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Chromosomal distribution patterns of the (AC)10
microsatellite and other repetitive sequences, and their use in chromosome rearrangement analysis of Avena species
Journal: Genome
Manuscript ID gen-2016-0146.R2
Manuscript Type: Article
Date Submitted by the Author: 30-Sep-2016
Complete List of Authors: Fominaya, Araceli; Universidad de Alcalá de Henares, Biomedicina y Biotecnología Loarce, Yolanda; Universidad de Alcala de Henares, Biomedicina y Biotecnología Montes, Alexander; Universidad de Alcalá de Henares, Biomedicina y Biotecnología Ferrer, Esther; Universidad de Alcalá de Henares, Biomedicina y Biotecnología
Keyword: Avena, chromosome structure, fluorescence in situ hybridization (FISH), repetitive DNA, microsatellite
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Chromosomal distribution patterns of the (AC)10 microsatellite and other
repetitive sequences, and their use in chromosome rearrangement
analysis of Avena species
Araceli Fominaya1, Yolanda Loarce, Alexander Montes, and Esther Ferrer.
Department of Biomedicine and Biotechnology, University of Alcalá, Alcalá de Henares,
Spain.
Complete address: Department of Biomedicine and Biotechnology, University of Alcalá,
Campus Universitario, Ctra. Madrid-Barcelona Km 33,600, 28871 Alcalá de Henares, Madrid,
Spain.
Corresponding author1: Araceli Fominaya; [email protected]
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Abstract
Fluorescence in situ hybridization (FISH) was used to determine the physical location of
the (AC)10 microsatellite in metaphase chromosomes of six diploid species (AA or CC
genomes), two tetraploid species (AACC genome), and five cultivars of two hexaploid
species (AACCDD genome) of the genus Avena, a genus in which genomic relationships
remain obscure. A preferential distribution of the (AC)10 microsatellite in the
pericentromeric and interstitial regions was seen for both the A- and D-genome
chromosomes, while in C-genome chromosomes the majority of signals were located
in the pericentromeric heterochromatic regions. New large chromosome
rearrangements were detected in two polyploid species: an intergenomic translocation
involving chromosomes 17AL and 21DS in A. sativa cv. Araceli, and another involving
chromosomes 4CL and 21DS in all the analyzed cultivars of A. byzantina. The latter
4CL-21DS intergenomic translocation differentiates clearly between A. sativa and A.
byzantina. Searches for common hybridization patterns on the chromosomes of
different species revealed chromosome 10A of A. magna and 21D of hexaploid oats to
be very similar in terms of the distribution of 45S and Am1 sequences. This suggests a
common origin for these chromosomes and supports a CCDD rather than an AACC
genomic designation for this species.
Keywords: Avena, chromosome structure, fluorescence in situ hybridization (FISH),
repetitive DNA.
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Introduction
The genus Avena contains approximately 30 species, two of which are important crop
species: Avena sativa L. and A. byzantina C. Koch. These species are also described as
homotypic subspecies (Rodionova et al. 1994; Diederichsen 2008). A. strigosa Schreb
is also cultivated in some areas, and is an important resource of resistance for
economically important diseases of oats such as cereal cyst nematode (caused by
Heterodera avenae Woll) and crown rust (caused by Puccinia coronata) (Loskutov and
Rines 2011; Rines et al. 2007). Many wild Avena species are also of economic interest
given their possession of genes potentially useful in crop improvement (Loskutov and
Rines 2011). Research into the differentiation of chromosome structure may provide
important information for the management of useful Avena genes via interspecific
hybridization.
Avena species can be divided into diploid, tetraploid and hexaploid groups with
a base chromosome number of seven. Diploid species have either an A or C genome,
tetraploids have either A, B or A, C genomes, and hexaploids have three genomes i.e.,
A, C and D. A-genome diploid species have five minor genomes - As, Al, Ad, Ap and Ac -
whereas C genome diploids have two minor genomes - Cv and Cp (Thomas 1992;
Loskutov and Rines 2011). Information on genome structure differences among related
species has been provided by C-banding (Fominaya et al. 1988a, 1988b; Linares et al.
1992; Jellen et al. 1993a, 1993b; Shelukhina et al. 2007; Shelukhina et al. 2008a,
2008b; Badaeva et al. 2011; Chaffin et al. 2016), genomic in situ hybridization (GISH)
(Chen and Armstrong, 1994; Jellen et al. 1994; Leggett and Markhand, 1995; Katsiotis
et al. 1996), and fluorescence in situ hybridization (FISH) of homologous repetitive
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sequences (Fominaya et al. 1995; Linares et al. 1996, 1998; Irigoyen et al. 2001; Sanz
et al. 2010; Luo et al. 2014, 2015).
The cytogenetic positions of specific repetitive sequences have been useful in
revealing the structural evolution of chromosomes in Avena species. For example,
information on the relative locations of ribosomal 45S and 5S DNA in diploid and
polyploid species has produced evidence regarding the structural evolution of the
chromosomes carrying these sequences (Linares et al. 1996; Badaeva et al. 2010, 2011;
Tomás et al. 2016), while nucleotide similarity among diploid and polyploid rDNA
copies has revealed some of their phylogenetic and genomic relationships (Peng et al.
2010). A small number of satellites, such as As120a in A. strigosa, and Am1 in A.
murphyi, have also been useful in revealing chromosome structure. As120a is
dispersed on the chromosomes of the A genome (Linares et al. 1998) while obvious
signals of Am1 repeats have been detected on those of the C genome (Fominaya et al.
1995). Other tandem repeats appear in more restricted locations in pericentromeric
positions. For example, CCS1 Avena-700 appears all around the centromeric regions
(Tomás et al. 2016) whereas A336 (isolated from chromosome 18D) appears in the
centromeric regions of A- and D-genome chromosomes (Luo et al. 2015). Low copy
genes represented by families of resistance gene analogues (Sanz et al. 2012), or which
code for endosperm proteins (Fominaya et al. 2016), have also been located on
specific chromosomes of diploid and hexaploid species, even allowing for the
identification of certain homeologous regions in hexaploids. However, the above
findings are insufficient to clarify the complex homology relationships within Avena.
New sequences with chromosome distributions that give further clues in this respect
are much needed.
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Microsatellites, or simple sequence repeats (SSRs), are tandemly repeated sets
of a few base pairs (1-6) that can vary extensively in terms of the number of times they
are repeated. They form a large part of non-coding regions, but are also found in
transcribed regions (see a review by Kalia et al. 2011). Their repeated nature has
facilitated in situ hybridization studies, and many papers report differences in their
density, distribution and composition (Pinto et al. 2003; Oliveira et al. 2006; Fuentes et
al. 2009; Cuadrado et al. 2008; Cuadrado and Jouve, 2010; Molnár et al. 2011;
Carmona et al. 2013; Kejnovský et al. 2013; Han et al. 2015). In oats, SSRs have been
used in: (i) the construction of genetic maps (Pal et al. 2002; Jannink and Gardner
2005; Becher 2007; Wight et al. 2010; Oliver et al. 2010, 2011a, 2011b; Song et al.
2015), (ii) to examine the association of microsatellites with other repetitive elements
(Li et al. 2000), (iii) in population genetics studies and genotyping analyses (He and
Bjørnstad 2012), (iv) to identify relationships among oat species (Li et al. 2000; 2009),
and (v) to determine the transferability of A. sativa SSR to A. strigosa germplasm (Da-
Silva et al. 2011). However, no report discusses the use of FISH to determine the
distribution of any microsatellite on the Avena chromosomes.
Since the (AC)10 motif has been described as common in oats (Li et al. 2000; Pal
et al. 2002; Becher 2007; He and Bjørnstad 2012), diploid and polyploid species of
Avena were subjected to (AC)10-FISH to reveal the overall distribution of this repetitive
element in their chromosomes. The resulting patterns were compared in order to
detect homology among the examined species. Repetitive sequences such As120a and
Am1, in combination with 45S and 5S rDNA sequences, were also used to identify
chromosomes. Karyotypes for the different Avena species, including all the above
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sequences, were analyzed, and differences in the chromosome structure of polyploid
species examined.
Material and Methods
Plant materials
Table 1 shows the Avena species used in the present study. These include wild diploid
and tetraploid forms, as well as several cultivars of two hexaploid species (A. sativa
and A. byzantina). These were kindly provided by different germplasm resource
centres.
Mitotic chromosome preparation
Mitotic chromosomes were prepared as described in earlier work (Fominaya et al.
1995) with some modifications. Briefly, seeds of all the examined species/cultivars
were germinated on moistened filter paper for 48 h at 25o C. To synchronize cell
division and accumulate metaphases, the germinated seed were then exposed to a
temperature of 4o C for 72 h followed by 24 h at 25o C. Oat root tips were excised and
placed in ice-cold water for 24 h and fixed for at least a further 24 h in ethanol-acetic
acid (3:1). They were then kept in that mixture at -20o C until use. Chromosomes were
prepared using enzymatically (cellulose, peptinase) digested root tips prior to
squashing the meristematic cells in a drop of 60% acetic acid on a clean microscope
slide. After removal of the coverslips by freezing, the slides were air dried for further
processing.
DNA probes
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The microsatellite sequence (AC)10, with biotin-11-dUTP incorporated at both ends,
was produced (automated synthesis) by TIB MOLBIOL. Four repetitive DNA probes
were used for chromosome identification: (1) pAs120a, a satellite DNA sequence
specific to the oat A genome, containing an insert of 114 bp isolated from A. strigosa
(Linares et al. 1998); (2) pAm1, a satellite DNA sequence specific to the oat C genome,
containing an insert of 464 bp isolated from A. murphyi (Solano et al. 1992); (3) p45S, a
ribosomal probe derived from A. strigosa (Sanz et al. 2010), and (4) pTa794, a satellite
DNA sequence containing a 410 bp 5S rDNA gene and the intergenic spacer isolated
from T. aestivum (Gerlach and Dyer 1980). These clones were amplified and labelled by
PCR with digoxigenin11-dUTP or biotin16-dUTP (Roche). These repetitive probes were
used in FISH both simultaneously and sequentially after hybridization with the (AC)10
probe.
Fluorescence in situ hybridization
Chromosome preparations were treated with RNase, fixed with 4% (w/v)
paraformaldehyde, and dehydrated in an ethanol series before air drying, according to
Fominaya et al. (1995). Between the RNAse and paraformaldehyde treatments, the
preparations were washed in 2xSSC (saline-sodium citrate). Hybridization mixture (30
µl) containing 50% (v/v) formamide, 2 x SSC, 10% (w/v) sodium dodecyl sulphate (SDS),
10% (w/v) dextran sulphate, 50 µg/ml of Escherichia coli DNA, and 2.6 pmol of the
microsatellite (AC)10 sequence, was denatured for 15 min at 75o C and then applied to
each chromosome preparation. The preparations were then covered with plastic
coverslips and the chromosomes and probe denatured at 75o C for 7 min using a
programmable thermal controller (PT-100, M.J. Research Inc.). Hybridization was
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performed at 37o C in a humidity chamber overnight. Post-hybridization washing was
performed in 4 x SSC/0.2% Tween-20, agitating for 10 min at room temperature (RT).
The detection of biotin was performed at 37o C in a humidity chamber, incubating the
chromosome preparations for 1 h in streptavidin-Cy3 (Sigma) in 5% (W/V) BSA. The
preparations were then rinsed for 10 min in 4 x SSC/0.2% Tween-20 at RT. 4´,6´-
diamidine-2´-phenylindole dihydrochloride (DAPI) was used as a counterstain. The
preparations were the mounted in Vectashield (Vector). Reprobing FISH and probe
detection were performed as described in Linares et al. (1998).
Images were obtained using a Zeiss Axiophot microscope equipped with a
fluorescent lamp and appropriate filters, and recorded using a CCD camera (Nikon DS).
The images were pseudo-coloured in blue (chromosomes) and pink or green (signals),
merged, and optimized for brightness and contrast using Adobe Photoshop.
Results
(AC)10-FISH signal patterns in diploid species
The karyotypes of the present diploid species were previously described in studies
involving conventional staining (Rajhathy and Thomas 1974) and C-banding (Fominaya
et al. 1988a, 1988b; Badaeva et al. 2005; Shelukhina et al. 2008a, 2008b). FISH has
previously been used to reveal the number and physical locations of 45S and 5S
ribosomal loci in the chromosomes of the examined diploid species (Linares et al.
1996; Shelukhina et al. 2008a; Tomás et al. 2016). The nomenclature used in the above
papers is followed here to designate both the A-genome and C-genome chromosomes.
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To identify individual chromosomes labelled with (AC)10 repeats, the slides were
reprobed with 45S and 5S ribosomal sequences.
When the (AC)10 oligonucleotide probe was hybridized with metaphases of the
diploid species, two signals patterns were clearly identified (Fig. 1). One showed
discrete, well-defined bands in the pericentromeric and interstitial regions of the A-
genome chromosomes (Fig. 1a, 1c, 1e, 1g, and 1m); the other showed very strong
bands in the pericentromeric regions and dispersed signals throughout the arms of the
C-genome diploid species chromosomes (Fig. 1i, 1k, and 1m).
In A. strigosa, the (AC)10 probe produced signal patterns in each chromosome
(Fig. 1a and 1m) except for chromosome 2. Distinct signal patterns were observed in
the pericentromeric regions of each chromosome, with chromosomes 1, 3, and 4
showing very strong signals. In chromosomes 1 and 4 they covered a large region
around the centromeres. Chromosome 1 also showed a strong signal in the distal
region of the long arm. Chromosomes 6 and 7 showed only weak signals in the
pericentromeric region, while 5 and 6 showed very strong signals in the interstitial
region of the long arms. Chromosomes 2 and 3 were identifiable by their 45S and 5S
rDNA signals (Fig. 1b and 1m).
For A. damascena, all chromosomes possessed obvious (AC)10 signals except for
3 and 5 (Fig. 1c and 1m). Chromosomes 1, 4, and 6 showed signals on both sides of the
centromeric region, while 2 and 7 showed signals on only one side. 45S and 5S rDNA
was used to identify chromosomes 3 and 6 (Fig. 1d and 1m).
For A. longiglumis, the (AC)10 probe produced signals in the interstitial region of
the long arms as well as close to the pericentromeric region in all chromosomes except
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3 and 6 (Fig. 1e and 1m). Chromosomes 1 and 3 showed signals with the 45S and 5S
rDNA probes (1f and 1m). For A. canariensis, the (AC)10 probe produced strong signals
in the interstitial regions of all chromosomes except number 6 (Fig. 1g and 1m). One
strong signal on chromosome 1 was produced near the 45S rDNA loci (Fig. 1h and 1m).
In contrast, no signals were detected near the 45S rDNA loci of chromosome 3.
Chromosome 7 also returned a strong signal at the end of the short arm. On the
whole, signals in A. longiglumis and A. canariensis were less intense than those
observed in the other two A-genome species.
A. eriantha (Fig. 1i and 1m) and A. ventricosa (Fig. 1k and 1m) showed strong
similarity in their signal patterns. The (AC)10 probe produced clear, bright signals in the
pericentromeric regions of all the chromosomes of these C-genome species. Scattered
signals were evident in most of the chromosomes, especially on the short arms of
chromosomes 6 and 7.
(AC)10-FISH signal patterns in tetraploid species
Sequential FISH analysis was performed on the AACC-tetraploid species A. magna and
A. murphyi, first using the (AC)10 probe on mitotic metaphase chromosomes (Fig. 2a
and 2c), and then using the 45S and Am1 probes simultaneously on the same cells
(Figs. 2b and 2d). This allowed the chromosome of these two species to be assigned to
either the A or C genome. The chromosomes were numbered 1-14 according to the
nomenclature of Linares et al. (1996). This was based on the chromosome arm ratio,
relative length, and FISH patterns for the four repetitive probes. The resulting
karyotype was taken as the reference karyotype (Fig. 2e).
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In both A. magna and A. murphyi, the A-genome chromosomes showed
discrete (AC)10 signals in the interstitial regions, whereas the C-genome chromosomes
showed strong (AC)10 signals in the pericentromeric regions. Comparison of the A-
genome chromosomes of these tetraploid species revealed differences in the number
of signals and in the intensity of some of these. In the karyotype of A. magna more
discrete signals were seen than in that of A. murphyi. Several chromosomes, such as
6A, 11A and 13A, each showed two signals of similar intensity. In contrast, no A-
genome chromosome of the A. murphyi showed more than one signal, and the
intensity of these signals was highly variable across chromosomes. Very conspicuous
signals were recorded in the short arm of chromosomes 12A and 13A. It should be
noted that the signal patterns of the A-genome chromosomes of these two species are
more similar in their intensity to those of A. longiglumis and A. canariensis than to
those of A. strigosa and A. damascena. Very strong signals were seen on all C-genome
chromosomes of both species, covering a large area of the pericentromeric regions.
Clear signals were also seen at the ends of the long arms of chromosomes 2C and 4C of
A. magna, and on those of 2C and 6C of A. murphyi. These chromosomes also showed
strong Am1 signals (related to heterochromatin) in similar positions.
(AC)10-FISH signal patterns in hexaploid species
The usefulness of the (AC)10 probe in karyotyping the two AACCDD hexaploid species
of cultivated oats - i.e., three cultivars of A. sativa (Figs. 3a, 3d, and Fig. 4) and two of
A. byzantina - was tested (Fig. 4). Both simultaneous and sequential FISH was then
performed using on the same cells, As120a or Am1, in combination with a ribosomal
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probe (45S or 5S) (Fig. 3b, 3e, 3f and 4). This allowed all the chromosomes to be
assigned to the A, C or D genome. The nomenclature used for the reference hexaploid
karyotype (Fig. 4) was that proposed by Sanz et al. (2010) who used the same
repetitive probes as in the present work.
Most of both the A- and D-genome chromosomes showed discrete signals of
(AC)10 sequences in the interstitial regions. The signals in the C-genome
chromosomes, however, covered a large region either side of the centromeres. For all
the cultivars analyzed, the (AC)10 hybridization signals were less intense on the D-
genome chromosomes than the A-genome chromosomes (Fig. 4). Indeed, the
hybridization of this chromosome marker differentiated every chromosome of each
cultivar (Fig. 4). The chromosomes of all five cultivars were further examined in an
attempt to identify diagnostic signals common to them all. In A. sativa, chromosomes
8A, 13A, 15A, 16A and 19A showed either interstitial, pericentromeric or terminal
signals common to all three of its cultivars, although differences in intensity were
evident (e.g., in the interstitial signal on chromosome 8A, and in the pericentromeric
signal on chromosome 15A). Chromosomes 11A, 15A and 19A of A. byzantina showed
identical signal patterns in both the cultivars analyzed. Moreover, the signals seen on
chromosomes 15A and 19A were the same in both A. byzantina and A. sativa.
The C-genome chromosomes showed strong (AC)10 signals in the
pericentromeric region of every chromosome (Fig. 4). In addition, distinct signals were
observed in the interstitial and terminal regions of the long arms of some
chromosomes, with some intra- and interspecific variation observed. Common signals
in the interstitial regions of the long arms appeared on chromosome 5C of all five
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analyzed cultivars, and more faintly on chromosome 4C of the A. sativa cultivars. The
(AC)10–FISH distribution pattern on the D-genome chromosomes was similar to that
observed on the A-genome chromosomes (Fig. 4), although the signals were less
intense. Among the three A. sativa cultivars, similar patterns were found on
chromosomes 10D, 14D, and 20D. The two A. byzantina cultivars showed similar
patterns for chromosomes 10D, 20D and 21D. A comparison of the A. sativa and A.
byzantina signal patterns revealed strong similarities between chromosomes 10D and
20D. By contrast, an important difference between the two species affected
chromosome 21D. A. byzantina showed a conspicuous signal on the short arm of this
chromosome which was absent in A. sativa. Other minor differences affecting other
chromosomes were also seen between the two species; for example, hybridization
signals were terminally located on chromosome 9D of A. byzantina but interstitially
located on that of A. sativa.
Discussion
The (AC)10 regions in the diploid and polyploid species of Avena mainly appeared as
sharp, thin bands in the pericentromeric and interstitial positions of the A- and D-
genome chromosomes. These regions have been characterized as euchromatin
(Fominaya et al. 1988a; Linares et al. 1992; Jellen et al. 1993a, 1993b; Shelukhina et al.
2008b; Badaeva et al. 2011). This agrees with observations in barley and Rumex
acetosa, in which the distribution of (AC)10-FISH signals and euchromatic regions
appear closely correlated (Cuadrado et al. 2008; Kejnovský et al. 2013). This suggests
that blocks of this microsatellite lie within regions containing single copy sequences. In
the present work, however, the location of the (AC)10 hybridization signals in the C-
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genome chromosomes was very similar to the C-banding of the centromeric and
pericentromeric regions. This indicates that (AC)10 is either a component of these
regions or of similar sequences of C-banded heterochromatin (Fominaya et al. 1988b;
Linares et al. 1992; Jellen et al. 1993a, 1993b; Shelukhina et al. 2008b; Badaeva et al.
2011). However, no strict correlation was seen between (AC)10 and the C-bands in
terminal positions. Thus, the terminal C-bands of 3C and 5C in hexaploid species must
be composed of sequences others than (AC)10.
The somatic chromosomes of A. sativa and A. byzantina have been
characterized by C-banding (Linares et al. 1992; Jellen et al. 1993a, 1993b; Badaeva et
al. 2011). FISH and GISH techniques have also been used to make detailed descriptions
of them (Chen and Armstrong 1994; Jellen et al. 1994; Leggett and Markhand 1995;
Linares et al. 1998; Linares et al. 2000, 2001; Sanz et al. 2010). However, these studies
failed to detect chromosome polymorphism among cultivars, except where large
chromosome arrangements had occurred (Jellen and Beard 2000; Sanz et al. 2010).
The existance of intra-cultivar variation detected could raise doubts on the validity of
using information provided by SSR-FISH to make inferences on inter-species
differentiation. Only highly conserved signal patterns in chromosomes of different
cultivars of one species should be used for detect interspecific polymorphism. In the
present study, contrasted interspecific polymorphisms were observed fairly frequently
(Fig. 4). The (AC)10 pattern on chromosome 21D, with a strong signal in the terminal
region of the short arm in the cultivars of A. byzantina but absent from those of A.
sativa, differentiates these species. In addition, this chromosome showed a unique
(AC)10 pattern in the non-terminal region of the short arm of A. sativa cv. Araceli.
Moreover, changes were evident in the position of several hybridization signals in A.
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byzantina cv. Kanota compared to A. sativa. These seem to follow a pattern in which
the Kanota signals lie in a terminal position, whereas those of the others cultivars are
in interstitial positions (e.g., on the long arm of chromosome 17A and both arms of 8A
and 9D chromosomes). The polymorphisms observed could have been caused by
changes in the number of copies of the microsatellite (e.g., via amplifications or
deletions) during the differentiation of the species and less likely in that affecting
cultivars (Kalia et al. 2011). However, determining the chromosome distribution of
SSRs in different cultivars allowed to evaluate the cytogenetic diversity within each
Avena species. This is especially significant in species where chromosome
rearrangements have played an important role in the differentiation within and
between species (Jellen and Beard 2000; Sanz et al. 2010).
The existance of translocations and inversions between parents used in genetic
mapping have complicated the obtention of a robust consensus genetic map in oats
(Oliver et al. 2013; Chaffin et al. 2016). Detection of changes in signal position of SSRs
in those parental lines, migth contribute to establish a more complete assignments of
linkage groups to specific chromosomes and explain some uneven distribution of
markers along the linkage groups. The present work using (AC)10-FISH provides
evidence of new large translocations. A. sativa cv. Araceli carries a translocation
involving the long arm of chromosome 17A and the short arm of 21D (Figs. 3e, 3f, and
4). This translocation was detected using C-genome specific sequences (Am1) and
ribosomal 45S, but the location of the (AC)10 hybridization signals helped to outline the
interchange (Figs. 4 and 5). This cultivar has not taken part of any mapping population
but if a similar translocation affected to a parental line the consensus linkage groups
merged 18 and merged 28 would be likely altered (Chaffin et al. 2016; Yan et al. 2016).
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A second intergenomic translocation detected by (AC)10-FISH affected the satellite of
chromosome 21D and the long arm of chromosome 4C in the two cultivars of A.
byzantina (Fig. 6). This 4CL-21DS translocation might explain the lack of markers and
the short genetic distances observed for chromosome 21D in the map for the cross
between A. sativa cv. Ogle and A. byzantina cv. Kanota (Oliver et al. 2013). Thus, It is
noteworthy that (AC)10–FISH allowed the detection of the 4CL-21DS intergenomic
translocation, but the detection of other putative chromosome rearrangements
between these two cultivars is no less interesting. For example, that likely affecting
chromosome 9D might explain the reduced genetic distance observed in the
corresponding linkage group KO17 (Oliver et al. 2013).
Sanz et al. (2010) classified the different types of intergenomic translocations
seen in the cultivars of A. byzantina and A. sativa into three classes: (i) common
translocations, present in homologous chromosomes of all closely related hexaploid
oat species; (ii) species-specific translocations involving certain chromosomes,
exclusive to each hexaploid species; and (iii) cultivar-specific, exclusive to some
cultivars of crop oats. Since the new intergenomic translocation 17AL-21DS (Fig. 5) is
seen only in A. sativa cv. Araceli, its origin must lie within the breeding programme for
this cultivar, and should therefore be identified as cultivar-specific. In contrast, the
intergenomic translocation 4CL-21DS detected in A. byzantina should be identified as
species-specific.
Based on molecular cytogenetic studies, a genomic designation of CCDD has
been suggested for the tetraploid species involved in the formation of the AACCDD-
genome hexaploid species (see Fominaya et al. 2006). The change was proposed since
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the species thought to be the donor of the A genome, A. strigosa, had repetitive
sequences that failed to hybridize with the chromosomes of AACC tetraploids, but did
hybridize with those of the AACCDD hexaploids (Linares et al. 1998). In the present
work, the similar degree of (AC)10 signalling among chromosomes of the reference A
genome of A. magna and the D-genome chromosomes of the hexaploid species may
indicate close proximity between these genomes, even though no individual
chromosome maintained an (AC)10 pattern in common with those seen in the
tetraploid and hexaploid species. This was likely due to the many rearrangements that
have occurred during the evolution of the genus (Chen and Armstrong 1994; Jellen et
al. 1994; Leggett and Markhand 1995; Linares et al. 1998; Linares et al. 2000, 2001;
Sanz et al. 2010). However, the hybridization patterns observed for the 45S and Am1
repetitive sequences on chromosome 10A of the tetraploid species A. magna (Fig. 2)
were identical to those on chromosome 21D of the hexaploid oat species, reinforcing
the idea that a close relationship exists between the A genome of the reference A.
magna genome and the D genome of the reference A. sativa genome (Fig. 4). In
contrast, no similar hybridization patterns were observed in the other tetraploid
species A. murphyi. The above observation regarding A. magna is supported by
comparisons of molecular linkage maps (Oliver et al. 2011b). For example, a region
containing several crown rust resistant QTLs, which are anchored to chromosome 9D
of hexaploid oats (Jackson et al. 2009), was found in the genetic map constructed from
an A. magna recombinant inbred line population. One A. magna SNP has been mapped
to chromosome 20D of the physically-anchored consensus map of hexaploid oats
(Oliver et al. 2013).
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Indirect observations argue against the involvement of A. strigosa in the
formation of the ancestral tetraploid AACC. Molecular studies have revealed the
dissimilarity between the A. strigosa genome and the A genome of tetraploid oat
species (Linares et al. 1998; Peng et al. 2010; Oliver et al. 2011a). Chromosome pairing
studies of the hybrid between a synthetic allotetraploid (involving A. strigosa and A.
clauda) and A. magna showed highly irregular pairing, indicating that the two A.
magna genomes differed considerably from those of the diploid species involved in the
tetraploid (Ladizinsky 2012). Genotypic by sequencing (GBS) has recently returned a
large SNP dataset for numerous accessions belonging to species with different
genomes and levels of ploidy. Comparing genetic distances between in silico
tetraploids (obtained by combining information for the A. strigosa SNPs and two C-
genome species) and A. magna, Chew et al. (2016) raised serious doubts about the
involvement of A. strigosa in the ancestral tetraploid AACC. If it is not involved, the D-
genome donor of the hexaploid species must have been the tetraploid species A.
magna or a closely related species. Thus, the hexaploid forms might came into
existence via the allopolyploid convergence of species with the CCDD genome and
others with the A genome. In addition, Chew et al. (2016) came to the conclusion that
both the tetraploidization and hexaploidization events may have occurred in
northwest Africa, followed by the radiation of the hexaploid oats to their current
worldwide distribution. The results of the above authors' analyses revealed strong
genetic similarity between the in silico and extant hexaploids, suggesting an ancestral
hexaploid oat participated in the creation of different hexaploid Avena species. More
recently, Yan et al. (2016) extent substantially the Avena GBS studies and present
strong evidences to justify the CCDD genome identity of the tetraploids species A.
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insularis, A. magna (A. maroccana) and A. murphyi. These authors examine the genetic
similarities of fifty-one possible combinations of diploids with tetraploids using GBS
markers and demonstrate that all in silico hexaploid comprised of CCDD genome
tetraploid plus A-genome diploids clustered closely with the extant hexaploids. The
closest in silico matches to the extant hexaploids included the CCDD tetraploids plus A.
longiglumis which led to the authors to suggest a possible role of these species in the
formation of the hexaploids. The similarity of intensity in (AC)10-FISH signals of the A.
longiglumis accession studied here and the A (D) genome of the tetraploids would not
agree with that proposal. However, more A. longiglumis accessions should be studied
study to clarify this.
In conclusion, (AC)10-FISH patterns have allowed differenciate all the
chromosomes of the Avena species analyzed. This has resulted in more complete and
specific karyotypes than the obtained using C-banding and FISH with the so far
available repetitive probes. However, it will be interesting to extent this study to
several accessions of diploid and tetraploid species for quantifying the magnitude of of
intra- and interspecific variation. Moreover, the analysis carried out on hexaploid
species shows the utility of this SSR to identify new translocations undetected by the
other karyotyping methods. Increasing the number of microsatellites used in FISH-
based studies on oats might provide valuable information on the structure of the
genomes and chromosomes of this genus, as well as help explain the incongruities of
genetic oat maps. The economical and easy applicability of this technique compared to
conventional FISH involving cloned sequences will facilitate this task.
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Acknowledgements
The authors thank the Ministerio de Ciencia e Innovación of Spain (AGL210-17042) and the
Universidad de Alcalá (UAH GC2014-002 and UAH CCG2014/EXP-068) for their support of
this work.
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Figure 1.- FISH microphotographs showing the distribution of repetitive sequences on
metaphase chromosomes of diploid species. A. strigosa (a, and b), A. damascena (c,
and d), A. longiglumis (e, and f), A. canariensis (g, and h), A. eriantha (i, and j), and A.
ventricosa (k, and l), afther DAPI staining and in situ hybridization with biotin-labelled
probes (pink) or digoxigenin-labelled probes (green): (a), (c), (e), (g), (i) and (k)
fluorescence in situ hybridization (FISH) with (AC)10 probe; (b), (d), (f), (h), (j), and (l)
simultaneous FISH with p45S and p5S probes. (m) Karyotypes of each diploid species
analysed showing a single chromosome of each homologous group chosen from the
metaphases in a-l. Note that chromosomes carried signals from p45S and p5S are
shown in duplicate on karyotypes at the right side of chromosomes with (AC)10 signals.
Scale bar = 10 µm.
Figure 2.- FISH performed on mitotic metaphase of tetraploid species A. magna (a, and
b), and A. murphyi (c, and d). (a) FISH of biotin-labelled (AC)10 (pink) probe. (b) The
same cell as in a after simultaneous FISH with the biotin-labelled pAm1 (pink) and
digoxigenin-labelled p45S (green) probes. (c) FISH of biotin-labelled (AC)10 (pink) probe.
(d) The same cell as in c after simultaneous FISH with the biotin-labelled pAm1 (pink)
and digoxigenin-labelled p45S (green) probes. (e) Karyotypes showing a single
chromosome of each homologous group chosen from the metaphases in a and c. The
reference karyotypes was made from the metaphases b and d for A. magna and A.
murphyi, respectively. They are based on the hybridization patterns of Am1 (pink) and
45S (green) sequences and following the nomenclature of Linares et al. (1996). Scale
bar = 10 µm.
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Figure 3.- FISH performed on metaphase chromosomes of hexaploid species A. sativa
cvs. Ogle (a) and Araceli (d) using (AC)10 probe (pink). Chromosomes are
counterstained with DAPI. (b) The same cell as in a after double FISH with pAs120a
(green) and p45S (pink) probes. (c) The same cell as in a after rehybridizing with pAm1
(green) and p5S (pink) probes. (e) The same cell as in d after double FISH with pAs120a
(green) and p5S (pink) probes. (f) The same cell as d after rehybridizing with pAm1
(pink) and p45S (green) probes. In e, arrows indicate the translocated chromosome
pair 21D; asterisks indicate the translocated chromosome pair 17A. Scale bar = 10 µm.
Figure 4.- (AC)10-FISH (pink) karyotypes from each of three cultivars of hexaploid
species A. sativa and two cultivars of hexaploid species A. byzantina. Each
chromosome probed with (AC)10 was identified by the hybridization patterns of
repetitive sequences after simultaneous and sequential FISH with pAs120a, pAm1,
p45S and p5S probes and reprobing of the same cell. According to Sanz et al. (2010),
the reference karyotype was based on the hybridization patterns of pAs120a (green),
p45S (pink) and p5S (pink) probes which identified the A-genome chromosomes; the
hybridization patterns of both pAm1 (green) and p5S (pink) wich identified the C-
genome chromosomes; and the hybridization patterns of pAm1 (green), p45S (pink)
and p5S (pink) probes which identified the D-genome chromosomes. Chromosomes of
reference karyotype were chosen from the same metaphase and corresponding to cv.
Ogle (Figs. 3 b, and 3c).
Figure 5.- Diagram showing the formation of a intergenomic translocation detected in
cv. Araceli compared to A. sativa cv. Ogle and affecting to chromosomes 17A and 21D.
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FISH signals using different probes are illustrated. In (a) probes pAs120a, pAm1 and
p45S. In (b) probe (AC)10.
Figure 6.- Diagram showing the formation of the intergenomic translocation in A.
byzantina (compared to A. sativa). (AC)10 signals are illustrated.
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Table 1. Avena species used in this study, including ploidy level, genomic composition,
accession numbers (or cultivar names) and provider.
Species Ploidy Genomic
composition
Accession Provider
A. strigosa Schreb 2x AsAs PI 258727 National Small Grains Collection, Betsville, USA.
A. damascena 2x AdAd CAV 0258 Plant Research Centre, Ottawa, Canada.
A. longiglumis Dur. 2x AlAl PI 367390 National Small Grains Collection, Betsville, USA.
A. canariensis Baum 2x AcAc WIR-292 N.I. Vavilov Research Institute, Russia.
A. eriantha 2x CpCp PI 657579 National Small Grains Collection, Betsville, USA.
A. ventricosa 2x CvCv PI 657338 National Small Grains Collection, Betsville, USA.
A. magna Murph et Terr 4x AACC PI 659402 National Small Grains Collection, Betsville, USA.
A. murphyi Ladiz. 4x AACC PI 657382 National Small Grains Collection, Betsville, USA.
A. sativa L. cv Ogle 6x AACCDD Plant Research Centre, Ottawa, Canada.
A. sativa L. cv Cobeña 6x AACCDD Cobeña National Institute of seeds, Madrid, Spain.
A. sativa L. cv Araceli 6x AACCDD Araceli National Institute of seeds, Madrid, Spain.
A. byzantina C Koch cv Culta 6x AACCDD WIR 5206 N.I. Vavilov Research Institute, Russia.
A. byzantina C Koch cv Kanota 6x AACCDD 2265 Plant Research Centre,Ottawa, Canada.
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17A 21D
A.sativa
cv Ogle
A.sativa
cv Araceli
17AL-21DS 21DS-17AL
a
17A 21D
A.sativa
cv Ogle
A.sativa
cv Araceli
b
120a
Dapi
45S Am1 (AC)
10
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