Direct cell extraction from fresh and stored soil samples: Impact on microbial viability and community compositions
Introduction
Despite the abundant and diverse microorganisms in soil samples, the majority of soil bacteria and archaea remain uncultured (Steen et al., 2019), which hampers our understanding of the functions of these prokaryotes from soil microbial communities. Recent development of various single-cell techniques using directly extracted microbial cells provides valuable phenotypic and genomic information of these uncultured microbes (Eichorst et al., 2015). Also, such directly extracted soil microbial cells have been used for high-throughput culturing (Wang et al., 2014), direct quantification of bacterial abundance (Bressan et al., 2015; Frossard et al., 2016; Khalili et al., 2019), and extraction of high-molecular-weight DNA (Robe et al., 2003; Williamson et al., 2011). However, the relative low yield and low viability of typical soil cell extraction procedures remain a major challenge, and hence, how well the directly extractable soil cells represent the original soil samples remains largely unknown.
Intensive efforts have been invested to improve the direct microbial cell extraction efficiency from soil samples by focusing on the following aspects: i) separation of microbial cells from soil organic matter and soil particles. Physical dispersion (e.g. blending and sonication) and chemical dispersion (e.g., ionic or non-ionic buffers) are used alone or together to detach cells from soil particle surfaces (Bakken, 1985; Courtois et al., 2001; Lindahl and Bakken, 1995; Williamson et al., 2011). Previous studies have shown that physical and chemical dispersions largely determine cell extraction efficiencies (Courtois et al., 2001; Khalili et al., 2019; Williamson et al., 2011). But the cell extraction efficiency is highly variable depending on soil textures (Amalfitano and Fazi, 2008). ii) purification of the dispersed microbial cells. Several density gradient media have been used to purify microbial cells from soil matrices, including Nycodenz (Lindahl and Bakken, 1995), Histodenz (Frossard et al., 2016), sucrose (Liu et al., 2010), and sodium bromide (Laflamme et al., 2005). Nycodenz density gradient centrifugation is one of the most commonly used purification methods. Higher Nycodenz concentration has been reported to be beneficial for improving the overall soil cell extraction efficiency (Eichorst et al., 2015; Holmsgaard et al., 2011). iii) increasing the number of extraction/purification procedures. For example, three sequential rounds of extraction recover more cells than a single-pass extraction (Williamson et al., 2011). Despite these various methods developed, with currently reported soil cell extraction procedures, both dead and live cells are recovered after Nycodenz density centrifugation (Burkert et al., 2019; Whiteley et al., 2003). Also, cell extraction efficiencies reported in literature are largely based on the total number of cells extracted that includes both live and dead cells. Therefore, to truly assess the extraction efficiency meaningful for downstream microbial phenotypic characterization, it is important to focus on the efficiency of viable cell extraction along with examining the viable microbial community compositions of cells extracted from soils.
Another aspect to consider is how soil sample storage conditions affect the efficiency of viable cell extraction from soil samples. Soil samples are often stored before conducting physiological or molecular biological experiments on them. Many studies have examined the effect of soil storage conditions on microbial communities, but the results of these studies are inconsistent. Some studies have found that temperature and duration of storage have no effect on the overall microbial community composition (Dolfing, 2004; Lauber et al., 2010; Rubin et al., 2013). However, other studies have demonstrated that storage conditions significantly change soil microbial community composition (Černohlávková et al., 2009; Cui et al., 2014; Piao et al., 2010; Tzeneva et al., 2009). In these studies, the microbial community diversities were measured at the DNA level; however, it is unknown whether the various soil storage conditions significantly impact the viability and recovery of soil-extractable cells and soil-viable microbial community compositions.
Lastly, to evaluate cell viability, cells are often fluorescently labeled using live/dead staining reagents and quantified using microscopy or flow cytometry (Emerson et al., 2017). However, this technique does not provide any information on the viable microbial community composition. Viability PCR has been used in cell cultures or environmental samples (Carini et al., 2016; Emerson et al., 2017; Nocker et al., 2007). Viability dyes, such as propidium monoazide or ethidium monoazide, bind to DNA from dead or compromised cells and the dye-bound DNA is degraded when exposed to certain wavelength of light, enabling the analysis of DNA originated from viable cells only. In this study, both live/dead staining and viability PCR were used to evaluate the impact of extraction procedures and soil storage conditions on the viability and microbial community composition of soil-extractable cells using soil samples having diverse ranges of physicochemical properties.
In this study, we aimed to improve the yield and viability of soil extractable cells with two sequential rounds of cell extraction procedure. By comparing different physical and chemical dispersion methods, and Nycodenz density gradient medium concentrations in soil samples having diverse physicochemical properties, we expected to identify the combination offering the highest cell viability and yield. In addition, using the optimized cell extraction procedure, we sought to assess the effect of soil storage conditions (4 °C, −80 °C, and air-drying) on yield, viability, and community composition of soil extractable cells. We hypothesized that storage at 4 °C would be suitable for maintaining viable microbial cells in soil samples because storage at −80 °C and air-drying may exert physiological stresses on soil microbes.
Section snippets
Soils
Four surface soils (0–10 cm depth) were collected from sites in Oklahoma (Table 1). Soil A was a loam soil taken from outside of the new warming experimental plots created in 2009 (34°58′45″ N, 97°31′15″ W) (Guo et al., 2018). Soil B was a clay loam soil taken from outside of the old warming experimental plots created in 1999 (34°58′44″ N, 97°31′29″ W) (Zhou et al., 2012). Soil C (sandy loam soil) and Soil D (loam soil) were obtained from outside of the switchgrass plots in the Third Street
Determining the optimal protocol for microbial cell extraction from soil
We evaluated the yield and viability of soil extractable cells using four extraction combinations of physical dispersion, chemical dispersion, and Nycodenz concentration. All extractions were performed with two sequential rounds (Fig. 1) in different types of soils, including loam, sandy loam and clay loam (Table 1). The total yields of soil extractable cells with two rounds of extraction and purification ranged from 4.5 × 106 to 2.6 × 107/g dry soil (Fig. 2A). Overall, more extractable cells
Discussion
Extraction of microbial cells from soil is a critical step for the application of many microbial discovery campaigns, including those performed at single-cell resolution. For example, microbial diversity in soil has been extensively mined for the discovery of novel antibiotics, anti-cancer compounds, enzymes, and organisms (Hover et al., 2018; Knight et al., 2003; Pham and Kim, 2012). Previous work on extraction methods often focused on the improvement of cell recovery efficiency evaluated at
Conclusions
Obtaining a large number of viable cells that represent the microbial community in soil as close as possible is often the first step for many microbiological applications. We found that implementation of a protocol that features the use of a blender + Tween 20 + 80% Nycodenz provides the optimal combination for direct viable soil bacteria extraction among conditions tested in the present study. First and second rounds of cell extraction resulted in different microbial community compositions,
Data availability
Raw sequences of 16S rRNA amplicon genes are available in NCBI SRA database (www.ncbi.nlm.nih.gov/sra) under accession number PRJNA644647.
Declaration of competing interest
The authors declare that they have no known competing financial interests or personal relationships that could have appeared to influence the work reported in this paper.
Acknowledgements
We thank Colin T. Bates for help in collecting Soil C and Soil D. The project depicted is sponsored by the Defense Advanced Research Projects Agency (Agreement W911NF1920013). The content of the information does not necessarily reflect the position or the policy of the Government, and no official endorsement should be inferred.
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