A Rapid DNA Extraction Method for PCR Amplification From Wetland Soils
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ORIGINAL ARTICLE
A rapid DNA extraction method for PCR amplification fromwetland soilsJ. Li1, B. Li1, Y. Zhou2, J. Xu2 and J. Zhao2
1 College of Life Sciences, Inner Mongolia University, Huhhot, China
2 College of Environment and Resources, Inner Mongolia University, Huhhot, China
Introduction
Ammonia oxidation is the fist step in nitrification, a key
process and limiting step in the global nitrogen cycle
(Leininger et al. 2006). Ammonia-oxidizing bacteria
(AOB) and the recently found ammonia-oxidizing organ-
isms belonging to the archaeal domain (AOA) play
important roles in the nitrogen cycle (You et al. 2009).
Ammonia oxidation is now believed to be driven by these
two major microbial groups. AOA have been found in
various habitats including hot ⁄ thermal springs (Hatzenp-
ichler et al. 2008), oceans (Beman et al. 2008), fresh water
(Santoro et al. 2008) and soil (Tourna et al. 2008). How-
ever, they are very difficult to culture outside of these
habitats because of their slow growth rates and their
sensitivity to some organic substances. Up to now, only
AOAs such as Nitrosopumilus maritimu, Nitrosocaldus
yellowstonii, Nitrososphaera gargensis (You et al. 2009)
were obtained. Cultivation-independent methods play
important roles in helping us to understand the diversity
and distribution of these microbes.
Ammonia oxidation-related microbes are low in number
and are hardly detectable using 16S rRNA (Junier et al.
2010). Therefore, alternative functional markers such as
specific metabolic-pathway-related key enzymes, e.g., those
involved in ammonia oxidation, have been used for ecolog-
ical studies (Hermansson and Lindgren 2001). To amplify
the amoA gene from AOA and AOB, an improved
approach based on the dispersal of soils with glass beads is
used to release ammonia-oxidizing microbes that are
strongly adherent on soil colloids or located within the
inner microporosity of soil aggregates (Robe et al. 2003).
Many DNA extraction methods have been reported.
SDS-based methods (Zhou et al. 1996) use CTAB or
PVPP (Juniper et al. 1999) to remove humic substances;
Al2(SO4)3 extraction methods (Dong et al. 2006; Persoh
et al. 2008) use Al2(SO4)3 to remove humic substances
and electroelution methods (Kallmeyer and Smith 2009)
purify DNA directly extracted from marine sediments
with an electroelution apparatus. DNA extraction solu-
tions contain EDTA (Tsai and Olson 1992; Zhou et al.
1996; Miller et al. 1999; Martin-Laurent et al. 2001),
which can combine with the divalent ions. It is very
important to obtain nucleic acids from various environ-
mental samples because DNA techniques allow less biased
access to a greater portion of uncultivable microbes and
Keywords
ammonia-oxidizing archaea, ammonia-
oxidizing bacteria, calcium chloride, glass
bead, SDS method.
Correspondence
Ji Zhao, College of Environment & Resources,
Inner Mongolia University, Huhhot 010021,
China.
E-mail: [email protected]
2010 ⁄ 1633: received 16 September 2010,
revised 1 March 2011 and accepted 15 March
2011
doi:10.1111/j.1472-765X.2011.03047.x
Abstract
Aims: We tested a method of rapid DNA extraction from wetland soil samples
for use in the polymerase chain reaction.
Methods and Results: The glass bead ⁄ calcium chloride ⁄ SDS method obtained
in the present study was compared with the calcium chloride ⁄ SDS ⁄ enzymatic
extraction method and the UltraClean� Soil DNA Isolation Kit. Rapid DNA
extraction could be completed within about two hours without purification
steps.
Conclusions: This study succeeded in establishing a fast soil DNA extraction
protocol that can be applied to various environmental sources that are rich in
humic acid content.
Significance and Impact of the Study: The method provides a technology with
high-quality DNA extraction from soils for testing the diversity of AOB and
AOA.
Letters in Applied Microbiology ISSN 0266-8254
626 Letters in Applied Microbiology 52, 626–633 ª 2011 The Society for Applied Microbiology
ª 2011 The Authors
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also provide a useful tool for studying the structure and
diversity of microbial communities (Robe et al. 2003).
Many soil DNA extraction methods have been reported,
such as a liquid nitrogen grinding method (Volossiouk
et al. 1995), a microwave-based rupture method (Orsini
and Romano-Spica 2001), an SDS-based method (Zhou
et al. 1996), a bead-beating lysis method (Miller et al.
1999), a rapid freeze-and-thaw method (Tsai and Olson
1992), a cation-exchange method (Jacobsen and Rasmus-
sen 1992), a solvent-based bead-beating method (Chen
et al. 2006), an MS laboratory method (Martin-Laurent
et al. 2001), a Nycodenz gradient separation method
(Helene et al. 2005), an Al2(SO4)3 extraction method
(Persoh et al. 2008), our laboratory-devised calcium chlo-
ride ⁄ SDS ⁄ enzyme DNA extraction method (Li et al.
2010) and our laboratory-devised glass bead ⁄ calcium
chloride ⁄ SDS DNA extraction method, which was
reported in this study. All DNA extraction methods focus
on humic substances. To get high-purity DNA from soil,
these methods generally include a subsequent purification
step, such as Sepharose 4B, Sephadex G-200, Sephadex
G-50 (Jackson et al. 1997) or electroelution (Kallmeyer
and Smith 2009). In our laboratory-devised calcium chlo-
ride ⁄ SDS ⁄ enzyme DNA extraction method, we also
focused on these substances and obtained a method that
is more efficient at removing humic acids from wetland
soil because it uses a humic-substance-removal solution
combined with calcium chloride solution. However, this
method could only be used for 16S rDNA amplification
and functional gene amplification from certain soils (in
this study). The glass bead ⁄ calcium chloride ⁄ SDS DNA
extraction method is based on the humic-substance-
removal technique derived from the calcium chlo-
ride ⁄ SDS ⁄ enzyme DNA extraction method, and it can
save time when used for functional gene amplification. In
particular, ammonia oxidation-related microbes can be
studied by this method. One commercial DNA purifica-
tion kit and two laboratory-devised methods, a calcium
chloride ⁄ SDS ⁄ enzyme DNA extraction method (Li et al.
2010) and an improved glass bead ⁄ calcium ⁄ chloride ⁄ SDS
method, were used to extract DNA directly from soil. The
amoA gene and 16S rDNA were amplified to estimate the
effectiveness of the different DNA extraction procedures.
Materials and methods
DNA extraction from soil
The physicochemical properties of the four soils used in
this study are presented in Table 1: Microbial biomass
carbon according to the chloroform fumigation extraction
method (Vance et al. 1987), organic carbon content in a
Elementar Liqui TOC Analyzer (Germany), total nitrogen
content with semimicro-Kjeldahl determination (Cole
et al. 1946), grain size distribution in a Microtrac S3500
(Montogomeryville, PA, USA). The experiment was con-
ducted in the Inner Mongolian steppes (sites W1, W2)
(43�38¢N, 116�42¢E) and Xilin River (sites W3, W4)
(44�08¢N, 117�08¢E) in the Inner Mongolia Autonomous
Region, China. Fresh soil samples were sieved (2 mm
mesh) and stored at )20�C. DNA was extracted from
four soil samples using a commercial kit (UltraClean�Soil DNA Isolation kit, Mobio Laboratories Inc., Carls-
bad, CA, USA) according to the manufacturers’ recom-
mendations (http://www.mobio. com ⁄ soil-dna-isolation ⁄ultraclean-soil-dna-isolation-kit.html) and using two pro-
cedures developed in our laboratory.
The steps of glass bead ⁄ calcium ⁄ chloride ⁄ SDS method
and the calcium chloride ⁄ SDS ⁄ enzyme DNA extraction
method are as follows (see Figs 1 and 2, respectively). A
humic-substance-removal solution containing 0Æ1 mol l)1
Tris, 0Æ1 mol l)1 Na4P2O7, 0Æ1 mol l)1 Na2EDTA, 1%
PVP (w ⁄ v), 0Æ1 mol l)1 NaCl and 0Æ05% Triton X-100
(v ⁄ v), pH 10Æ0. DNA extraction buffer containing
0Æ1 mol l)1 Tris–HCl, 1Æ5 mol l)1 NaCl and 1% CTAB,
pH 8Æ0. The mixture was homogenized using a Vortex-
Genie� 2 (Mobio Laboratories) for glass bead ⁄ cal-
cium ⁄ chloride ⁄ SDS method. If the nucleic acid mix
showed a white precipitate, 500 ll of a sterile, ice-cold
carbonate dissolution mix (0Æ43 mol l)1 glacial acetic acid,
0Æ43 mol l)1 sodium acetate, and 0Æ17 mol l)1 sodium
chloride, pH 4Æ6) (Kallmeyer and Smith 2009) was added,
followed by incubation for 20 min on ice with 0Æ6 volume
of isopropyl alcohol and centrifugation at 12 000 g for
5 min. Finally, 50 ll of TE buffer was added.
PCR amplification of 16 S rDNA and the amoA gene
To test the quality of the DNA extraction methods, 16S
rDNA and amoA gene amplification was performed on
Table 1 Properties of soil sample used in DNA extraction
Soil properties W1 W2 W3 W4
Size (lm) and %
1000 lm 100 100Æ00 100Æ00 100Æ00
500 lm 99Æ89 99Æ67 100Æ00 100Æ00
250 lm 96Æ8 90Æ31 91Æ56 96Æ41
100 lm 68Æ62 53Æ37 30Æ71 53Æ14
50 lm 47Æ23 33Æ12 15Æ28 30Æ05
10 lm 16Æ62 13Æ70 3Æ79 6Æ67
5 lm 7Æ86 6Æ49 0Æ98 2Æ22
2 lm 1Æ298 0Æ93 0Æ00 0Æ00
Organic carbon (g kg)1) 70Æ69 62Æ60 25Æ08 2Æ37
Total nitrogen (g kg)1) 2Æ115 2Æ037 1Æ089 1Æ7
Microbial biomass carbon
(mg kg)1)
987Æ01 731Æ21 246Æ35 756Æ10
J. Li et al. A rapid DNA extraction method from wetland soils
ª 2011 The Authors
Letters in Applied Microbiology 52, 626–633 ª 2011 The Society for Applied Microbiology 627
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DNA obtained directly from the four soils. Three repli-
cates were analysed for the glass bead ⁄ calcium ⁄ chlo-
ride ⁄ SDS method. The 16S rDNA was amplified in a
thermocycler from 1 ll of extracted soil DNA template
with a total volume of 25 ll by using 2Æ0 ll of
2Æ5 mmol l)1 dNTP, 1Æ0 ll of 0Æ01 mol l)1 27F (5¢-AGA
GTT TGA TCM TGG CTC AG-3¢) (see Table 2), 1Æ0 ll
of 0Æ01 mol l)1 1492R (5¢-TAC GGH TAC CTT GTT
ACG ACT T-3¢) (see Table 2), 2Æ5 ll of 10· buffer (Pro-
mega, Madison, WI), and 0Æ2 ll of 5 U ll)1 Taq DNA
polymerase under the following conditions: 5 min at
94�C, 30 cycles of 30 s at 94�C, 30 s at 55�C, and 80 s at
The nucleic acids were washed with 70% ethanol and
air-dried, 50 µl of TE buffer was added
600-µl collected supernatant was incubated for 20min on ice with 0·6 volume of isopropyl alcohol,
centrifuged at 12 000 g for 5 min
800-µl collected supernatant + equal volume ofchloroform-isoamyl-alcohol (24 : 1) in the 2-ml
centrifuge tube, centrifuged at 12 000 g for 5 min
900-µl collected supernatant + equal volume ofphenol-chloroform-isoamyl-alcohol (25 : 24 : 1) in the
2-ml centrifuge tube, centrifuged at 12 000 g for 5min
0·3 g soils
2-ml centrifuge tube + three 2·5-mm-diameterglass beads or 3·0-mm-diameter glass beads
1 ml of a humic-substance-removal solution wasadded
Homogenized for 2 min at maximum speed, centrifuged at 12 000 g for 2 min at ambient
temperature, followed by decanting of the supernatant
Calcium chloride solution was added (1 ml, 0·5 mol
l–1), homogenized for 2 min at maximum speed, centrifuged at 12 000 g for 2 min at ambient
temperature, followed by decanting of the supernatant
DNA extraction buffer (800 µl) was added
Homogenized for 5 s at maximum speed
200 µl 20% SDS was added, mixing up and down
and incubation for 10 min at 65°C, centrifuged at
12 000 g for 2 min
Figure 1 The steps of glass bead ⁄ calcium ⁄ chloride ⁄ SDS method.
The nucleic acids were washed with 70% ethanol and
air-dried, followed by addition of 50 µl TE buffer
500-µl collected supernatant was incubated for 20 min on ice with 0·6 volume of isopropyl alcohol in the
1·5-ml centrifuge tube and centrifuged at 12 000 g
600-µl collected supernatant + equal volume ofchloroform-isoamyl-alcohol (24 : 1) in the 1·5-ml
centrifuge tube and centrifuged at 12 000 g
800-µl collected supernatants + equal volume ofphenol-chloroform-isoamyl-alcohol (25 : 24 : 1) in the
2-ml centrifuge tube and centrifuged at 12 000 g
1 g soil + 2-ml centrifuge tube
Homogenized and centrifuged at 12 000 g for 5 min atambient temperature, the supernatant was then
decanted
1 ml of 0·5 mol l–1 CaCl2 solution was added,homogenized, and centrifuged at 12 000 g for 5 min
The supernatant was then decanted, 1 ml of 0·05 mol
l–1 sodium oxalate (pH 7·96) was added,homogenized and centrifuged at 12 000 g for 5 min
and decanting of the supernatant
700 µl of DNA extraction buffer was added, then
homogenized and 100 µl of 100 g l–1 lysozyme wasadded, mixed up and down several times and
incubated for 30 min at 37°C 200 rpm in a tableconcentrator, then 200 µl 20% SDS was added and
incubated for 1 h, centrifuged at 12 000 g
900-µl collected supernatant + equal volume of phenol-chloroform-isoamyl-alcohol (25 : 24 : 1) in the
2-ml centrifuge tube and centrifuged at 12 000 g
700-µl collected supernatant + equal volume ofchloroform-isoamyl-alcohol (24 : 1) in a 1·5-ml
centrifuge tube and centrifuged at 12 000 g
Figure 2 The steps of calcium chloride ⁄ SDS ⁄ enzyme DNA extraction
method.
A rapid DNA extraction method from wetland soils J. Li et al.
628 Letters in Applied Microbiology 52, 626–633 ª 2011 The Society for Applied Microbiology
ª 2011 The Authors
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72�C, and an additional 10-min cycle at 72�C. The 16S
rDNA PCR products were then separated by electro-
phoresis on a 1% agarose gel. The AmoA gene of AOB
was amplified using nested PCR. The first round of the
nested PCR amplification from 2 ll of extracted soil
DNA template was conducted in a total volume of 50 ll
by using 4Æ0 ll of 2Æ5 · 10)3 mol l)1 dNTP, 1Æ0 ll of
1Æ0 · 10)9 mol l)1 A189 (5¢-GGN GAC TGG GAC TTC
TGG-3¢) (see Table 2), 1Æ0 ll of 1Æ0 · 10)9 mol l)1
amoA-2R (5¢-CCC CTC KGS AAA GCC TTC TTC-3¢)(see Table 2), 5Æ0 ll of 10 · buffer (Promega) and 0Æ4 ll
of 5 U ll)1 Taq under the following conditions: 5 min at
94�C, 30 cycles of 40 s at 94�C, 40 s at 55�C, 40 s at
72�C, and an additional 10-min cycle at 72�C. The second
round of the nested PCR amplification from 2 ll of
extracted soil DNA template was conducted in a total vol-
ume of 50 ll using 4Æ0 ll of 2Æ5 · 10)3 mol l)1 dNTP,
1Æ0 ll of 1Æ0 · 10)9 mol l)1 amoA-1F (5¢-GGG GTT TCT
ACT GGT GGT-3¢) (see Table 2) 1Æ0 ll of 1Æ0 ·10)9 mol l)1 amoA-2R (5¢-CCC CTC KGS AAA GCC
TTC TTC-3¢) (see Table 2), 5Æ0 ll of 10 · buffer (Pro-
mega) and 0Æ4 ll of 5 U ll)1 Taq under the following
conditions: 5 min at 94�C, 30 cycles of 20 s at 94�C, 20 s
at 55�C, 20 s at 72�C, and an additional 10-min cycle at
72�C. The AmoA gene of AOA was PCR amplified from
2 ll of extracted soil DNA template in a total volume of
50 ll using 8Æ0 ll of 2Æ5 · 10)3 mol l)1 dNTP, 1Æ0 ll of
1Æ0 · 10)9 mol l)1 A19F (5¢-ATG GTC TGG CTW AGA
CG-3¢) (see Table 2), 1Æ0 ll of 1Æ0 · 10)9 mol l)1 A643R
(5¢-TCC CAC TTW GAC CAR GCG GCC ATC CA-3¢)(see Table 2), 5Æ0 ll of 10 · buffer (Promega) and 0Æ4 ll
of 5 U ll)1 Taq under the following conditions: 3 min at
95�C, 35 cycles of 30 s at 94�C, 30 s at 55�C, 1 min at
72�C, and an additional 10-min cycle at 72�C.
Cloning and sequencing
PCR products of the AmoA gene from AOB were purified
using a DNA purification kit (AxyPrep Biosciences,
Hangzhou, China) according to the manufacturers’ recom-
mendations, ligated into pMD-19T and then transformed
into chemically competent Escherichia coli DH-5a (pro-
vided by the biochemistry laboratory of Inner Mongolia
University, Huhhot, China). Clones were randomly
selected for further analysis. Plasmid DNA was isolated
from individual clones and sequenced by Invitrogen
(Shanghai, China) using M13 forward and reverse primers.
Phylogenetic analysis of AmoA
Gene sequences from AOB were edited, and the vector
sequences were deleted using the CLC Sequence Viewer
5 (http://www.clcbio.com). All sequences were analysed
using megaBlast (http://blast.ncbi.nlm.nih.gov/Blast.cgi?
PROGRAM=blastn&BLAST_PROGRAMS=megaBlast&
PAGE_TYPE=BlastSearch&SHOW_DEFAULTS=on&LINK_
LOC=blasthome) to select the closest reference sequences,
all amoA nucleotide sequences were aligned using
Clustal X software, and an N-J tree (Jukes-Cantor
correction) was constructed using mega software
(Tamura et al. 2007). The bootstrap value was 1000 and
the model was selected using the Kimura-2 parameter.
AmoA gene sequence accession numbers
The sequences identified in this study were submitted to
GenBank under accession numbers HM481179–HM481197.
Results
Comparison of the three soil DNA extraction methods
DNA was extracted from four soil samples using three
methods (see the Materials and methods) (Fig. 3). The
two methods devised in our laboratory do not contain
EDTA in the DNA extraction buffer and use a humic-
substance-removal solution and calcium chloride solution
to remove these substances before cell lysis. The glass
bead ⁄ calcium chloride ⁄ SDS DNA extraction method
obtains DNA that is about 23 kb in length, and the
procedure can be completed within approximately two
hours. In comparison with the calcium chloride ⁄ SDS ⁄enzyme DNA extraction method, which needs 4 h (Li
et al. 2010), this method is faster. The glass bead ⁄ calcium
Table 2 List of PCR primers
Name Sequence References Primer synthesis by
27F 5¢-AGA GTT TGA TCM TGG CTC AG-3¢ Martin-Laurent et al. (2001) Invitrogen
1492R 5¢-TAC GGH TAC CTT GTT ACG ACT T-3¢ Martin-Laurent et al. (2001) Invitrogen
amoA-1F 5¢-GGG GTT TCT ACT GGT GGT-3¢ Horz et al. (2004) Invitrogen
amoA-2R 5¢-CCC CTC KGS AAA GCC TTC TTC-3¢ Horz et al. (2004) Invitrogen
A189 5¢- GGN GAC TGG GAC TTC TGG-3¢ Horz et al. (2004) Invitrogen
A19F 5¢-ATG GTC TGG CTW AGA CG-3¢ Leininger et al. (2006) Invitrogen
A643R 5¢- TCC CAC TTW GAC CAR GCG GCC ATC CA-3¢ Treusch et al. (2005) Invitrogen
J. Li et al. A rapid DNA extraction method from wetland soils
ª 2011 The Authors
Letters in Applied Microbiology 52, 626–633 ª 2011 The Society for Applied Microbiology 629
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chloride ⁄ SDS DNA extraction method saves time and
can be used for PCR amplification (Fig. 4) such as that of
16S rDNA and especially for functional genes (amoA
gene).
Characterization of the new DNA extraction method
The calcium chloride ⁄ SDS ⁄ enzyme DNA extraction
method (Li et al. 2010) was efficient in removing humic
substances using the humic-substance-removal solution
combined with the calcium chloride solution, which can
combine with humic substances (Yuan et al. 2000; Davis
et al. 2002; Zhou et al. 2005). These processes are per-
formed only in the first two steps (see the Materials and
methods). As the subsequent steps include lysozyme treat-
ment and heat treatment, they can lead to the release of
humic substances from incompletely degraded animal and
plant cells. For some soils, the humic substances released
during the following steps under lysozyme and heating
treatment cannot be removed. The sensitivity of PCR for
DNA extracted from environmental samples is less than
that for purified genomic DNA. This reduction could be
attributed to humic substances or other interfering com-
pounds present in the soil or sediments (Tsai and Olson
1992). Thus, the calcium chloride ⁄ SDS ⁄ enzyme DNA
extraction method could only be used to amplify 16S
rDNA in all soils and the amoA gene from some of the
soils in this study. Thus, the question remains: how to
remove humic substances from incompletely degraded
animal and plant cells? Larger glass beads were chosen to
disperse the cells from the soil particles, allowing most
dead animal and plant cells to release the humic sub-
stances into the humic-substance-removal solution and
calcium chloride solution in the first two steps. Therefore,
the humic substances are fully removed, and DNA
obtained by the glass bead ⁄ calcium ⁄ chloride ⁄ SDS DNA
extraction method can be used to amplify functional
genes.
(a) (b)
2000 bp
M111222333444111222333444Round 2 Round 1 4 3 2 1 M
1000 bp750 bp500 bp250 bp100 bp
2000 bp1000 bp750 bp500 bp250 bp100 bp
Figure 4 Gel electrophoresis of ammonia-oxidizing bacteria microbial genomic amoA and AOA microbial genomic gene fragment amplification
from four different soils by glass bead ⁄ calcium chloride ⁄ SDS method.
Glass Bead-Calcium Chloride-SDS method
Ultra CleanSoil DNAIsolation
Kit
CalciumChloride-SDS
-EnzymaticMethod4 4 4 3 3 3 2 2 2 1 1 1 M
4 3 2 1 4 3 2 1
23130 bp9416 bp6557 bp4362 bp2322 bp2027 bp
564 bp
Figure 3 Gel electrophoresis of microbial genomic DNA (three dupli-
cates) from four different soils by three methods.
Table 3 Results of PCR amplification of 16S
rDNA, amoA gene fragments from ammonia-
oxidizing bacteria (AOB) and ammonia-
oxidizing archaea (AOA) carried out with the
UltraClean� Soil DNA Isolation Kit, calcium
chloride ⁄ SDS ⁄ enzymatic and glass beads ⁄calcium chloride ⁄ SDS method
Gene
fragment Primer pair
Glass
bead ⁄ calcium
chloride ⁄ SDS
method
Calcium
chloride ⁄ SDS ⁄enzymatic
method
UltraClean�soil DNA
isolation kit
16S rDNA 27F ⁄ 1492R ++++ ++++ ++++
AOB amoA A189 ⁄ 2Rw + ) )1F ⁄ 2Rww ++++ ++ )
AOA amoA A19F ⁄ A643R ++++ ) )
The single star represents round 1 of nested PCR, and the double star represents round 2 of nested
PCR. ++++ means that PCR product of the target gene fragment can be obtained from four
different soils by one of the three DNA extraction methods. +++ represents only three different
soils, ++ only two difference soils, + only one soil, ) represents no PCR product of the target gene
fragment can be obtained from four different soils by any one of the DNA extraction methods.
A rapid DNA extraction method from wetland soils J. Li et al.
630 Letters in Applied Microbiology 52, 626–633 ª 2011 The Society for Applied Microbiology
ª 2011 The Authors
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PCR amplification of 16S rDNA and the amoA gene
The results of PCR amplification of 16S rDNA and amoA
are presented in Table 3. The DNA obtained by the three
DNA extraction methods from the four soils was used as a
template to amplify 16S rDNA (Fig. not shown). The spec-
ificity of the different primer combinations was tested, and
the primer combination consisting of amoA-1F and amoA-
2R provided the most reliable performance in these studies
(Rotthauwe et al. 1997). The AmoA gene was amplified
GU931351
clone-A-4|HM481182
clone-A-3|HM481181
clone-A-5|HM481183
clone-A-1|HM481179
clone-A-2|HM481180
GU225888
clone-C-6|HM481191
EU515194
FJ853362
clone-B-2|HM481185
clone-B-3|HM481186
clone-B-1|HM481184
HM113507
GQ143593
clone-D-2|HM481194
GU931355
EU625025
GU931352
clone-B-5|HM481187
FJ890584
Nitrosospira-sp.LT2MFa|AY189145
clone-C-2|HM481188
clone-C-7|HM481192
FJ447346
Nitrosospira-multiformis|DQ228454
AF239880
clone-C-4|HM481190
clone-C-3|HM481189
Nitrosospira-sp.40KI|AJ298687
clone-D-1|HM481193
clone-D-4|HM481196
EU625184
clone-D-5|HM481197
clone-D-3|HM481195
AY249690
AB474979
Nitrosomonas-marina|AF272405
Nitrosomonas-oligotropha|AF272406
Nitrosomonas-ureae|AF272403
Nitrosomonas-eutropha|AJ298713
100
52100
8999
100
63
5459
72
99
9199
99
97
65
91
87
6687
6364
84
66
61
82
65100
8459
0·05
Cluster 1
Cluster 2
Cluster 3
Figure 5 Phylogenetic tree based on amoA partial sequences was conducted using MEGA ver. 4Æ0 (Tamura, Dudley, Nei and Kumar 2007). Boot-
strap values >50% are shown at each node. Numbers at each branch points indicate the percentage supported by bootstrap based on 1000 repli-
cates. Bar indicates 0Æ05 substitution per nucleotide.
J. Li et al. A rapid DNA extraction method from wetland soils
ª 2011 The Authors
Letters in Applied Microbiology 52, 626–633 ª 2011 The Society for Applied Microbiology 631
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using nested PCR because of low abundance of AOB in
our soil samples (Horz et al. 2004). Aliquots of the first
round of PCR products were used as the templates for the
second round of PCR (see the part of Materials and meth-
ods). The primer pairs selected were A189 ⁄ amo-2R and
amo-1F ⁄ amoA-2R for the first and second rounds of
nested PCR, respectively. The other primer pairs (Junier
et al. 2010) were not tested in this study. The PCR product
from the amoA gene of AOB was 491 bp. AmoA of AOB
was amplified from only one of the four soil samples in
the first round of nested PCR with the glass bead ⁄ cal-
cium ⁄ chloride- ⁄ SDS DNA extraction method (Fig. 4a).
However, the target bands were obtained from all four soil
samples in the second round of nested PCR (Fig. 4a).
AOB were not detected in soil samples W3 or W4 by the
calcium chloride ⁄ SDS ⁄ enzyme DNA extraction method.
The abundance and the composition of the indigenous
bacterial community are dependent on the DNA recovery
method used (Martin-Laurent et al. 2001), as clearly dem-
onstrated by our results. The amoA gene of AOA could be
amplified by general PCR from all soils using the primer
pairs A19F ⁄ A643R (Treusch et al. 2005; Leininger et al.
2006) (Fig. 4b). This finding may indirectly show that the
richness of AOA is higher than that of AOB. AmoA gene
copies from Crenarchaeota (Archaea) are up to 3000-fold
more abundant than bacterial amoA genes (Leininger et al.
2006). AOA amoA genes are more abundant, often as
much as 80 times moreso than AOB amoA genes (Caffrey
et al. 2007). Our results are consistent with the results of
these previous studies.
Phylogenetic relationships
Four clone libraries of the amoA gene were constructed
from the W1, W2, W3 and W4 soil samples. Five ran-
domly selected clones were sequenced. A phylogenetic tree
based on partial amoA sequences was constructed using
mega ver. 4.0 (Tamura, Dudley, Nei, and Kumar 2007). In
this study, 19 clones were obtained from the four soils:
clones A-1 to A-5 belong to the W1 soil sample, clones B-1
to B-3 and B-5 belong to the W2 soil sample, clones C-2
to C-4, C-6 and C-7 belong to the W3 soil sample and
clones D-1 to D-5 belong to the W4 soil sample. These
clones received the accession numbers HM481179–
HM481197 from GenBank, respectively (Fig. 5).
The amoA sequences of AOB were divided into three
clusters that were related to Nitrosospira. Nitrosomonas was
not detected in these soil samples. Cluster 1, a Nitrosospir-
a-like group, included five W1 clones, four W2 clones, one
W3 clone and one W4 clone. Cluster 2 included two W3
clones. Cluster 3 included two W3 clones and four W4
clones. The AmoA gene sequences indicated that Nitroso-
spira of AOB may be the main nitrifiers in these four
different soils. Our results are consistent with the findings
of Mohamed et al. (2010).
Conclusion
This study succeeded in establishing a fast soil DNA
extraction protocol that can be applied to various envi-
ronmental sources that are rich in humic acid content. In
particular, the glass bead ⁄ calcium chloride ⁄ SDS method
provides a rapid new approach for studying the diversity
of AOB and ammonia-oxidizing archaea (AOA) in wet-
land and grassland soils.
Acknowledgements
This work was financially supported by the Key Project of
National Programs for Fundamental Research and Devel-
opment (2009CB125909). We thank Dr Alexander Buy-
antuyev for scientific paper writing classes, who is
teaching in success Sino-US for Conservation, Energy and
Sustainability Science. We thank our parents for the sup-
port and understanding these years.
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