Sterol, n-alcohol and n-alkane composition of living fen plants

In groundwater-fed fen peatlands, the surface biomass decays rapidly and, as a result, highly humified peat is formed. A high degree of humification constrains palaeoecological studies because reliable identification of plant remains is hampered. Organic geochemistry techniques as a means of identifying historical plant communities have been successfully applied tobog peat. The method has also been applied to fen peat, but without reference to the composition of fen plants. We have applied selected organic geochemistry methods to determine the composition of the neutral lipid fractions from 12 living fen plants, to investigate the potential for the distributions to characterize and separate different fen plants and plant groups. Our results show correspondence with previous studies, e.g. C23 and C25n-alkanes dominating Sphagnum spp. and C27 to C31 alkanes dominating vascular plants. However, we also found similarities in n-alkane distributions between Sphagnum spp. and the below ground parts of some vascular plants. We tested the efficiency of different n-alkane ratios to separate species and plant groups. The ratios used for bog studies (e.g. n-C23/n-C25 and n-C23/n-C29) did not work as consistently for fen plants. Some differences in sterol distribution were found between vascular plants and mosses; in general vascular plants had a higher concentration of sterols. When distributions of n-alkanes, n-alkane ratios and sterols were all included as variables, redundancy analysis (RDA) separated different plant groups into their own clusters. Our results imply that the pattern for bog biomarkers cannot directly be applied to fen environments. Nevertheless, they encourage further testing to determine whether or not the identification of plant groups, plants or plant parts from highly humified peat is possible by applying fen species-specific biomarker proxies.

(Table T1) N-alkane, n-alcohol and n-fatty acid concentrations in ODP Site 184-1147 and 184-1148 sediments

Lipid compositions of sediments recovered during Ocean Drilling Program Leg 184 in the South China Sea have been identified and quantified. The identified lipids can be ascribed to terrigenous and marine sources. Terrigenous lipids are mainly C27, C29, C31 n-alkanes, C26, C28, C30 n-fatty acids, and n-alcohols, which were derived from leaf waxes of higher land plants and transported to the sea by airborne dust or fresh water. Marine lipids, mainly C37 and C38 alkenones, C30 diol, and C30 and C32 keto-ols, were from microalgae, notably haptophytes and eustigmatophytes. Elevated concentrations and accumulation rates of both terrigenous and marine lipids in the interval 202-245 meters composite depth (mcd) and 0-166 mcd were postulated to be related to the development of the East Asian monsoon at 6-8 Ma and enhanced variations of the developed East Asian monsoon after 3.2 Ma, respectively. The pronounced late Oligocene input of terrigenous lipids reflects the paleoenvironment of a newly opened, narrow basin, with restricted ocean waters and the proximity of continental runoff.

Microbial community, biomarker concentrations and their isotopic signature in sediment of Gullfaks and Tommeliten methane seeps in the Northern North Sea

Gullfaks is one of the four major Norwegian oil and gas fields, located in the northeastern edge of the North Sea Plateau. Tommeliten lies in the greater Ekofisk area in the central North Sea. During the cruises HE 208 and AL 267 several seep locations of the North Sea were visited. At the Heincke seep at Gullfaks, sediments were sampled in May 2004 (HE 208) using a video-guided multiple corer system (MUC; Octopus, Kiel). The samples were recovered from an area densely covered with bacterial mats where gas ebullition was observed. The coarse sands limited MUC penetration depth to maximal 30 centimeters and the highly permeable sands did not allow for a high-resolution, vertical subsampling because of pore water loss. The gas flare mapping and videographic observation at Tommeliten indicated an area of gas emission with a few small patches of bacterial mats with diameters <50 cm from most of which a single stream of gas bubbles emerged. The patches were spaced apart by 10-100 m. Sampling of sediments covered by bacterial mats was only possible with 3 small push cores (3.8 cm diameter) mounted to ROV Cherokee. These cores were sampled in 3 cm intervals. Lipid biomarker extraction from 10 -17 g wet sediment was carried out as described in detail elsewhere (Elvert et al., 2003; doi:10.1080/01490450303894). Briefly, defined concentrations of cholestane, nonadecanol and nonadecanolic acid with known delta 13C-values were added to the sediments prior to extraction as internal standards for the hydrocarbon, alcohol and fatty acid fraction, respectively. Total lipid extracts were obtained from the sediment by ultrasonification with organic solvents of decreasing polarity. Esterified fatty acids (FAs) were cleaved from the glycerol head group by saponification with methanolic KOH solution. From this mixture, the neutral fraction was extracted with hexane. After subsequent acidification, FAs were extracted with hexane. For analysis, FAs were methylated using BF3 in methanol yielding fatty acid methyl esters (FAMES). The fixation for total cell counts and CARD-FISH were performed on-board directly after sampling. For both methods, sediments were fixed in formaldehyde solution. After two hours, aliquots for CARD-FISH staining were washed with 1* PBS (10mmol/l sodium phosphate solution, 130mmol/l NaCl, adjusted to a pH of 7.2) and finally stored in a 1:1 PBS:ethanol solution at -20°C until further processing. Samples for total cell counts were stored in formalin at 4°C until analysis. For sandy samples, the total cell count/CARD-FISH protocol was optimized to separate sand particles from the cells. Cells were dislodged from sediment grains and brought into solution with the supernatant by sonicating each sample onice for 2 minutes at 50W. This procedure was repeated four times and supernatants were combined. The sediment samples were brought to a final dilution of 1:2000 to 1:4000 and filtered onto 0.2µm GTTP filters (Millipore, Eschbonn, Germany).