (days-weeks) needed to obtain stable permeation rates of the gaseous standards (caused by e.g. disturbances in adsorption-desorption equilibria of gaseous tracers on tube walls). These challenges are however minor in comparison to the challenges exhibited by methods not based on IDA. The method is thus a great improvement for the determination of chemical forms of gaseous Hg and have been successfully applied in microcosm experiments (Paper I, Björn et al50, Larsson et al.60) and for Hg speciation analysis in natural gases (Larsson et al.90). Further, Baya and Hintelmann91 were, for the first time, able to quantify MeHg and DMeHg in the Arctic lower troposphere using this methodology (average detected concentrations of 5.5 ± 2.0 and 2.3 ± 3.6 13 pg/m3 of MeHg and 2.8 ± 3.6 and 4.1 ± 2.3 pg/m3 for DMeHg in Hudson bay and the high Arctic, respectively). They could thus support the possibility that MeHg bioaccumulating in the Arctic system may partly originate from MeHg and DMeHg volatilized from oceans. 1.1.2 Methylation and demethylation rates and rate constants Methylmercury accumulated in fish originates from HgII methylated by sulfate and/or iron reducing bacteria under anoxic conditions in soils, waters and sediments.9-15 The concentration of MeHg in fish is thus under control of the activity of HgII methylating bacteria, the concentration and availability of HgII for these bacteria (i.e. speciation of dissolved, adsorbed and solid HgII), as well as of the rate of MeHg demethylation.42 Because all these factors vary among ecosystems, so will the expected net methylation rates of HgII. The rates for HgII methylation and MeHg demethylation in natural environments are traditionally described by pseudo first-order kinetic models (Equation 1) where the rates of methylation and demethylation, rm and rd, are calculated as the products of concentrations of HgII and MeHg, and the methylation and demethylation rate constants, km, and kd (d-1), respectively.45 Typically the rate constants, km and kd, are experimentally determined using isotopically enriched aqueous AHgII and MeBHg tracers. Figure 3 illustrates the expected MeHg/HgII ratio for AHgII and MeBHg as a function of time, following first-order kinetics (Equation 1). The rate constants are typically determined within the timeframe when rm>>rd for AHgII and rm<<rd for MeBHg (typically 1-48 h). By assuming negligible demethylation and methylation of formed MeAHg and BHgII, respectively, during this time period, km and kd can be calculated by Equation 2 and Equation 3, respectively. For the calculation of km, the pool of HgII is assumed to be several orders of magnitude larger than the pool of MeHg formed and can be approximated as constant during the time of incubation. 14 Figure 3. Expected MeHg/HgII ratio as a function of time as a consequence of firstorder methylation and demethylation of the AHgII and MeBHg tracers, enriched in isotope A and B, respectively. A situation is described where steady state is reached with rm = rd. Equation 1 [ [ ] ] ] [ [ ] Equation 2 [MeHg] [ ] Equation 3 ( [ ] [ 15 ]) [ ] ) In paper II, km and kd, were instead calculated by fitting a nonlinear reversible reaction model, Equation 5 (integrated from Equation 4), to determined MeHg concentrations (formed from a HgII tracer) as a function of time (Figure 1 in Paper II). This approach does not require the assumptions made in Equation 2 and Equation 3 and allows estimating rate constants also for changes in ambient Hg. Experimental conditions may induce a net methylation of ambient Hg as a consequence of changes in the environmental conditions (increased temperature and mixing of sediment slurries). In paper II, we were able to compare km determined for ambient Hg and km determined for traditional aqueous AHgII tracers and our newly synthesized solid/adsorbed tracers. Due to the typically small net methylation of ambient Hg, the km values were associated with large uncertainties and the approach is thus primary useful for method development and evaluation purposes. In our experiment, the km values for ambient Hg were 20-30% lower when calculated from Equation 2, as compared when calculated from Equation 5. This suggests that by neglecting demethylation a reasonably small (considering the experimental complexity and typical variability associated with determination of km), however statistically significant, error is induced. The magnitude of this error is expected to vary considerably between samples depending on the magnitude of the methylation and demethylation rates. The nonlinear reversible reaction Equation 4 [ [ [HgII ] ) ] Hg] ) [ ][ [ [HgII ] ) ] Hg] ) Equation 5 [ Hg] ) ) ( ( )[ ) ( 16 )) [ ] ] model requires a larger minimum number of data points compared to the traditional approach, based on Equation 2 and Equation 3, and the latter approach may thus be more practical in large scale surveys and monitoring studies. The AHgII and MeBHg tracers are typically added as labile aqueous species at concentrations corresponding to 10-100 % of ambient MeHg and Hg.50 The current consensus concerning the availability of HgII for uptake in bacteria responsible for methylation is that i) dissolved complexes of HgII constitute the available pool (neutral Hg-S and specific Hg-thiol complexes have been suggested as particular available)44, 48, 101 and ii) precipitation and adsorption of HgII to the solid and adsorbed phases limit the pool available for methylation.92-94 It is generally assumed that added aqueous tracers have a higher availability than ambient HgII.45,50 This have also been experimentally supported (Paper II).45 The terms potential, specific or conditional rate/rate constant have thus been used to acknowledge the presumably overestimated km.50 For the determination of biogeochemically more relevant values on km and kd, we have proposed solid and adsorbed phase isotopically enriched Hg tracers to be used (Paper II, see 2.2.3) As discussed below (see 3.2); there are reasons to consider, in contrary to the general view, the existence of a sediment MeHg pool that is not readily available for demethylation. Assuming the presence of HgII and MeHg pools that are not readily available for methylation and demethylation reactions, Equation 1 should include one second term for HgII and one for MeHg (Equation 6) in addition to the once describing pools readily available for methylation, HgIIA and MeHgA. Equation 6 [ [ [ ] ] ] [ [ 17 ] ] [ [ [ ] ] ] 1.1.3 Determination of methylation rate constants using solid or adsorbed chemical forms of HgII (paper II) In paper II, we synthesized the following solid and adsorbed HgII isotope tracers; α-199HgS(s), β-201HgS(s), HgII reacted with Mackinawite (≡FeS200 HgII or ≡FeS-202HgII), and HgII bound to natural organic matter (NOM196 HgII). These tracers were incubated in brackish water estuarine sediment slurries together with the traditionally used aqueous HgII nitrate tracer, 198 Hg(NO3)2(aq). Determined average km values are shown in Equation 7 and followed the order; β-201HgS(s) < α-199HgS(s) < ≡FeS-202HgII < NOM-196HgII < 198Hg(NO3)2(aq). The constants were calculated using the nonlinear curve fitting of Equation 5 and thus a km value could also be assigned for ambient Hg (0.011 ± 0.005 d−1), calculated from a small increase in the MeHg/HgII ratio (an experimental artifact due to disturbance of sediment layering and increased temperature). As a comparison, a km value of 0.010 ± 0.0011 d−1 for ambient Hg was calculated from rate constants determined from solid/adsorbed tracers and with the distribution of ambient HgII between solid (HgS) and organically adsorbed phases (Hg-NOM) as determined using Hg LIII-edge EXAFS. The good correspondence between the measured and calculated values of km for ambient Hg is a strong support for the new methodology used. It was concluded that specific solid and adsorbed HgII tracers are much better representatives of ambient Hg than aqueous phase tracers like 198Hg(NO3)2(aq), which yielded a km 12 times higher than the value estimated for ambient Hg. It was furthermore shown that net methylation of solid/adsorbed tracers, in addition to thermodynamic properties of solid/adsorbed HgII phases, was controlled by the kinetics of dissolution/desorption (Figure 4 in paper II). Equation 7 ) ) [ [ [ ) )] 18 [ ] ] ] Applying this solid/adsorbed-phase tracer methodology to other systems requires knowledge of the chemical solid/adsorbed-phase speciation of ambient HgII in the sample. Even though current approaches to obtain such information (Hg-EXAFS measurements, sequential extraction methods, or chemical equilibrium modeling) have constraints, they can be used to make qualified assumptions about the speciation of Hg. For the sediment used in papers II-IV, Hg LIII-edge EXAFS measurements (and speciation modeling) suggested a solid-phase speciation of 70 % as β-HgS(s) and 30 % as Hg(SR)2 (paper II). In paper III and IV we demonstrate how the proposed approach also can be applied to differentiate the reactivity of different geochemical pools of Hg in systems of larger scale. 1.2 Scale of experiment – from micro- to mesocosms A goal in science is to recognize and determine the causality in order to be able to explain, predict and understand ongoing or coming natural phenomena. This requires experiments at multiple scales and with variable and increasing complexity.95-97 Microcosm (micro = small; cosm = world) provides less complex and more controlled conditions, giving an opportunity to study individual processes than cannot be singled out in larger scale experiments. According to scaling theory, some patterns and processes will however only be evident over a certain threshold of scale and complexity.95 The number of experiments conducted at mesocosm (meso=intermediate) or field scale have thus increased during the last 30 years.97 The mesocosm experiments summarized by Petersen et al.97 had a median volume of 1.7 m3 and a median duration of 49 days. As concluded by the authors, this is a small and brief scale in relation to the physical and time scale of ecosystems. They further identified the presence of walls as a problem since the biological, material and energy exchange with the outside world is restricted and the walls also provide surfaces for growth of artificial edge habitats. The third and last main limitation of mesocosm experiment originates from experimental artifacts arising from the decisions made by the experimental designer (i.e. number of replicates, size, duration, control of additives etc). It should be noted that field and whole ecosystem experiments also suffer from scale dependence since all ecosystems vary in physical scale, manipulations are done by experiment designer and the time scale of experiments /monitoring is limited. 19 We studied methylation of solid and adsorbed phases of HgII in microcosm (up to 0.005 L of sediment slurries; paper II) as well as in mesocosms (2000 L of water and intact sediment cores; papers III-IV). Even though absolute rates of net methylation between tracers differed, the order and the relative differences of availability for methylation of the tracers was the same in micro- and mesocosms (Table 3, 3.1). Similar conclusions concerning the availability of solid/adsorbed HgII phases can thus be drawn from both scales. This illustrates that traditional microcosm incubation for determination of km and kd are useful experimental tools that do reflect environmental processes occurring also in larger scale. This is not obvious since sediments are dynamic and complex systems with a drastic change in chemical properties with depth. Thus, mixing of sediment into slurries likely alters the chemical and biological properties of the material. Important differences between the microcosm sediment slurries and the mesocosm experiment were: i) the use of intact sediment cores in the mesocosm study (keeping the natural redox gradient and presumably bacterial community structure), ii) establishment of a pelagic‒sediment coupling in the mesocosm systems and maintenance of a continuous supply of autochthonous organic carbon to the benthic zone, and iii) that atmospheric and terrestrial loadings of HgII and MeHg could be simulated in a realistic way in the mesocosm. The combination of molecular scale detail (i.e. solid phase speciation of Hg II and MeHg) with the more complex meso-scale experimental system help to significantly improve our biogeochemical understanding of Hg in natural, complex systems. 20 3. Mercury methylation, bioaccumulation evasion and This thesis contains a summary of three experimental studies, as illustrated in Figure 4, covering the processes of mercury methylation, demethylation and bioaccumulation. Figure 4. Illustration summarazing the three experimental studies in this thesis 21 3.1 Methylation of HgII Mercury methylation in sediments is mediated by specific strains of sulfate and iron reducing bacteria.12-15 It is generally accepted that methylation of Hg occurs inside the cell,98-99 even if the transportation mechanisms of HgII through the cell membrane is not clear. Different dissolved complexes of HgII have been suggested to be available for uptake by methylating bacteria including neutral Hg-sulfide complexes and Hg complexes with specific low molecular mass thiols.44,48,100-101 Nano-particulate (colloidal) HgS(s) has recently been proposed to be directly available for bacterial uptake, as judged from studies using pure bacterial cultures.46,102 Proposed mechanisms for uptake of such particles are however lacking. In accordance with bacterial culture studies, we detected methylation in sediment slurries of HgII likely originating from nanoparticles (<0.02 µm) of α-HgS(s) (paper II). Our study showed that methylation of solid/adsorbed HgII phases is controlled by thermodynamics and as well as kinetics of HgII dissolution/desorption. The higher availability for methylation of nano-particualte HgS(s) than crystalline micro-particulate HgS(s) observed in previous bacterial culture experiments46,102, might thus also be explained by higher desorption rates from smaller particles instead of a direct bacterial uptake of HgS(s) nanoparticles. Until further evidence for direct bacterial uptake of HgS(s) nano-particles can be demonstrated, it is reasonable to retain the consensus stating uptake of only dissolved HgII species. The phase distribution of HgII in sediments is largely shifted to the solid and adsorbed phases (typical solid-liquid partition coefficient, Kd, of Hg in sediments is 103.5-6 (L kg-1)).43, 68 The main chemical forms of HgII in these phases include HgII adsorbed to thiol groups in natural organic matter,65,103 or at the surfaces of FeS(s) minerals104 and incorporated in the crystalline Hg phases cinnbar (α-HgS) and metacinnabar (β-HgS).105 Remarkably few studies have discussed, or studied in detail, the importance of solid phase speciation, even though it has been generally accepted that precipitation and adsorption of HgII are important processes limiting Hg methylation.42-45 Dissolution of HgS(s) and desorption of HgII from surfaces are to a large extent controlled by the composition of the pore water chemistry.103,106-107 Formation rates of MeHg, derived from complex natural system at realistic conditions, are thus required to evaluate different solid and adsorbed HgII 22 species contribution to MeHg formation. In papers II-IV we provide such quantitative data, which previously have not been available (Table 3; net methylation represented as the MeHg/HgII molar ratio, further discussed in paper III). We conclude, that the solid/adsorbed phase speciation of HgII is a major controlling factor for rates of MeHg net formation. This was shown in traditional sediment slurries (paper II) as well as in mesocosm systems with intact sediments (i.e. maintained natural redox gradient, presumably maintained bacterial community structure) and a continuous supply of autochthonous organic carbon to the benthic zone from pelagic food webs with different structure and productivity. The higher availability of HgII-NOM to methylating bacteria, as compared to HgS(s) phases (papers II-IV, Table 3) can be explained by the higher thermodynamic stability of HgS(s). As shown by EXAFS measurements,66 HgII bind to NOM by two-coordinated complexation to thiol-groups, and when these are saturated, HgII binds to weaker O/N sites. The estimated concentration of thiol-groups (RHS) in the NOM material used in papers IIIV (~25 µmol RHS g-1 NOM)79 and the concentrations of HgII in the HgIINOM tracer (~3 µmol g-1 NOM) suggest a supply of thiol-groups large enough for the formation of a HgII-(SR)2 complex. In the mesocosm systems (papers III and IV), we observed higher net methylation rates in the sediment of 204HgIIwt (204HgII(aq) added to the water of the mesocosm) than of the Table 3. Average net methylation, as MeHg/HgII ratio (± Standard Error,SE), of HgII determined in paper II (n=5) and paper III-IV (range for 3 mesocosm treatments, n=3-9) Paper II 198 196 β- Hg (aq) II Hg -NOM 201 α- Papers III-IV II HgS(s) 199 HgS(s) ≡FeS- 200 Hg II Ambient Hg 0.96 (0.004) 204 HgIIWt 0.050 (0.003) 201 II 0.0054 (0.0007) β- 0.026 (0.006) – 0.045 (0.01) Hg -NOMsed 0.0077 (0.0008) – 0.0092 (0.001) 200 0.00040 (0.00003) – 0.00067 (0.0001) HgSsed 0.0078 (0.0008) 0.044 (0.004) 0.0087 (0.0002) Ambient Hg 23 0.0068 (0.0007) – 0.0085 (0.0008) 201 HgII-NOMsed tracer (injected 5 mm below the sediment surface). As discussed in paper III, we suggest that 204HgIIwt is deposited to the surface of the sediment as primary bound to NOM particles present in the water column and that differences in binding strength to the NOM is a contributing cause for the higher net methylation of 204HgIIwt compared to 201HgII-NOMsed. The variation in reactivity between different types of HgII-NOM complexes is however most likely smaller (because Hg will always bind to an excess of RSH groups with similar binding strength) than the difference in reactivity between HgII-NOM and β-HgS(s). For HgII reacted with Mackinawite (FeS(s)), the availability for methylation of a newly prepared tracer was similar as of 196HgII-NOM (paper II). The availability of the ≡FeS-202HgII tracer when it had been aged for 24 days before the incubation was however lower and similar to the availability of β-HgS(s), suggesting a gradual dissolution of the Mackinawite by HgII and precipitation of β-HgS(s) (as previously shown in adsorption104 and Hg EXAFS studies79). Our results support the idea that precipitation of β-HgS(s) in sediment is an important “sink” for HgII that limits the bioavailability of HgII for methylating bacteria.92-94 Pure β-HgS(s) is metastable at temperatures below 315°C but only slowly transforms to α-HgS(s).108 The inclusion of impurities also affects the stability of β-HgS(s) in natural systems. It is plausible that βHgS(s) precipitated in sediment pore water, with a complex chemical composition, is less stable (shows a greater solubility) than commercially available β-HgS(s) and β-HgS(s) precipitated in more pure model systems (MQ water). Further, β-HgS(s) is (as typically for sulfur minerals) a nonstoichiometric solid and differences in the stoichiometry (i.e. Hg/S ratio) may be a second cause of differing availability between β-HgS(s) phases. Indeed, differentiated solubility of β-HgS(s) phases has been demonstrated in laboratory experiment.109 In addition to the solid/adsorbed HgII speciation, MeHg formation is controlled by additional environmental processes limiting or enhancing the bioavailability of HgII or the activity of methylating bacteria. In field studies, variations in MeHg formation and concentrations among sites have been correlated to the concentrations of dissolved sulfide, NOM and to pH.42 The effects of these chemical factors are complex since they may affect MeHg formation in multiple ways. For example, NOM immobilizes HgII in sediments by adsorption42,66,106 but may also increase the solubility of β24 HgS(s),106 inhibit β-HgS(s) precipitation, and enhance bacterial activity, resulting in a potentially increased methylation rate.110 Further, specific low molecular mass HgII-thiols have been suggested to be available for methylating bacteria.100-101 The possible HgII species accumulated and methylated by bacteria in natural environments are still under debate mainly due to the uncertainties in the chemical speciation of HgII in pore water.49 For sulfide, correlation to MeHg concentrations has been suggested to be an effect of decreased availability of HgII due to a higher concentration of charged dissolved HgII-sulfide complexes at higher concentrations of sulfide.48,92,111 Finally, the observed correlation between MeHg concentration in sediments and pH has been suggested to be caused by an increased association with solid phases of HgII at lower pH values, thus limiting the availability of HgII.112 Climate change scenarios for the Baltic Sea region predict an increased terrestrial input of allochthonous NOM and nutrients to lakes and estuaries.113 This may fuel the pelagic bacterial pathway114-116, reduce phytoplankton primary production and cause a shift from a phytoplankton based to a bacteria based pelagic food web with decreased sedimentation of autochthonous NOM as a consequence. We hypothesized that this could decrease the activity of methylating bacteria and thus also MeHg formation. In the reversed direction, we hypothesized that increased sedimentation of autochthonous NOM, caused by an increased biomass from increased nutrients load to lakes and estuaries as a consequence of eutrophication,117 could increase the production of MeHg. It is obvious from the number of factors influencing MeHg formation and as discussed later, its bioaccumulation, that properly conducted meso- and large scale experiments are needed if the effect of e.g. climate change or eutrophication is to be predicted. In paper IV, methylation of geochemical Hg pools in mesocosm model ecosystems with different pelagic food web structure and productivity are discussed. In the experiment, three different treatment schemes were applied: high and low addition of nutrients (referred to as NPhigh and NPlow, respectively) and addition of a humic soil extract (simulating an increased terrestrial load of humic material, referred to as HSE). For NPhigh mesocosms, fluctuations in the net formation of MeHg from 201HgII-NOMsed tracer correlated to that of primary production in the pelagic zone (measured as primary production rate or chlorophyll α), whereas only small fluctuation 25 in net Hg methylation and primary production was observed in HSE mesocosms. This shows that net methylation of HgII may respond quickly to changes in pelagic productivity (days in these mesocosm systems). The fluctuation in Hg methylation observed for β-200HgSsed was less pronounced than for 201HgII-NOMsed. This suggests that formation of MeHg from β200 HgSsed tracer was limited by a slow rate of dissolution of HgII from the solid phase i.e. the dissolution process was the rate limiting step. Interestingly, net methylation of 204Hgwt (simulating recent atmospheric and terrestrial HgII loads) increased with time in HSE mesocosm and did not show the same pattern as the 201HgII-NOMsed tracer. The higher (however not statistically different) average net methylation of 204Hgwt tracer in HSE was opposite to the hypothesis proposed prior to the experiment, expecting a lower net methylation of also recent HgII loads due to a lower primary production. A number of different possible explanations are discussed in paper IV. The results in paper IV again emphasize the importance of the chemical speciation of solid/adsorbed forms of HgII. It is clear that depending on the chemical speciation of solid/adsorbed HgII, ecosystems can be expected to differ with respect to the outcome and magnitude of the response to environmental changes. 3.2 Demethylation of MeHg Processes of MeHg demethylation in surface waters include both biotic and photo induced abiotic mechanisms.39,118-119 In sediments, demethylation has been ascribed mainly to biological processes.39,120-121 Significant abiotic demethylation has also been suggested, but a mechanistic understanding is lacking.122-123 In the mesocosm systems (paper III), we report steady-state MeHg/HgII ratios in the sediment obtained from net demethylation of the Me198Hg-NOMsed tracer, and net methylation of HgII solid/adsorbed phase tracers as well as of ambient Hg (during the 52 days on experiment). Based on these quotients it was estimated that up to 30% of the Me198Hg-NOMsed tracer was not readily available for demethylation. This observation is consistent with previous findings from Marvin-Dipasquale et al.124 An initial quick demethylation of added tracers (also observed in papers III-IV and by Marvin-Dipasquale et al.), has been used in other studies to determine the typical MeHg turnover, (km+kd)-1 of 1-3 days.125 These turnover rates are however misguiding. They are determined from the initial decrease in MeHg 26 when the rate of demethylation is highly exceeding the rate of methylation (rm << rd, Figure 3), as controlled by the high availability of MeHg tracer added as an aqueous labile complex, and do not take into account the pool of MeHg not readily available for demethylation. Instead, turnover rates determined from the Me198Hg-NOMsed tracer (paper III, SI) were on the order of 90 days. It is still uncertain if the mechanism for stabilization of MeHg (making it less available for demethylation), simply is formation of complexes with thiol-groups in NOM, or if additional processes are involved. As illustrated in paper III, these processes are potentially very important for the amount of MeHg accumulated in biota and further research to clarify mechanisms for MeHg stabilization in sediments is warranted. 3.3 Evasion of Hg In paper I, evasion of gaseous chemical forms of Hg, i.e. Hg0, MeHg and DMHg, was determined from sediment˗water microcosm systems containing sediments contaminated with Hg from chloro alkali industry and pulp from paper industry. Emission of MeHg(g) (chemical speciation modeling suggested evasion of MeHg as a neutral CH3HgSH0 complex) was characterized by a transient trend (Figure 2 in paper 1) with highest emission rates reached after 12 days (110 ± 41 and 140 ± 51 fmol h-1 for ambient MeHg and MeHg formed from added 201HgII(aq) tracer, respectively). This transient trend is similar to trends for MeHg concentrations in other sediment incubation experiments (e.g. Figure 1 in paper II). Also, the sediment concentration of ambient MeHg increased 3 times during the course of the experiment whereas the gaseous emission of ambient MeHg was significantly higher in the beginning of the experiment. Our data thus suggest that gaseous emission of MeHg in sediment is controlled by recently methylated MeHg rather than by the total pool of MeHg in sediment. Indeed, estimated sediment−water flux of MeHg from costal marine systems reveals variations among sites and also seasonal variations have been observed.39,126130 At sites in the continental shelf of southern New England, the seasonal variation in MeHg flux was also correlated to seasonal changes in MeHg gross production, in line with our observation.127 As previously discussed adsorption of MeHg to e.g. NOM particles may possibly stabilize MeHg and prevent demethylation (see 3.2). Adsorption of MeHg to solid phases may also be the reason for the higher sediment concentration, but lower evasion, 27 of ambient MeHg compared to Me201Hg from the microcosms observed in paper I. Treatments of the microcosms (dark, light and dark with addition of acetate) did not cause any significant difference in MeHg evasion. For the evasion of Hg0, the treatments suggested a predominance of photo induced oxidation of Hg0 rather than reduction of HgII in this system (light radiation from a tungsten lamp giving radiation in the visual spectral range with an overall lower intensity than solar radiation). The transport of Hg from sediment to water column occurs via diffusion, advection and/or resuspension of particles.131 The importance of in situ gross MeHg production, aqueous MeHg speciation and total concentration of MeHg in the sediment for the sediment−water mass transfer of MeHg can thus be expected to vary among ecosystem depending on the dominant transportation mechanism. 3.4 Bioaccumulation of mercury Both HgII and MeHg are accumulated in micro-sized seston but little is known about the underlying mechanisms. Current literature suggests passive diffusion of lipophilic mercury species such as HgCl2, CH3HgCl and low molecular mass thiol complexes of MeHg into plankton cells.132-135 The similar abilities of HgCl2 and CH3HgCl to pass lipophilic membranes suggest that these chemical forms should have similar accumulation efficiencies.134 MeHg and HgII are however distributed differently within the cells and this result in a higher transfer efficiency of MeHg.134,136 The fraction of total Hg occurring as MeHg thus typically increases from 0.31.5% in phytoplankton to 2-22% in zooplankton (data compiled by Mason et al.38) and >90 % in piscivorous fish.39,137 In paper III and IV, we quantified HgII and MeHg accumulated in seston and benthic invertebrates (Chironomids, Amphipods, Polycheates and Bivalves), after 8 weeks of experiment, from ambient Hg, and from HgII and MeHg tracers added to the brackish water-sediment mesocosms. The accumulation is presented as the biota−sediment accumulation factor (BSAF), which is the 28 Table 4. Accumulation of Ambient Hg (Hg occuring as MeHg (%), MeHg-BSAF and HgII-BSAF) and stable isotope analysis (δ13C and δ15N (‰)) in seston and benthic invertebrates from mesocosm experiment systems (± 1 SE). MeHg (% of Hg) BSAF MeHg BSAF HgII δ13C (‰) δ15N (‰) Seston 50-100 µm 100-300 µm 300 µm 8.6 (4.0) n=9 4.8 (2.2) n=9 0.39 (0.06) n=9 n=8 n=9 n=8 16 (5.3) 6.7 (4.7) 0.15 (0.04) n=7 n=9 17 (10) 7.5 (4.3) 0.19 (0.06) n=8 -23 (1.6) n=8 n=7 -25 (1.5) -20 (1.5) n=5 8.1 (0.4) n=8 n=7 8.8 (0.5) 9.4 (1.1) n=5 Amphipoda 63 (11) n=3 22 (6) n=8 0.063 (0.050) n=4 -19 n=1 7.3 n=1 Polycheate 29 (9) n=9 36 (14) n=9 0.58 (0.08) n=9 -22 (0.3) n=9 9.4 (0.1) n=9 Mussel 8.6 (0.5) n=9 28 (2) n=9 2.2 (0.2) n=9 -22 (0.2) n=9 7.1 (0.1) n=9 Chironomidae 5.6 (1.5) n=4 16 (2.2) n=7 2.2 (0.3) n=5 -22 (0.3) n=5 8.5 (0.1) n=5 concentration ratio of HgII or MeHg between biota and sediment (pmol g-1 d.w./pmol g-1 d.w.). Accumulation in seston is typically given as the biota accumulation factor (concentration ratio between biota and water), but because the concentration in the water was below the detection limits for most tracers, BSAF was used also for seston. The average percent of ambient Hg occurring as MeHg, MeHg-BSAF and HgII-BSAF for ambient Hg, and δ13C and δ15N (‰) (used to evaluated trophic and foraging dynamics) in seston and benthic invertebrates are summarized in Table 4. Seston (suspended material including living organism as well as inorganic and organic particles138) was collected with plankton nets at size fractions of 50-100, 100-300 and >300 µm. The δ15N value in seston was comparable to the values in benthic invertebrates. This is similar to findings by Eagles Smith et al139: chironomids, amphipods and seston with a size over 80 µm (assigned by the authors as zooplankton) had similar δ15N values whereas the ratio in phytoplankton was lower. This suggests that primarily zooplankton species made up the seston fractions collected (> 50 µm) from the mesocosm. The fraction of total Hg occurring as MeHg in seston collected (Table 4) was also within the range typical for zooplankton (2-22 %).38 Traditional paradigms envision production of phytoplankton to constitute the base of aquatic food webs140 and the concentrations of MeHg in fish to be a 29 consequence of dietary exposure of Hg throughout the food web.16,141 Bioaccumulation and magnification schemes and models are therefore often based on MeHg entering the food web by accumulation in phytoplankton from surrounding water. MeHg and HgII accumulating in pelagic plankton will thus originate from either the sediment via advection, diffusion and resuspention of particles or from terrestrial and atmospheric sources.131 Even though fish concentration of MeHg typically increases with trophic level,17-18 large variations are found among ecosystems and species positioned at the same trophic level.18,139,142 Factors regulating the production of MeHg, the entry of MeHg into the food web as well as the trophic transfer of MeHg have been suggested to explain these variations.139,142 The relative importance of these factors is however poorly understood.131,142-143 Factors suggested includes e.g. concentration of dissolved organic carbon (DOC),110,135 pH,144 rates of primary production,145-146 atmospheric deposition of sulfate147 and of HgII 27-28 as well as the growth rate148 and age149 of the biota and the pelagic food web structure.18 As discussed in paper IV, we observed higher accumulation of ambient MeHg, and MeHg originating from Me199Hgwt and 204HgIIwt tracers in seston in HSE compared to NPlow and NPhigh treated mesocosm. This may to some extent be explained by a higher concentration of DOM circulating in the water column, complexing and keeping the concentrations of Hg and MeHg added as aqueous tracers at a higher level in the water phase of HSE mesocosms. Even though higher rates of sedimentation were observed in HSE mesocosm, the sedimentation of Hg and MeHg obviously was overridden by the effect of higher concentrations of DOC in the water column per se. As discussed in paper IV, this was likely not the only explanation for the higher MeHg concentrations in seston originating from Me199Hgwt and 204HgIIwt tracer. Additional plausible factors that may have contributed include algal bloom dilution150, a higher degree of accumulation of MeHg-DOM complexes by bacteria and/or larger biomagnification due to an additional trophic level151 introduced in HSE mesocosm. Several studies have stressed the importance of pelagic food web couplings to the benthic zone for trophic transfer of nutrients and energy152 as well as MeHg.137,139,142-143 Benthic organisms can accumulate MeHg from the dissolved MeHg fraction and via sediment ingestion.153 Aquatic organisms feeding on benthic invertebrates, so called benthivores, thus provide a 30 secondary pathway for the transfer of MeHg from sediment to the pelagic food web (in addition to MeHg entering the food web via accumulation in phytoplankton after transfer of MeHg from sediment to water). In the reversed direction, benthic organisms feeding on deposited planktonic material and necrophages may forage on fish carcasses with a high MeHg concentration. Together, the pelagic-to-benthic and the benthic-to-pelagic foraging results in a trophic feedback cycle of MeHg that not only preserves MeHg within the biota compartment, but may also result in higher MeHg levels in benthivores and piscivorous fish.142 Figure 5 illustrates the trophic transfer pathways in the aquatic food web. Amphipods feed both on suspended particulate matter in the water column by filtration, and detritus and sediment by deposit feeding.154-155 Amphipods showed higher MeHg-BSAF and HgII-BSAF for Me199Hgwt tracer, and lower for Me198Hg-NOMsed added 0.5 cm below the sediment surface, in comparison to the other benthic invertebrates (Figure 6 and Figure 7). Figure 5. Illustration of biaccumualtion and biomagnification of MeHg from sediment and water to the benthic and pelagic foodweb. Solid lines represents abiotc transportation processes and dashed lines bioaccumulation and magnification. 31 This suggests that the Amphipods to a larger extent feed on material originating from the water column in comparison to the other benthic invertebrates. Chironomids and Bivalves (mussels), well-known filter feeders, had similar concentrations of MeHg and HgII originated from the tracers and from ambient Hg. They also had a similar fraction of Hg occurring as MeHg (Table 4). Polychaetes (ragworms) had higher %C, %N, δ15N (‰) as well as a generally higher MeHg-BSAF of sediment tracers. This suggests that Polychaetes, by their digestion of sediment, were exposed for higher concentrations of MeHg than chironomids and bivalves that primary filter feeds. Sediment digestion as a primary exposure route of Hg for Polychaetes have also previously been shown.153 As shown in Figure 6 and Figure 7, HgII and MeHg from tracers added to the water (Me199Hgwt and 204HgIIwt) accumulated to a higher extent than tracers injected into the sediment (MeHg196Hg-NOMsed, 201HgII-NOMsed and β200 HgSsed) in both seston and benthic invertebrates. We therefore conclude newly imported HgII and MeHg from terrestrial and atmospheric sources to be more available for accumulation in seston and benthic invertebrates than HgII and MeHg previously accumulated in the sediment or MeHg formed in situ from previously accumulated HgII. Furthermore, benthic invertebrates accumulated MeHg from the MeHg196Hg-NOMsed tracer and MeHg formed from 201HgII-NOMsed and β-200HgSsed tracers to a much higher extent than seston. This suggests that benthic invertebrates may play an important role in transferring MeHg accumulated or in situ formed in the sediment to the pelagic food web. Our results in papers III and IV thus emphasize that the traditional bioaccumulation and biomagnification pathways of mercury (MeHg in water → phytoplankton → zooplankton → fish) are too simplified. 32 Figure 6. MeHg and HgII accumulation from tracers added 0.5 cm below the sediment surface in seston and benthic invertebrates (shown as MeHgand HgII-BSAF ± 1 SD) 33 Figure 7 MeHg and HgII accumulation from tracers added to the water column in seston and benthic invertebrates (shown as MeHg- and HgIIBSAF ± 1 SD) 34 4. Implication and final remarks In papers I-IV we concluded that: the solid and adsorbed speciation of HgII is a principle factor controlling the rate and net methylation of Hg terrestrial and atmospheric sources of HgII and MeHg are more available for methylation, as well as for bioaccumulation, than sediment pools of HgII and MeHg a fraction of MeHg in sediments is not readily available for demethylation or evasion, but still available for bioaccumulation in benthic invertebrates Extensive efforts have been undertaken to reduce anthropogenic emissions of Hg since the health effects of MeHg showed in e.g. pollution catastrophes (Minamata, Japan, 1950’s and Iraq, 1970’s).35,156 These actions have indeed resulted in decreased atmospheric depositions of Hg and downward trends of mercury concentration in fish in Sweden and the USA, for examples, have also been observed.4,32-34,157 While further efforts are planned, negotiated and under implementation there are still large uncertainties how further decreased anthropogenic Hg emissions will affect MeHg concentrations in fish.37 Two main concerns are that i) the response time for levels of MeHg in fish may be on the order of decades or up to centuries due to a continuous leakage and export of Hg stored in soils, and that ii) decreased anthropogenic depositions may be counteracted by other environmental changes such as climate changes and eutrophication.25,31,33 In the METALLICUS (Mercury Experiment to Assess Atmospheric Loading in Canada and the United States) project, the response time of reduced atmospheric depositions has been simulated in mesocosm and whole ecosystem scale experiments.25,27-28 It was concluded that HgII deposited directly to the water surface was quickly methylated. The increase of the concentrations of Hg in fish was immediate, suggesting a very fast response time between changes in rates of atmospheric Hg deposition and Hg concentrations in fish. As pointed out in the METALLICUS studies, the fast response time is only true for systems receiving the major Hg input from the 35 atmosphere as a load directly onto the water body, and not indirectly via runoff from terrestrial ecosystems. For aquatic systems with a relative large watershed area, the response time may be delayed up to centuries due to the legacy of Hg stored and gradually leached and exported from soil. In the METALLICUS whole ecosystem study, isotopically enriched Hg were also added to the watershed (forest and wetland), however these loadings could not, during 3 years after first load addition, be detected in the biota.25 Table 5 summarizes literature data on the relative contribution from terrestrial and atmospheric sources of Hg (note: also including Hg0) and MeHg to different aquatic systems. As shown, terrestrial imports of Hg is higher than atmospheric imports in most estuaries and lakes where the loadings of Hg has been modeled. Transfer of MeHg from sediment to the water systems, determined using flux chambers or pore water MeHg concentration gradients, is typically interpreted as net methylation of Hg accumulated in sediments.39, 129-130 Thus, the possible mobilization of MeHg from sediment into the water phase is neglected. We show that HgII recently deposited to the sediment surface is more readily available for methylation processes than the already accumulated pool of HgII (paper III). It is also shown that newly formed MeHg was the main source of MeHg evasion from the sediment system (paper I). Based on our results, we suggest that recently (months-years) deposited HgII and MeHg contribute to a significantly higher degree to sediment-water fluxes than HgII and MeHg already stored in sediments for a longer time. Separating the contribution from recent and past Hg deposited deposition from field observations is however challenging. It emphasizes the need for quantitative data on the availability of specific geochemical pools of Hg for methylation and bioaccumulation. Such data were successfully derived from our mesocosm scale system, allowing modeling of MeHg formation and bioaccumulation in unprecedented detail. Studies in the METALLICUS project are loading experiments where the atmospheric deposition of Hg is simulated by isotopically enriched, aqueous HgII tracers. Thus, the study is restricted to a comparison of the reactivity of recent, labile Hg loadings with the reactivity of the entire Hg pool (i.e. ambient Hg) without differentiating between younger and older fractions (corresponding to recent and past loadings) of the sediment pool. 36 Table 5. Terretrial/atmospheric ratios for import of total Hg and MeHg to the water body of oceans, estuaries and lakes. The total contribution from terrestrial and atmospheric sources to the total Hg and MeHg import to the water are given in paranthesis. Terrestrial/Atmospheric input ratios (100·(Terrestrial+Atmospheric)/(Total inputs)) Ref total Hg MeHg Ocean Global (pre. industrial) Global (current) Estuaries Global Estuarine San Francisco Bay Tokyo Bay Long Island Sound NY/NJ Harbor Estuary Chesapeake bay Lakes Superior Michigan Onondaga Little Rock Lake Clear Lake Lake Champlain Big Dam West Spring Lake 158 0.030 (100 %) 0.065 (100 %) 158 159 160 161 162 163 164 165 165 165 165 166 167 168 169 1 (98 %) 1.5 (6.4 %) 1.9 (19 %) 7.9 (100 %) 31 (100 %) 1.6 (79 %) − − (<4 %) − 6.9 (33%) 27 (76 %) 4.2 (30 %) 0.6 (87 %) 0.31 (44 %) 310 (91 %) only atm. (40 %) 188 (100 %) 1.6 (100 %) 10 (74 %) 0.09 (93.9 %) only terr. (26 %) − (0 %) only terr. (6 %) − (0 %) − − only terr. (91 %) 0.51 (15 %) In papers III-IV, we constructed simple mass balance budgets to illustrate different scenarios in an estuarine environment. (Figure 8, Paper III (Figure 5 and Table 1), Paper IV (Figure 5)). The origin of MeHg in sediment and biota was calculated from the determined ratios of net methylation and demethylation, and the Biota Sediment Accumulation Factors (BSAF) derived from specific HgII and MeHg tracers. These tracers simulated more recently imported HgII and MeHg from atmospheric and terrestrial sources, as well as older, stored sediment pools of HgII and MeHg. A challenge when applying these types of models is the selection of scales, including the time and the depth in the sediment at which methylation and demethylation reactions are considered most active. We used calculated cumulative terrestrial and atmospheric loads of HgII and MeHg, typical for estuarine environments during a 2 months period, and an active sediment layer of 1.5 cm in our model to match the experimental scale from which our quantitative data was derived. Since sediments store the largest reservoirs of 37 Hg in lakes and estuaries, the mass of sediment considered as “active” can be expected to largely impact the results of Hg mass balance budgets. For estuarine mass balance budgets, “active” sediment layer of 1 and 15 cm has previously been assumed for Chesapeake and San Francisco Bay, respectively160,164 and the timescale is typically year-1.160-164 It is easy to understand that it has been difficult to establish a clear relationship between MeHg in fish and the concentrations of Hg or MeHg in sediment among ecosystems when comparing the mass budget of MeHg in sediment and biota (Figure 8) and by looking at the variations of terrestrial and atmospheric inputs among ecosystem (Table 5). Because of differences in the availability for methylation and bioaccumulation, specific geochemical Hg pools give very different predicted contributions to MeHg in sediment, seston and benthic organisms (Figure 8, Paper III (Figure 4-5)). Since such data have not previously been available, we need to reevaluate the importance of sediment pools versus newly imported Hg from atmospheric and terrestrial sources. Most urgently, there is an obvious risk Figure 8. Mass balance budget calculations (denoted model A, in paper III) for pools of MeHg in sediment and biota (seston, Amphipodas and benthic invertebrates) consiting of newly imported MeHg and HgII from terrestrial and atmospheric sources and older sediment pools of MeHg and HgII (having a composition of 70 % β-HgS and 30 % Hg-NOM). 38 that contributions of MeHg in fish from terrestrial sources of MeHg and HgII are underestimated. From the different Hg loading and solid phase speciation scenarios postulated (Paper III) we conclude that at constant loading rates, it can be expected that the sediment pools’ contribution to MeHg in sediment and biota is governed by the solid-phase speciation of HgII and the formation of MeHg pools not readily available for demethylation. In paper IV, we calculated mass balance budgets for MeHg in sediment and seston under the scenarios simulated in NPlow, NPhigh and HSE mesocosm. Although associated with large uncertainties, the model suggested that at predicted climate change scenarios for Scandinavia, the concentration of MeHg in plankton could double due to increased inflow of MeHg and Hg II and an increased availability of Hg for MeHg formation and bioaccumulation. For the eutrophication scenario, only small changes in sediment and seston concentrations of MeHg was predicted. Even though the availability of geochemical pools of HgII and MeHg for methylation, demethylation and bioaccumulation will differ among sites, our data can, until similar data have been obtained also from other ecosystems, be used to improve our understanding of Hg biogeochemistry and to predict the effect of environmental changes or changes in Hg loading rates. As future outlooks following this thesis work I suggest some key research questions to address important knowledge gaps in Hg biogeochemistry related to environmental changes, atmospheric and terrestrial loading rate changes as well as Hg and MeHg bioaccumulation in fish: Determination of methylation rates of solid/adsorbed phase tracers and solid phase speciation in other types of ecosystems. Such data could allow an evaluation to what extent differences in the solid phase speciation of Hg among ecosystems could explain differences in sediment as well as biota concentrations of MeHg. Studying mechanisms and processes leading to accumulation of persistent MeHg pools in sediments. Such knowledge is at the present scant and the importance of such pools in sediments is not well recognized. Application of the mesocosm scale experiment on fresh water system. We experimentally demonstrated how environmental 39 changes such as global warming and eutrophication may affect MeHg formation and bioaccumulation of Hg in an estuarine system. Such data is also needed for freshwater ecosystems where the responses might differ in direction and magnitude. Addressing these three key questions will broaden our understanding of Hg biogeochemistry and help understand ways to mitigate the anthropogenic contribution of MeHg in the environment. 40 Acknowledgements Mathias, jag vill tacka dig mest av allt. För allt du gav och du lärde mig, jag vet att du hade varit stolt. Vi hade säkert suttit o diskuterat små detaljer i avhandlingen utan att förstå varandra alls (o till slut kanske insett att vi menade samma sak). Tack för att du var min allra bästa vän och livskamrat under så många år, tack för vår underbara dotter. Jag kommer alltid älska dig och berätta för din dotter om vilken omtänksam och underbar pappa hon haft. Vi saknar dig väldigt här nere! Tack Ida, du är underbar! De finns så många stunder som jag inte skulle klarat av utan dig! Tack för all stöttning och att du låtit mig vara en sån stor del av ditt liv. Ett stort tack till min o Frejas familj som stöttat och hjälpt med allt från kärlek o värme till hjälp med barnpassning o alla små ting: mamma, pappa, Eva, svärmor Susanne, svärfar Eskil, bror Jens med familj, Mathias syskon med respektive och övrig familj till Mathias, moster Kerstin. I would like to thank the staff at the Department of Chemistry and Umeå Marine Sciences Centre for providing me extra support and help so I could come back to work again and finish my thesis. I felt a great support and a genuine care from you. A special thanks to my supervisors and co-authors (especially Erik B, Ulf, and Mats) for listening and for the extra support. During my time in Umeå, I always felt I was surrounded by people who were true friends, and people that would support me if I ever needed it. When my life then was turned upside down, I got at so much more support than I ever could have imagined. Also from friends I just got to know or that I lost contact with. So I would like to thank all of you who in small and big ways showed your support. Even if I did not have time to have all the coffees, dinners and movie nights you suggested, the gesture meant a lot to me. 41 I would like to thank the Department of Chemistry and Umeå Marine Sciences Centre for giving me the chance to opportunity to do research. Tack till min underbara huvudhandledare Erik! Tack för att du gav mig vägledning såväl utrymme att utvecklas och växa. Tack för allt roligt vi haft tillsammans under de här åren. Min tid som doktorand har varit spännande, rolig och helt fantastisk, och mycket av det beror på att du lagt ner din tid och själ i våra forskningsprojekt och i att vägleda mig i forskningen. Tack också för att du varit en av mina närmsta vänner och stöttat mig i både framgångar och motgångar. Tack för skratten, guidningen in i vinernas värld och inte minst alla fartfyllda och legendariska stunder på dansgolvet! Ulf, tack för att du delar med dig så mycket av din passion för forskning. Det är verkligen inspirerande och jag är väldigt glad att jag fått jobba med dig. Tack också för att du, trots ett fullspäckat schema, tog dig tiden att läsa min avhandling och ge feedback. Erik L, tack för support och all praktiskt hjälp med galna mesocosm-idéer. Någon uppskjutning av en mesocosm till rymden blev det inte (och inte heller sediment-tårta), men de kändes som vi fixade saker som tekniskt var i samma klass. Tack till mina medförfattare: speciellt Mats för ditt engagemang och stöttning och Agneta, utan din kompetens hade mesocosm-projektet inte varit möjligt. Tack Tom, för att du guidade mig under första tiden som doktorand, det blev ett stort tomrum i gruppen sen du slutade och jag saknar din humor och personlighet. Thanks to my super-mesocosm-team including Minh and Helen!!! The mesocosm project and my time as a PhD student would not have been the same without the two of you!!! Tack Lasse för två oförglömliga sommar-projekt i Vietnam och Kambodja. Tack till övriga kollegor i forskningsgruppen: Lars, Sylvain, Andreas, Max, Rose-Marie, Solomon och Wolfgang. Tack Yvonne för tiden som kontorskompisar och för din vänskap. Tack till alla er andra som bidragit på olika sätt till arbetet som ligger till grund för artiklarna: Tom Larsson, Anna Karlsson, Ida Tjerngren, Johan Nordbäck (Swedish Geotechnical Institute), Dan Boström, Per Hörstedt, Per-Olof Westlund, Andrey Shchukarev, Staffan Åkerblom och framför allt ett stort tack till Henrik Larsson och övrig teknisk personal på UMF. 42 Har så många underbara vänner att tacka och jag kommer inte (dagen innan tryck) kunna komma ihåg att ta med alla. Tack till Åsa o Frasse, Sandra och Erik, Tuva-Li och Nicklas för barnpassning, trevligt sällskap och goa middagar/luncher. Tack Åsa, också för ditt stöd sista halvåret. Tack till alla som blivit, eller varit, del av ”analytisk kemi” för trevliga fikaraster och vilda analyt-fester! Tack Anna N för att du visade mig Australien. Tack Lisa och Thomas för trevliga spelkväller och goda middagar. Tack Andreas för din vänskap och att du berikat både mitt och Mathias liv. När jag tänker på dig som vän tänker jag på när du, flera kvällar i rad, kom till mig på sjukhuset och satt o skrattade med mig framför TVn, du gjorde verkligen skillnad då! Tack Sarah för sällskap till magdansen, hoppas vi får chans att dansa ihop fler gånger. Tack Kristina, Jonas, Emil, Josefina, matgruppen och alla andra vänner som berikar mitt liv! Till sist, Tack till min underbara och älskade dotter Freja! Du och jag har en underbar liten familj ihop! 43 References 1. Selin, N. E.; Jacob, D. J.; Yantosca, R. M.; Strode, S.; Jaegle, L.; Sunderland, E. M., Global 3-D Land-Ocean-Atmosphere Model for Mercury: Present-Day Versus Preindustrial Cycles and Anthropogenic Enrichment Factors for Deposition (Vol 22, Artn No Gb3099, 2008). Global Biogeochemical Cycles 2008, 22 (3). 2. Sunderland, E. M.; Gobas, F.; Branfireun, B. A.; Heyes, A., Environmental Controls on the Speciation and Distribution of Mercury in Coastal Sediments. Mar. Chem. 2006, 102 (1-2), 111-123. 3. Selin, N. E.; Sunderland, E. M.; Knightes, C. D.; Mason, R. A., Sources of Mercury Exposure for US Seafood Consumers: Implications for Policy. Environ. Health Perspect. 2010, 118 (1), 137-143. 4. Johansson, K.; Bergbäck, B.; Tyler, G., Impact of Atmospheric Long Range Transport of Lead, Mercury and Cadmium on the Swedish Forest Environment. Water, Air, & Soil Pollution: Focus 2001, 1 (3-4), 279-297. 5. Selin, N. E., Science and Strategies to Reduce Mercury Risks: A Critical Review. Journal of Environmental Monitoring 2011, 13 (9), 2389-2399. 6. Camargo, J. A., Which Source of Mercury Pollution. Nature 1993, 365 (6444), 302-302. 7. Berg, T.; Fjeld, E.; Steinnes, E., Atmospheric Mercury in Norway: Contributions from Different Sources. Sci. Total Environ. 2006, 368 (1), 39. 8. Jiang, G. B.; Shi, J. B.; Feng, X. B., Mercury Pollution in China. Environ. Sci. Technol. 2006, 40 (12), 3672-3678. 9. Jensen, S.; Jernelov, A., Biological Methylation of Mercury in Aquatic Organisms. Nature 1969, 223 (5207), 753-&. 10. StLouis, V. L.; Rudd, J. W. M.; Kelly, C. A.; Beaty, K. G.; Flett, R. J.; Roulet, N. T., Production and Loss of Methylmercury and Loss of Total Mercury from Boreal Forest Catchments Containing Different Types of Wetlands. Environ. Sci. Technol. 1996, 30 (9), 2719-2729. 11. Lehnherr, I.; St Louis, V. L.; Hintelmann, H.; Kirk, J. L., Methylation of Inorganic Mercury in Polar Marine Waters. Nat. Geosci. 2011, 4 (5), 298302. 12. Gilmour, C. C.; Henry, E. A.; Mitchell, R., Sulfate Stimulation of Mercury Methylation in Fresh-Water Sediments. Environ. Sci. Technol. 1992, 26 (11), 2281-2287. 13. Compeau, G. C.; Bartha, R., Sulfate-Reducing Bacteria - Principal Methylators of Mercury in Anoxic Estuarine Sediment. Appl. Environ. Microb. 1985, 50 (2), 498-502. 44 14. Fleming, E. J.; Mack, E. E.; Green, P. G.; Nelson, D. C., Mercury Methylation from Unexpected Sources: Molybdate-Inhibited Freshwater Sediments and an Iron-Reducing Bacterium. Appl. Environ. Microb. 2006, 72 (1), 457-464. 15. Kerin, E. J.; Gilmour, C. C.; Roden, E.; Suzuki, M. T.; Coates, J. D.; Mason, R. P., Mercury Methylation by Dissimilatory Iron-Reducing Bacteria. Appl. Environ. Microb. 2006, 72 (12), 7919-7921. 16. Hall, B. D.; Bodaly, R. A.; Fudge, R. J. P.; Rudd, J. W. M.; Rosenberg, D. M., Food as the Dominant Pathway of Methylmercury Uptake by Fish. Water Air and Soil Pollution 1997, 100 (1-2), 13-24. 17. Cabana, G.; Rasmussen, J. B., Modeling Food-Chain Structure and Contaminant Bioaccumulation Using Stable Nitrogen Isotopes. Nature 1994, 372 (6503), 255-257. 18. Cabana, G.; Tremblay, A.; Kalff, J.; Rasmussen, J. B., Pelagic Food-Chain Structure in Ontario Lakes - a Determinant of Mercury Levels in Lake Trout (Salvelinus-Namaycush). Can. J. Fish. Aquat. Sci. 1994, 51 (2), 381389. 19. USEPA, EPA Mercury Study Report to Congress; Office of Air Quality and Standards and Office of Research and Developement Washington (DC), 1997. 20. Cai, Y.; Li Y.; Yin Y.; Liu G., Advances in Speciation Analysis of Mercury in the Environment. In Environmental Chemistry and Toxicology of Mercury, Liu, G.; Cai., Y; O'Driscoll N., Ed. Wiley: New Jersey, 2012. 21. Clarkson, T. W.; Magos, L., The Toxicology of Mercury and Its Chemical Compounds. Crit. Rev. Toxicol. 2006, 36 (8), 609-662. 22. Karagas, M. R.; Choi, A. L.; Oken, E.; Horvat, M.; Schoeny, R.; Kamai, E.; Cowell, W.; Grandjean, P.; Korrick, S., Evidence on the Human Health Effects of Low-Level Methylmercury Exposure. Environ. Health Perspect. 2012, 120 (6), 799-806. 23. Hakanson, L.; Nilsson, A.; Andersson, T., Mercury in Fish in Swedish Lakes. Environmental Pollution 1988, 49 (2), 145-162. 24. Lindqvist, O.; Johansson, K.; Aastrup, M.; Andersson, A.; Bringmark, L.; Hovsenius, G.; Hakanson, L.; Iverfeldt, A.; Meili, M.; Timm, B., Mercury in the Swedish Environment - Recent Research on Causes, Consequences and Corrective Methods. Water Air and Soil Pollution 1991, 55 (1-2), R11&. 25. Harris, R. C.; Rudd, J. W. M.; Amyot, M.; Babiarz, C. L.; Beaty, K. G.; Blanchfield, P. J.; Bodaly, R. A.; Branfireun, B. A.; Gilmour, C. C.; Graydon, J. A.; Heyes, A.; Hintelmann, H.; Hurley, J. P.; Kelly, C. A.; Krabbenhoft, D. P.; Lindberg, S. E.; Mason, R. P.; Paterson, M. J.; Podemski, C. L.; Robinson, A.; Sandilands, K. A.; Southworth, G. R.; Louis, V. L.; Tate, M. T., Whole-Ecosystem Study Shows Rapid Fish- 45 Mercury Response to Changes in Mercury Deposition. P. Natl. Acad. Sci. USA 2007, 104 (42), 16586-16591. 26. U.S. Environmental Protection Agency (2009) 2008 National Listing of Fish Advisories (EPA Fact Sheet EPA-823-F-09-007). Available at www.epa.gov. Accessed December 3. 27. Orihel, D. M.; Paterson, M. J.; Blanchfield, P. J.; Bodaly, R. A.; Hintelmann, H., Experimental Evidence of a Linear Relationship between Inorganic Mercury Loading and Methylmercury Accumulation by Aquatic Biota. Environ. Sci. Technol. 2007, 41 (14), 4952-4958. 28. Orihel, D. M.; Paterson, M. J.; Gilmour, C. C.; Bodaly, R. A.; Blanchfield, P. J.; Hintelmann, H.; Harris, R. C.; Rudd, J. W. M., Effect of Loading Rate on the Fate of Mercury in Littoral Mesocosms. Environ. Sci. Technol. 2006, 40 (19), 5992-6000. 29. Sunderland, E. M.; Mason, R. P., Human Impacts on Open Ocean Mercury Concentrations. Global Biogeochemical Cycles 2007, 21 (4). 30. Munthe, J.; Bodaly, R. A.; Branfireun, B. A.; Driscoll, C. T.; Gilmour, C. C.; Harris, R.; Horvat, M.; Lucotte, M.; Malm, O., Recovery of MercuryContaminated Fisheries. Ambio 2007, 36 (1), 33-44. 31. Åkerblom, S.; Nilsson, M.; Yu, J.; Ranneby, B.; Johansson, K., Temporal Change Estimation of Mercury Concentrations in Northern Pike (Esox Lucius L.) in Swedish Lakes. Chemosphere 2012, 86 (5), 439-445. 32. Rasmussen, P. W.; Schrank, C. S.; Campfield, P. A., Temporal Trends of Mercury Concentrations in Wisconsin Walleye (Sander Vitreus), 19822005. Ecotoxicology 2007, 16 (8), 541-550. 33. Monson, B. A., Trend Reversal of Mercury Concentrations in Piscivorous Fish from Minnesota Lakes: 1982-2006. Environ. Sci. Technol. 2009, 43 (6), 1750-1755. 34. French, T. D.; Campbell, L. M.; Jackson, D. A.; Casselman, J. M.; Scheider, W. A.; Hayton, A., Long-Term Changes in Legacy Trace Organic Contaminants and Mercury in Lake Ontario Salmon in Relation to Source Controls, Trophodynamics, and Climatic Variability. Limnol. Oceanogr. 2006, 51 (6), 2794-2807. 35. UNEP Chemical Branch, D., The Global Atmosperic Mercury Assessment: Sources, Emissions and Transport; Geneva, 2008. 36. Pacyna, E. G.; Pacyna, J. M.; Sundseth, K.; Munthe, J.; Kindbom, K.; Wilson, S.; Steenhuisen, F.; Maxson, P., Global Emission of Mercury to the Atmosphere from Anthropogenic Sources in 2005 and Projections to 2020. Atmospheric Environment 2010, 44 (20), 2487-2499. 37. UNEP Chemical Branch, D. Mercury, the Negotiation Process. http://www.unep.org/hazardoussubstances/Mercury/Negotiations/tabid/332 0/Default.aspx (accessed December 4). 46 38. Mason, R. P.; Choi, A. L.; Fitzgerald, W. F.; Hammerschmidt, C. R.; Lamborg, C. H.; Soerensen, A. L.; Sunderland, E. M., Mercury Biogeochemical Cycling in the Ocean and Policy Implications. Environmental Research 2012, 119, 101–117. 39. Fitzgerald, W. F.; Lamborg, C. H.; Hammerschmidt, C. R., Marine Biogeochemical Cycling of Mercury. Chem. Rev. 2007, 107 (2), 641-662. 40. UNEP, Global Mercury Assessment; UNEP: Geneva, Switzerland, 2002. 41. Templeton, D. M.; Ariese, F.; Cornelis, R.; Danielsson, L. G.; Muntau, H.; Van Leeuwen, H. P.; Lobinski, R., Guidelines for Terms Related to Chemical Speciation and Fractionation of Elements. Definitions, Structural Aspects, and Methodological Approaches (IUPAC Recommendations 2000). Pure Appl. Chem. 2000, 72 (8), 1453-1470. 42. Benoit, J. M.; Gilmour, C. C.; Heyes, A.; Mason, R. P.; Miller, C. L., Geochemical and Biological Controls over Methylmercury Production and Degradation in Aquatic Ecosystems. 2003; p 262-297. 43. Hammerschmidt, C. R.; Fitzgerald, W. F., Geochemical Controls on the Production and Distribution of Methylmercury in near-Shore Marine Sediments. Environ. Sci. Technol. 2004, 38 (5), 1487-1495. 44. Benoit, J. M.; Gilmour, C. C.; Mason, R. P., The Influence of Sulfide on Solid Phase Mercury Bioavailability for Methylation by Pure Cultures of Desulfobulbus Propionicus (1pr3). Environ. Sci. Technol. 2001, 35 (1), 127-132. 45. Hintelmann, H.; Keppel-Jones, K.; Evans, R. D., Constants of Mercury Methylation and Demethylation Rates in Sediments and Comparison of Tracer and Ambient Mercury Availability. Environ. Toxicol. Chem. 2000, 19 (9), 2204-2211. 46. Graham, A. M.; Aiken, G. R.; Gilmour, C. C., Dissolved Organic Matter Enhances Microbial Mercury Methylation under Sulfidic Conditions. Environ. Sci. Technol. 2012, 46 (5), 2715-2723. 47. Drott, A.; Lambertsson, L.; Bjorn, E.; Skyllberg, U., Importance of Dissolved Neutral Mercury Sulfides for Methyl Mercury Production in Contaminated Sediments. Environ. Sci. Technol. 2007, 41 (7), 2270-2276. 48. Benoit, J. M.; Gilmour, C. C.; Mason, R. P.; Heyes, A., Sulfide Controls on Mercury Speciation and Bioavailability to Methylating Bacteria in Sediment Pore Waters. Environ. Sci. Technol. 1999, 33 (6), 951-957. 49. Skyllberg, U., Chemical Speciation of Mercury in Soil and Sediment In Environmental Chemistry and Toxicology of Mercury, First Edition, Guangliang Liu, Yong Cai, Nelson O'Driscoll, Ed. John Wiley & Sons, Inc.: 2012. 50. Bjorn, E.; Larsson, T.; Lambertsson, L.; Skyllberg, U.; Frech, W., Recent Advances in Mercury Speciation Analysis with Focus on Spectrometric 47 Methods and Enriched Stable Isotope Applications. Ambio 2007, 36 (6), 443-451. 51. USEPA, Method 3200, Mercury Species Fractionation and Quantification by Microwave Assisted Extraction, Selective Solvent Extraction and/or Solid Phase Extraction. 2005. 52. Liu, J. R.; Valsaraj, K. T.; Devai, I.; DeLaune, R. D., Immobilization of Aqueous Hg(II) by Mackinawite (FeS). Journal of Hazardous Materials 2008, 157 (2-3), 432-440. 53. Qian, J.; Skyllberg, U.; Frech, W.; Bleam, W. F.; Bloom, P. R.; Petit, P. E., Bonding of Methyl Mercury to Reduced Sulfur Groups in Soil and Stream Organic Matter as Determined by X-Ray Absorption Spectroscopy and Binding Affinity Studies. Geochim. Cosmochim. Acta 2002, 66 (22), 38733885. 54. Pandey, S. K.; Kim, K. H.; Brown, R. J. C., Measurement Techniques for Mercury Species in Ambient Air. Trac-Trends in Analytical Chemistry 2011, 30 (6), 899-917. 55. Leopold, K.; Foulkes, M.; Worsfold, P., Methods for the Determination and Speciation of Mercury in Natural Waters-a Review. Analytica Chimica Acta 2010, 663 (2), 127-138. 56. Krupp, E. M.; Milne, B. F.; Mestrot, A.; Meharg, A. A.; Feldmann, J., Investigation into Mercury Bound to Biothiols: Structural Identification Using ESI-Ion-Trap Ms and Introduction of a Method for Their HPLC Separation with Simultaneous Detection by ICP-MS and ESI-MS. Anal. Bioanal. Chem. 2008, 390 (7), 1753-1764. 57. Drott, A. Chemical Speciation and Transformation of Mercury in Contaminated Sediments. Swedish University of Agricultural Sciences, Umeå, 2009. 58. Lin, C.-J.; Singhasuk, P.; Pehkonen, S. O., Atmospheric Chemistry of Mercury. In Environmental Chemistry and Toxicology of Mercury, Guangliang Liu, Y. C., Nelson O'Driscoll, Ed. 2012. 59. Larsson, T.; Bjorn, E.; Frech, W., Species Specific Isotope Dilution with on Line Derivatisation for Determination of Gaseous Mercury Species. J. Anal. At. Spectrom. 2005, 20 (11), 1232-1239. 60. Larsson, T.; Frech, W., Species-Specific Isotope Dilution with Permeation Tubes for Determination of Gaseous Mercury Species. Analytical Chemistry 2003, 75 (20), 5584-5591. 61. EPA, U., Method 1631, Revision E: Mercury in Water by Oxidation, Purge and Trap, and Cold Vapour Atomic Fluorescence Spectrometry Washington, DC, 2002. 62. Lambertsson, L.; Bjorn, E., Validation of a Simplified Field-Adapted Procedure for Routine Determinations of Methyl Mercury at Trace Levels 48 in Natural Water Samples Using Species-Specific Isotope Dilution Mass Spectrometry. Anal. Bioanal. Chem. 2004, 380 (7-8), 871-875. 63. Drott, A.; Lambertsson, L.; Bjorn, E.; Skyllberg, U., Potential Demethylation Rate Determinations in Relation to Concentrations of MeHg, Hg and Pore Water Speciation of MeHg in Contaminated Sediments. Mar. Chem. 2008, 112 (1-2), 93-101. 64. USEPA, Method 3052, Microvawe Assisted Acid Digestion of Siliceous and Organically Based Matrices; 1996. 65. Skyllberg, U., Competition among Thiols and Inorganic Sulfides and Polysulfides for Hg and MeHg in Wetland Soils and Sediments under Suboxic Conditions: Illumination of Controversies and Implications for MeHg Net Production. J. Geophys. Res-Biogeo. 2008, 113, G00C03. 66. Skyllberg, U.; Bloom, P. R.; Qian, J.; Lin, C. M.; Bleam, W. F., Complexation of Mercury(II) in Soil Organic Matter: EXAFS Evidence for Linear Two-Coordination with Reduced Sulfur Groups. Environ. Sci. Technol. 2006, 40 (13), 4174-4180. 67. Lambertsson, L.; Lundberg, E.; Nilsson, M.; Frech, W., Applications of Enriched Stable Isotope Tracers in Combination with Isotope Dilution GCICP-MS to Study Mercury Species Transformation in Sea Sediments During in Situ Ethylation and Determination. J. Anal. At. Spectrom. 2001, 16 (11), 1296-1301. 68. Nater, E. A.; Cook, B. D., Lmmb 051 Mercury in Plankton. In Lake Michigan Mass Balance Methods Compendium (Http://Www.Epa.Gov/Greatlakes/Lmmb/Methods), USEPA: 1996. 69. Qvarnstrom, J.; Frech, W., Mercury Species Transformations During Sample Pre-Treatment of Biological Tissues Studied by HPLC-ICP-MS. J. Anal. At. Spectrom. 2002, 17 (11), 1486-1491. 70. Lin, C. J.; Pongprueksa, P.; Lindberg, S. E.; Pehkonen, S. O.; Byun, D.; Jang, C., Scientific Uncertainties in Atmospheric Mercury Models I: Model Science Evaluation. Atmospheric Environment 2006, 40 (16), 2911-2928. 71. Nguyen, H. T.; Kim, K. H.; Shon, Z. H.; Hong, S., A Review of Atmospheric Mercury in the Polar Environment. Critical Reviews in Environmental Science and Technology 2009, 39 (7), 552-584. 72. Choe, K. Y.; Gill, G. A., Isolation of Colloidal Monomethyl Mercury in Natural Waters Using Cross-Flow Ultrafiltration Techniques. Mar. Chem. 2001, 76 (4), 305-318. 73. Stordal, M. C.; Gill, G. A.; Wen, L. S.; Santschi, P. H., Mercury Phase Speciation in the Surface Waters of Three Texas Estuaries: Importance of Colloidal Forms. Limnol. Oceanogr. 1996, 41 (1), 52-61. 74. Guentzel, J. L.; Powell, R. T.; Landing, W. M.; Mason, R. P., Mercury Associated with Colloidal Material in an Estuarine and an Open-Ocean Environment. Mar. Chem. 1996, 55 (1-2), 177-188. 49 75. USEPA Method 3051a; Microwave Assisted Acid Digestion of Sediments, Sludges, Soils and Oils. 2007. 76. Bernaus, A.; Gaona, X.; Valiente, M., Characterisation of Almaden Mercury Mine Environment by XAS Techniques. Journal of Environmental Monitoring 2005, 7 (8), 771-777. 77. Lowry, G. V.; Shaw, S.; Kim, C. S.; Rytuba, J. J.; Brown, G. E., Macroscopic and Microscopic Observations of Particle-Facilitated Mercury Transport from New Idria and Sulphur Bank Mercury Mine Tailings. Environ. Sci. Technol. 2004, 38 (19), 5101-5111. 78. Kim, C. S.; Brown, G. E.; Rytuba, J. J., Characterization and Speciation of Mercury-Bearing Mine Wastes Using X-Ray Absorption Spectroscopy. Sci. Total Environ. 2000, 261 (1-3), 157-168. 79. Skyllberg, U.; Drott, A., Competition between Disordered Iron Sulfide and Natural Organic Matter Associated Thiols for Mercury(II)-an EXAFS Study. Environ. Sci. Technol. 2010, 44 (4), 1254-1259. 80. Richet, P.; Bottinga, Y.; Javoy, M., Review of Hydrogen, Carbon, Nitrogen, Oxygen, Sulfur, and Chlorine Stable Isotope Fractionation among Gaseous Molecules. Annual Review of Earth and Planetary Sciences 1977, 5, 65-110. 81. Heumann, K. G., Isotope-Dilution Mass-Spectrometry (IDMS) of the Elements. Mass Spectrom. Rev. 1992, 11 (1), 41-67. 82. Sturup, S., The Use of ICPMS for Stable Isotope Tracer Studies in Humans: A Review. Anal. Bioanal. Chem. 2004, 378 (2), 273-282. 83. Trace Science International. (accessed December 5). 84. Larsson, T. Instrumental and Methodological Developments for Isotope Dilution Analysis of Gaseous Mercury Species. Umeå University Umeå, 2007. 85. Rosenfeld, W. D.; Silverman, S. R., Carbon Isotope Fractionation in Bacterial Production of Methane. Science 1959, 130 (3389), 1658-1659. 86. Yin, R. S.; Feng, X. B.; Shi, W. F., Application of the Stable-Isotope System to the Study of Sources and Fate of Hg in the Environment: A Review. Applied Geochemistry 2010, 25 (10), 1467-1477. 87. Feng, X.; Foucher, D.; Hintelmann, H.; Yan, H.; He, T.; Qiu, G., Tracing Mercury Contamination Sources in Sediments Using Mercury Isotope Compositions. Environ. Sci. Technol. 2010, 44 (9), 3363-3368. 88. Ohata, M.; Ichinose, T.; Furuta, N.; Shinohara, A.; Chiba, M., Isotope Dilution Analysis of Se in Human Blood Serum by Using High-Power Nitrogen Microwave-Induced Plasma Mass Spectrometry Coupled with a Hydride Generation Technique. Analytical Chemistry 1998, 70 (13), 27262730. 50 http://www.tracesciences.com/hg.htm 89. Hoelzl, R.; Hoelzl, C.; Kotz, L.; Fabry, L., The Optimal Amount of Isotopic Spike Solution for Ultratrace Analysis by Isotope Dilution Mass Spectrometry. Accreditation and Quality Assurance 1998, 3 (5), 185-188. 90. Larsson, T.; Frech, W.; Bjorn, E.; Dybdahl, B., Studies of Transport and Collection Characteristics of Gaseous Mercury in Natural Gases Using Amalgamation and Isotope Dilution Analysis. Analyst 2007, 132 (6), 579586. 91. Baya, A. P. H., Holger, The Measurement of Organic Mercury Species in the Artic Troposphere. In International Conference of Mercury as a Global Pollutant Halifax, Canada, 2011; pp 22-23. 92. Dyrssen, D.; Wedborg, M., The Sulfur-Mercury(II) System in NaturalWaters. Water Air and Soil Pollution 1991, 56, 507-519. 93. Ravichandran, M.; Aiken, G. R.; Ryan, J. N.; Reddy, M. M., Inhibition of Precipitation and Aggregation of Metacinnabar (Mercuric Sulfide) by Dissolved Organic Matter Isolated from the Florida Everglades. Environ. Sci. Technol. 1999, 33 (9), 1418-1423. 94. Wolfenden, S.; Charnock, J. M.; Hilton, J.; Livens, F. R.; Vaughan, D. J., Sulfide Species as a Sink for Mercury in Lake Sediments. Environ. Sci. Technol. 2005, 39 (17), 6644-6648. 95. Wiens, J. A., Spatial Scaling in Ecology. Functional Ecology 1989, 3 (4), 385-397. 96. Petersen, J. E.; Kemp, W. M.; Bartleson, R.; Boynton, W. R.; Chen, C. C.; Cornwell, J. C.; Gardner, R. H.; Hinkle, D. C.; Houde, E. D.; Malone, T. C.; Mowitt, W. P.; Murray, L.; Sanford, L. P.; Stevenson, J. C.; Sundberg, K. L.; Suttles, S. E., Multiscale Experiments in Coastal Ecology: Improving Realism and Advancing Theory. Bioscience 2003, 53 (12), 1181-1197. 97. Petersen, J. E.; Cornwell, J. C.; Kemp, W. M., Implicit Scaling in the Design of Experimental Aquatic Ecosystems. Oikos 1999, 85 (1), 3-18. 98. Choi, S. C.; Bartha, R., Cobalamin-Mediated Mercury Methylation by Desulfovibrio-Desulfuricans Ls. Appl. Environ. Microb. 1993, 59 (1), 290295. 99. Choi, S. C.; Chase, T.; Bartha, R., Enzymatic Catalysis of Mercury Methylation by Desulfovibrio-Desulfuricans Ls. Appl. Environ. Microb. 1994, 60 (4), 1342-1346. 100. Schaefer, J. K.; Morel, F. M. M., High Methylation Rates of Mercury Bound to Cysteine by Geobacter Sulfurreducens. Nat. Geosci. 2009, 2 (2), 123-126. 101. Schaefer, J. K.; Rocks, S. S.; Zheng, W.; Liang, L. Y.; Gu, B. H.; Morel, F. M. M., Active Transport, Substrate Specificity, and Methylation of Hg(II) in Anaerobic Bacteria. P. Natl. Acad. Sci. USA 2011, 108 (21), 8714-8719. 102. Zhang, T.; Kim, B.; Leyard, C.; Reinsch, B. C.; Lowry, G. V.; Deshusses, M. A.; Hsu-Kim, H., Methylation of Mercury by Bacteria Exposed to 51 Dissolved, Nanoparticulate, and Microparticulate Mercuric Sulfides. Environ. Sci. Technol. 2012, 46 (13), 6950-6958. 103. Feyte, S.; Gobeil, C.; Tessier, A.; Cossa, D., Mercury Dynamics in Lake Sediments. Geochim. Cosmochim. Acta 2012, 82, 92-112. 104. Jeong, H. Y.; Klaue, B.; Blum, J. D.; Hayes, K. F., Sorption of Mercuric Ion by Synthetic Manocrystalline Mackinawite (FeS). Environ. Sci. Technol. 2007, 41 (22), 7699-7705. 105. Charnock, J. M.; Moyes, L. N.; Pattrick, R. A. D.; Mosselmans, J. F. W.; Vaughan, D. J.; Livens, F. R., The Structural Evolution of Mercury Sulfide Precipitate: An XAS and XRD Study. Amer. Mineral. 2003, 88 (8-9), 11971203. 106. Slowey, A. J., Rate of Formation and Dissolution of Mercury Sulfide Nanoparticles: The Dual Role of Natural Organic Matter. Geochim. Cosmochim. Acta 2010, 74 (16), 4693-4708. 107. Waples, J. S.; Nagy, K. L.; Aiken, G. R.; Ryan, J. N., Dissolution of Cinnabar (HgS) in the Presence of Natural Organic Matter. Geochim. Cosmochim. Acta 2005, 69 (6), 1575-1588. 108. Paquette, K. E.; Helz, G. R., Inorganic Speciation of Mercury in Sulfidic Waters: The Importance of Zero-Valent Sulfur. Environ. Sci. Technol. 1997, 31 (7), 2148-2153. 109. Mikac, N.; Foucher, D.; Niessen, S.; Fischer, J. C., Extractability of HgS (Cinnabar and Metacinnabar) by Hydrochloric Acid. Anal. Bioanal. Chem. 2002, 374 (6), 1028-1033. 110. Lambertsson, L.; Nilsson, M., Organic Material: The Primary Control on Mercury Methylation and Ambient Methyl Mercury Concentrations in Estuarine Sediments. Environ. Sci. Technol. 2006, 40 (6), 1822-1829. 111. Benoit, J. M.; Mason, R. P.; Gilmour, C. C., Estimation of Mercury-Sulfide Speciation in Sediment Pore Waters Using Octanol-Water Partitioning and Implications for Availability to Methylating Bacteria. Environ. Toxicol. Chem. 1999, 18 (10), 2138-2141. 112. Winfrey, M. R.; Rudd, J. W. M., Environmental Factors Affecting the Formation of Methylmercury in Low ph Lakes. Environ. Toxicol. Chem. 1990, 9 (7), 853-869. 113. Meier, H. E. M., Baltic Sea Climate in the Late Twenty-First Century: A Dynamical Downscaling Approach Using Two Global Models and Two Emission Scenarios. Climate Dynamics 2006, 27 (1), 39-68. 114. Jansson, M.; Karlsson, J.; Blomqvist, P., Allochthonous Organic Carbon Decreases Pelagic Energy Mobilization in Lakes. Limnol. Oceanogr. 2003, 48 (4), 1711-1716. 115. Karlsson, J.; Jonsson, A.; Meili, M.; Jansson, M., Control of Zooplankton Dependence on Allochthonous Organic Carbon in Humic and Clear-Water Lakes in Northern Sweden. Limnol. Oceanogr. 2003, 48 (1), 269-276. 52 116. Sandberg, J.; Andersson, A.; Johansson, S.; Wikner, J., Pelagic Food Web Structure and Carbon Budget in the Northern Baltic Sea: Potential Importance of Terrigenous Carbon. Marine Ecology Progress Series 2004, 268, 13-29. 117. Elmgren, R., Understanding Human Impact on the Baltic Ecosystem: Changing Views in Recent Decades. Ambio 2001, 30 (4-5), 222-231. 118. Schaefer, J. K.; Yagi, J.; Reinfelder, J. R.; Cardona, T.; Ellickson, K. M.; Tel-Or, S.; Barkay, T., Role of the Bacterial Organomercury Lyase (MerB) in Controlling Methylmercury Accumulation in Mercury-Contaminated Natural Waters. Environ. Sci. Technol. 2004, 38 (16), 4304-4311. 119. Sellers, P.; Kelly, C. A.; Rudd, J. W. M.; MacHutchon, A. R., Photodegradation of Methylmercury in Lakes. Nature 1996, 380 (6576), 694-697. 120. Oremland, R. S.; Culbertson, C. W.; Winfrey, M. R., Methylmercury Decomposition in Sediments and Bacterial Cultures - Involvement of Methanogens and Sulfate Reducers in Oxidative Demethylation. Appl. Environ. Microb. 1991, 57 (1), 130-137. 121. Billen, G.; Joiris, C.; Wollast, R., Bacterial Methylmercury-Mineralizing Activity in River Sediments. Water Research 1974, 8 (4), 219-225. 122. Deacon, G. B., Volatilization of Methylmercuric Chloride by HydrogenSulfide. Nature 1978, 275 (5678), 344-344. 123. Martin-Doimeadios, R. C.; Tessier, E.; Amouroux, D.; Guyoneaud, R.; Duran, R.; Caumette, P.; Donard, O. F. X., Mercury Methylation/Demethylation and Volatilization Pathways in Estuarine Sediment Slurries Using Species-Specific Enriched Stable Isotopes. Mar. Chem. 2004, 90 (1-4), 107-123. 124. Marvin-DiPasquale, M.; Agee, J.; McGowan, C.; Oremland, R. S.; Thomas, M.; Krabbenhoft, D.; Gilmour, C. C., Methyl-Mercury Degradation Pathways: A Comparison among Three Mercury-Impacted Ecosystems. Environ. Sci. Technol. 2000, 34 (23), 4908-4916. 125. Heyes, A.; Mason, R. P.; Kim, E. H.; Sunderland, E., Mercury Methylation in Estuaries: Insights from Using Measuring Rates Using Stable Mercury Isotopes. Mar. Chem. 2006, 102 (1-2), 134-147. 126. Hammerschmidt, C. R.; Fitzgerald, W. F.; Lamborg, C. H.; Balcom, P. H.; Visscher, P. T., Biogeochemistry of Methylmercury in Sediments of Long Island Sound. Mar. Chem. 2004, 90 (1-4), 31-52. 127. Hammerschmidt, C. R.; Fitzgerald, W. F., Methylmercury Cycling in Sediments on the Continental Shelf of Southern New England. Geochim. Cosmochim. Acta 2006, 70 (4), 918-930. 128. Gill, G. A.; Bloom, N. S.; Cappellino, S.; Driscoll, C. T.; Dobbs, C.; McShea, L.; Mason, R.; Rudd, J. W. M., Sediment-Water Fluxes of 53 Mercury in Lavaca Bay, Texas. Environ. Sci. Technol. 1999, 33 (5), 663669. 129. Choe, K. Y.; Gill, G. A.; Lehman, R. D.; Han, S.; Heim, W. A.; Coale, K. H., Sediment-Water Exchange of Total Mercury and Monomethyl Mercury in the San Francisco Bay-Delta. Limnol. Oceanogr. 2004, 49 (5), 15121527. 130. Covelli, S.; Faganeli, J.; Horvat, M.; Brambati, A., Porewater Distribution and Benthic Flux Measurements of Mercury and Methylmercury in the Gulf of Trieste (Northern Adriatic Sea). Estuarine Coastal and Shelf Science 1999, 48 (4), 415-428. 131. Mason, R. P.; Lawrence, A. L., Concentration, Distribution, and Bioavailability of Mercury and Methylmercury in Sediments of Baltimore Harbor and Chesapeake Bay, Maryland, USA. Environ. Toxicol. Chem. 1999, 18 (11), 2438-2447. 132. Leaner, J. J.; Mason, R. P., The Effect of Thiolate Organic Compounds on Methylmercury Accumulation and Redistribution in Sheepshead Minnows, Cyprinodon Variegatus. Environ. Toxicol. Chem. 2001, 20 (7), 1557-1563. 133. Golding, G. R.; Kelly, C. A.; Sparling, R.; Loewen, P. C.; Rudd, J. W. M.; Barkay, T., Evidence for Facilitated Uptake of Hg(II) by Vibrio Anguillarum and Escherichia Coli under Anaerobic and Aerobic Conditions. Limnol. Oceanogr. 2002, 47 (4), 967-975. 134. Mason, R. P.; Reinfelder, J. R.; Morel, F. M. M., Uptake, Toxicity, and Trophic Transfer of Mercury in a Coastal Diatom. Environ. Sci. Technol. 1996, 30 (6), 1835-1845. 135. Luengen, A. C.; Fisher, N. S.; Bergamaschi, B. A., Dissolved Organic Matter Reduces Algal Accumulation of Methylmercury. Environ. Toxicol. Chem. 2012, 31 (8), 1712-1719. 136. Pickhardt, P. C.; Fisher, N. S., Accumulation of Inorganic and Methylmercury by Freshwater Phytoplankton in Two Contrasting Water Bodies. Environ. Sci. Technol. 2007, 41 (1), 125-131. 137. Becker, D. S.; Bigham, G. N., Distribution of Mercury in the Aquatic FoodWeb of Onondaga Lake, New-York. Water Air and Soil Pollution 1995, 80 (1-4), 563-571. 138. Wallace, J. B.; Merritt, R. W., Filter-Feeding Ecology of Aquatic Insects. Annual Review of Entomology 1980, 25, 103-132. 139. Eagles-Smith, C. A.; Suchanek, T. H.; Colwell, A. E.; Anderson, N. L., Mercury Trophic Transfer in a Eutrophic Lake: The Importance of HabitatSpecific Foraging. Ecological Applications 2008, 18 (8), A196-A212. 140. Rand, P. S.; Stewart, D. J., Prey Fish Exploitation, Salmonine Production, and Pelagic Food Web Efficiency in Lake Ontario. Can. J. Fish. Aquat. Sci. 1998, 55 (2), 318-327. 54 141. Tsui, M. T. K.; Wang, W. X., Uptake and Elimination Routes of Inorganic Mercury and Methylmercury in Daphnia Magna. Environ. Sci. Technol. 2004, 38 (3), 808-816. 142. Bowling, A. M.; Hammerschmidt, C. R.; Oris, J. T., Necrophagy by a Benthic Omnivore Influences Biomagnification of Methylmercury in Fish. Aquatic Toxicology 2011, 102 (3-4), 134-141. 143. Lawrence, A. L.; Mason, R. P., Factors Controlling the Bioaccumulation of Mercury and Methylmercury by the Estuarine Amphipod Leptocheirus Plumulosus. Environmental Pollution 2001, 111 (2), 217-231. 144. Wiener, J. G.; Stokes, P. M., Enhanced Bioaccumulation of Mercury, Cadmium and Lead in Low-Alkalinity Waters - an Emerging Regional Environmental Problem. Environ. Toxicol. Chem. 1990, 9 (7), 821-823. 145. Pickhardt, P. C.; Folt, C. L.; Chen, C. Y.; Klaue, B.; Blum, J. D., Algal Blooms Reduce the Uptake of Toxic Methylmercury in Freshwater Food Webs. P. Natl. Acad. Sci. USA 2002, 99 (7), 4419-4423. 146. Allen, E. W.; Prepas, E. E.; Gabos, S.; Strachan, W. M. J.; Zhang, W. P., Methyl Mercury Concentrations in Macroinvertebrates and Fish from Burned and Undisturbed Lakes on the Boreal Plain. Can. J. Fish. Aquat. Sci. 2005, 62 (9), 1963-1977. 147. Drevnick, P. E.; Canfield, D. E.; Gorski, P. R.; Shinneman, A. L. C.; Engstrom, D. R.; Muir, D. C. G.; Smith, G. R.; Garrison, P. J.; Cleckner, L. B.; Hurley, J. P.; Noble, R. B.; Otter, R. R.; Oris, J. T., Deposition and Cycling of Sulfur Controls Mercury Accumulation in Isle Royale Fish. Environ. Sci. Technol. 2007, 41 (21), 7266-7272. 148. Swanson, H. K.; Johnston, T. A.; Schindler, D. W.; Bodaly, R. A.; Whittle, D. M., Mercury Bioaccumulation in Forage Fish Communities Invaded by Rainbow Smelt (Osmerus Mordax). Environ. Sci. Technol. 2006, 40 (5), 1439-1446. 149. Evans, M. S.; Lockhart, W. L.; Doetzel, L.; Low, G.; Muir, D.; Kidd, K.; Stephens, G.; Delaronde, J., Elevated Mercury Concentrations in Fish in Lakes in the Mackenzie River Basin: The Role of Physical, Chemical, and Biological Factors. Sci. Total Environ. 2005, 351, 479-500. 150. Luengen, A. C.; Flegal, A. R., Role of Phytoplankton in Mercury Cycling in the San Francisco Bay Estuary. Limnol. Oceanogr. 2009, 54 (1), 23-40. 151. Watras, C. J.; Bloom, N. S., Mercury and Methylmercury in Individual Zooplankton - Implications for Bioaccumulation. Limnol. Oceanogr. 1992, 37 (6), 1313-1318. 152. Vander Zanden, M. J.; Essington, T. E.; Vadeboncoeur, Y., Is Pelagic TopDown Control in Lakes Augmented by Benthic Energy Pathways? Can. J. Fish. Aquat. Sci. 2005, 62 (6), 1422-1431. 55 153. Wang, W. X.; Stupakoff, I.; Gagnon, C.; Fisher, N. S., Bioavailability of Inorganic and Methylmercury to a Marine Deposit Feeding Polychaete. Environ. Sci. Technol. 1998, 32 (17), 2564-2571. 154. Dewitt, T. H.; Ozretich, R. J.; Swartz, R. C.; Lamberson, J. O.; Schults, D. W.; Ditsworth, G. R.; Jones, J. K. P.; Hoselton, L.; Smith, L. M., The Influence of Organic-Matter Quality on the Toxicity and Partitioning of Sediment-Associated Fluoranthene. Environ. Toxicol. Chem. 1992, 11 (2), 197-208. 155. Dahl, E., Deep-Sea Carrion Feeding Amphipods - Evolutionary Patterns in Niche Adaptation. Oikos 1979, 33 (2), 167-175. 156. Clifton, J. C., Mercury Exposure and Public Health. Pediatric Clinics of North America 2007, 54 (2), 237-+. 157. Hrabik, T. R.; Watras, C. J., Recent Declines in Mercury Concentration in a Freshwater Fishery: Isolating the Effects of De-acidification and Decreased Atmospheric Mercury Deposition in Little Rock Lake. Sci. Total Environ. 2002, 297 (1-3), 229-237. 158. Mason, R. P.; Sheu, G. R., Role of the Ocean in the Global Mercury Cycle. Global Biogeochemical Cycles 2002, 16 (4). 159. Rolfhus, K. R.; Fitzgerald, W. F., Linkages between Atmospheric Mercury Deposition and the Methylmercury Content of Marine Fish. Water Air and Soil Pollution 1995, 80 (1-4), 291-297. 160. MacLeod, M.; McKone, T. E.; Mackay, D., Mass Balance for Mercury in the San Francisco Bay Area. Environ. Sci. Technol. 2005, 39 (17), 67216729. 161. Sakata, M.; Marumoto, K.; Narukawa, M.; Asakura, K., Mass Balance and Sources of Mercury in Tokyo Bay. Journal of Oceanography 2006, 62 (6), 767-775. 162. Balcom, P. H.; Fitzgerald, W. F.; Vandal, G. M.; Lamborg, C. H.; Rolfllus, K. R.; Langer, C. S.; Hammerschmidt, C. R., Mercury Sources and Cycling in the Connecticut River and Long Island Sound. Mar. Chem. 2004, 90 (14), 53-74. 163. Balcom, P. H.; Hammerschmidt, C. R.; Fitzgerald, W. F.; Lamborg, C. H.; O'Connor, J. S., Seasonal Distributions and Cycling of Mercury and Methylmercury in the Waters of New York/New Jersey Harbor Estuary. Mar. Chem. 2008, 109 (1-2), 1-17. 164. Mason, R. P.; Lawson, N. M.; Lawrence, A. L.; Leaner, J. J.; Lee, J. G.; Sheu, G. R., Mercury in the Chesapeake Bay. Mar. Chem. 1999, 65 (1-2), 77-96. 165. Qureshi, A.; MacLeod, M.; Scheringer, M.; Hungerbuhler, K., Mercury Cycling and Species Mass Balances in Four North American Lakes. Environmental Pollution 2009, 157 (2), 452-462. 56 166. Suchanek, T. H.; Cooke, J.; Keller, K.; Jorgensen, S.; Richerson, P. J.; Eagles-Smith, C. A.; Harner, E. J.; Adam, D. P., A Mass Balance Mercury Budget for a Mine-Dominated Lake: Clear Lake, California. Water Air and Soil Pollution 2009, 196 (1-4), 51-73. 167. Gao, N.; Armatas, N. G.; Shanley, J. B.; Kamman, N. C.; Miller, E. K.; Keeler, G. J.; Scherbatskoy, T.; Holsen, T. M.; Young, T.; McIlroy, L.; Drake, S.; Olsen, B.; Cady, C., Mass Balance Assessment for Mercury in Lake Champlain. Environ. Sci. Technol. 2006, 40 (1), 82-89. 168. Ethier, A. L. M.; Mackay, D.; Toose-Reid, L. K.; O'Driscoll, N. J.; Scheuttammer, A. M.; Lean, D. R. S., The Development and Application of a Mass Balance Model for Mercury (Total, Elemental and Methyl) Using Data from a Remote Lake (Big Dam West, Nova Scotia, Canada) and the Multi-Species Multiplier Method. Applied Geochemistry 2008, 23 (3), 467481. 169. Hines, N. A.; Brezonik, P. L., Mercury Inputs and Outputs at a Small Lake in Northern Minnesota. Biogeochemistry 2007, 84 (3), 265-284. 57
© Copyright 2024 Paperzz