AEM
Home Help [Feedback] [For Subscribers] [Archive] [Search] [Contents]
This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrowReprints and Permissions
Right arrow Copyright Information
Right arrow Books from ASM Press
Right arrow MicrobeWorld
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Lovell, C. R.
Right arrow Articles by Bagwell, C. E.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Lovell, C. R.
Right arrow Articles by Bagwell, C. E.
Agricola
Right arrow Articles by Lovell, C. R.
Right arrow Articles by Bagwell, C. E.

 Previous Article  |  Next Article 

Applied and Environmental Microbiology, November 2001, p. 5308-5314, Vol. 67, No. 11
0099-2240/01/$04.00+0   DOI: 10.1128/AEM.67.11.5308-5314.2001
Copyright © 2001, American Society for Microbiology. All rights reserved.

Recovery and Phylogenetic Analysis of nifH Sequences from Diazotrophic Bacteria Associated with Dead Aboveground Biomass of Spartina alterniflora

Charles R. Lovell,1,* Michael J. Friez,2 John W. Longshore,2 and Christopher E. Bagwell1,dagger

Department of Biological Sciences, University of South Carolina, Columbia, South Carolina 29208,1 and Molecular Diagnostics Laboratory, Greenwood Genetic Center, Greenwood, South Carolina 296462

Received 4 June 2001/Accepted 21 August 2001


    ABSTRACT
Top
Abstract
Text
References

DNA was extracted from dry standing dead Spartina alterniflora stalks as well as dry Spartina wrack from the North Inlet (South Carolina) and Sapelo Island (Georgia) salt marshes. Partial nifH sequences were PCR amplified, the products were separated by denaturing gradient gel electrophoresis (DGGE), and the prominent DGGE bands were sequenced. Most sequences (109 of 121) clustered with those from alpha -Proteobacteria, and 4 were very similar (>99%) to that of Azospirillum brasilense. Seven sequences clustered with those from known gamma -Proteobacteria and five with those from known anaerobic diazotrophs. The diazotroph assemblages associated with dead Spartina biomass in these two salt marshes were very similar, and relatively few major lineages were represented.


    TEXT
Top
Abstract
Text
References

Low elevations of salt marshes along the Atlantic and northern Gulf of Mexico coasts of temperate North America are characterized by extensive monoculture stands of the smooth cordgrass Spartina alterniflora (35). Spartina marshes support high rates of macrophyte primary production and microbially mediated nutrient cycling. Numerous studies indicate that primary production (16, 37) and decomposition (15, 19, 38) in Spartina marshes are nitrogen limited. In these systems, diazotrophy (N2 fixation) is an important source of "new" nitrogen (8, 23, 40).

A significant but often overlooked focus of diazotrophy in salt marshes is dead aboveground Spartina biomass, particularly standing dead biomass (19, 33). There are quite large amounts of standing dead biomass at all times of the year, with ratios of dead to live aboveground biomass exceeding 1:1 during the winter and spring months (7, 31). Standing dead biomass is partially mineralized and frequently very dry (17) but supports substantial microbial activity (17-19), which is greatly stimulated when the material becomes wet through tidal action or precipitation (17). Rates of diazotrophy in moist standing dead Spartina are among the highest reported for decomposing plant materials (see Table 4 in reference 19).

Relatively little attention has been given to the microorganisms involved in decomposition of and diazotrophy in dead aboveground Spartina biomass. Much of the microbial biomass in standing dead materials consists of fungal hyphae (18). Cyanobacteria are present but occur chiefly in clay-rich surface films (18), while diazotrophy occurs primarily on and within the decaying biomass itself (19). It seems that the predominant diazotrophs in this material are heterotrophic bacteria, but the types of organisms present have not been determined.

Recent applications of molecular biological methods have greatly facilitated the study of natural bacterial communities and functionally significant taxa within them (9, 34, 39, 42). In particular, PCR amplification has been used to recover segments of nifH, the structural gene encoding the nitrogenase iron protein, from various types of environmental samples, including marine and freshwater plankton (1, 3, 44), termite hindguts (11, 20), microbial mats and aggregates (21, 22, 43), terrestrial soils (28, 29, 32, 41), the rhizoplanes of rice (Oryza sativa) (36) and of shoal grass (Halodule wrightii) (10), and the rhizosphere of Spartina (14). PCR amplification of nifH sequences followed by their separation through denaturing gradient gel electrophoresis (DGGE) has been used to examine the complexity and stability of the diazotroph assemblage found in the Spartina rhizosphere (25-27), and sequence analysis of the DGGE bands has been used to determine phylogenetic relationships of the diazotrophic organisms represented (14). While such methods have certain inherent limitations and biases (25, 42), they provide an efficient means to profile the diazotrophs associated with dead aboveground Spartina biomass and to determine the phylogenetic affiliations of these organisms.

In this study we determined the types of diazotrophic heterotrophic bacteria present in standing dead and loose, recently deposited (wrack) Spartina biomass, as defined by recoverable partial nifH sequences resolved by DGGE. Our primary objectives were to assess the diversity of these assemblages and to identify the major phylogenetic groups of organisms that are capable of contributing to N2 fixation in dead aboveground Spartina biomass.

Sampling sites. Samples of standing dead Spartina stalks and Spartina wrack were collected from the short-form Spartina zones in two different salt marsh systems. The Crab Haul Creek Basin site in the North Inlet estuary, near Georgetown, S.C. (79°12'W, 33°20'N), was located in the intertidal zone approximately 50 m from the nearest tidal creek and was sampled on 31 August 2000. The Doboy Sound site on Sapelo Island, Ga. (31°23'N, 81°17'W), was located in the intertidal zone near Doboy Sound (Georgia Coastal Ecosystems Long Term Ecological Research Site 6) and was sampled on 1 August 2000. The upper, approximately 10-cm lengths of dry standing dead stalks were collected. Dry wrack, which consisted of loose stalks (litter) recently deposited on the sediment surface, was collected from deposits lying near the sampling locations for standing dead stalks. Standing dead stalks and wrack were transferred to sterile Whirl-Pak bags and stored at -70°C pending DNA extraction.

DNA extraction. Standing dead and wrack stalks were broken up into 2-cm fragments. DNA was extracted from the samples using a direct lysis procedure described previously (13, 25). DNA extracts were further purified and concentrated using the Wizard DNA clean-up system following the manufacturer's instructions (Promega, Madison, Wis.). DNA quality and quantity were assessed by agarose gel electrophoresis and fluorometry, respectively.

PCR amplification of nifH. PCR was performed using Taq DNA polymerase (Qiagen, Valencia, Calif.) in a reaction mixture containing (25-µl reaction volume) 25 ng of template DNA, 1.5 mM MgCl2, 2 µM deoxynucleoside triphosphate (dNTP) mixture, 0.5 pmol of each primer, and 10 µg of bovine serum albumin. The nifH primers used were those of Piceno et al. (25) and are specific for heterotrophic diazotrophs. These primers were designed to have low degeneracy, which is needed for DGGE applications, and are not expected to amplify nifH sequences from cyanobacteria, Frankia spp., and methanogens. Primer design and testing have been described previously (25). Amplification was initiated by a denaturation step at 94°C for 2 min and proceeded in two phases: (i) a 20-cycle touchdown program (94°C for 45 s, 58°C for 30 s, decreasing 0.5°C/cycle, and 70°C for 30 s), and (ii) 20 cycles of a standard amplification program at a 48°C annealing temperature for 30 s. A final extension step at 70°C for 2 min was used. Multiple individual reactions were performed for each sample. PCR products were pooled (200-µl final volume per sample) and stored as alcohol precipitates at -20°C. Prior to DGGE, amplimers were recovered by centrifugation and dissolved in 15 µl of TE (10 mM Tris-HCl [pH 8.0], 1 mM EDTA).

DGGE. nifH amplimers were electrophoresed on denaturing gradient gels (1-mm thick, 6.5% polyacrylamide, 78 to 89% denaturant, where 100% denaturant contains 7 M urea and 40% formamide) at 48°C for 1,900 V · h using the Bio-Rad (Hercules, Calif.) DCode universal mutation detection system. Gels were stained for 30 min in TE with SYBR Gold (Molecular Probes, Eugene, Oreg.) and documented using the Alpha Imager 2000 (Alpha Innotech Corp., San Leandro, Calif.). Gel plugs were collected from all well-resolved bands in the profiles using wide-bore micropipette tips and stored in 50 µl of distilled water at -20°C. Gel bands were designated homoduplexes or heteroduplexes following previously described methods (25).

Amplimer cloning and identification of different cloned amplimer sequences. Amplimers from DGGE gel plugs were recovered by reamplification and cloned as described previously (14). Recombinant colonies were maintained on Luria-Bertani agar plates containing 100 µg of ampicillin ml-1. Clones were screened for appropriately sized insert by amplification using primers specific for the SP6 and T7 RNA polymerase binding sites (14). Restriction fragment length polymorphism analysis was employed to assess gel band amplimer composition (i.e., homogeneous or heterogeneous) and to identify different clones for sequencing (14).

DNA sequencing and analysis. Recombinant plasmids were purified from selected clones by using the Qiagen Plasmid Mini Kit. Plasmid concentrations were determined fluorometrically. Sequencing reactions used T7 and Sp6 primers and ABI (Applied Biosystems, Foster City, Calif.) BigDye version 2.0 chemistry. Sequences were determined using an ABI 3100 genetic analyzer. For phylogenetic reconstructions, nifH sequences from numerous different known diazotrophs and from various environmental sources were selected using the Blast search feature of the NCBI GenBank database (2). Nucleotide sequences were translated, and the inferred amino acid sequences were aligned (5) and checked by hand for proper alignment of conserved marker residues (14). Neighbor-joining phylogenies (30) were constructed in MEGA version 2.0 (12) using percent dissimilarity distances and pairwise deletion of gaps and missing data. The use of alternative amino acid distance measures (e.g., Poisson and gamma correction for multiple substitutions) or tree construction methods (neighbor joining or Unweighted Pair Group Method Using Arithmetic Averages) had no significant effect on the resulting dendrogram topology (data not shown). NifH amino acid sequences from Methanobacterium thermoautotrophicum (accession no. AE00916) and Methanosarcina barkeri (X56072) were used as outgroup taxa. Bootstrapping (6) was used to estimate the reliability of phylogenetic reconstructions (500 replicates).

All dead aboveground Spartina biomass samples yielded strong amplification products, although the North Inlet samples produced substantially stronger amplification than the Sapelo Island samples (Fig. 1). DGGE yielded 16 well-resolved nifH amplimer bands from North Inlet standing dead biomass and 9 bands from wrack. Due to somewhat lower yields of amplification products from the Sapelo Island samples, only five robust bands were recovered from the standing dead material and four bands from wrack. All of these bands were successfully sampled, and the amplimers were cloned and screened for unique sequences. An artifact band, which was described previously (25), was also observed in each sample lane. A total of 54 different partial nifH sequences were recovered from standing dead Spartina and 24 from Spartina wrack collected at North Inlet. Twenty-one different sequences were recovered from the standing dead material and 20 from the wrack from Sapelo Island.


View larger version (108K):
[in this window]
[in a new window]
  		FIG. 1.   Denaturing gradient gel images showing nifH amplimers from dead aboveground Spartina biomass. PCR and DGGE conditions are described in Materials and Methods. Lanes: A, North Inlet standing dead Spartina; B, North Inlet Spartina wrack; C, Sapelo Island standing dead; D, Sapelo Island wrack; Art., artifact.

The partial nifH sequences were initially translated and examined for key, highly conserved amino acid residues that are important in nitrogenase iron protein structure and function (4, 24). Within the segments analyzed, 11 amino acids, including (Klebsiella pneumoniae [J01740] numbering) Lys15 and Ser16 (within the MgATP binding domain), Arg100 (the ADP-ribosylation site), Asp125 (possibly involved in protein conformation changes), Asp129 (involved in ATP hydrolysis), Arg140 and Lys143 (contribute to salt bridge formation), and four conserved Cys residues (numbers 38, 85, 97, and 132, two of which coordinate the Fe4S4 cluster), were used as markers for determining sequence accuracy. Four sequences had one substitution each: NIS2-1 and SIW2-6, Cys85 replaced by Arg85; NIS3-2, Ser16 replaced by Trp16; and NIW8-1, Cys97 replaced by Arg97. All sequences were used in subsequent analyses.

The sequences from dead aboveground Spartina biomass and their closest affiliations with known diazotrophs on the basis of sequence similarity are listed in Table 1. As has been reported in numerous previous studies of environmental nifH sequences (1, 3, 14, 29, 36, 41, 43, 44), these sequences fell into three major clusters. The overwhelming majority of dead Spartina nifH sequences were affiliated with a cluster defined by sequences from alpha -Proteobacteria and well supported by bootstrapping (Fig. 2). Forty-six of 54 sequences (85%) from the North Inlet standing dead sample, all 24 of the sequences from North Inlet wrack (100%), 19 of 21 sequences (90%) from the Sapelo Island standing dead sample, and 17 of 20 sequences (85%) from Sapelo Island wrack were from presumptive alpha -Proteobacteria. These sequences were further subdivided into a number of smaller clusters, some of which contained nifH sequences from known diazotrophs.

                              
View this table:
[in this window]
[in a new window]
  		TABLE 1.   Similarities of dead aboveground Spartina biomass NifH amino acid sequences to the most similar sequences from known diazotrophic bacterial speciesa



View larger version (20K):
[in this window]
[in a new window]
  		FIG. 2.   Phylogenetic analysis of dead aboveground Spartina biomass NifH amino acid sequences from presumptive alpha -Proteobacteria, from various known alpha -Proteobacteria, and from selected unknown, presumptive alpha -Proteobacteria from other sources. NIS, North Inlet standing dead Spartina; NIW, North Inlet Spartina wrack; SIS, Sapelo Island standing dead Spartina; SIW, Sapelo Island Spartina wrack. The percentage of 500 bootstrap samples that supported each branch is shown. Bootstrap values below 50% are not shown.

Several sequences from North Inlet standing dead Spartina biomass were closely affiliated with purple nonsulfur bacteria, and seven had substantial similarity (>= 96%) to the Rhodobacter sphaeroides NifH sequence (Table 1). Several sequences from all sample types were over 95% similar to the Gluconacetobacter diazotrophicus sequence. Another group of eight sequences from North Inlet samples were substantially similar (>= 95%) to NifH sequences from rhizobia. Seven of these were over 97% similar to a Bradyrhizobium japonicum sequence. Another substantial sequence grouping, predominantly from the Sapelo Island standing dead sample, was strongly affiliated with the NifH sequence from Azospirillum brasilense. Four of these had 99% or greater similarity to the A. brasilense sequence, and two were identical to it. The NifH sequences of A. brasilense and Azospirillum lipoferum are 99.3% similar, so at least four of the dead Spartina biomass NifH sequences were very likely from Azospirillum species and two seemingly from a strain of A. brasilense. This finding confirms the prediction of Newell et al. (19) that Azospirillum-like organisms may be involved in degradation of standing dead Spartina biomass. There were also many sequences that were not closely affiliated with any known diazotrophs among the alpha -Proteobacteria. Blast searches of the NCBI GenBank database revealed only a few sequences from other types of environmental samples that had meaningful similarity to any sequences from dead aboveground Spartina biomass. Among these were four sequences recovered from the Spartina rhizosphere (14).

The second major cluster containing sequences from dead aboveground Spartina biomass was characterized by sequences from gamma -Proteobacteria (Fig. 3). This cluster contained three sequences from standing dead Spartina whose positions were ambiguous. When these three sequences were omitted and the tree was reconstructed, the gamma -Proteobacteria cluster was strongly supported by bootstrap analysis (60% for the cluster as a whole, 96 and 91% for the two major subclusters). Omitting these sequences also raised the bootstrap score for the alpha -Proteobacteria cluster from 76 to 99%. One of the remaining seven presumptive gamma -Proteobacteria sequences was very strongly affiliated with the Azotobacteriaceae, with over 99% similarity to the NifH sequences of Azomonas agilis and Azotobacter chroococcum (Table 1). For comparison, the NifH sequences of A. chroococcum and Azotobacter vinelandii are 99.3% similar. Two other sequences also had substantial similarity (>= 95%) to sequences from azotobacteria. The only other sequence with strong similarity to a sequence from a known organism was a North Inlet standing dead sequence that was >98% similar to the sequence from Pseudomonas stutzeri. As was the case for sequences from presumptive alpha -Proteobacteria, few environmental sequences were substantially similar to those from dead aboveground Spartina biomass, and these were from the Spartina rhizosphere.


View larger version (34K):
[in this window]
[in a new window]
  		FIG. 3.   Phylogenetic analysis of dead aboveground Spartina biomass NifH amino acid sequences from presumptive gamma -Proteobacteria, from various known gamma -Proteobacteria, and from selected unknown, presumptive gamma -Proteobacteria from other sources. NIS, North Inlet standing dead Spartina; NIW, North Inlet Spartina wrack; SIS, Sapelo Island standing dead Spartina; SIW, Sapelo Island Spartina wrack. The percentage of 500 bootstrap samples that supported each branch is shown. Bootstrap values below 50% are not shown.

Only five sequences recovered from dead aboveground Spartina biomass were affiliated with the remaining major NifH sequence cluster, the anaerobes (Fig. 4). While the closest affiliations of these sequences to any from known organisms were all with sulfate-reducing bacteria, none of the dead Spartina NifH sequences were sufficiently similar to any sequence from a known diazotroph to permit even presumptive identification. Two sequences from the North Inlet standing dead sample were similar to sequences from Spartina rhizosphere, but since the rhizosphere core samples contained both roots and sediments, and the dead aboveground biomass samples all carried a small amount of sediment, these sequences may be from sediment diazotrophs rather than species closely affiliated with the decomposing plant materials.


View larger version (35K):
[in this window]
[in a new window]
  		FIG. 4.   Phylogenetic analysis of dead aboveground Spartina biomass NifH amino acid sequences from unknown, presumptive anaerobic bacterial sequences, from various known anaerobic bacteria, and from selected unknown, presumptive anaerobic bacteria from other sources. NIS, North Inlet standing dead Spartina; NIW, North Inlet Spartina wrack; SIS, Sapelo Island standing dead Spartina; SIW, Sapelo Island Spartina wrack. The percentage of 500 bootstrap samples that supported each branch is shown. Bootstrap values below 50% are not shown.

NifH sequences recovered from dead Spartina biomass reflected a diazotroph assemblage of very limited diversity, consisting almost exclusively of alpha -Proteobacteria. Some of these organisms are apparently related to known diazotrophs, including Azospirillum brasilense, Bradyrhizobium japonicum, Gluconacetobacter diazotrophicus, and Rhodobacter sphaeroides. Very few sequences from dead Spartina biomass were affiliated with the other major NifH sequence groups. However, it is noteworthy that among the few sequences recovered from presumptive gamma -Proteobacteria, several were quite similar to those from known diazotrophs, including Azomonas agilis, Azotobacter chroococcum, and Pseudomonas stutzeri. While it is certainly possible that some sequences were lost due to PCR biases or other artifacts (25, 42), identical methods have yielded much more diverse sequence collections from other sample types (14; Lovell et al., unpublished data). It appears that while the relatively harsh (partially mineralized and frequently dry) microenvironments represented by dead aboveground Spartina biomass can support impressive rates of diazotrophy (19) when wet, they pose a substantial challenge for many diazotrophic biota and consequently harbor a very restricted range of organisms.

Nucleotide sequence accession numbers. The nifH sequences determined in this study are available in the GenBank database under accession numbers AF389702 to AF389823.


    ACKNOWLEDGMENTS

We acknowledge Steven Newell for assistance with Sapelo Island sampling site identification and the Belle W. Baruch Institute for Marine and Coastal Research for access to North Inlet sampling sites.

This research was supported by NSF award DEB-9903623 to C.R.L.


    FOOTNOTES

* Corresponding author. Mailing address: Department of Biological Sciences, University of South Carolina, Columbia, SC 29208. Phone: (803) 777-7036. Fax: (803) 777-4002. E-mail: lovell{at}biol.sc.edu.

dagger Present address: Environmental Sciences Division, Oak Ridge National Laboratory, Oak Ridge, TN 37831.


    REFERENCES
Top
Abstract
Text
References

1. Affourtit, J., J. P. Zehr, and H. W. Paerl. 2001. Distribution of nitrogen-fixing microorganisms along the Neuse River Estuary, North Carolina. Microb. Ecol. 41:114-123[Medline].
2. Benson, D. A., M. S. Boguski, D. J. Lipman, J. Ostell, and B. F. F. Ouellette. 1998. GenBank. Nucleic Acids Res. 26:1-7[Abstract/Free Full Text].
3. Braun, S. T., L. M. Proctor, S. Zani, M. T. Mellon, and J. P. Zehr. 1999. Molecular evidence for zooplankton-associated nitrogen-fixing anaerobes based on amplification of the nifH gene. FEMS Microbiol. Ecol. 28:273-279[CrossRef].
4. Dean, D. R., and M. R. Jacobson. 1992. Biochemical genetics of nitrogenase, p. 763-834. In G. Stacey, R. H. Burris, and H. J. Evans (ed.), Biological nitrogen fixation. Chapman and Hall, New York, N.Y.
5. Devereux, J., P. Haeberli, and O. Smithies. 1984. A comprehensive set of sequence analysis programs for the VAX. Nucleic Acids Res. 12:387-395.
6. Felsenstein, J. 1985. Confidence limits on phylogenies: an approach using the bootstrap. Evolution 39:783-791[CrossRef].
7. Gallagher, J. L., R. J. Reimold, R. A. Linthurst, and W. J. Pfeiffer. 1980. Aerial production, mortality, and mineral accumulation-export dynamics in Spartina alterniflora and Juncus roemerianus plant stands in a Georgia salt marsh. Ecology 61:303-312[CrossRef].
8. Hanson, R. B. 1983. Nitrogen fixation activity (acetylene reduction) in the rhizosphere of salt marsh angiosperms, Georgia, USA. Bot. Mar. 26:49-59.
9. Head, I. M., J. R. Saunders, and R. W. Pickup. 1998. Microbial evolution, diversity, and ecology: a decade of ribosomal RNA analysis of uncultivated microorganisms. Microb. Ecol. 35:1-21[CrossRef][Medline].
10. Kirshtein, J. D., H. W. Paerl, and J. Zehr. 1991. Amplification, cloning, and sequencing of a nifH segment from aquatic microorganisms and natural communities. Appl. Environ. Microbiol. 57:2645-2650[Abstract/Free Full Text].
11. Kudo, T., M. Ohkuma, S. Moriya, S. Noda, and K. Ohtoko. 1998. Molecular phylogenetic identification of the intestinal anaerobic microbial community in the hindgut of the termite Reticulitermes speratus, without cultivation. Extremophiles 2:155-161[CrossRef][Medline].
12. Kumar, S., K. Tamura, I. B. Jakobsen, and M. Nei. MEGA2: molecular evolutionary genetics analysis, version 2.0. Bioinformatics, in press.
13. Lovell, C. R., and Y. M. Piceno. 1994. Purification of DNA from estuarine sediments. J. Microbiol. Methods 20:161-174[CrossRef].
14. Lovell, C. R., Y. M. Piceno, J. M. Quattro, and C. E. Bagwell. 2000. Molecular analysis of diazotroph diversity in the rhizosphere of the smooth cordgrass Spartina alterniflora. Appl. Environ. Microbiol. 66:3814-3822[Abstract/Free Full Text].
15. Marinucci, A. C., J. E. Hobbie, and J. V. K. Helfrich. 1983. Effect of litter nitrogen on decomposition and microbial biomass in Spartina alterniflora. Microb. Ecol. 9:27-40.
16. Morris, J. T. 1991. Effects of nitrogen loading on wetland ecosystems with particular reference to atmospheric deposition. Annu. Rev. Ecol. Syst. 22:257-279[CrossRef].
17. Newell, S. Y., R. D. Fallon, R. M. Cal Rodriguez, and L. C. Groene. 1985. Influence of rain, tidal wetting and relative humidity on release of carbon dioxide by standing-dead salt-marsh plants. Oecologia 68:73-79[CrossRef].
18. Newell, S. Y., R. D. Fallon, and J. D. Miller. 1989. Decomposition and microbial dynamics for standing, naturally positioned leaves of the salt-marsh grass Spartina alterniflora. Mar. Biol. 101:471-481[CrossRef].
19. Newell, S. Y., C. S. Hopkinson, and L. A. Scott. 1992. Patterns of nitrogenase activity (acetylene reduction) associated with standing, decaying shoots of Spartina alterniflora. Estuar. Coast. Shelf Sci. 35:127-140[CrossRef].
20. Ohkuma, M., S. Noda, R. Usami, K. Horikoshi, and T. Kudo. 1996. Diversity of nitrogen fixation genes in the symbiotic intestinal microflora of the termite Reticulitermes speratus. Appl. Environ. Microbiol. 62:2747-2752[Abstract].
21. Olson, J. B., T. F. Steppe, R. W. Litaker, and H. W. Paerl. 1998. N2-fixing microbial consortia associated with the ice cover of Lake Bonney, Antarctica. Microb. Ecol. 36:231-238[CrossRef][Medline].
22. Olson, J. B., R. W. Litaker, and H. W. Paerl. 1999. Ubiquity of heterotrophic diazotrophs in marine microbial mats. Aquat. Microb. Ecol. 19:29-36.
23. Patriquin, D. G., and C. R. McClung. 1978. Nitrogen accretion, and the nature and possible significance of N2 fixation (acetylene reduction) in a Nova Scotian Spartina alterniflora stand. Mar. Biol. 47:227-242[CrossRef].
24. Peters, J. W., K. Fisher, and D. R. Dean. 1995. Nitrogenase structure and function: a biochemical-genetic perspective. Annu. Rev. Microbiol. 49:335-366[CrossRef][Medline].
25. Piceno, Y. M., P. A. Noble, and C. R. Lovell. 1999. Spatial and temporal assessment of diazotroph assemblage composition in vegetated salt marsh sediments using denaturing gradient gel electrophoresis analysis. Microb. Ecol. 38:157-167[CrossRef][Medline].
26. Piceno, Y. M., and C. R. Lovell. 2000. Stability in natural microbial communities. I. Nutrient addition effects on rhizosphere diazotroph assemblage composition. Microb. Ecol. 39:32-40[CrossRef][Medline].
27. Piceno, Y. M., and C. R. Lovell. 2000. Stability in natural microbial communities. II. Plant resource allocation effects on rhizosphere diazotroph assemblage composition. Microb. Ecol. 39:41-48[CrossRef][Medline].
28. Poly, F., L. Ranjard, S. Nazaret, F. Gourbière, and L. J. Monrozier. 2001. Comparison of nifH gene pools in soils and soil microenvironments with contrasting properties. Appl. Environ. Microbiol. 67:2255-2262[Abstract/Free Full Text].
29. Rosado, A. S., G. F. Duarte, L. Seldin, and J. D. Van Elsas. 1998. Genetic diversity of nifH gene sequences in Paenibacillus azotofixans strains and soil samples analyzed by denaturing gradient gel electrophoresis of PCR-amplified gene fragments. Appl. Environ. Microbiol. 64:2770-2779[Abstract/Free Full Text].
30. Saitou, N., and M. Nei. 1987. The neighbor-joining method: a new method for reconstructing phylogenetic trees. Mol. Biol. Evol. 4:406-425[Abstract].
31. Schubauer, J. P., and C. S. Hopkinson. 1984. Above- and belowground emergent macrophyte production and turnover in a coastal marsh ecosystem, Georgia. Limnol. Oceanogr. 29:1052-1065.
32. Shaffer, B. T., F. Widmer, L. A. Porteous, and R. J. Seidler. 2000. Temporal and spatial distribution of the nifH gene of N2-fixing bacteria in forests and clearcuts in western Oregon. Microb. Ecol. 39:12-21[CrossRef][Medline].
33. Thomson, A. D., and K. L. Webb. 1984. The effect of chronic oil pollution on salt-marsh nitrogen fixation (acetylene reduction). Estuaries 7:2-11.
34. Tunlid, A. 1999. Molecular biology: a linkage between microbial ecology, general ecology and organismal biology. Oikos 85:177-189.
35. Turner, R. E. 1976. Geographic variations in salt marsh macrophyte production: a review. Contrib. Mar. Sci. 20:47-68.
36. Ueda, T., Y. Suga, N. Yahiro, and T. Matsuguchi. 1995. Remarkable N2-fixing bacterial diversity detected in rice roots by molecular evolutionary analysis of nifH gene sequences. J. Bacteriol. 177:1414-1417[Abstract/Free Full Text].
37. Valiela, I., and J. M. Teal. 1974. Nutrient limitation in salt marsh vegetation, p. 547-563. In R. J. Riemold, and W. H. Queen (ed.), Ecology of halophytes. Academic Press, New York, N.Y.
38. Valiela, I., J. M. Teal, S. D. Allen, R. Van Etten, D. Goehringer, and S. Volkmann. 1985. Decomposition in salt marsh ecosystems: the phases and major factors affecting disappearance of above-ground organic matter. J. Exp. Mar. Biol. Ecol. 89:29-54[CrossRef].
39. Ward, D. M., M. J. Ferris, S. C. Nold, and M. M. Bateson. 1998. A natural view of microbial biodiversity within hot spring cyanobacterial mat communities. Microbiol. Mol. Biol. Rev. 62:1353-1370[Abstract/Free Full Text].
40. Whiting, G. J., and J. T. Morris. 1986. Nitrogen fixation (C2H2 reduction) in a salt marsh: its relationship to temperature and an evaluation of an in situ chamber technique. Soil Biol. Biochem. 18:515-521[CrossRef].
41. Widmer, S., B. T. Shaffer, L. A. Porteous, and R. J. Seidler. 1999. Analysis of nifH gene pool complexity in soil and litter at a Douglas fir forest site in the Oregon Cascade mountain range. Appl. Environ. Microbiol. 65:374-380[Abstract/Free Full Text].
42. Zehr, J. P., and D. G. Capone. 1996. Problems and promises of assaying the genetic potential for nitrogen fixation in the marine environment. Microb. Ecol. 32:263-281[Medline].
43. Zehr, J. P., M. Mellon, S. Braun, W. Litaker, T. Steppe, and H. W. Paerl. 1995. Diversity of heterotrophic nitrogen fixation genes in a marine cyanobacterial mat. Appl. Environ. Microbiol. 61:2527-2532[Abstract].
44. Zehr, J. P., M. T. Mellon, and S. Zani. 1998. New nitrogen-fixing microorganisms detected in oligotrophic oceans by amplification of nitrogenase (nifH) genes. Appl. Environ. Microbiol. 64:3444-3450[Abstract/Free Full Text].

Applied and Environmental Microbiology, November 2001, p. 5308-5314, Vol. 67, No. 11
0099-2240/01/$04.00+0   DOI: 10.1128/AEM.67.11.5308-5314.2001
Copyright © 2001, American Society for Microbiology. All rights reserved.


This article has been cited by other articles:


This Article
Right arrow Abstract Freely available
Right arrow Full Text (PDF)
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Similar articles in this journal
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Download to citation manager
Right arrowReprints and Permissions
Right arrow Copyright Information
Right arrow Books from ASM Press
Right arrow MicrobeWorld
Citing Articles
Right arrow Citing Articles via HighWire
Right arrow Citing Articles via Google Scholar
Google Scholar
Right arrow Articles by Lovell, C. R.
Right arrow Articles by Bagwell, C. E.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Lovell, C. R.
Right arrow Articles by Bagwell, C. E.
Agricola
Right arrow Articles by Lovell, C. R.
Right arrow Articles by Bagwell, C. E.

Home Help [Feedback] [For Subscribers] [Archive] [Search] [Contents]
J. Bacteriol. Microbiol. Mol. Biol. Rev. Eukaryot. Cell All ASM Journals