uid=AND,o=lter,dc=ecoinformatics,dc=org all public read SP021 Robert P. Griffiths

Oregon State University;Dept. of Forest Science;321 Richardson Hall Corvallis OR 97331-5752 USA

(541) 737-6559 bbgriff@peak.org griff@for.orst.edu Robert P. Griffiths

Oregon State University;Dept. of Forest Science;321 Richardson Hall Corvallis OR 97331-5752 USA

(541) 737-6559 bbgriff@peak.org griff@for.orst.edu Principal Investigator Alan K. Swanson Other Researcher Robert P. Griffiths

Oregon State University;Dept. of Forest Science;321 Richardson Hall Corvallis OR 97331-5752 USA

(541) 737-6559 bbgriff@peak.org griff@for.orst.edu Abstractor Robert P. Griffiths

Oregon State University;Dept. of Forest Science;321 Richardson Hall Corvallis OR 97331-5752 USA

(541) 737-6559 bbgriff@peak.org griff@for.orst.edu Creator 2011-09-14 To better understand the effects vegetation has on forest soils, we established a number of sampling transects running from old-growth (OG) forests into stands with different vegetation or transects within different vegetation types without an OG component. Each transect was made up of 75 meter segments in both the OG and “treatment” stands. Soil samples and field observations were made at 5 meter-intervals along these segments. Where indicated, the OG portion of the transect acted as a pseudocontrol. The types of vegetation assemblages studied were: (1) a 26 year-old young stand (YS), (2) 6 sites showing normal to fast recovery (FAST) ranging in age from 29 to 36 years, (3) 5 sites showing slow recovery (SLOW) after clear-cutting ranging in age from 27 to 36 years, (4) 4 degraded (DEGRAD) sites ranging in age from 26 to 35 years, (5) 2 grass sites (GRASS), 26 years and undisturbed, and (6) a bracken fern site (FERN) aged at 26 years. Of these, the DEGRAD, GRASS and FERN sites showed much higher levels of denitrification potential than the other sites suggesting that mineralized fixed nitrogen was being lost from these sites at higher rates than the other vegetation types. Ectomycorrhizal mats were also essentially absent from sites as well. The concentration of living roots was highest in the YS and GRASS sites. The lowest concentrations of labile or biologically active organic carbon as measured by laboratory respiration rates, was found in the DEGRAD sites. The lowest levels of mineralizable (labile) organic nitrogen were found in the FERN site. Litter depth was lowest in the YS and GRASS sites and highest in the FERN site. There were a number of differences found between FAST and SLOW sites that reflected the different NNP activities in these stands. The concentration of ectomycorrhizal mats was greater in the FAST stands. Additionally, litter depth, field respiration rates were all greatest in the FAST stands, all of these patterns would be expected from stands with greater NPP. The concentration of mineralizable nitrogen, extractable ammonium and denitrification potentials were all lowest in the FAST stands suggesting that more organic nitrogen is being cycled and utilized by the faster growing trees. The higher concentration of mycorrhizal mats in these sites could provide the mechanism for cycling organic nitrogen a more rapid rate that in the SLOW sites where they are not as numerous. soil properties succession inorganic nutrients plants LTER controlled vocabulary Long-Term Ecological Research (LTER) Andrews Experimental Forest site thesaurus inorganic nutrients LTER core research areas References Griffiths, R. P., Bradshaw, G. A., Marks, B., and G. W. Lienkaemper. 1996. Spatial distribution of ectomycorrhizal mats in coniferous forests of the Pacific Northwest, USA. Plant and Soil 180:147-158. Griffiths, R.P., Homann, P.S., and Riley, R. (1998) Denitrification enzyme activity of Douglas-fir and red alder forest soils of the Pacific Northwest. Soil Biology and Biochemistry 30, 1147-1157. Groffman, P.M., and Tiedje, J.M. 1989. Denitrification in north temperate forest soils: relationships between denitrification and environmental factors at the landscape scale. Soil Biology & Biochemistry 21, 621-626. Hunt, H.W., Ingham, E.R., Coleman, D.C., Elliott, E.T., and Reid, C.P.P. (1988) Nitrogen limitation of production and decomposition in prairie, mountain meadow, and pine forest. Ecology 69, 1009-1016. Ingham, E R., Coleman, D.C., and Moore, J.C. (1989) An analysis of food-web structure and function in a shortgrass prairie, a mountain meadow, and a lodgepole pine forest. Biology and Fertility of Soils 8, 29-37. Keeney, D.R., and Bremner, J.M. 1966. Comparison and evaluation of laboratory methods of obtaining an index of soil nitrogen availability. Agronomical Journal 58, 498-503. Keeney, D.R., and Nelson, D.W. 1982. Nitrogen-inorganic forms. In Methods of soil analysis. Edited by A.L. Page, R.H. Miller, and D.R. Keeney. American Society of Agronomy, Madison, Wis. pp. 643-698. Köchy, M. and Wilson, S.D. (1997) Litter decomposition and nitrogen dynamics in aspen forest and mixed-grass prairie. Ecology 78, 732-739. Perry, D.A., Amaranthus, M.P., Borchers, J.G., Borchers, S.L. and Brainerd, R.E. (1989) Bootstrapping in ecosystems Biological Science 39, 230-237. Popenoe, J.H., Bevis, K.A., Gordon, B.R., Sturhan, N.K., and Hauxwell, D.L. (1992) Soil - vegetation relationships in Franciscan terrain of Northwestern California. Soil Science 56, 1951-1952. Ross, D.J., Tate, K.R., and Feltham, C.W. (1996) Microbial biomass, and C and N mineralization, in litter and mineral oils of adjacent mountain ecosystems in the southern beech (Nothofagus) forest and a tussock grassland. Tabatabai, M. A., and J. A. Bremner. (1969) Use of p-nitrophenyl phosphate for assay of soil phosphatase activity. Soil Biology & Biochemistry 1,301 - 307. Yakimenko, E.Y. (1997) Soil comparative evolution under grasslands and woodlands in the forest zone of Russia. In Management of Carbon Sequestration in Soil, eds. R. Lal, J. K. Kimble, and B.A. Stewart, pp. 391-404. CRC Press, New York. Zou, X., D. Binkley, and K. G. Doxtader. (1992) A new method for estimating gross phosphorus mineralization and immobilization rates in soils. Plant & Soil 147,243 - 2 Student workers conducting field measurements at the H.J. Andrews during the summer of 1996: Alan Swanson, Paul Graphton, Amy Rousseau, Jodi Garton, and Thomas Barnes. Alan Swanson was the field research team supervisor. Lousia Hooven conducted some of the laboratory analyses. Alan Swanson, Paul Graphton, Amy Rousseau, Jodi Garton, Lousia Hooven and Thomas .The National Science Foundation provided financial support Data Use Agreement: The re-use of scientific data has the potential to greatly increase communication, collaboration and synthesis within and among disciplines, and thus is fostered, supported and encouraged. This Data Set is released under the Creative Commons license CC BY "Attribution" (see: https://creativecommons.org/licenses/by/4.0/). Creative Commons license CC BY - Attribution is a license that allows others to distribute, remix, tweak, and build upon your work (even commercially), as long as you are credited for the original creation. This license accommodates maximum dissemination and use of licensed materials. It is considered professional conduct and an ethical obligation to acknowledge the work of other scientists. The Data User is asked to provide attribution of the original work if this data package is shared in whole or by individual parts or used in the derivation of other products. A recommended citation is provided for each Data Set in the Andrews LTER data catalog (see: http://andlter.forestry.oregonstate.edu/data/catalog/datacatalog.aspx). A generic citation is also provided for this Data Set on the website https://portal.edirepository.org in the summary metadata page. Data Users are thus strongly encouraged to consider consultation, collaboration and/or co-authorship with the Data Set Creator. While substantial efforts are made to ensure the accuracy of data and associated documentation, complete accuracy of data sets cannot be guaranteed and all data are made available "as is." The Data User should be aware, however, that data are updated periodically and it is the responsibility of the Data User to check for new versions of the data. The data authors and the repository where these data were obtained shall not be liable for damages resulting from any use or misinterpretation of the data. General acknowledgement: Data were provided by the HJ Andrews Experimental Forest research program, funded by the National Science Foundation's Long-Term Ecological Research Program (DEB 2025755), US Forest Service Pacific Northwest Research Station, and Oregon State University. If data used in publication, the PI will be listed as a co-author. Whenever these data are presented in whatever form, the PI will be acknowledged. http://andlter.forestry.oregonstate.edu/data/abstract.aspx?dbcode=SP021 1996-07-01 1996-09-30 All Organisms All Organisms Highest common category (ca. kingdom) Fungi Division or Phylum Basidiomycota Division or Phylum Basidiomycetes Order Phallales Family Hysterangiaceae Genus Hysterangium Family Gomphaceae Genus Gautieria Vegetation can profoundly influence both the chemistry and biology of soils; altering soils in a way that enhances plant community resiliency to perturbation (Perry et al.1989). To a large degree, this finding explains why forests that have been disturbed by fire, disease, wind-throw, harvesting or other factors typically return to the same vegetative assemblage that was present before the disturbance. For instance comparative studies between grasslands and forests have shown large differences in soil chemistry (Göceoðlu, 1988; Hart et al., 1992; Popenoe et al., 1992; Ross et al., 1996; Yakimenko, 1997); litter decomposition rates (Hunt et al., 1988; Köchy and Wilson, 1997) and food web compositions (Hunt et al., 1987; Ingham at al., 1989). The main objective of this study was to run a survey on the effects of different types of vegetation and rates of early succession on forest soil properties. In past studies, we had observed significant differences in soil properties in a chronosequence of post-clear-cut stands ranging in age from 5 to 40 years (seed data in study code SP07: “Disturbance effects on soil processes (stand age study))”. We found significant differences in soil properties between 5 year-year old stands and old-growth stands. The differences were essentially nonexistent after 40 years. We wanted to determine if we could detect differences in soils associated with different vegetation types (i.e. GRASS and FERN) as well as soils associated with stands with different rates of recovery after clear-cutting. The extreme on this continuum is the DEGRAD sites where essentially no conifers have become reestablished after harvest. The SLOW sites were those that did not have canopy closure after approximately 30 years and the FAST sites were ones that did. The main focus of Synthesis Area “B” of LTER4 is early plant succession. Our study was designed to provide preliminary information about how the rate of early succession might impact soil processes. The current study was an important first step before conducting a much more comprehensive study of early succession sites conducted during 1998 and 1999. The results of this more recent study are reported in the data file entitled “Influence of coniferous tree invasion on forest meadow soil properties” (study code SP012). The current study also laid the groundwork for a data set entitled “Effects of bracken fern invasions on soil processes in clear-cut marginal sites” completed in 1997. In addition, it laid the groundwork for a 1998 study of forest meadow invasion by conifers in a data set entitled “Influence of coniferous tree invasion on forest meadow soil” (See SP016).

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Andrews Forest LTER Program US Forest Service Pacific Northwest Research Station 3200 SW Jefferson Way Corvallis OR 97331

hjaweb@fsl.orst.edu http://andrewsforest.oregonstate.edu/ Robert P. Griffiths

Oregon State University;Dept. of Forest Science;321 Richardson Hall Corvallis OR 97331-5752 USA

(541) 737-6559 bbgriff@peak.org griff@for.orst.edu Andrews Forest LTER Site

Forest Ecosystems and Society Department in Forestry Oregon State University 201K Richardson Hall Corvallis OR 97331-5752

(541) 737-8480 lterweb@fsl.orst.edu http://andrewsforest.oregonstate.edu/ Field Methods - SP021 At each sample location along these transects, a 4.7 x 10 cm soil core was taken for subsequent analysis. The samples were transported to the laboratory in an ice chest and subsequently stored at 15 degrees C until the initiation of analyses, usually within 16 h of their receipt. The following measurements were made in the field: litter depth, mineral soil respiration, soil and air temperature, light levels and ectomycorrhizal mat characteristics. Field (forest floor) respiration rates were measured with a nondispersive, infrared CO2 analyzer (Li-Cor, LI-6200). Measurements were made over a period of 1 min after the chamber gas reached ambient CO2 concentration. The instrument was calibrated on site against a known standard at each location. A Q10 adjustment was made for ambient soil temperature. Electronic thermometers calibrated at 0°C with ice water measured soil temperature. The temperature probes were inserted into the mineral soil to a depth of 10 cm. The distribution of ectomycorrhizal mats was determined visually in the field by inspecting the relative abundance of mats in 4.7 x 10 cm cores. Two distinct mat types were scored: (1) mats similar to those of the genus Hysterangium and (2) mats similar to those of the genus Gautieria. This approach has been used successfully in the past to document ectomycorrhizal mat distribution patterns in coniferous forests of the Pacific Northwest (Griffiths et al. 1996). Laboratory Methods - SP021 In preparation for laboratory analyses, all soils were sieved through a 2-mm sieve. Soil moisture was determined by drying duplicate 10 g field-moist sieved soils at 100 degrees C for at least 8 h. The percent soil moisture was calculated by dividing the difference between wet and dry samples and dividing that number by the dry wt., which was then multiplied by 100. Soil pH was measured in 1:10 (soil:distilled water) slurries of oven-dried (100 degrees C) soil. These slurries were shaken for 1 h prior to reading pH values with a Sigma model E4753 electrode. Soil organic matter was measured by loss-on-ignition at 550 degrees C for 6 h after oven drying at 100 degrees C. The dry mass of live roots within the cores was measured by removing by hand roots in cores that had been dried for 8 h at 100 degrees C. Denitrification potential was measured using a method by Groffman and Tiedje (1989) as modified by us (Griffiths et al., 1998). Each reaction vessel (25-mL Erlenmeyer flask) contained 5 g of less than 2 mm, field-moist soil. Flasks were sealed with rubber serum bottle stoppers and purged with Ar to displace O2 in the headspace gas. After purging with Ar, 2 mL of a 1 mM solution of glucose and NO3- was added to each flask. Flasks were subsequently incubated at 25 degrees C for 1 h. This preincubation period was used because previous time-series experiments showed a lag in N2O production during this period. The same experiments have shown linear N2O production rates during the following 2-4 h (unpublished data). After the preincubation period, 0.5 mL of headspace gas was removed from the reaction vessel and injected into a gas chromatograph (GC) fitted with an electron capture detector (Hewlett Packard model 5890 GC, connected to a Hewlett Packard model 3396 integrator). The integrator was calibrated by the external calibration method with known gas standards. A second headspace N2O analysis was made after an additional 2-h incubation at 25 degrees C. The net N2O released over this 2-h period was used to estimate N2O production rates. Laboratory respiration measurements were made on field-moist, sieved soils (4 g dry weight). These rates represent the basal respiration rate for soil microorganisms. Soils were brought to 75% moisture content by the addition of enough sterile deionized water to equal 3 g water per 25-mL Erlenmeyer flask. Once sealed with serum bottle stoppers, the flasks were incubated at 24 degrees C for 14 days after which headspace CO2 concentrations were measured using gas chromatography. This was a measure of labile soil carbon. The same GC and integrator as were used for this assay as that used to measure N2O, but in this case a flame ionization detector and a methanizer in series were used. Substrate induced respiration (SIR) was also measured in these soils. The reaction vessels were prepared as before except 0.1 mL of 1 M glucose solution was added to the reaction vessel and the assay for CO2 evolution rates were calculated from the difference between the headspace CO2 concentrations after the first h incubation and the concentration 2 h later. SIR was calculated by subtracting CO2 evolution rates without the glucose amendment from the rates in the presence of glucose. Extractable ammonium was determined by shaking 10 g of field-moist soil with 50 mL 2 M KCl for 1 h (Keeney and Nelson 1982), adding 0.3 mL 10 M NaOH to the slurry, and measuring ammonium concentration with an Orion model 95-12 ammonium electrode (Orion Research Inc., Boston, MA). Mineralizable N was measured by the waterlogged technique of Keeney and Bremner (1966). For each analysis, 10 g of field-moist soil were added to 53 mL of distilled water in a 20 x 125 mm screw-cap test tube, and incubated at 40 degrees C for 7 d. Then 53 mL of 4 M KCl was added to the slurry, and ammonium concentration was determined with the ammonium electrode. Mineralizable N was calculated as the difference between initial and final ammonium concentrations. Beta-glucosidase activity was determined by the spectrophotometric assay of Tabatabai and Bremmer (1969), as modified by Zou et al. (1992). One mL of 10 mM p-nitrophenyl b-D glucopyranoside substrate was added to duplicate 1-mL subsamples containing a soil slurry (1 gdw in 1 mL deionized H2O). The tubes were shaken and then placed with duplicate controls without substrate in a 30 degrees C water bath for 2 h. After incubating, 1 mL of 10 mM p-nitrophenyl b-D glucopyranoside was added to the controls, and all reactions were immediately stopped by the addition of 2 mL of 0.1 M tris[hydroxymethyl]aminomethane at pH 12.0. The mixtures were centrifuged for 5 min at 500 x g. From the supernatant, 0.2 mL was diluted with 2.0 mL deionized water. The optical density was measured at 410 nm, and a standard curve was prepared from 0.02 to 1.0 micro-mol/mL p-nitrophenol (pNP). Sampling frequency: One set of measurements for each transect at each Sampling transects ran from old-growth (OG) forests into stands with different vegetation or were stand-alone transects within each vegetation type or successional type. Each transect was made up of 75 meter segments in both the OG and “treatment” stands. Soil samples and field observations were made at 5 meter-intervals along these segments. Andrews Experimental Forest (HJA) -122.26172200 -122.10084700 44.28196400 44.19770400 1631 1631 meter Cascade Head Experimental Forest -123.99172777 -123.89730000 45.06476948 45.03130000 Sherri L. Johnson

US Forest Service ;Pacific NW Research Station ;3200 SW Jefferson Way Corvallis OR 97331 USA

541-758-7771 sherri.johnson2@usda.gov sherri.johnson@oregonstate.edu https://www.fs.fed.us/research/people/profile.php?alias=sherrijohnson Principal Investigator Julia A. Jones

Oregon State University;Department of Geosciences; Wilkinson Hall 104 Corvallis OR 97331-5506 USA

(541) 737-1224 Julia.Jones@oregonstate.edu geojulia@comcast.net http://ceoas.oregonstate.edu/profile/jones/ http://orcid.org/0000-0001-9429-8925 Principal Investigator Matthew G Betts

Department of Forest Ecosystems and Society; 201E Richardson Hall; College of Forestry; Oregon State University Corvallis OR 97331

(541) 737-3841 matt.betts@oregonstate.edu http://www.fsl.orst.edu/flel/index.htm Principal Investigator Michael P. Nelson

Department of Forest Ecosystems and Society; 201K Richarson Hall; College of Forestry; Oregon State University Corvallis OR 97331

541-737-9221 mpnelson@oregonstate.edu http://www.michaelpnelson.com http://orcid.org/0000-0001-6917-4752 Principal Investigator David Bell david.bell@usda.gov david.bell@oregonstate.edu https://lemma.forestry.oregonstate.edu/about/david-bell Principal Investigator The H.J. Andrews Experimental Forest is a living laboratory that provides unparalleled opportunities for the study of forest and stream ecosystems in the central Cascade Range of Oregon. Since 1980, as a part of the National Science Foundation Long Term Ecological Research (NSF-LTER) program, the Andrews Experimental Forest has become a leader in the analysis of forest and stream ecosystem dynamics. Long-term field experiments and measurement programs have focused on climate dynamics, streamflow, water quality, and vegetation succession. Currently researchers are working to develop concepts and tools needed to predict effects of natural disturbance, land use, and climate change on ecosystem structure, function, and species composition. The Andrews Experimental Forest is administered cooperatively by the USDA Forest Service Pacific Northwest Research Station, Oregon State University and the Willamette National Forest. Funding for the research program comes from the National Science Foundation (NSF), US Forest Service Pacific Northwest Research Station, Oregon State University, and other sources. Data were provided by the HJ Andrews Experimental Forest research program, funded by the National Science Foundation's Long-Term Ecological Research Program (DEB 2025755), US Forest Service Pacific Northwest Research Station, and Oregon State University. National Science Foundation: DEB1440409 The Andrews Forest is situated in the western Cascade Range of Oregon, and covers the entire 15,800-acre (6400-ha) drainage basin of Lookout Creek. Elevation ranges from 1350 to 5340 feet (410 to 1630 m). Broadly representative of the rugged mountainous landscape of the Pacific Northwest, the Andrews Forest contains excellent examples of the region's conifer forests and associated wildlife and stream ecosystems. These forests are among the tallest and most productive in the world, with tree heights of often greater than 250 ft (75 m). Streams are steep, cold and clean, providing habitat for numerous aquatic organisms. 1 SP02101 Chemical and biochemical characteristics of soils along transects in stands with different vegetation and successional characteristics.: SP02101.csv 46410 d95e1cdd1ec4934e8693d5b1a3270306 1 \r\n column , " http://andlter.forestry.oregonstate.edu/ltermeta/ltersearch/dataaccess.aspx?docid=SP02101_v1.csv TRANSECT Transect number going from og control to treatment stand numeric(2,0) number 1.000000 natural 29.0000 47.0000 POSITION Position along each 75 meter leg; each 5 meters apart numeric(2,0) number 1.000000 whole 0.0000 75.0000 TREATMENT Treatment type; OG=oldgrowth; DEGRAD=degraded; YS=young stand char(5) Treatment type; OG=oldgrowth; DEGRAD=degraded; YS=young stand SOILTEMP Soil temperature measured with Licor numeric(5,1) degrees Celsius 0.100000 real 9.0000 25.0000 AIRTEMP Air temperature measured with Licor numeric(5,1) degrees Celsius 0.100000 real 8.0000 40.0000 LIGHT Amount of light measured with Licor numeric(5,1) micromoles per square meter per second 0.100000 real 0.0000 2000.0000 MOIST Percent moisture: ((wet-dry)/dry)*100 numeric(5,1) percent 0.100000 real 7.0000 200.0000 BULKDENS Bulk density numeric(4,2) grams per square centimeter 0.010000 real 0.0000 1.0000 LITTER Litter depth numeric(4,1) centimeters 0.100000 real 0.0000 25.0000 ROOTS Dry mass of living roots in 4.7 x 10 cm core numeric(5,3) grams 0.001000 real 0.0000 3.0000 HYSTER Percentage of core containing mycorrhizal mats like those of the genus Hysterangium numeric(3,0) percent 1.000000 whole 0.0000 100.0000 GAUT Percentage of core containing mycorrhizal mats like those of the genus Gautieria numeric(3,0) percent 1.000000 whole 0.0000 100.0000 DENIT Denitrification potential (dry weight basis, as N) numeric(6,2) nanograms per gram per hour 0.010000 real 0.0000 450.0000 EXAMM Extractable ammonium (dry weight basis) numeric(5,1) micromoles per gram 0.100000 real 0.0000 15.0000 MINN Mineralizable nitrogen (dry weight basis) numeric(5,1) micromoles per gram 0.100000 real 0.0000 70.0000 B_GLUC Beta-glucosidase activity (dry weight basis) numeric(5,3) micromoles per gram per hour 0.001000 real 0.0000 1.0000 LABRESP Laboratory respiration rates (dry weight basis) numeric(5,1) micrograms per gram per hour 0.100000 real 0.0000 200.0000 FLDRESP Field respiration rates numeric(5,1) grams per square meter per day 0.100000 real 0.0000 70.0000 NOTNULL SP02101.GAUT SP02101.HYSTER SP02101.POSITION SP02101.TRANSECT SP02101.TREATMENT 589 grams per square centimeter micromoles per g per hour nanograms/gram*hour grams per square meter per day micrograms per gram per hour micromoles per square meter per second centimeters; .01 meters micromoles per gram percent; a number grams; 0.001 kilogram Degrees Celsius; a common unit of temperature; constantToSI=273.18 dimensionless number, i.e., ratio, count