Abstract
The nitrogen cycle is greatly influenced by soil microbes through their transformation of different nitrogen compounds. Additionally, microbial diversity is profoundly modified by plant root exudates in the rhizosphere. Hence, root exudates indirectly control different processes in the nitrogen cycle by modifying the microbial community in the rhizosphere. We are beginning to understand more about the roles of plant root exudates in nitrogen fixation, nitrification, denitrification, anaerobic ammonium oxidation (anammox), dissimilatory nitrate reduction to ammonium (DNRA), nitrate reduction, nitrogen mineralization, and, finally, nitrogen uptake in the rhizosphere. Root exudates release chemoattractant compounds (flavonoids) into the rhizosphere; as a result, rhizobia move toward legume roots for colonization through a chemotactic process. The rhizobium–legume interaction is a very complex process involving root exudates, nod genes, and other compounds released from rhizobia and legume plants. Moreover, after nodulation, atmospheric nitrogen can be fixed and transformed into ammonia through biological processes involving the nitrogenase enzyme. Root exudates are also used as a carbon energy source by different microbial communities involved in asymbiotic nitrogen fixation, denitrification, and the DNRA and anammox processes. Chemical fertilizers, including synthetic nitrogen fertilizers, are also used for improving crop yields of different cereals and other vegetables in modern agricultural practices. Excess ammonia is further oxidized and converted into nitrite by Nitrosomonas, and, finally, nitrate is formed by Nitrobacter in a nitrification process in freshwater and soil ecosystems. In contrast, anammox, which is a two-step process, operates mainly in marine ecosystems and sediments. Better knowledge of these processes is needed so that urgent attention can be paid to optimizing the use of nitrogen fertilizers and minimizing their contributions to climate change and nitrogen pollution.
Access provided by Autonomous University of Puebla. Download chapter PDF
Similar content being viewed by others
Keywords
1 The Nitrogen Cycle: An Overview
In general, the nitrogen (N) cycle in different ecosystems and environments can be summarized as a process of oxidation–reduction chemical reactions catalyzed by archaea, rhizospheric microorganisms, algae, and plants (Fig. 8.1). Of the total six nitrogen compounds, nitrate is completely oxidized, while ammonium is a fully reduced form of nitrogen are regulated by these organisms. Free nitrogen gas, an inorganic form of N, is present in the atmosphere and is not accessible to most living organisms, but N can be fixed (biochemically), transported into plants and other living things, and converted into its organic forms by diazotrophic prokaryotes and also by lightning (geochemically) (Vitousek et al. 2013). These prokaryotes may be archaea or bacteria, free living or in mutualistic cooperation, and can reduce nitrogen to ammonia (Hoffman et al. 2014). Further, ammonia is biologically incorporated into amines, transported from soil into different parts of plants, and finally converted into diverse organic compounds (Krapp 2015). Additionally, through the nitrification process, ammonium can easily be oxidized by soil microbes and converted into nitrite, nitrate, and hydroxylamine (Hayatsu et al. 2008). The nitrification and two-step oxidation processes are biologically performed by bacteria or archaea, known as ammonium-oxidizing archaea (AOAs) and ammonium-oxidizing bacteria (AOBs), and nitrite-oxidizing bacteria, respectively (Prosser and Nicol 2012). Recently, the complete ammonia oxidation (comammox) process has been described; through this biological process, both oxidative steps (conversion of ammonium into nitrite and into nitrate) are performed by a single organism, Nitrospira (Daims et al. 2015; van Kessel 2015). In contrast, the denitrification process—including reduction of nitrate to nitrite, nitric oxide, nitrous oxide, and, ultimately, free nitrogen gas—is executed by soil microbes, including fungi, bacteria, and archaea (Hayatsu et al. 2008). In addition to nitrification and denitrification, two other processes—dissimilatory nitrate reduction to ammonia and anaerobic ammonium oxidation (anammox)—are included in the N cycle (Rütting et al. 2011). The DNRA process—in which nitrate is used as an electron acceptor under microaerophilic/anaerobic conditions, reduced to nitrite, and finally converted into ammonia—is performed by fungi and bacteria, while nitrogen (Welsh et al. 2014) and free N2 are finally produced in the anammox process from nitrate via nitrous oxide and hydrazine as intermediate forms (Kartal et al. 2011; van Niftrik et al. 2012).
The concept of the N cycle changed at the beginning of the twenty-first century after the discovery of archaea and as a result of human interference in the form of chemical fertilizer manufacturing to enhance crop production in current agricultural practices (Offre et al. 2013). After the discovery of archaea and their nitrogen fixation capabilities in freshwater and marine sediments, the newly discovered roles of prokaryotes in the N cycle were discussed by researchers (Prosser and Nicol 2012). AOAs are broadly disseminated and capable of nitrification in acidic soil, but this process may be inhibited by high concentrations of ammonium (Verhamme et al. 2011). The impact of human activities on the N cycle has been estimated by data showing that the total amount of nitrogen fixation by the Haber–Bosch process in addition to other anthropogenic activity by human (210 Tg N/year) is greater than than the total amount of N-fixation by asymbiotic and symbitic process (203 Tg N/year). The use of chemical fertilizers in legume cultivation is essential for human nutrition (Erisman et al. 2008). A total of 120 Tg N year−1 of N fertilizer is synthesized by chemical catalysis in the Haber–Bosch process, and 50% of the total N fertilizer that is produced is used in three major crops (Table 8.1): wheat (18%), rice (16%), and maize (16%) (Ladha et al. 2016). Plants themselves cannot fix atmospheric nitrogen and are not directly involved in the nitrification process, but they can uptake or assimilate nitrate (Vitousek et al. 1997) or ammonium from soil or water through their roots, depending on which substrate is suitable for uptake in different environments (Smith et al. 1999). Production and use of chemical fertilizers pose serious threats to the environment because they result in eutrophication of marine water and freshwater, and emission of the potent greenhouse gas N2O (Ravishankara et al. 2009). After nitrogen fertilization of soil, nitrate and ammonium ions are generated, and some are taken up by plant roots, but most of the fertilizer is used as a substrate by nitrifiers and denitrifiers, causing substantial loss of N through production of N2O in the denitrification process (Mosier et al. 1998; Shcherbak et al. 2014). Moreover, it is now very clear that plants are involved indirectly and regulate the N cycle by controlling the population of prokaryotes and fungi by releasing root exudates (Bardgett et al. 2014; Finzi et al. 2015). In this chapter, we discuss recent progress in research on root exudates and their involvement in pathways of N cycle nitrification, denitrification, etc.
2 Root Exudates: Current-Status
The rhizosphere is the active zone in soil where nutrients secreted from plant roots support microbial growth and biological activity, and exchange of nutrients is mobilized (Hamilton and Frank 2001; Landi et al. 2006; Zhu et al. 2014). This is a very densely populated area of soil, where the root system of one plant competes with others by invasion into their root systems to acquire mineral nutrients, water, and space (Ryan and Delhaize 2001). Soil microorganisms (protozoa, bacteria, fungi, etc.) also contend with each other to utilize nutrient sources of organic materials (Bais et al. 2004). One of the most important metabolic processes in plant roots is secretion of a variety of compounds into the rhizosphere (Badri and Vivanco 2009). In this process, 5–21% of photosynthetically fixed carbon is secreted through plant roots in the form of root exudates (Marschner 1995; Derrien et al. 2004). The quality and amount of root exudates varies with the age and species of the plant and also depends on abiotic and biotic factors (Jones et al. 2004).
Root exudates are composed of low and high molecular weight compounds (Badri and Vivanco 2009) and include soluble and insoluble compounds produced by specialized cells, including border cells (Huang et al. 2014) in the roots of all plants (Table 8.2). The exudates regulate the microbial community in the rhizosphere (Hirsch et al. 2003) and act as signaling molecules that attract or repel microorganisms in the rhizosphere and provide nutrient support for microbes to establish a plant–microbe relationship (Hirsch et al. 2003; Dennis et al. 2010). Exopolysaccharides and some soluble and antagonist compounds help to regulate biotic and abiotic conditions for plants (Huang et al. 2014).
Mucilage is a type of root exudate secreted from aerial and underground roots of plants (Bennett et al. 2020). Compounds in mucilage secreted from aerial roots of Sierra Mixe corn and from underground roots of maize have been analyzed (McCully and Boyer 1997). Different polysaccharides, phospholipids, and proteins are found in mucilage (Read et al. 2003). Secretion of mucilage from roots is a common process in cereal crops, including barley, wheat, and sorghum (Kislev and Werker 1978; Sinha et al. 2002; Carter et al. 2019). In an in vitro analysis, the amount of mucilage synthesized was 11–47 mg of dry matter per gram of root (Nguyen 2003). The mucilage diffusion rate and quantity are determined by whether the root is grown in a nutrient solution or in water (Sealey et al. 1995). Mucilage secreted into soil helps to enhance the aggregation capability of soil, which promotes aeration of soil, prevents soil erosion, and supports root growth to maintain a continuous flow of water in the rhizosphere. Moreover, mucilage also protects the meristem of the root from toxic compounds (Read et al. 2003). To date, the quantity of mucilage secreted from plant roots into the rhizosphere remains unknown.
Plant roots also release different gases (CO2, H2, and ethylene) after different metabolic activities by microbes and plants in the rhizosphere. For example, CO2 diffuses into the rhizosphere after carbohydrate respiration in the process of plant–microbe interaction (Phillips et al. 1999). Accumulation of CO2 in the rhizosphere enhances Ca2+ production and uptake by plants through dissolution of CaCO3 (Dakora and Phillips 2002).
3 Root Exudates and Different Processes in the Nitrogen Cycle
3.1 Root Exudates, Asymbiotic Relationships, and Nitrogen Fixation
Diazotrophic bacteria in the rhizospheres of cereals, grasses, and nonleguminous crops can fix environmental N2 asymptotically in temperate and tropical agricultural systems. Asymbiotic N fixation is also performed in soil by different endophytic and free-living bacteria (Roper and Ladha 1995). Upto 60 kg ha−1 of N can be fixed asymbiotically by diazotrophic bacteria in soil around different varieties of nonleguminous crops (Cleveland et al. 1999; Gupta et al. 2006). One modern technique includes use of a radioisotope tracer in which a 15N-enriched radiolabeled compound is used for quantification of asymbiotically fixed N in graminaceous plants. This has enabled estimation of a significant economic profit from asymbiotic fixed N in soil (Kennedy and Islam 2001; Hurek et al. 2002). Moreover, through molecular approaches, a diversity of culturable and nonculturable N-fixing microbes have been identified in the rhizospheres of cereals and nonleguminous plants (Hurek et al. 2002; Buckley et al. 2007).
Root exudates are continuously secreted from plant roots (Greer-Phillips et al. 2004) and influence the population and metabolic activity of diazotrophic and free-living bacteria in the rhizosphere (Fig. 8.1). Bacteria move in a favorable direction in the rhizosphere by flagellar rotation in response to release of specific chemical compounds from root exudates; this is known as chemotaxis (Eisenbach 1996). Thus, root exudates can indirectly control asymbiotic N fixation (Steenhoudt and Vanderleyden 2000). For example, Azospirillum brasilense is chemotactically attracted to compounds secreted from root exudates in the rhizosphere and consequently colonizes the root surface (Steenhoudt and Vanderleyden 2000). In contrast, different N sources [NH4Cl, KNO3, NH4NO3, and urea (CO[NH2]2)] can interfere with colonization by Azospirillum in rice and wheat plants (Naher et al. 2018). The root volume, shoot dry biomass, and N content in shoots is reduced in corn when the population of Azospirillum is reduced and less nitrogenase activity occurs. A total of nine amino acids (asparagine, serine, aspartic acid, glutamic acid, phenylalanine, valine, threonine, alanine, and tryptophan), six sugars (galactose, glucose, xylose, sucrose, arabinose, and fructose), and four organic acid (fumarate, malate, citrate, and succinate) have been identified in exudates from corn roots. The organic acids and five of the sugars (excluding glucose) secreted from root exudates are used by Azospirillum as energy sources in the rhizosphere (Pereira et al. 2020). Interestingly, indole acetic acid (IAA) has been synthesized in vitro by Azospirillum, using root exudates from lentil (Lens culinaris), bean (Phaseolus vulgaris L.), radish (Raphanus sativus L.), tomato (Lycopersicum esculentum), rice (Oryza sativa L.), canola (Brassica napus L.), and clover (Trifolium alexandrinum L.) plants grown in a medium supplemented with L-tryptophan, a precursor of IAA. A supernatant of Azospirillum A3 grown in a medium containing root exudates from different plants enhanced the growth of rice roots (Moghaddam et al. 2012). In a recent study, glutamic acid (30μM L−1) stimulated chemotaxis by 2.9 and 7.4 times (in comparison with control conditions) in the rhizospheres of cabbage and lettuce plants, and it acted as a signaling molecule for chemotaxis and colonization of the cabbage and lettuce roots. In a pot assay, the biomass, chlorophyll content, and available N significantly increased in lettuce bacterized with Azospirillum Ac63 by improving the quality of root exudates and enhancing secretion of glutamic acid in the rhizosphere (Wang et al. 2020).
3.2 Symbiotic Nitrogen Fixation and Root Exudates
N fixation is a metabolic activity that synthesizes ammonia from environmental N by use of nitrogenase enzymes. In this process, the system consumes 5% of the energy produced by plant photosynthates (Dong and Layzell 2001). H2 is released as a by-product of N fixation in legumes. Some rhizobia have a hydrogenase (Hup) enzyme for uptake of H2 gas to produce energy by oxidation, but most rhizobia lack a hydrogenase enzyme and are unable to use H2 gas. Ultimately, therefore, the H2 gas diffuses into the rhizosphere from root nodules (Golding et al. 2012). H2 gas release after N fixation is also helpful for modification of the soil microbiome and contributes indirectly to plant growth (Dong and Layzell 2001). Simultaneously, H2 gas stimulates the hydrogen-oxidizing rhizobial community, which can indirectly boost plant growth–promoting activities, such as root elongation, by syntjesizing IAA (Ahmad et al. 2020) and retarding ethylene releases from plant roots (Ahmad et al. 2013). This is beneficial to nonleguminous and leguminous plants (Maimaiti et al. 2007).
It is well established that root exudates are involved in development of symbiotic relationships between legumes and rhizobia (Bradyrhizobium, Sinorhizobium, Rhizobium, Mesorhizobium, etc.) in the rhizosphere. This is known as Rhizobium–legume symbiosis (Oldroyd 2013; Philippot et al. 2013). Chemical compound releases from legume roots, especially releases of flavonoids (hesperetin, genistein, and naringenin), activate and synthesize nodulation factors (Hassan and Mathesius 2012) through initiation or catalysis of expression of nod genes in rhizobia (Begum et al. 2001). Nodulation factors are host specific and are classified as lipochitooligosaccharides (LPOs). They are secreted by rhizobia and stimulate initiation of the nodulation process (Limpens et al. 2015). Mechanistically, these discharged LPO molecules bind to special receptors located in the plasma membrane of epidermal cells on legume root hairs and initiate the process of nodulation by stimulating a calcium-dependent cascade (Ahmad et al. 2012; Oldroyd 2013). Flavonoids are continuously secreted into the rhizosphere from legume roots, but their concentrations increase and they act as chemoattractants when compatible Rhizobium species are present in the rhizosphere (Zuanazii et al. 1998). Moreover, symbiotic N-fixation is influenced by intercropping of faba beans and wheat. For example, the number of nodules and total dry weight of nodule/plant increases in faba beans after intercropping of faba beans and wheat, in comparison with monocropping. The nodulation process in faba beans is enhanced after intercropping through increases in the concentrations of chalcone, flavanol, hesperetin, and isoflavone in plant root exudates (Table 8.3). Furthermore, symbiotic N fixation is influenced by intercropping of faba beans and wheat (Liu et al. 2017). In a recent in vitro study, the effect of bis(2-ethylhexyl) phthalate (DEHP), a stress compound, on the quality and quantity of secreted root exudates was analyzed. Root exudates were collected from the roots of alfalfa (Medicago sativa), grown in hydroponic solution, and analyzed. This revealed that the root exudates were composed mainly of carbohydrates (28.6%), organic acids (15.58%), and lipids (13.87%), among a total of 314 identified compounds. Moreover, DEHP indirectly alters the nodulation process by retarding the rate of flavonoid diffusion from plant roots. Mechanistically, a lower concentration of DEHP suppresses the concentration of 4′,5-dihyrroxy-7- methoxyisoflavone (a flavonoid) in the root exudates and also influences carbohydrate metabolism (Wang et al. 2020).
Proteins secreted from rhizobia are also involved in determining the host specificity of rhizobium–legume interactions. There are three known mechanisms of protein secretion in rhizobia. The first study on secretion of proteins elicited that the type I secretion system was induced by nodulation factors (NodD and NodO) and flavonoids involved in symbiosis of Rhizobium leguminosarum bv. viciae (de Maagd 1989). In another mechanism, nodulation outer proteins are released by the type III secretion system in rhizobia. Activation of the type III secretion system in Bradyrhizobium japonicum requires NodW factors, NodD1, and flavonoids (Krause et al. 2002). Type III secretion systems have also been reported in Sinorhizobium fredii USDA257 (Krishnan et al. 2003), Bradyrhizobium elkanii (Okazaki et al. 2009), and Mesorhizobium loti MAFF303999 (Okazaki et al. 2010). Nodulation outer proteins (NOPs)—including nopA, nopC, nopB, nopL, nopX, and nopP—are secreted from the type III secretion system of S. fredii USDA257 (Deakin and Broughton 2009).
Several studies have shown that the rhizobial nodulating capacity of legumes at the genus and species levels of rhizobia is influenced by proteins secreted by the type III secretion system (Krishnan et al. 2003; Ausmees et al. 2004; Okazaki et al. 2009, 2010).
4 Root Exudates Control Loss of Nitrogen Through Denitrification and the Anammox Process in the Nitrogen Cycle
One of the key processes in the N cycle is nitrification, in which different nitrogen compounds are converted into nitrate through microbial processes (Fig. 8.1). The nitrification process depends on the types of nitrogen compounds and microbial metabolic activity in the rhizosphere (Subbarao et al. 2007). In this process, less mobile ammonium is converted into mobile nitrate through enzymatic processes (Subbarao et al. 2009). Nitrate formed in the rhizosphere is less utilized by plants than ammonium. Nitrification may not be beneficial, because it may increase loss of fertilizer N through leaching and denitrification (Subbarao et al. 2006). Recovery of N and improvement of nitrogen use efficiency through inhibition of nitrification is a key strategy to control loss of N in the rhizosphere (Subbarao et al. 2009). Some plants release certain compounds from root exudates that inhibit or suppress the nitrification process, and this is known as biological nitrification inhibition (BNI) (Subbarao et al. 2006). Recently, to evaluate the BNI process, a luminescent assay was developed for detection of the ammonium oxidation process (conversion of ammonia into nitrite) in the rhizosphere, in which recombinant Nitrosomonas europaea was used as a bioindicator (Subbarao et al. 2007). BNI compounds were tested in various species of plants, such as cereals, legumes, and plants from tropical and temperate regions. BNI activity ranged between 0 and 18.3 AT (inhibitor allylthiourea/gm of root dry weight day−1) unit in root exudates from 18 different species of field grass, pearl millet, cereals, legumes, and vegetables. Among pasture grasses, BNI activity was greatest in Brachiaria decumbens and B. humidicola (Subbarao et al. 2007). Many low- and high-BNI genotypes have been detected in B. humidicola pasture grass. In a pot experiment, B. humidicola suppressed around 90% of the nitrification process by releasing BNI compounds into the rhizosphere, and the soil concentration of ammonium, as an inorganic form of nitrogen, remained unchanged (Subbarao et al. 2007). Plants that release only small amounts of BNI compounds have been shown not to inhibit the nitrification process; most of the ammonia is oxidized and converted into nitrate in soil (Zakir et al. 2008; Subbarao et al. 2012). Similarly, after screening, studies have revealed that other cereal crops (maize, wheat, rice, and barley) do not secrete BNI compounds in their root exudates (Lata et al. 1999). Moreover, legumes do not interfere in the nitrification process, because they lack BNI capacity. Synthesis and exudation of BNI compounds by sorghum, B. humidicola, and Leymus racemosus is influenced by the form of nitrogen applied to soil. When nitrate was applied to soil, BNIs were not released from the roots, whereas after ammonia application to soil, BNIs compounds were synthesized (Subbarao et al. 2013). Methyl 3-(3-hydroxyphenyl) propionate (MHPP) inhibits the denitrification process and has been identified in root exudates from sorghum grown in ammonia-treated soil. MHPP inhibits the nitrification process via the ammonia monooxygenase (AMO) enzymatic pathway but does not interfere in the hydroxylamine oxidoreductase (HAO) enzymatic pathway of Nitrosomonas (Zakir et al. 2008). The BNI process can be exploited for management of soil denitrification processes in agronomic approaches.
Root exudates are equally important in serving as a C source for growth of the bacterial population involved in the denitrification process (Zhai et al. 2013). The denitrification process is inhibited by BNI compounds in root exudates, while bacterial use of this C source to oxidize ammonia creates equilibrium in the N cycle in the rhizosphere. After the denitrification process in the rhizosphere of wheat, N2O is released into the environment (Table 8.3). The rate of emission of N2O is directly influenced by nirS (nitrite reductase) gene abundance in Rhodobacterales and Pseudomonadales in the rhizosphere (Ai et al. 2017). Two interlinked and important key processes in the N cycle that operate in different ecosystems (estuarine water, freshwater, and the ocean) are the anammox process and denitrification (Francis et al. 2007; Zhu et al. 2010). Between 31% and 41% of N2 is emitted from the rhizosphere of rice, while only 2–3% of N2 is released from nonrhizospheric soil via the anammox process (Nie et al. 2018). A total of 79% of N loss in marine ecosystems occurs through the anammox process. In contrast, denitrification accounts for 87% of N loss in freshwater and soil (Schubert et al. 2006). The diversity of anammox bacteria in the rhizospheres of submerged plants and sediments is influenced by the concentrations of nitrate, ammonia, and organic matter, and by redox potential and oxygen availability (Lee and Francis 2017). The most important parameters for the anammox process are the availability of dissolved oxygen (Oshiki et al. 2016) and salinity (Sonthiphand et al. 2014) in submerged ecosystems. The ammonia-to-nitrate molar ratio also influences the anammox process. A phylogenetic analysis indicated that the anammox bacteria Brocadia fuigida and Scalindua wagneri and the nirS denitrifying bacteria Herbaspirillum and Pseudomonas were the dominant species in sediment around declined Potamogeton crispus. It was suggested that a sudden decline in submerged macrophytes would increase the abundance of anammox bacteria and denitrifying bacteria in a relatively short time (Hu et al. 2020).
5 Root Exudates and the DNRA Process
The DNRA process is very critical in our understanding of soil ecosystems in microaerophilic conditions and in the presence of nitrate (Stein and Klotz 2016). While free N releases in atmosphere resulted loss of N during the denitrification and anammox processes (Canfield et al. 2010). Through N gas emissions, significant loss of N occurs in the denitrification and anammox processes, although the DNRA process helps to retain N in the form of ammonia in aquatic systems (An and Gardner 2002). Ammonia is further taken up by plant roots, enhancing plant growth. In the DNRA process, highly mobile nitrate and nitrite are reduced to ammonia (An and Gardner 2002). DNRA activity is widely detected in soils or environments with microaerophilic conditions, such as wetland systems (Gao et al. 2017; Zhang et al. 2017), terrestrial (forest, grassland, agriculrural land, dessert) habitats, floodplains (Jones et al. 2017), and marine sediments (Cheng et al. 2016). The DNRA process is also influenced by the C-to-N and carbon-to-nitrate ratios in both terrestrial and aquatic systems (Robertson et al. 2016; Zhou et al. 2017).
Chemolithoautotrophic and heterotrophic bacteria and other diverse microbes are involved in the DNRA process (Pang and Ji 2019). Additionally, the nrfA gene, which encodes nitrite reductase, has been developed as a biomarker gene for the DNRA process (Welsh et al. 2014). This gene has been identified in diverse groups of bacteria: Planctomycetes, Chloroflexi, Bacteroides, Acidobacteria, Planctomycetes, Firmicutes, and Verrucomicrobia (Welsh et al. 2014). The microbial diversity surrounding plant roots is greatly influenced by root exudates in terrestrial and aquatic habitats, and the DNRA process is indirectly affected by root exudates as the population of microbes is manipulated. For example, in a recent study, the DNRA rate, the abundance of Chthiniobacter, and the total organic matter content were correlated in rhizospheric and nonrhizospheric soil. The DNRA rates were higher in rhizospheric soils where larger populations of Chthiniobacter were recorded than in nonrhizospheric soil because of the greater availability of C sources in rhizospheric soil (Pan et al. 2020).
6 Nitrogen Mineralization and Uptake by Plant Roots
Proteins and peptides from decomposed material from living organisms in soil is an immobilized form of an organic source of nitrogen. This complex form of organic N is converted into amino acids by protease and further degraded into NH4 by the bacterial community in the rhizosphere (Ahmad et al. 2014). Peptidases secreted in root exudates from Medicago enhance N mineralization in the rhizosphere (De-la-Pena and Vivanco 2010). Additionally, Godlewski and Adamczyk (2007) reported that proteases were secreted in root exudates from 15 different types of wild and agricultural plant species. Later, they concluded that secretion of proteases from wheat (Adamczyk et al. 2008) and allium (Adamczyk et al. 2009) was a strategy on the part of the plants to mineralize complex organic forms of N into simple forms for utilization of nitrogen. Root uptake of amino acids from soil was studied using a proteomic and isotopic method in which radiolabeled glycine was used as a source of nitrogen for uptake by Lolium perenne plants (Thornton et al. 2007). The microbial community in the rhizosphere also releases proteases and break down proteins into amino acids. Proteases in root exudates or in the rhizosphere digest protein and convert it into amino acids to facilitate N uptake by plant roots. These limited findings clearly indicate that root exudates facilitate mineralization of N and its further uptake by plants. In the N mineralization process, rhizospheric microbes secrete proteases that break down complex forms of N (in proteins and peptides) into simple organic forms (in amino acids) and further convert them into ammonium. Carbon is one of the growth-limiting factors for microbes. Thus, this limitation is partially controlled by exudates that are secreted from roots, move through soil, and transform it into rhizospheric soil (Lynch and Whipps 1990).
7 Conclusion
The biochemistry of root exudates is still not fully understood and varies between different species of plants. Because the exact mechanisms of plant root exudate secretion are not fully understood, many aspects of the biological processes of plant–microbe interactions are still unknown. Characterization of molecules that influence microbial diversity in the rhizosphere and metabolic profiling of root exudates are ongoing processes aimed at increased understanding of the roles of root exudates in plant–microbe interactions. Rhizospheric microbial diversity and root exudate compounds are involved directly and indirectly in different processes in the nitrogen cycle in the rhizosphere and in other ecosystems. More physiological study of root exudation mechanisms is needed for greater understanding of the biochemistry of the nitrogen cycle in the rhizosphere.
References
Achouak W, Abrouk D, Guyonnet J, Barakat M, Ortet P, Simon L, Lerondelle C, Heulin T, Haichar FE (2019) Plant hosts control microbial denitrification activity. FEMS Microbiol Ecol 95:fiz021
Adamczyk B, Godlewski M, Zimny J, Zimny A (2008) Wheat (Triticum aestivum) seedlings secrete proteases from the roots and, after protein addition, grow well on medium without inorganic nitrogen. Plant Biol 10:718–724
Adamczyk B, Godlewski M, Smolandera A, Kitunen V (2009) Degradation of proteins by enzymes exuded by Allium porrum roots—a potentially important strategy for acquiring organic nitrogen by plants. Plant Physiol Biochem 47:919–925
Ahmad E, Zaidi A, Khan MS, Oves M (2012) Heavy metal toxicity to symbiotic nitrogen-fixing microorganism and host legumes. In: Zaidi A, Wani PA, Khan MS (eds) Toxicity of heavy metals to legumes and bioremediation. Springer-Verlag, Wien, pp 29–44
Ahmad E, Khan MS, Zaidi A (2013) ACC deaminase producing Pseudomonas putida strain 328 PSE3 and Rhizobium leguminosarum strain RP2 in synergism improves growth, nodulation and 329 yield of pea grown in alluvial soils. Symbiosis 61:93–104
Ahmad E, Zaidi A, Khan MS (2014) Response of PSM inoculation to certain legumes and cereal crops. In: Khan MS, Zaidi A, Musarrat J (eds) Phosphate solubilising microorganisms: principles and application of microphos technology. Springer-Verlag, Cham, pp 175–206
Ahmad E, Sharma SK, Sharma PK (2020) Deciphering operation of tryptophan-independent pathway in high IAA producing Micrococcus aloeverae DCB-20. FEMS Microbiol Lett 367:fnaa 190
Ai C, Liang G, Wang X, Sun J, He P, Zhou W (2017) A distinctive root-inhabiting denitrifying community with high N2O/(N2O+N2) product ratio. Soil Biol Biochem 109:118–123
An S, Gardner WS (2002) Dissimilatory nitrate reduction to ammonium (DNRA) as a nitrogen link, versus denitrification as a sink in a shallow estuary (Laguna Madre/Baffin Bay, Texas). Marine Ecol Prog Ser 237:41–50
Ausmees N, Kobayashi H, Deakin WJ, Marie C, Krishnan HB, Broughton WJ, Perret X (2004) Characterization of NopP, a type III secreted effector of Rhizobium sp. strain NGR234. J Bacteriol 186:4774–4780
Badri DV, Vivanco JM (2009) Regulation and function of root exudates. Plant Cell Environ 32:666–681
Bais HP, Park SW, Weir TL, Callaway RM, Vivanco JM (2004) How plants communicate using the underground information superhighway. Trends Plant Sci 9:26–32
Bardgett RD, Mommer L, De Vries FT (2014) Going underground: root traits as drivers of ecosystem processes. Trends Ecol Evol 29:692–699
Begum AA, Leibovitch S, Migner P, Zhang F (2001) Specific flavonoids induced nod gene expression and pre-activated nod genes of Rhizobium leguminosarum increased pea (Pisum sativum L.) and lentil (Lens culinaris L.) nodulation in controlled growth chamber environments. J Exp Bot 52:1537–1543
Bennett AB, Pankievicz VC, Ané JM (2020) A model for nitrogen fixation in cereal crops. Trends Plant Sci 25:226–235
Buckley DH, Huangyutithan V, Hsu SF, Nelson TA (2007) Stable isotope probing with N15 reveals novel noncultivated diazotrophs in soil. Appl Environ Microbiol 73:3196–3204
Canfield DE, Glazer AN, Falkowski PG (2010) The evolution and future of Earth’s nitrogen cycle. Science 330:192–196
Carter AY, Ottman MJ, Curlango-Rivera G, Huskey DA, D’Agostini BA, Hawes MC (2019) Drought-tolerant barley: II. Root tip characteristics in emerging roots. Agronomy 9:220
Chen T, Liu Y, Zhang B, Sun L (2019) Plant rhizosphere, soil microenvironment, and functional genes in the nitrogen removal process of bioretention. Environ Sci Process Impacts 21:2070–2079
Cheng L, Li X, Lin X, Hou L, Liu M, Li Y, Liu S, Hu X (2016) Dissimilatory nitrate reduction processes in sediments of urban river networks: spatiotemporal variations and environmental implications. Environ Pollut 219:545–554
Cleveland CC, Townsend AR, Schimel DS, Fisher H, Howarth RW, Hedin LO, Perakis SS, Latty EF, Von Fischer JC, Elseroad A, Wasson MF (1999) Global patterns of terrestrial biological nitrogen (N2) fixation in natural ecosystems. Global Biogeochem Cycles 13:623–645
Coskun D, Britto DT, Shi W, Kronzucker HJ (2017) How plant root exudates shape the nitrogen cycle. Trends Plant Sci 22:661–673
D’Angioli AM, Viani RA, Lambers H, Sawaya AC, Oliveira RS (2017) Inoculation with Azospirillum brasilense (Ab-V4, Ab-V5) increases Zea mays root carboxylate-exudation rates, dependent on soil phosphorus supply. Plant and Soil 410:499–507
Daims H, Lebedeva EV, Pjevac P, Han P, Herbold C, Albertsen M, Jehmlich N, Palatinszky M, Vierheilig J, Bulaev A, Kirkegaard RH (2015) Complete nitrification by Nitrospira bacteria. Nature 528:504–509
Dakora FD (2000) Commonality of root nodulation signals and nitrogen assimilation in tropical grain legumes belonging to the tribe Phaseoleae. Aust J Plant Physiol 27:885–892
Dakora FD, Phillips DA (2002) Root exudates as mediators of mineral acquisition in low-nutrient environments. Plant and Soil 245:35–47
Dardanelli MS, de Córdoba FJ, Estévez J, Contreras R, Cubo MT, Rodríguez-Carvajal MÁ, Gil-Serrano AM, López-Baena FJ, Bellogín R, Manyani H, Ollero FJ (2012) Changes in flavonoids secreted by Phaseolus vulgaris roots in the presence of salt and the plant growth–promoting rhizobacterium Chryseobacterium balustinum. Appl Soil Ecol 57:31–38
de Maagd RA, Wijfjes AH, Spaink HP, Ruiz-Sainz JE, Wijffelman CA, Okker RJ, Lugtenberg BJ (1989) NodO, a new nod gene of the Rhizobium leguminosarum biovar viciae sym plasmid pRL1JI, encodes a secreted protein. J Bacteriol 171:6764–6770
Deakin WJ, Broughton WJ (2009) Symbiotic use of pathogenic strategies: rhizobial protein secretion systems. Nat Rev Microbiol 7:312–320
De-la-Pena C, Vivanco JM (2010) Root–microbe interactions: the importance of protein secretion. Curr Proteomics 7:265–274
Dennis PG, Miller AJ, Hirsch PR (2010) Are root exudates more important than other sources of rhizodeposits in structuring rhizosphere bacterial communities? FEMS Microbiol Ecol 72:313–327
Derrien D, Marol C, Balesdent J (2004) The dynamics of neutral sugars in the rhizosphere of wheat: an approach by 13C pulse–labelling and GC/C/IRMS. Plant and Soil 267:243–253
Dong Z, Layzell DB (2001) H2 oxidation, O2 uptake and CO2 fixation in hydrogen treated soils. Plant and Soil 229:1–12
Eisenbach M (1996) Control of bacterial chemotaxis. Mol Microbiol 20:903–910
Erisman JW, Sutton MA, Galloway J, Klimont Z, Winiwarter W (2008) How a century of ammonia synthesis changed the world. Nat Geosci 1:636–639
Finzi AC, Abramoff RZ, Spiller KS, Brzostek ER, Darby BA, Kramer MA, Phillips RP (2015) Rhizosphere processes are quantitatively important components of terrestrial carbon and nutrient cycles. Glob Chang Biol 21:2082–2094
Francis CA, Beman JM, Kuypers MM (2007) New processes and players in the nitrogen cycle: the microbial ecology of anaerobic and archaeal ammonia oxidation. ISME J 1:19–27
Gao D, Li X, Lin X, Wu D, Jin B, Huang Y, Liu M, Chen X (2017) Soil dissimilatory nitrate reduction processes in the Spartina alterniflora invasion chronosequences of a coastal wetland of southeastern China: dynamics and environmental implications. Plant Soil 421:383–399
Godlewski M, Adamczyk B (2007) The ability of plants to secrete proteases by roots. Plant Physiol Biochem 45:657–664
Golding A, Zou Y, Yang X, Flynn B, Dong Z (2012) Plant growth promoting H2-oxidizing bacteria as seed inoculants for cereal crops. Agric Sci 3:510–516
Greer-Phillips SE, Stephens BB, Alexandre G (2004) An energy taxis transducer promotes root colonization by Azospirillum brasilense. J Bacteriol 186:6595–6604
Guo M, Gong Z, Miao R, Su D, Li X, Jia C, Zhuang J (2017) The influence of root exudates of maize and soybean on polycyclic aromatic hydrocarbons degradation and soil bacterial community structure. Ecol Eng 99:22–30
Gupta VV, Roper MM, Roget DK (2006) Potential for non-symbiotic N2-fixation in different agroecological zones of southern Australia. Soil Res 44:343–354
Haichar FZ, Santaella C, Heulin T, Achouak W (2014) Root exudates mediated interactions belowground. Soil Biol Biochem 77:69–80
Hamilton EW III, Frank DA (2001) Can plants stimulate soil microbes and their own nutrient supply? Evidence from a grazing tolerant grass. Ecology 82:2397–2402
Hartwig UA, Maxwell CA, Joseph CM, Phillips DA (1990) Chrysoeriol and luteolin released from alfalfa seeds induce nod genes in Rhizobium meliloti. Plant Physiol 92:116–122
Hassan S, Mathesius U (2012) The role of flavonoids in root–rhizosphere signalling: opportunities and challenges for improving plant–microbe interactions. J Exp Bot 63:3429–3444
Hayatsu M, Tago K, Saito M (2008) Various players in the nitrogen cycle: diversity and functions of the microorganisms involved in nitrification and denitrification. Soil Sci Plant Nutr 54:33–45
Hirsch AM, Bauer WD, Bird DM, Cullimore J, Tyler B, Yoder JI (2003) Molecular signals and receptors: controlling rhizosphere interactions between plants and other organisms. Ecology 84:858–868
Hoffman BM, Lukoyanov D, Yang ZY, Dean DR, Seefeldt LC (2014) Mechanism of nitrogen fixation by nitrogenase: the next stage. Chem Rev 114:4041–4062
Hu J, Zhou Y, Lei Z, Liu G, Hua Y, Zhou W, Wan X, Zhu D, Zhao J (2020) Effects of Potamogeton crispus decline in the rhizosphere on the abundance of anammox bacteria and nirS denitrifying bacteria. Environ Pollut 260:114018
Huang XF, Chaparro JM, Reardon KF, Zhang R, Shen Q, Vivanco JM (2014) Rhizosphere interactions: root exudates, microbes, and microbial communities. Botany 92:267–275
Hurek T, Handley LL, Reinhold-Hurek B, Piché Y (2002) Azoarcus grass endophytes contribute fixed nitrogen to the plant in an unculturable state. Mol Plant-Microbe Interact 15:233–242
Janczarek M, Skorupska A (2011) Modulation of rosR expression and exopolysaccharide production in Rhizobium leguminosarum bv. trifolii by phosphate and clover root exudates. Int J Mol Sci 12:4132–4155
Jones DL, Hodge A, Kuzyakov Y (2004) Plant and mycorrhizal regulation of rhizodeposition. New Phytol 163:459–480
Jones ZL, Jasper JT, Sedlak DL, Sharp JO (2017) Sulfide-induced dissimilatory nitrate reduction to ammonium supports anaerobic ammonium oxidation (anammox) in an open-water unit process wetland. Appl Environ Miccrobiol 83(15)
Kartal B, Maalcke WJ, de Almeida NM, Cirpus I, Gloerich J, Geerts W, den Camp HJ, Harhangi HR, Janssen-Megens EM, Francoijs KJ, Stunnenberg HG (2011) Molecular mechanism of anaerobic ammonium oxidation. Nature 479:127–130
Kennedy IR, Islam NJ (2001) The current and potential contribution of asymbiotic nitrogen fixation to nitrogen requirements on farms: a review. Austr J Exp Agric 41:447–457
Kidd DR, Ryan MH, Hahne D, Haling RE, Lambers H, Sandral GA, Simpson RJ, Cawthray GR (2018) The carboxylate composition of rhizosheath and root exudates from twelve species of grassland and crop legumes with special reference to the occurrence of citramalate. Plant and Soil 424:389–403
Kislev M, Werker E (1978) Mucilage on the root surface and root hairs of sorghum: heterogeneity in structure, manner of production and site of accumulation. Ann Bot 42:809–816
Krapp A (2015) Plant nitrogen assimilation and its regulation: a complex puzzle with missing pieces. Curr Opin Plant Biol 25:115–122
Krause A, Doerfel A, Göttfert M (2002) Mutational and transcriptional analysis of the type III secretion system of Bradyrhizobium japonicum. Mol Plant Microbe Interact 15:1228–1235
Krishnan HB, Lorio J, Kim WS, Jiang G, Kim KY, DeBoer M, Pueppke SG (2003) Extracellular proteins involved in soybean cultivar–specific nodulation are associated with pilus-like surface appendages and exported by a type III protein secretion system in Sinorhizobium fredii USDA257. Mol Plant Microbe Interact 16:617–625
Ladha J, Tirol-Padre A, Reddy C et al (2016) Global nitrogen budgets in cereals: a 50-year assessment for maize, rice, and wheat production systems. Sci Rep 6:19355
Landi L, Valori F, Ascher J, Renella G, Falchini L, Nannipieri P (2006) Root exudate effects on the bacterial communities, CO2 evolution, nitrogen transformations and ATP content of rhizosphere and bulk soils. Soil Biol Biochem 38:509–516
Lata JC, Durand J, Lensi R, Abbadie L (1999) Stable coexistence of contrasted nitrification statuses in a wet tropical savanna system. Funct Ecol 13:762–763
Lee JA, Francis CA (2017) Spatiotemporal characterization of San Francisco Bay denitrifying communities: a comparison of nirK and nirS diversity and abundance. Microb Ecol 73:271–284
Li X, Gao D, Hou L, Liu M (2019) Soil substrates rather than gene abundance dominate DNRA capacity in the Spartina alterniflora ecotones of estuarine and intertidal wetlands. Plant Soil 436:123–140
Limpens E, van Zeijl A, Geurts R (2015) Lipochitooligosaccharides modulate plant host immunity to enable endosymbioses. Annu Rev Phytopathol 53:311–334
Liu Y, Guan D, Jiang X, Ma M, Li L, Cao F, Chen H, Shen D, Li J (2015) Proteins involved in nodulation competitiveness of two Bradyrhizobium diazoefficiens strains induced by soybean root exudates. Biol Fertil Soils 51:251–260
Liu YC, Qin XM, Xiao JX, Tang L, Wei CZ, Wei JJ, Zheng Y (2017) Intercropping influences component and content change of flavonoids in root exudates and nodulation of faba bean. J Plant Int 12:187–192
Lu Y, Zhou Y, Nakai S, Hosomi M, Zhang H, Kronzucker HJ, Shi W (2014) Stimulation of nitrogen removal in the rhizosphere of aquatic duckweed by root exudate components. Planta 239:591–603
Lynch JM, Whipps JM (1990) Substrate flow in the rhizosphere. Plant Soil 129:1–10
Maimaiti J, Zhang Y, Yang J, Cen YP, Layzell DB, Peoples M, Dong Z (2007) Isolation and characterization of hydrogen-oxidizing bacteria induced following exposure of soil to hydrogen gas and their impact on plant growth. Environ Microbiol 9:435–444
Marschner H (1995) Mineral nutrition of higher plants. Academic, London
McCully ME, Boyer JS (1997) The expansion of maize root-cap mucilage during hydration changes in water potential and water content. Physiol Plant 99:169–177
Moghaddam MMM, Emtiazi G, Salehi Z (2012) Enhanced auxin production by Azospirillum pure cultures from plant root exudates. J Agric Sci Technol 14:985–994
Moscatiello R, Squartini A, Mariani P, Navazio L (2010) Flavonoid-induced calcium signalling in Rhizobium leguminosarum bv. viciae. New Phytol 188:814–823
Mosier A, Kroeze C, Nevison C, Oenema O, Seitzinger S, Van Cleemput O (1998) Closing the global N2O budget: nitrous oxide emissions through the agricultural nitrogen cycle. Nutr Cycl Agroecosyst 52:225–248
Naher K, Miwa H, Okazaki S, Yasuda M (2018) Effects of different sources of nitrogen on endophytic colonization of rice plants by Azospirillum sp. B510. Microbes Environ 2018:17186
Nguyen C (2003) Rhizodeposition of organic C by plants: mechanisms and controls. Agronomie 23:375–396
Nie Y, Wang M, Zhang W, Ni Z, Hashidoko Y, Shen W (2018) Ammonium nitrogen content is a dominant predictor of bacterial community composition in an acidic forest soil with exogenous nitrogen enrichment. Sci Environ 624:407–415
O’Neal L, Akhter S, Alexandre GA (2019) PilZ-containing chemotaxis receptor mediates oxygen and wheat root sensing in Azospirillum brasilense. Front Microbiol 10:312
Offre P, Spang A, Schleper C (2013) Archaea in biogeochemical cycles. Annu Rev Microbiol 67:437–457
Okazaki S, Zehner S, Hempel J, Lang K, Gottfert M (2009) Genetic organization and functional analysis of the type III secretion system of Bradyrhizobium elkanii. FEMS Microbiol Lett 295:88–95
Okazaki S, Okabe S, Higashi M, Shimoda Y, Sato S, Tabata S (2010) Identification and functional analysis of type III effector proteins in Mesorhizobium loti. Mol Plant Microbe Interact 23:223–234
Oldroyd GED (2013) Speak, friend, and enter: signalling systems that promote beneficial symbiotic associations in plants. Nat Rev Microbiol 11:252–263
O'Neal L, Vo L, Alexandre G (2020) Specific root exudates compounds sensed by dedicated chemoreceptors shape Azospirillum brasilense chemotaxis in the rhizosphere. Appl Environ Microbiol 86(15):e01026–e01020. https://doi.org/10.1128/AEM.01026-20
Oshiki M, Ali M, Shinyako-Hata K, Satoh H, Okabe S (2016) Hydroxylamine-dependent anaerobic ammonium oxidation (anammox) by “Candidatus Brocadia sinica”. Environ Microbiol 18:3133–3143
Pan H, Qin Y, Wang Y, Liu S, Yu B, Song Y, Wang X, Zhu G (2020) Dissimilatory nitrate/nitrite reduction to ammonium (DNRA) pathway dominates nitrate reduction processes in rhizosphere and non-rhizosphere of four fertilized farmland soil. Environ Res 1:109612
Pang Y, Ji G (2019) Biotic factors drive distinct DNRA potential rates and contributions in typical Chinese shallow lake sediments. Environ Pollut 254:112903
Pereira LC, Bertuzzi Pereira C, Correia LV, Matera TC, Santos RF, Carvalho CD, Osipi EA, Braccini AL (2020) Corn responsiveness to Azospirillum: accessing the effect of root exudates on the bacterial growth and its ability to fix nitrogen. Plan Theory 9:923
Philippot L, Raaijmakers JM, Lemanceau P, Van Der Putten WH (2013) Going back to the roots: the microbial ecology of the rhizosphere. Nat Rev Microbiol 11:789–799
Phillips DA, Joseph CM, Yang GP, Martinez-Romero E, Sanborn JR, Volpin H (1999) Identification of lumichrome as a Sinorhizobium enhancer of alfalfa root respiration and shoot growth. Proc Natl Acad Sci U S A 22:12275–12280
Prosser JI, Nicol GW (2012) Archaeal and bacterial ammonia-oxidisers in soil: the quest for niche specialisation and differentiation. Trends Microbiol 20:523–531
Ravishankara AR, Daniel JS, Portmann RW (2009) Nitrous oxide (N2O): the dominant ozone-depleting substance emitted in the 21st century. Science 326:123–125
Read DB, Bengough AG, Gregory PJ, Crawford JW, Robinson D, Scrimgeour CM, Young IM, Zhang K, Zhang X (2003) Plant roots release phospholipid surfactants that modify the physical and chemical properties of soil. New Phytol 157:315–321
Robertson EK, Roberts KL, Burdorf LD, Cook P, Thamdrup B (2016) Dissimilatory nitrate reduction to ammonium coupled to Fe (II) oxidation in sediments of a periodically hypoxic estuary. Limnol Ocean 61:365–381
Roper MM, Ladha JK (1995) Biological N2 fixation by heterotrophic and phototrophic bacteria in association with straw. In: Management of biological nitrogen fixation for the development of more productive and sustainable agricultural systems 1995. Springer, Dordrecht, pp 211–224
Rütting T, Boeckx P, Müller C, Klemedtsson L (2011) Assessment of the importance of dissimilatory nitrate reduction to ammonium for the terrestrial nitrogen cycle. Biogeosciences 8:1779–1791
Ryan PR, Delhaize E (2001) Function and mechanism of organic anion exudation from plant roots. Annu Rev Plant Physiol Mol Biol 52:527–560
Schubert CJ, Durisch-Kaiser E, Wehrli B, Thamdrup B, Lam P, Kuypers MM (2006) Anaerobic ammonium oxidation in a tropical freshwater system (Lake Tanganyika). Environ Microbiol 8:1857–1863
Sealey LJ, McCully ME, Canny MJ (1995) The expansion of maize root-cap mucilage during hydration. Kinetics Physiol Plant 93:38–46
Shcherbak I, Millar N, Robertson GP (2014) Global metaanalysis of the nonlinear response of soil nitrous oxide (N2O) emissions to fertilizer nitrogen. Proc Natl Acad Sci U S A 111:9199–9204
Sinha Roy S, Mittra B, Sharma S, Das TK, Roy BCR (2002) Detection of root mucilage using an antifucose antibody. Ann Bot 89:293–299
Smith VH, Tilman GD, Nekola JC (1999) Eutrophication: impacts of excess nutrient inputs on freshwater, marine, and terrestrial ecosystems. Environ Pollut 100:179–196
Sonthiphand P, Hall MW, Neufeld JD (2014) Biogeography of anaerobic ammonia-oxidizing (anammox) bacteria. Front Microbiol 5:399
Srivastava P, Sharma PK, Dogra RC (1999) Inducers of nod genes of Rhizobium ciceri. Microbiol Res 154:49–55
Steenhoudt O, Vanderleyden J (2000) Azospirillum, a free-living nitrogen-fixing bacterium closely associated with grasses: genetic, biochemical and ecological aspects. FEMS Microbiol Rev 24:487–506
Stein LY, Klotz MG (2016) The nitrogen cycle. Curr Biol 26:94–98
Subbarao GV, Ishikawa T, Ito O, Nakahara K, Wang HY, Berry WL (2006) A bioluminescence assay to detect nitrification inhibitors released from plant roots: a case study with Brachiaria humidicola. Plant Soil 288:101–112
Subbarao GV, Rondon M, Ito O, Ishikawa T, Rao IM, Nakahara K, Lascano C, Berry WL (2007) Biological nitrification inhibition (BNI)—is it a widespread phenomenon? Plant Soil 294:5–18
Subbarao GV, Nakahara K, Hurtado MP, Ono H, Moreta DE, Salcedo AF, Yoshihashi AT, Ishikawa T, Ishitani M, Ohnishi-Kameyama M, Yoshida M, Rondon M, Rao IM, Lascano CE, Berry WL, Ito O (2009) Evidence for biological nitrification inhibition in Brachiaria pastures. Proc Natl Acad Sci U S A 106:17302–17307
Subbarao GV, Sahrawat KL, Nakahara K, Ishikawa T, Kishii M, Rao IM, Hash CT, George TS, Srinivasa Rao P, Nardi P, Bonnett D, Berry W, Suenaga K, Lata JC (2012) Biological nitrification inhibition—a novel strategy to regulate nitrification in agricultural systems. Adv Agron 114:249–302
Subbarao GV, Nakahara K, Ishikawa T, Ono H, Yoshida M, Yoshihashi T, Zhu Y, Zakir HAKM, Deshpande SP, Hash CT, Sahrawat KL (2013) Biological nitrification inhibition (BNI) activity in Sorghum and its characterization. Plant and Soil 366:243–259
Thornton B, Osborne SM, Paterson E, Cash P (2007) A proteomic and targeted metabolomic approach to investigate change in Lolium perenne roots when challenged with glycine. J Exp Bot 58:1581–1590
Usyskin-Tonne A, Hadar Y, Yermiyahu U, Minz D (2020) Elevated CO2 has a significant impact on denitrifying bacterial community in wheat roots. Soil Biol Biochem 142:107697
van Kessel MA, Speth DR, Albertsen M, Nielsen PH, den Camp HJ, Kartal B, Jetten MS, Lücker S (2015) Complete nitrification by a single microorganism. Nature 528:555–559
van Niftrik L, Jetten MSM (2012) Anaerobic ammonium-oxidizing bacteria: unique microorganisms with exceptional properties. Microbiol Mol Biol Rev 76:585–596
Velmourougane K, Prasanna R, Singh S, Chawla G, Kumar A, Saxena AK (2017) Modulating rhizosphere colonisation, plant growth, soil nutrient availability and plant defense enzyme activity through Trichoderma viride–Azotobacter chroococcum biofilm inoculation in chickpea. Plant and Soil 421:157–174
Verhamme DT, Prosser JI, Nicol GW (2011) Ammonia concentration determines differential growth of ammonia-oxidising archaea and bacteria in soil microcosms. ISME J 5:1067–1071
Vitousek PM, Aber JD, Howarth RW, Likens GE, Matson PA, Schindler DW, Schlesinger WH, Tilman DG (1997) Human alteration of the global nitrogen cycle: sources and consequences. Ecol Appl 7:737–750
Vitousek PM, Menge DN, Reed SC, Cleveland CC (2013) Biological nitrogen fixation: rates, patterns and ecological controls in terrestrial ecosystems. Philos Trans R Soc B 368:20130119
Vranova V, Rejsek K, Formanek P (2013) Aliphatic, cyclic, and aromatic organic acids, vitamins, and carbohydrates in soil: a review. Sci World J, Article ID-524239
Wang YF, Wang JF, Xu ZM, She SH, Yang JQ, Li QS (2020) L-glutamic acid induced the colonization of high-efficiency nitrogen-fixing strain Ac63 (Azotobacter chroococcum) in roots of Amaranthus tricolor. Plant and Soil 451:357–370
Welsh A, Chee-Sanford JC, Connor LM, Löffler FE, Sanford RA (2014) Refined NrfA phylogeny improves PCR-based nrfA gene detection. Appl Environ Microbiol 80:2110–2119
Zakir HAKM, Subbarao GV, Pearse SJ, Gopalakrishnan S, Ito O, Ishikawa T, Kawano N, Nakahara K, Yoshihashi T, Ono H, Yoshida M (2008) Detection, isolation and characterization of a root-exuded compound, methyl 3-(4-hydroxyphenyl) propionate, responsible for biological nitrification inhibition by sorghum (Sorghum bicolor). New Phytol 180:442–451
Zhai X, Piwpuan N, Arias CA, Headley T, Brix H (2013) Can root exudates from emergent wetland plants fuel denitrification in subsurface flow constructed wetland systems? Ecol Eng 61:555–563
Zhang J, Subramanian S, Zhang Y, Yu O (2007) Flavone synthases from Medicago truncatula are flavanone-2-hydroxylases and are important for nodulation. Plant Physiol 144:741–751
Zhang Z, Qiao M, Li D, Yin H, Liu Q (2016) Do warming-induced changes in quantity and stoichiometry of root exudation promote soil N transformations via stimulation of soil nitrifiers, denitrifiers and ammonifiers? Eur J Soil Biol 74:60–68
Zhang CB, Liu WL, Han WJ, Guan M, Wang J, Liu SY, Ge Y, Chang J (2017) Responses of dissimilatory nitrate reduction to ammonium and denitrification to plant presence, plant species and species richness in simulated vertical flow constructed wetlands. Wetland 37:109–122
Zhou M, Butterbach-Bahl K, Vereecken H, Brüggemann N (2017) A meta-analysis of soil salinization effects on nitrogen pools, cycles and fluxes in coastal ecosystems. Glob Chang Biol 23:1338–1352
Zhu G, Jetten MS, Kuschk P, Ettwig KF, Yin C (2010) Potential roles of anaerobic ammonium and methane oxidation in the nitrogen cycle of wetland ecosystems. Appl Microbiol Biotechnol 86:1043–1055
Zhu B, Gutknecht JL, Herman DJ, Keck DC, Firestone MK, Cheng W (2014) Rhizosphere priming effects on soil carbon and nitrogen mineralization. Soil Biol Biochem 76:183–192
Zuanazzi JAS, Clergeot PH, Quirion JC, Husson HP, Kondorosi A, Ratet P (1998) Production of Sinorhizobium meliloti nod gene activator and repressor flavonoids from Medicago sativa roots. Mol Plant Microbe Interact 11:784–794
Acknowledgments
The authors are grateful to the Application of Microorganisms Agriculture and Allied Sectors (AMAAS) Network Project, Indian Council of Agricultural Research (ICAR), New Delhi, India.
Author information
Authors and Affiliations
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2021 The Author(s), under exclusive license to Springer Nature Switzerland AG
About this chapter
Cite this chapter
Ahmad, E., Sharma, P.K., Khan, M.S. (2021). Roles of Root Exudates in Different Processes in the Nitrogen Cycle in the Rhizosphere. In: Cruz, C., Vishwakarma, K., Choudhary, D.K., Varma, A. (eds) Soil Nitrogen Ecology. Soil Biology, vol 62. Springer, Cham. https://doi.org/10.1007/978-3-030-71206-8_8
Download citation
DOI: https://doi.org/10.1007/978-3-030-71206-8_8
Published:
Publisher Name: Springer, Cham
Print ISBN: 978-3-030-71205-1
Online ISBN: 978-3-030-71206-8
eBook Packages: Biomedical and Life SciencesBiomedical and Life Sciences (R0)