Abstract
Due to disruption of soil aggregates and cell lysis and the subsequent release of organic C and N, increased microbial N transformation processes can be observed after freeze–thaw cycles. In a microcosm study, we investigated the influence of plant residues with different C/N ratios (lucerne-clover-grass-mix and wheat straw) on N transformations and the abundance pattern of the corresponding functional genes in an arable soil after freezing and thawing. Unfrozen soil samples, continuously incubated at 10°C, served as control. Concentration of soil NH +4 , NO −3 , and water-extractable organic C (WEOC) as well as genes involved in nitrification and denitrification, quantified by real-time PCR, were determined before freezing and 1, 3, and 7 days after thawing. The amounts of inorganic N and WEOC as well as the investigated gene abundance pattern did hardly differ between control samples and samples subjected to freezing and thawing that have been amended with straw. In contrast, clear alterations of the measured parameters and abundances were observed after freezing and thawing in samples being amended with the lucerne-clover-grass-mix compared to the control samples.
Explore related subjects
Discover the latest articles, news and stories from top researchers in related subjects.Avoid common mistakes on your manuscript.
Introduction
Factors driving microbial N cycle in soils during the vegetation period have been studied in detail in the last decades. It has been clearly shown that many factors such as mineral N and available C contents, oxygen concentration, soil water content, pH value, and temperature (Davidson and Kingerlee 1997) influence the N transformation rates. Although high denitrification rates during the winter months have been observed accounting for up to 30% of the annual N2O emissions from agricultural soils (Ruser et al. 1998), there is still a lack of understanding how N turnover is regulated during the cold time of the year (Phillips 2008).
Legumes and legume–grass mixtures, frequently used as green manure in organic farming, might be one factor influencing N turnover in winter. These plants are cropped in autumn, remain on the fields over winter, and supply plants in the following vegetation period with N. Due to the low C/N ratio of green manures compared to other plant residues (e.g., straw of cereals, which is left on the fields after harvest in autumn), more N is also available for microbial activities. However, it is poorly understood how and under which conditions the N of the plant residues is transformed during the winter months. We expected that due to freeze–thaw processes and the increased amounts of available C, e.g., microbes involved in denitrification will become more abundant depending on the quality and amount of applied N.
Therefore, we investigated the influence of two common agricultural plant residues (wheat straw and lucerne-clover-grass-mix) considerably differing in their C quality and C/N ratio on nitrifiers and denitrifiers based on abundance of the functional genes for the ammonia monooxygenase gene amoA and the nitrite reductase genes nirK and nirS, respectively, and on mineral N fractions (NO −3 and NH +4 ) after a freeze–thaw cycle.
Materials and methods
The experimental site is located on the research farm “Klostergut Scheyern” in Southern Germany (48°30.0′ N; 11°20.7′ N). Soil samples were taken from an arable field (Cambisol) in September 2008 several weeks after harvest of summer wheat. The upper 20 cm of the plowed soil horizon were sampled and characterized as follows: 22% clay, 36% silt, and 42% sand; 1.5% organic C, C/N ratio of 10.0; pH value 5.8 (0.01 M CaCl2). The soil was sieved at 2 mm and air-dried at room temperature.
Wheat straw and growth of a lucerne-clover-grass-mix were chosen as organic amendment reflecting common agricultural situations at field sites in autumn and winter. The different plant residues exhibited similar C contents (43.6% and 42.1%, respectively) but differed considerably in their C/N ratios (126.6 and 10.1, respectively), recalcitrance, and biodegradability (Mueller et al. 1998; Nicolardot et al. 2007; Wang et al. 2004). The residues were air-dried and ball-milled (Retsch MM2, Germany) before application.
The experiment was set up in the following way: 50 g soil was amended with 2 g of the respective plant residues and incubated in cylinders of 4-cm height and a volume of 100 cm3. Thus, similar amounts of C were added to the soil (corresponding to 222 dt C ha−1), however of different quality and C/N ratios. Per treatment and sampling time point, four independent replicate cylinders were prepared. All samples were equilibrated during a pre-incubation period of 2 weeks at 10°C and 60% water holding capacity. Half of the samples were then frozen for 3 days at −20°C and afterwards returned to 10°C; the other half of the samples remained constant at 10°C. Sampling was carried out at day 0 (day before freezing) and days 4, 6, and 10 (1, 3, and 7 days after thawing), respectively.
Aliquots of soil samples were immediately extracted with 0.01 M CaCl2 [soil/CaCl2 ratio 1:2 (wt/wt)] according to Zsolnay (2003). Both NH +4 –N and NO −3 –N concentrations were measured using the Nanocolor Ammonium 3 and Nanocolor Nitrat 50 kit (Merck, Germany), respectively. The concentrations of water-extractable organic C (WEOC) were determined by DIMATOC 100 (DIMATEC, Germany) in the extracts.
The remaining soil was stored at −20°C until soil DNA was extracted according to Griffiths et al. (2000). Gene abundances of functional genes related to nitrification [archaeal amoA (AOA) and bacterial amoA (AOB)] and denitrification (nirK and nirS) were measured by SybrGreen-based quantitative real-time PCR, using the 7300 Real-Time PCR System (Applied Biosystems, Germany) as described by Hai et al. (2009). Briefly, the reaction volumes consisted of 25 µl including 12.5 μl Power SYBR® Green PCR Master Mix (Applied Biosystems), 0.5 μl 3% BSA (Sigma-Aldrich, Germany), 0.625 μl DMSO (Sigma, Germany), 2 μl DNA template, 0.5 μl of each primer (10 µM, Table 1), and 8.375 μl 0.1% DEPC water. All samples and standard curves (serial plasmid dilutions from 101 to 106 gene copies µl−1) were performed in triplicates, and at least four negative controls without DNA template were run per plate. Amplification efficiencies of 81–86% (amoA AOA), 79–82% (amoA AOB), 85–90% (nirK), and 86–91% (nirS) were achieved. Copy numbers were related to 1 g of dry soil.
Statistical analyses were carried out using SPSS 11.5. Prior to analysis, data were checked for normal distribution and homogeneity of variances by the Kolmogorov–Smirnov test and the Levene test, respectively. The effect of the freeze–thawing, respectively, of the organic amendments at a given time point were tested on significance with the t test (P < 0.05).
Results and discussion
Due to the low N input in the straw treatment, soil NH +4 and NO −3 concentrations did not differ between the samples treated by freezing and thawing and the control samples constantly kept at 10°C. The measured concentrations remained low (3.3–5.5 µg NO −3 –N and up to 0.3 µg NH +4 –N g−1, respectively) and did not change during the investigation period (Fig. 1a, b). Similar observations were made for the soil WEOC contents in this treatment (28.3–54.2 µg C g−1; Fig. 1c). In contrast, addition of the lucerne-clover-grass-mix significantly increased the soil NO −3 –N (56.5–113.6 µg g−1), NH +4 –N (54.0–70.6 µg g−1), and WEOC (126.3–195.8 µg g−1) concentrations compared to the straw amendment (Fig. 1a–c). In this treatment, freezing and thawing significantly increased the amount of NH +4 –N and WEOC and led to lower NO −3 –N concentrations compared to the non-frozen control samples.
It is generally accepted that the amount of available inorganic N is one of the factors regulating denitrification rates in soil (Phillips 2008). Our results support our hypothesis that this is not only true for the vegetation period but can be extended to the winter period. Clark et al. (2009) could show that nitrification was the cause of NO −3 accumulation in frozen soils, and this process was consequently limited by NH +4 availability. Therefore, higher NH +4 concentrations are often associated with increased NO −3 concentrations (Elliott and Henry 2009).
High amounts of NH +4 during mid-winter thawing periods might be a result of increased soil protease activity, which is also related to the availability of C (Mrkonjic Fuka et al. 2009). In our study, we found higher concentrations of WEOC in the samples amended with the lucerne-clover-grass-mix (Fig. 1c) and correlating higher NH +4 concentrations. Moreover, WEOC determines denitrification activities (Phillips 2008). Thus, WEOC affects N turnover in two ways: on the one hand it stimulates the protease activity and the formation of inorganic N, and on the other hand it is a prerequisite for denitrification.
According to the different amounts of soil inorganic N and readily available organic C in the two treatments, higher abundances of genes involved in nitrification (AOA 0.8–1.6 × 106 and AOB 0.2–1.1 × 107 amoA copies g−1; Fig. 2a, b) and denitrification (nirK 2.0–2.5 × 108 and nirS 0.4–1.6 × 107 copies g−1; Fig. 2c, d) were determined in the soil amended with lucerne-clover-grass-mix. Interestingly, somewhat higher archaeal amoA (AOA; 4.7–9.7 × 105 copies g−1) than bacterial amoA (AOB; 1.8–5.8 × 105 copies g−1) gene copies were found in the straw-amended samples, whereas lucerne-clover-grass-mix-amended samples showed the opposite behavior (Fig. 2a, b). However, the influence of freezing and thawing resulted in both treatments in increased AOA/AOB ratios compared to the non-frozen control soil (Fig. 2b).
The result that AOB are more affected by the freeze–thaw event compared to AOA also supports the hypotheses by Schleper et al. (2005) and Valentine (2007) who presumed that archaea are more tolerant to stress conditions than bacteria. Several studies also showed that AOA/AOB ratios increase with decreasing availability of C and N (Leininger et al. 2006). It was also speculated that AOA might be more closely attached to soil particles which might result in a certain protection of AOA compared to AOB.
Concerning the genes involved in denitrification, the straw-amended samples also revealed lower copy numbers of both, nirK (0.4–1.5 × 108 copies g−1) and nirS (1.4–4.6 × 106 copies g−1) genes (Fig. 2c, d). However, both treatments exhibited considerably more nirK than nirS gene copies and showed decreased copy numbers after 1 day of thawing compared to the non-frozen control.
The higher nirK copy numbers could reflect a possible niche differentiation for microbes harboring one of the two functionally redundant nitrite reductases, where nirK-possessing bacteria could preferentially colonize habitats with more available C and N. This trend has also been observed when hotspots in soil exhibiting high amounts of available C and N have been compared with low activity areas (e.g., rhizosphere vs. bulk soil) (Sharma et al. 2005). In the legume mix-amended samples, a fast recovery of nirK copy numbers was detected, which was also found by Sharma et al. (2006), whereas the straw-amended soil showed a decrease in gene copies also in the control samples during the incubation period.
Our results indicate that the amount and quality of applied N have distinct effects on the abundance of genes involved in N cycling and the corresponding N transformations during freezing and thawing events. This is in line with previous studies showing the close link between the different transformation processes of the nitrogen cycle (Nannipieri and Paul 2009). This study indicates that the nitrogen stored in legumes, which are often used as green manure in agriculture, can fast be mineralized, nitrified, and denitrified during winter time as a result of freezing and thawing cycles. It could be considered if nitrification inhibitors applied after thawing might help to reduce transformations of the formed NH +4 into NO −3 and thus reduce N losses via leaching of NO −3 and emission of N2O and N2 by denitrification.
Reference
Braker G, Fesefeldt A, Witzel KP (1998) Development of PCR primer systems for amplification of nitrite reductase genes (nirK and nirS) to detect denitrifying bacteria in environmental samples. Appl Environ Microbiol 64:3769–3775
Clark K, Chantigny MH, Angers DA, Rochette P, Parent LE (2009) Nitrogen transformations in cold and frozen agricultural soils following organic amendments. Soil Biol Biochem 41:348–356
Davidson EA, Kingerlee W (1997) A global inventory of nitric oxide emissions from soils. Nutr Cycl Agroecosyst 48:37–50
Elliott AC, Henry HAL (2009) Freeze–thaw cycle amplitude and freezing rate effects on extractable nitrogen in a temperate old field soil. Biol Fertil Soils 45:469–476
Griffiths RI, Whiteley AS, ƠDonnell AG, Bailey MJ (2000) Rapid method for coextraction of DNA and RNA from natural environments for analysis of ribosomal DNA- and rRNA-based microbial community composition. Appl Environ Microbiol 66:5488–5491
Hai B, Diallo NH, Sall S, Haesler F, Schauss K, Bonzi M, Assigbetse K, Chotte JL, Munch JC, Schloter M (2009) Quantification of key genes steering the microbial nitrogen cycle in the rhizosphere of sorghum cultivars in tropical agroecosystems. Appl Environ Microbiol 75:4993–5000
Henry S, Baudoin E, López-Gutiérrez JC, Laurent FM, Brauman A, Philippot L (2004) Quantification of denitrifying bacteria in soils by nirK gene targeted real-time PCR. J Microbiol Methods 59:327–335
Leininger S, Urich T, Schloter M, Schwark L, Qi J, Nicol GW, Prosser JI, Schuster SC, Schleper C (2006) Archaea predominate among ammonia-oxidizing prokaryotes in soils. Nature 442:806–809
Michotey V, Méjean V, Bonin P (2000) Comparison of methods for quantification of cytochrome cd1-denitrifying bacteria in environmental marine samples. Appl Environ Microbiol 66:1564–1571
Mrkonjic Fuka M, Engel M, Hagn A, Munch JC, Sommer M, Schloter M (2009) Changes of diversity pattern of proteolytic bacteria over time and space in an agricultural soil. Microb Ecol 57:391–401
Mueller T, Jensen LS, Nielsen NE, Magid J (1998) Turnover of carbon and nitrogen in a sandy loam soil following incorporation of chopped maize plants, barley straw and blue grass in the field. Soil Biol Biochem 30:561–571
Nannipieri P, Paul E (2009) The chemical and functional characterization of soil N and its biotic components. Soil Biol Biochem 41:2357–2369
Nicolardot B, Bouziri L, Bastian F, Ranjard L (2007) A microcosm experiment to evaluate the influence of location and quality of plant residues on residue decomposition and genetic structure of soil microbial communities. Soil Biol Biochem 39:1631–1644
Phillips RL (2008) Denitrification in cropping systems at sub-zero soil temperatures. A review. Agron Sustain Dev 28:87–93
Rotthauwe JH, Witzel KP, Liesack W (1997) The ammonia monooxygenase structural gene amoA as a functional marker: Molecular finescale analysis of natural ammonia-oxidizing populations. Appl Environ Microbiol 63:4704–4712
Ruser R, Schilling R, Steindl H (1998) Soil compaction and fertilization effects on nitrous oxide and methane fluxes in potato fields. Soil Sci Soc Am J 62:1587–1595
Schauss K, Focks A, Leininger S, Kotzerke A, Heuer H, Thiele-Bruhn S, Sharma S, Wilke BM, Matthies M, Smalla K, Munch JC, Amelung W, Kaupenjohann M, Schloter M, Schleper C (2009) Dynamics and functional relevance of ammonia-oxidizing archaea in two agricultural soils. Environ Microbiol 11:446–456
Schleper C, Jurgens G, Jonuscheit M (2005) Genomic studies of uncultivated archaea. Nat Rev Microbiol 3:479–488
Sharma S, Aneja MK, Mayer J, Munch JC, Schloter M (2005) Characterization of bacterial community structure in rhizosphere soil of grain legumes. Microb Ecol 49:407–415
Sharma S, Szele Z, Schilling R, Munch JC, Shloter M (2006) Influence of freeze–thaw stress on the structure and function of microbial communities and denitrifying populations in soil. Appl Environ Microbiol 72:2148–2154
Throbäck IN, Enwall K, Jarvis Å, Hallin S (2004) Reassessing PCR primers targeting nirS, nirK and nosZ genes for community surveys of denitrifying bacteria with DGGE. FEMS Microbiol Ecol 49:401–417
Valentine DL (2007) Adaptations to energy stress dictate the ecology and evolution of the Archaea. Nat Rev Microbiol 5:316–323
Wang WJ, Baldock JA, Dalal RC, Moody PW (2004) Decomposition dynamics of plant materials in relation to nitrogen availability and biochemistry determined by NMR and wet-chemical analysis. Soil Biol Biochem 36:2045–2058
Zsolnay Á (2003) Dissolved organic matter: artefacts, definitions, and functions. Geoderma 113:187–209
Acknowledgment
The authors wish to acknowledge financial support from the China Scholarship Council (CSC).
Author information
Authors and Affiliations
Corresponding author
Rights and permissions
About this article
Cite this article
Su, M., Kleineidam, K. & Schloter, M. Influence of different litter quality on the abundance of genes involved in nitrification and denitrification after freezing and thawing of an arable soil. Biol Fertil Soils 46, 537–541 (2010). https://doi.org/10.1007/s00374-010-0449-9
Received:
Revised:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1007/s00374-010-0449-9