19:I[42426,["/_next/static/immutable/chunks/1xctgzqre-wsy.js","/_next/static/immutable/chunks/06_-wz6pdtp2b.js","/_next/static/immutable/chunks/30e52g49hg40p.js","/_next/static/immutable/chunks/02yq6tul2z-oh.js","/_next/static/immutable/chunks/10bx_ec2vj7n_.js","/_next/static/immutable/chunks/33bfn03fo8xnt.js","/_next/static/immutable/chunks/0tfjf78scu61b.js","/_next/static/immutable/chunks/31xnvej4n1bi9.js"],"default"] 1a:Tf63,

Methodology from Spivak, AC and J Ossolinski. 2016. Limited effects of nutrient enrichment on bacterial carbon sources in salt marsh tidal creek sediments. Marine Ecology Progress Series. 544:107-130. 10.3354/meps11587

Sediment samples for organic matter composition were collected by placing a hard plastic sleeve around a polyvinyl chloride (PVC) corer (5 cm diameter x 15 cm deep) and then removing the corer. The plastic sleeve remained in place to maintain the integrity of the sediment column and mark the core location. The top 0.5 cm of each core was collected into pre-combusted vials and frozen (-80 deg C) until analysis.

Lipid biomarker compounds were extracted using a modified Bligh and Dyer (1959) method. Sediment samples were extracted with a chloroform : methylene chloride : phosphate buffer saline mixture (2:1:0.8, v:v:v) using a microwave-accelerated reaction system (MARS6); samples were heated to 80deg C for 10 min with continuous stirring. Following extraction, samples were partitioned and the organic phase was removed. The total lipid extract was concentrated under N2 and samples were separated on silica gel columns by eluting with chloroform, acetone (F1/2), and methanol (F3) (Guckert et al. 1985). The F3 (phospholipids) was dried under N2 and saponified with 0.5 M NaOH at 70 deg C for 4 h. Saponified samples were acidified and extracted three times with hexane. The extract was methylated with acidic methanol (95:5 methanol: HCl) and heated overnight at 70deg C to form fatty acid methyl esters (FAME). Samples were analyzed with an Agilent 7890 gas chromatograph with an effluent split ~70:30 between a 5975C mass spectrometer and a flame ionization detector. Peaks were separated on an Agilent DB-5 ms column (60 m, 0.25 mm inner diameter, 0.25 μm film). FAME concentrations were quantified using methyl heneicosanoate as an internal standard. FAs are designated A:BwC, where A is the number of carbon atoms, B is the number of double bonds, and C is the position of the first double bond from the aliphatic ‘w’ end of the molecule. The prefixes ‘i’ and ‘a’ refer to iso and anteiso methyl branched FAs and indicate whether the methyl group is attached to the penultimate or antepenultimate carbon atoms (Bianchi & Canuel 2011).

Stable carbon isotope ratios of FAMEs (F3) were determined by the WHOI Organic Mass Spectrometry Facility with a Hewlett-Packard 6890 GC interfaced to a DeltaPlus IRMS. Excess 13C was calculated per Eqs. 1 – 3, where samples collected prior to 13C label application were controls and PLFA concentrations were in units of moles m-2.

PLFA isotopic values were derived from the isotopic composition of FAMEs and corrected for the d13C of the carbon added during methylation using a mass balance approach. We analyzed total PLFA concentrations as well as concentrations and isotopic composition of compounds and subclasses representing algae (polyunsaturated fatty acids C20:4w6, C20:5w3; PUFA), bacteria (iso- and anteiso- branched C15:0, C17:0; BrFA), sulfate reducing bacteria (10-methyl C16:0), and a combination of algae and microbes (short chain fatty acids C12:0, C14:0; SCFA) (Perry et al. 1979, Kaneda 1991, Volkman et al. 1998). The d13C of PLFA subclasses was calculated as concentrated weighted averages. In order to evaluate the sources of carbon supporting sediment bacteria in the tidal creeks, PLFA isotopic values measured in initial sediment samples (i.e., pre-label application) were corrected for a -3 0/00 fractionation during lipid synthesis (Hayes 2001, Bouillon & Boschker 2006).

1b:T88e,Extracted from the NSF award abstract: This project will address how rates of benthic microalgal production respond to eutrophication and geomorphological changes in human-impacted tidal creeks. Excess nutrient loading increases benthic algal biomass and likely stimulates production rates but the magnitude of nutrient and geomorphological effects on rates of production is unknown. Will changes in benthic algal productivity affect algal-bacterial coupling? Furthermore, how is algal-bacterial coupling affected by geomorphological changes, which may be exacerbated by excess nutrient loading but can also occur in pristine marshes? This project will take advantage of the infrastructure of the TIDE project, a long-term saltmarsh eutrophication experiment at the Plum Island Ecosystem - Long Term Ecological Research site in Northeastern Massachusetts. Specifically, the PIs will measure benthic metabolism and examine algal- bacterial coupling in fertilized and ambient nutrient tidal creeks in the first field season. The following field season, they will compare sediment metabolism and carbon dynamics on slumped tidal creek walls (i.e. areas where low marsh has collapsed into the tidal creek) to that on the bottom of tidal creeks. In both years, gross and net production will be determined using an innovative triple oxygen isotope technique and traditional dissolved oxygen and inorganic carbon flux measurements. Comparisons between these methods will be useful in informing studies of sediment metabolism. Lipid biomarkers will be used to characterize the sources of organic matter to creek sediments, and stable isotope analysis of bacterial specific biomarkers to identify the sources of organic carbon utilized by sediment bacteria. The biomarkers will reveal whether sediment bacteria use organic matter substrates, such as benthic microalgal carbon, selectively or in proportion to availability. Overall, results from the proposed study will provide important information about how sediment carbon dynamics in shallow tidal creeks respond to long term eutrophication. Furthermore, findings will enhance understanding of the role of tidal creeks in coastal biogeochemistry.6:["$","$L19",null,{"dataset":{"_id":"668443","description":"

Sediment PLFA isotope values.

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BCO-DMO Data Processing Notes:

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\n-removed spaces from data
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It is frequently used as a detector in gas chromatography. Standalone FIDs can also be used in applications such as landfill gas monitoring, fugitive emissions monitoring and internal combustion engine emissions measurement in stationary or portable instruments.","type_acronym":"FID"},{"_id":"668452","name":"Agilent 7890 gas chromatograph","description":"effluent split ~70:30","type_id":"661","type_name":"Gas Chromatograph","type_desc":"Instrument separating gases, volatile substances, or substances dissolved in a volatile solvent by transporting an inert gas through a column packed with a sorbent to a detector for assay. 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Month samples were collected; mm

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Month of year; numeric 1 to 12.

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Core ID

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Core identification number or label; often used with ice, rock, sediment, or coral cores.

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Estuary where samples were collected.

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Sampling site identification.

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Number of hours elapsed since application of the 13C label; 0 represents samples collected immediately before label application.

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Time GMT defined as HHMM; time of day; generally reported in GMT as HHMM (hours and minutes) but may also be HH.H (decimal hours) or HHMMSS (hours; minutes and seconds); in EqPac time is reported as Hawaii local time

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Refers to whether the 13 label was added as NaHCO3 (ie BMA) or S. alterniflora (ie S alt) detritus.

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Experimental conditions applied to experimental units. In comparative experiments, members of the complementary group, the control group, receive either no treatment or a standard treatment.

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Concentration of a combination of algae and microbes; short chain fatty acid

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