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Doubled Haploidy in Model and Recalcitrant Species

Original Research ARTICLE

Front. Plant Sci., 08 December 2014 | https://doi.org/10.3389/fpls.2014.00675

Cellular dynamics during early barley pollen embryogenesis revealed by time-lapse imaging

  • 1Department of Physiology and Cell Biology, Leibniz Institute of Plant Genetics and Crop Plant Research, Gatersleben, Germany
  • 2Department of National Gene Bank and Genetic Resources, Agriculture Research Center, Giza, Egypt

Plants display a remarkable capacity for cellular totipotency. An intriguing and useful example is that immature pollen cultured in vitro can pass through embryogenic development to form haploid or doubled haploid plants. However, a lack of understanding the initial mechanisms of pollen embryogenesis hampers the improvement and more effective and widespread employment of haploid technology in plant research and breeding. To investigate the cellular dynamics during the onset of pollen embryogenesis, we used time-lapse imaging along with transgenic barley expressing nuclear localized Green Fluorescent Protein. The results enabled us to identify nine distinct embryogenic and non-embryogenic types of pollen response to the culture conditions. Cell proliferation in embryogenic pollen normally started via a first symmetric mitosis (54.3% of pollen observed) and only rarely did so via asymmetric pollen mitosis I (4.3% of pollen observed). In the latter case, proliferation generally originated from the vegetative-like cell, albeit the division of the generative-like cell was observed in few types of pollen. Under the culture conditions used, fusion of cell nuclei was the only mechanism of genome duplication observed.

Introduction

The life cycle of higher plants involves the alteration of sporophytic and gametophytic generations. Whereas the sporophyte constitutes the plant in its apparent form, the female and male gametophytes are reduced in size and have become depending on the sporophyte.

Under natural conditions, spontaneous formation of haploid embryos and plants in angiosperms can arise from female gametophytic cells but not from male gametophytic cells (McKone and Halpern, 2003). However, male gametophytes (i.e., immature pollen) cultivated in vitro, can be induced to become embryogenic and form sporophyte-like haploid embryos and plants. Through spontaneous or artificially triggered genome duplication, doubled haploids can arise that themselves are genuine sporophytes.

The value of haploid technology in plant research and breeding lies in the fact that the founder cells of doubled haploids are products of meiosis, and resultant plants constitute pools of diverse recombinant, yet genetically fixed individuals. Their recombinant genome is fixed through homozygosity of the doubled haploid plants produced. The employment of haploid technology has become widely used in breeding programs of many crop species (Germanà, 2011).

Doubled haploids are also widely used in genetic studies, such as QTL, gene mapping and marker-trait association (Murovec and Bohanec, 2012). Genetic transformation of embryogenic pollen allows for the production of instantly true-breeding transgenic plants (Kumlehn et al., 2006; Eudes and Chugh, 2008; Chauhan and Khurana, 2011). A novel approach for haploid induction has recently been developed by the genetic engineering of the centromeric region (Ravi and Chan, 2010).

Although distinct pathways of pollen embryogenesis have been proposed (Sunderland and Evans, 1980; Hu and Kasha, 1999), recent evidence hints at the presence of multiple pathways within one culture (Hu and Kasha, 1999; Kasha et al., 2001). Maraschin et al. (2005), using time-lapse studies, identified three such pathways within immature barley pollen cultures.

Spontaneous genome doubling can result in completely fertile doubled haploids. In barley and wheat, spontaneous doubling frequencies between 18 and 85% have been observed, (Jähne and Lörz, 1995; Hu and Kasha, 1999). Several mechanisms for plant genome doubling have been proposed: (i) endoreduplication, (ii) nuclear fusion, (iii) endomitosis, and (iv) c-mitosis (Jensen, 1974; d'Amato, 1989; González-Melendi et al., 2005; Kasha, 2005; Seguí-Simarro and Nuez, 2008). However, none of the proposed genome doubling mechanisms has ever been observed in living cells.

Despite the great value of pollen embryogenesis, very little is known about the underlying cellular mechanisms. In vacuolated immature pollen, embryogenesis can be induced by various treatments both in vivo and in vitro (Touraev et al., 1997). Due to the high amenability to pollen embryogenesis, barley has become a model species to study this phenomenon in temperate cereal crop species (Sunderland et al., 1974; Kasha, 2007).

This present paper is the first to give a full account of the initial cellular dynamics in the pollen embryogenesis process until the formation of growing multicellular structures. The approach relies on multi-dimensional (4D) live-cell imaging of transgenic pollen expressing the Green Fluorescence Protein (GFP) gene with nuclear localization signal using a temporal resolution of 3 min.

Results

Generation of Transgenic Barley Expressing SV40-NLS:GFP

A total of 71 primary transgenic (T0) plants were generated by co-culture of embryogenic pollen with Agrobacterium strain LBA4404/pSB1. This strain harbored a GFP gene fused to the Simian virus SV40 nuclear localization signal under the control of the maize UBIQUITIN1 promoter with first intron (Figure 1C). Ploidy and presence of the selectable marker gene HPT were checked by flow cytometry and PCR, respectively. Most regenerants were haploid (43.7%) or diploid (47.9%), while the remaining ones were tetra- (5.6%) or mixoploid (2.8%). Five spontaneously doubled haploid and 20 colchicine-treated plants were grown to maturity. Three colchicine-treated haploids did not set grain. The remaining 22 fertile doubled haploids contained the HPT selectable marker gene. Confocal Laser Scanning Microscopy (CLSM) analysis showed only a single line to accumulate appreciable amounts of GFP in its nuclei. This line was used to produce embryogenic pollen cultures from which 27 T1 regenerants were generated including 7 tetraploid, 5 triploid, and 15 diploid plants. Sexual progeny of 7 randomly selected diploid T1-lines were grown. To confirm integration of HPT and NLS:GFP, four T2-families were selected at random for DNA gel blot analysis (Figure 1A) and PCR (Figure 1B). Primer pairs and specific probe were selected to cover most functional parts of the T-DNA (Figure 1C). All plants contained both HPT and NLS:GFP (Figure 1B) and showed an identical T-DNA integration pattern (Figure 1A), confirming that the doubled haploid T1-lines were homozygous for the transgene. Nuclear localization of GFP in T0 transgenic plants was confirmed by CLSM (Figures 1D–F).

FIGURE 1
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Figure 1. Characterization of the doubled haploid SV40-NLS:GFP transgenic barley line displaying nucleus-specific accumulation of GFP. Randomly chosen T2-siblings (four per family) derived from four T1-plants (P11, P15, P21, P25) were analyzed for genomic T-DNA integration and transgene zygosity. (A) DNA gel blot analysis of HindIII-digested genomic DNA hybridized with an HPT-specific probe. The two bands seen per lane indicate genomic integration of two T-DNA copies. (B) PCR analysis with primer pairs specific for the HPT (upper band) and the GFP (lower band) genes. (C) Map of T-DNA with primer pairs and hybridization probe positions indicated. WT1, 2 and 3, wild type individuals of cv. “Igri”; LB, left border; ZmUBI1-int, maize UBIQUITIN1 promoter with first intron; HPT, hygromycin B phosphotransferase protein coding region; t35S, CaMV 35S gene terminator; tNOS, NOPALINE SYNTHASE gene terminator; eGFP, synthetic S65T green fluorescent protein coding region; NLS, SV40 Simian virus 40 nuclear localization signal; RB, right border. (D) Leaf tissue with GFP in the nuclei of guard and other epidermis cells. Chlorophyll autofluorescence shown in red. (E) GFP accumulation in the nuclei of a root tip. (F) GFP accumulation in nuclei of immature pollen after the second embryogenic pollen mitosis. Bar = 30 μm.

Live-Cell Imaging of Cultured Pollen Over Time

In eight separate experiments, the development of a total of 71 immature pollen was followed over a time span of up to 15 days. Of these pollen, 70 were (uni-nucleate) microspores and a single one bi-cellular. With a diameter of about 40 μm, the bi-cellular pollen was distinctly larger than the microspores, which were about 30 μm. Over time, the bi-nucleate pollen increased in size without showing any mitotic activity and started to accumulate starch (Supplementary Figures 1C,D) before dying on the second day of culture (Supplementary Figures 1E,F; see Supplementary movie 1). The small generative-like nucleus of this bi-cellular pollen remained spherical (Supplementary Figures 1A–D; see Supplementary movie 1). The remaining 70 immature pollen that were at the late microspore stage at the onset of observation showed various developmental patterns with regards to pollen mitosis I and to their final fate, so that nine different developmental pathways could be discerned (Table 1). The majority of pollen (61.1%; types I, II, and III) started the development with a symmetrical cell division, whereas types IV, V, and VI had in common to undergo asymmetric pollen mitosis I. In contrast to types I–VI, no mitotic activity was observed in types VII–IX.

TABLE 1
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Table 1. Types of pollen development as observed in live-cell imaging experiments during the initial 2 weeks of culture under conditions supportive for pollen embryogenesis.

The nucleus of type I pollen (54.3% overall) contained a single nucleolus (Figure 2A). Prior to mitosis, the nucleus migrated from a strictly peripheral to a more central position and began moving rapidly while increasing in size, with cytoplasmic strands radiating from the nuclear periphery (Figures 2B,C) (Supplementary movie 2). After symmetric first mitosis (Figure 2D), the two resulting daughter cells remained mitotically active. Despite numerous rounds of synchronized mitoses (Figures 2F,G), the pollen did temporarily not increase in size; during this period of time, the cytoplasmic proportion of the individual cells increased while the vacuoles accordingly dwindled in size (Figures 2A–H). This type of pollen did not show any detectable starch accumulation. Type I development represents the major pathway of pollen embryogenesis under the conditions used in this study.

FIGURE 2
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Figure 2. Time-lapse of type I development (embryogenic pollen) shown by synchronously acquired DIC and fluorescence images. (A) Uni-nucleate pollen (microspore) with nucleus close to pollen aperture. (B,C) The nucleus has migrated away from the pollen periphery and cytoplasmic strands are formed. The blurred fluorescence signal indicates the break-down of the nuclear envelope prior to mitosis. (D) Newly formed cell wall (DIC) and a pair of daughter nuclei (GFP) after mitosis. (E) Appearance of cytoplasmic strands indicating imminent second mitosis. (F,G) Newly formed intermediate cell wall (DIC) separates four cells (GFP) contained within the pollen envelope. (H) Additional cycles of mitosis create a multicellular structure. CS, cytoplasmic strand; CW, cell wall; N, nucleus; n, nucleolus; PA, pollen aperture. Bar = 20 μm.

Type II showed an early difference to type I development (2.9% overall; see Supplementary movie 3). Here the nucleus prior to mitosis did not move to a central position and remained opposite of the pollen aperture. Furthermore, the cytoplasm remained largely peripheral and did not form cytoplasmic strands upon mitosis (Supplementary Figures 2B–F). Despite the formation of two nuclei of equal size and shape, a cell wall remained absent as judged by Differential Interference Contrast (DIC) microscopy (Supplementary Figures 2B–G) an unopposed movement of the two daughter nuclei throughout the cytoplasm was observed (Supplementary Figures 2B,C). Later this pollen started to deposit starch from day 3 onwards (Supplementary Figure 2D) and shortly died as indicated by cell shrinkage and the loss of GFP signal in the nucleus (Supplementary Figures 2F–H).

In type III development (4.3% overall; see Supplementary movie 4), the nucleus remained opposite of the pollen aperture at the time of symmetric cell division (Figures 3A,B). In contrast to type II development, the two daughter nuclei moved to the center of the cell (Figure 3C) with cytoplasmic strands radiating from their surface (Figure 3D), but showed no further mitotic activity. Type III pollen gradually accumulated starch without increasing in size over time (Figures 3D–H). In contrast to type II, type III pollen remained viable for more than 2 weeks, i.e., during the entire time of observation as shown by GFP signal in their nuclei (Figure 3H).

FIGURE 3
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Figure 3. Type III development over time (non-embryogenic pollen) shown by synchronously acquired DIC and fluorescence images. After the initial symmetric division, the pollen remains bi-cellular, showing no further cell divisions but gradually accumulating starch while remaining viable throughout the observation period (14 days). (A) Uni-nucleate pollen with large vacuole and the nucleus residing opposite to the pollen aperture. (B,C) Symmetrical cell division. (D,E) Cell with two similar sized daughter nuclei and large vacuoles. (F–H) Increase of the cytoplasmic volume and starch accumulation. N, Nucleus; n, nucleolus; PA, pollen aperture; V, vacuole. Bar = 20 μm.

Of the pollen whose first mitosis was asymmetrical (types IV, V, and VI), only type IV followed an embryogenic pathway (4.3% overall; Figure 4, Supplementary movie 5). Type IV pollen significantly increased in size and cytoplasmic strands appeared prior to the first mitosis (Figure 4C). The nucleus, however, remained residing opposite of the pollen aperture (Figures 4A–D). The first mitosis was followed by an asymmetric cell division resulting in a large vegetative-like cell and a much smaller generative-like cell (Figure 4E). Whereas the latter remained inactive and opposite of the pollen aperture, the former showed active movements and the appearance of cytoplasmic strands that preceded a further mitosis (Figures 4F,G) resulting in two similar daughter nuclei (Figure 4H). Further synchronized divisions produced a multicellular structure that showed no sign of amyloplast formation and starch accumulation (Figures 4I–L). Compared to type I development, cell proliferation in type IV was delayed by several days. Over the time of observation, the generative-like cell degenerated in most cases; and although it remained viable in some cases, (Figures 4E–L).

FIGURE 4
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Figure 4. Time-lapse of type IV development (embryogenic pollen) shown by synchronously acquired DIC and fluorescence images. (A) Uni-nucleate pollen with large vacuole and thin layer of peripheral cytoplasm. (B) Uni-nucleate pollen increases in size. (C) Cytoplasmic strands appear prior to pollen mitosis I. (D–F) Large spherical vegetative-like nucleus and smaller ellipsoid generative-like nucleus after asymmetric division. (G–L) Synchronized mitotic events originate from the vegetative-like cell; note that the generative-like cell does not show any mitotic activity. CS, cytoplasmic strand; Gn, generative-like nucleus; PA, pollen aperture; V, vacuole; Vn, vegetative-like nucleus. Bar = 20 μm.

Developmental type V (2.9% overall) was very similar to developmental type II in terms of cell size, thin-layered cytoplasm, starch accumulation and ultimate cell degeneration, except for the fact that here the first pollen mitosis was asymmetric.

Type VI pollen (7.1% overall; Supplementary movie 6) was characterized by forming a larger than usual, spherical, generative-like cell (Figures 5A,B) that was capable of undergoing two successive symmetric and synchronized divisions (Figures 5C–H). The nuclei produced by the mitotic activity of the generative-like cell remained within the original boundaries as defined after the first asymmetric division (Figures 5B–H). Of particular note is the small size of nuclei originating from the generative-like cell as compared to those derived from the vegetative-like cell (Figures 5F–H).

FIGURE 5
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Figure 5. Time-lapse of type VI (non-embryogenic pollen). Development shown by synchronously acquired DIC and fluorescence images of GFP. Green arrows indicate vegetative-like nucleus and its daughter nuclei. White arrows indicate generative-like nucleus and its daughter nuclei (A,B). Asymmetric division resulted in a large vegetative-like and a small generative-like cell. (C,D) First mitosis of the vegetative nucleus; the spherical generative-like nucleus remains fixed opposite to the pollen aperture. (E,F) First mitosis of the generative-like cell. (G,H) Second symmetric and synchronized mitosis of the nuclei originated from the generative-like cell. Note that the nuclei derived from the generative-like nucleus are much smaller than those derived from the vegetative-like nucleus. Gn, generative-like nucleus; PA, pollen aperture; V, vacuole; Vn, vegetative-like nucleus. Bar = 20 μm.

Of the pollen that failed to undergo mitosis, developmental type VII (1.4% overall; Supplementary movie 7) showed a remarkable increase in nuclear size over time (Supplementary Figures 3C–E). The pollen itself, however, did not expand and neither did form amyloplasts for starch accumulation. Cytoplasmic strands were not visible and the nucleus eventually disintegrated into multiple micronuclei (Supplementary Figures 3G–H). Despite fragmentation of the nucleus (on end of day 2 × of culture), the cell was still alive when observation ended.

Developmental type VIII (2.8% overall) pollen became exceptionally large (diameter 60 μm) but did not show any particular signs of development before dying within the first 2–3 days of culture.

Immature pollen of developmental type IX (20.0% overall) did not show any developmental changes during the time of observation; this pollen died sooner or later.

Spontaneous Genome Doubling During Pollen Embryogenesis

Live-cell imaging revealed that nuclear fusion is a common process observed in more than 40% of the multicellular pollen and occurring throughout pollen embryogenesis (Figures 68; Supplementary movie 8) rather than being limited to a certain stage. Notably, polyploid products of multiple consecutive nuclear fusions were also frequently observed (Figures 6B,G,O, 8). In some extreme cases, such processes resulted in large tube-shaped nuclei (Figure 8E).

FIGURE 6
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Figure 6. Spontaneous genome doubling during pollen embryogenesis shown by synchronously acquired DIC and fluorescence images of GFP. (A) Two haploid nuclei after the first pollen mitosis. (B,C) Nuclei adhere to one another and eventually fuse to form a diploid nucleus. (D–F) Second mitosis producing a pair of diploid sister nuclei. (G–I) The two diploid nuclei adhere to one another and fuse to a tetraploid nucleus. (J,K) Third mitosis resulted in two tetraploid nuclei. (L–O) Fourth synchronized mitosis resulting in four tetraploid nuclei, two of which later fuse to a single octaploid nucleus. CW, cell wall; n, haploid genome. Bar = 20 μm.

More detailed information on the nuclear fusion process was obtained from electron microscopy studies. Nuclear fusion starts with a close alignment of two nuclei (Figures 7A, 8A–C), followed by fusion of the nuclear envelopes (Figures 7B,C). In some cases, cell wall was partially present at the site of the assumed nuclear fusion (Figures 7D,E). Nuclear fusion may account for the often occurring irregular shape of nuclei and the recurrent presence of cytoplasmic pockets within the nucleoplasm (Figures 7E,G). An intriguing observation was that of an elongated nucleus featuring a median invagination and unusual distribution of heterochromatin, which appeared to be absent from a narrow median band in the plane of the median constriction (Figure 7G).

FIGURE 7
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Figure 7. TEM micrographs of nuclear fusion at different stages of pollen embryogenesis. (A) Induced immature pollen during first day of culture with two nuclei in close vicinity. (B,C) Detail of (A) shows the absence of cell wall and the close proximity of the nuclear envelopes. Arrow indicates region of assumed membrane fusion. (D) Multicellular structure 7 days after initiation of pollen embryogenesis. (E) Two nuclei after fusion with incomplete cell wall formation near the site of nuclear fusion. (F) Multicellular structure 7 days after initiation of pollen embryogenesis. (G) Elongated nucleus with clear median constriction (arrowheads), cytoplasmic pockets and a narrow median band marking the site of fusion. CyP, cytoplasmic pocket; CW, cell wall; N, nucleus; n, nucleolus; V, vacuole. Bar = 20 μm.

FIGURE 8
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Figure 8. Variable ploidy level in a multicellular structure shown by synchronously acquired DIC and fluorescence images. (A,C,E) GFP. (B,D) DIC. (A,B) Haploid multicellular structure with cell walls and spherical nuclei. (C,D) Chimeric polyploid multicellular structure with irregular shaped nuclei often not separated by cell wall. Note the difference of nuclear sizes. Arrows refer to a possible triple fusion. (E) Multicellular structure with highly polyploid nuclei next to small spherical, likely haploid, nuclei. Bar = A,B,D–E = 10 μm; C = 1 μm.

The information gained from live-cell imaging and electron microscopy studies suggests that mitosis is not always followed by cell wall formation (Figures 68). Failure of cell wall formation can occur at any stage of pollen embryogenesis and so can nuclear fusion. This would explain the chimeric ploidy level often observed within individual multicellular structures (Figure 8E).

Discussion

Only a few previous studies have followed the embryogenic development of isolated pollen in culture, e.g., Indrianto et al. (2001) in wheat as well as Kumlehn and Lörz (1999) and Maraschin et al. (2005) in barley. In these pioneering observations, time intervals of several hours or days were used, thus allowing only for a sketchy outline of the process. We here present a detailed monitoring of pollen embryogenesis from the vacuolated immature uni-nucleate barley pollen (the pre-mitotic microspore) until the formation of growing multicellular structures using a temporal resolution of only 3 min. The use of transgenic barley expressing a GFP-construct with nuclear-localization signal further greatly improved the accuracy of observations.

Pollen Development in vitro

Populations of immature pollen in vitro always show variability in the developmental state of individuals. Reasons for this heterogeneity include that pollen is typically isolated using a number of different spikes at once, that the florets of a spike show a developmental gradient along the rachis, and that nutrient provision and signal perception even of each individual pollen grain may well depend on the particular position within the anther. In addition, pollen of hybrid plants (that are typically used to produce doubled haploids in breeding practice) or of outbreeding species are genetically diverse due to meiotic segregation. In our experiments, 58.6% of pollen analyzed eventually formed multicellular structures (Table 1). This agrees with observations by Maraschin et al. (2005) who identified only three developmental pathways; whereas the present study enabled us to distinguish nine different types of pollen response to the given culture conditions (Table 1).

Indrianto et al. (2001) in wheat and Maraschin et al. (2005) in barley showed that multicellular structures were only obtained from immature pollen that were enlarged after induction treatment. In the present study, however, the type I pollen grains that underwent cell proliferation most efficiently did temporarily not increase in size during the initiation of cell proliferation. A very similar scenario has been shown in cultures of isolated wheat zygotes (Kumlehn et al., 1999; Figure 2I), where an initial series of cell divisions result in a step-wise decrease in cell size without substantial enlargement of the whole proembryo prior to the onset of its exponential growth based upon proliferation of small, cytoplasmic rich cells that are characteristic for the proper of globular zygotic embryos. Likewise, the formation and ongoing proliferation of small cells is indicative of the embryogenic nature of type I pollen. Type IV pollen did temporarily increase in size, which was associated with a remarkable delay in first mitosis. The resultant vegetative-like cell then behaved like the microspore cell of type I pollen in undergoing embryogenic development involving a successive decrease in cell size over an initial series of mitoses followed by continued proliferation of small cells. By contrast, other pollen grains that increased in size shortly after inductive treatment (types II, V, and VIII) eventually accumulated starch in amyloplasts and did not show continuous cell proliferation. Since amyloplasts are not unambiguously recognized by differential interference contrast microscopy used in this study, we have investigated samples of comparable developmental stages of barley pollen embryogenesis also by transmission electron microscopy and thereby proved that these structures are indeed starch-containing granules (data not shown).

Successful induction of embryogenesis in uni-nucleate pollen was usually associated with a first symmetric mitosis (92.7% of embryogenic pollen; type I) and only rarely with a first asymmetric mitosis (7.3% of embryogenic pollen; type IV). In contrast to pollen response type IV, both microspore daughter cells contributed to the cell proliferation following a first symmetric pollen mitosis (type I).

A comparison between regular pollen maturation and pollen embryogenesis is shown in Figure 9. The developmental pathways identified show three main routes based on the type of the first pollen mitosis (Figures 9H,L,U). In the most common route, first mitosis was symmetric and the two daughter cells proliferated synchronously to eventually form an embryo-like structure (Figures 9H–K). Starch was not detected in early stages, though some amyloplasts appeared later on (Figures 9J,K). In the less common second route, pollen firstly divided asymmetrically to produce generative and vegetative-like cells (Figure 9L). Depending on the fate of the generative-like cell, two sub-routes were identified. In the first sub-route, only the vegetative-like cell proliferated (Figures 9M–O) while the generative-like cell remained opposite to the cell aperture and often degenerated within the period of observation (Figures 9M–P). In the second sub-route both generative and vegetative-like cells underwent mitosis (Figures 9Q–S). In the third route, pollen failed to undergo first mitosis and in some case the nucleus was degenerated into small micronuclei (Figure 9U).

FIGURE 9
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Figure 9. Schematic model of main developmental routes of pollen during regular maturation and pollen embryogenesis. (A) premitotic microspore, (B) commencement of starch accumulation in premitotic microspore, (C) product of asymmetric pollen mitosis I, (D) bicellular pollen with the generative cell deliberated from the cell periphery, (E) formation of two sperm via pollen mitosis II, (F) germination of mature pollen, (G) premitotic microspore with emerging small vacuoles, (H) bicellular pollen after symmetric 1st pollen mitosis, (I) 4-celled pollen after two rounds of symmetric cell divisions, (J) multi-cellular pollen, (K) pollen releasing proliferating tissue, (L) bicellular pollen after asymmetric 1st pollen mitosis, (M) tri-cellular pollen after symmetric division of the vegetative-like cell, (N) 5-celled pollen including a non-divided generative-like cell and 4 cells derived from the vegetative-like cell, (O) multicellular pollen including a non-divided generative-like cell and multiple cells derived from the vegetative-like cell, (P) multicellular pollen releasing proliferating tissue, (Q) tri-cellular pollen after symmetric division of the vegetative-like cell, (R) 4-nucleate pollen after division of the generative-like nucleus, (S) 6-nucleate pollen including 4 nuclei derived from the generative-like nucleus, (T) no information is available about pollen fate after stage S, (U) failure of cell division in microspore is associated with formation of micronuclei. GC, generative/generative-like cell; Gn, generative/generative-like nucleus; Mn, micro nucleus; N, nucleus; SC, sperm cell; St, starch; V, vacuole; Vn, vegetative/vegetative-like nucleus.

Nuclear Fusion Leads to Genome Doubling

Spontaneous genome doubling during pollen embryogenesis can produce doubled haploid plants that, in contrast to haploids, show normal fertility.

Sunderland et al. (1974) proposed the fusion of mitotic nuclei as an explanation for genome duplication in embryogenic pollen grains of Datura. An alternative mechanism was published by Seguí-Simarro and Nuez (2008) who observed that karyokinesis is followed by a disrupted cytokinesis, which allows the daughter nuclei to fuse within the same cytoplasm. Lee and Chen (1987) and Kasha (2005) claimed the fusion of generative and vegetative nuclei in cultures of barley pollen after the degradation or incomplete assembly of the separating cell wall.

Our observations revealed that mitosis is not always followed by cytokinesis which allows mitotic daughter nuclei to fuse. Indeed, nuclear fusion turned out to be the only means of genome doubling in the cultures analyzed in the present study. It could occur at any time during pollen embryogenesis, which explains the chimeric ploidy status of individual multicellular structures (Figures 6, 8) and plants. González-Melendi et al. (2005) showed that when nuclei coexist within the same cytoplasm, their envelopes may fuse. However, the same authors also argued that the absence of cell wall is not sufficient to explain nuclear fusion. There are indeed many examples of stable multinucleate cells that occur naturally, e.g., bi-nucleate tapetal cells, coenocytic endosperm and the female gametophyte, or can be experimentally-induced (Risueño et al., 1968; Nishihama et al., 2001; Park and Twell, 2001; Olsen, 2004). Consequently, hitherto unknown factors must exist, that stimulate attachment and fusion of nuclear envelopes (Chen et al., 1984; González-Melendi et al., 2005; Seguí-Simarro and Nuez, 2007).

Fusion between vegetative and generative nuclei was never observed in the present study. Every asymmetric pollen mitosis I ended with a physical barrier between vegetative and generative-like cells, which effectively precluded their respective nuclei from fusing. The integrity of the separating cell wall is also supported by the observation that in cases where generative-like cells were able to undergo symmetric divisions, all daughter cells remained within the boundary of the original generative-like cell (Figure 5).

The high frequency of whole genome duplication events and resultant polyploid nuclei observed is not associated with a corresponding proportion of high polyploidy amongst the regenerants, as was shown for example in the present study by the flow-cytometric analysis of the gfp-transgenic plants generated via agroinoculation of embryogenic pollen cultures. It is well conceivable that a ploidy larger than twice the normal somatic value can lead to disadvantages in further embryogenic development and regeneration which effects selection in favor of viable individuals in the ploidy range between 1 and 4 n with a further preference of diploids. Also in the ploidy-chimeric structures frequently found in this study, the same selection principle may effect a preferential development of cells and tissue domains having a ploidy within this tolerable range.

Summary and Perspective

Pollen embryogenesis can be followed after symmetric or asymmetric mitosis. The appearance of starch granules or pollen expansion prior to or right after pollen mitosis I is associated with failure of pollen embryogenesis under the conditions used in this study. Under the culture conditions used, nuclear fusion was the only mechanism of genome doubling and could occur at any developmental stage during pollen embryogenesis, provided cell wall formation had failed entirely or locally. In the rare occasion of a generative-like cell showing mitotic activity, the nuclei remained significantly smaller than those of normal embryonic cells. This makes the contribution of these cells to embryogenesis highly doubtful. Because cultures of immature pollen are highly heterogenic, it was necessary to follow the fate of individual pollen, in order to unambiguously identify and validate those developmental types that truly account for pollen embryogenesis.

The descriptive information provided here will be a valuable source for the evaluation of pollen cultures used to produce doubled haploid plants. This will especially apply for the establishment and improvement of protocols for recalcitrant species (e.g., rye and oats) or genotypes that have so far been hardly amenable to pollen embryogenesis. The thorough characterization of two embryogenic pathways and their unambiguous discrimination from seven non-embryogenic types of response as was performed in the present study we also consider as a vital prerequisite for future transcriptomics and metabolomics approaches relying on the collection of individually selected pollen, which may help to cope with the unavoidable heterogeneity in pollen populations. Also, the findings presented here on the mechanism and temporal occurrence of whole genome duplication events are likely to have implications on the utilization of embryogenic pollen cultures in induced mutagenesis, genetic transformation and genome engineering approaches with regards to zygosity and chimerism of the genetic alterations obtained in doubled haploids. In addition, the novel technical opportunities provided by the experimental setup established and utilized in the present study may facilitate the elucidation of the still unknown molecular triggers of pollen embryogenesis by over-time observation of fluorescence-tagged subcellular structures or candidate proteins essentially involved in this process.

Methods

Genetic Transformation of Barley using Embryogenic Pollen Cultures

Barley transformation of the winter type cv. Igri using hygromycin as selective agent in the culture media was performed as previously described (Kumlehn et al., 2006). The hypervirulent A. tumefaciens strain LBA4404/pSB1 (Komari et al., 1996) carrying the binary vector pGH252n was used to inoculate embryogenic pollen. The binary vector was cloned followed standard procedures described in detail in the Supplementary materials and methods section, and its introduction into agrobacteria was performed by electroporation.

Molecular Analysis of Transgenic Plants

Genomic DNA prepared from leaf material (Pallotta et al., 2000) was analyzed by standard PCR using primers for the coding sequence of the HPT gene GH-HYG-F1 (5′-GATCGGACGATTGCGTCGCA-3′) and GH-HYG-R2 (5′-TATCGGCACTTTGCATCGGC-3′), or GFP GH-GFP-F1 (5′-GGTCACGAACTCCAGCAGGA-3′) and GH-GFP-R2 (5′-TACGGCAAGCTGACCCTGAA-3′). For DNA gel blot analysis, genomic DNA was digested with HindIII, separated in 0.8% (w/v) agarose gel (30 μg per lane) and blotted onto Hybond N+ membrane (Amersham, Braunschweig, Germany) by capillary transfer under alkaline conditions according to the manufacturer's instructions. Membranes were hybridized with DIG-labeled HPT according to the manufacturer's instructions (Roche, Mannheim, Germany). Hybridization and detection was performed according to the protocol for non-radioactive DNA gel blot experiments (Roche, Mannheim, Germany).

Analysis of Reporter Gene Expression using Confocal Laser Scanning Microscopy

Leaves, roots and pollen from T0 transgenic plants were analyzed for the presence of GFP with a Zeiss LSM 510 META CLSM (Carl Zeiss Microscopy GmbH, Jena, Germany) using a 488 nm laser line for excitation. GFP signals were detected with a 505–530 nm bandpass filter. Auto-fluorescence of chlorophyll was detected with a 650 nm long-pass filter.

Ploidy Analysis and Colchicine Treatment

Ploidy level of regenerants was assessed using a Ploidy Analyser PA I (Partec GmbH, Münster, Germany). Nuclei were stained with CyStain UV (Partec GmbH, Münster, Germany) according to the manufacturer's instructions. Haploid regenerants were treated with colchicine to induce genome doubling (Takamura and Miyajima, 1996). A detailed description is provided in the Supplementary materials and methods section.

Live-Cell Imaging

Live-cell imaging was performed as described by Daghma (2011). Cultures of transgenic immature pollen were observed over a period of up to 15 days. Pollen was subjected to inductive treatment involving incubation of dissected anthers in 0.4 M mannitol at 25°C for 1 day followed by 4°C for 1 day before isolation and culturing in SMB medium for 1 day at 25°C in the dark. The capture of images was started immediately after pollen had been transferred into KBP medium. GFP was excited with a 488 nm argon-krypton laser line. DIC images were acquired with a HeNe 633 laser line. Z-stacks of 9 images were taken every three min with a spacing of 1.5–4 μm depending on expansion of pollen during the development. Scanning of every Z-stack took 80 s. To reduce the risk of bleaching, laser intensity was kept below 4% emission. The developmental progress of a total of 71 individual immature pollen grains was analyzed in five separate experiments.

Transmission Electron Microscopy

For transmission electron microscopy, pollen was prepared using high pressure freezing and freeze substitution as described by Daghma et al. (2011).

Author Contributions

Diaa Eldin S. Daghma, Jochen Kumlehn, and Michael Melzer designed the research. Diaa Eldin S. Daghma and Goetz Hensel performed the experiments and analyzed the data. Twan Rutten contributed to time-lapse imaging. Diaa Eldin S. Daghma, Goetz Hensel, and Jochen Kumlehn wrote the manuscript.

Conflict of Interest Statement

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

We thank Monika Wiesner, Kirsten Hoffie, Ingrid Otto and Andrea Mueller for their highly skilled technical support. This work was supported by the Forschungszentrum Jülich GmbH (GABI FUTURE).

Supplementary Material

The Supplementary Material for this article can be found online at: http://www.frontiersin.org/journal/10.3389/fpls.2014.00675/abstract

References

Chauhan, H., and Khurana, P. (2011). Use of doubled haploid technology for development of stable drought tolerant bread wheat (Triticum aestivum L.) transgenics. Plant Biotechnol. J. 9, 408–417. doi: 10.1111/j.1467-7652.2010.00561.x

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Chen, C. C., Kasha, K. J., and Marsolais, A. (1984). Segmentation patterns and mechanisms of genome multiplication in cultured microspores of barley. Can. J. Genet. Cytol. 26, 475–483.

Google Scholar

d'Amato, F. (1989). Polyploidy in cell differentiation. Caryologia 42, 183–211.

Google Scholar

Daghma, D. S. (2011). Structural Changes During the Initiation of Pollen Embryogenesis in Barley. Ph.D. dissertation, University of Martin Luther, Halle Saale, German.

Daghma, D. S., Kumlehn, J., and Melzer, M. (2011). The use of cyanobacteria as filler in nitrocellulose capillaries improves ultrastructural preservation of immature barley pollen upon high pressure freezing. J. Micros. 244, 79–84. doi: 10.1111/j.1365-2818.2011.03509.x

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Eudes, F., and Chugh, A. (2008). Nanocarrier based plant transfection and transduction. WO 2008/148223 A1, Patent Application 25. Available online at: http://www.lens.org/lens/patent/WO_2008_148223_A1

Germanà, M. A. (2011). Gametic embryogenesis and haploid technology as valuable support to plant breeding. Plant Cell Rep. 30, 839–857. doi: 10.1007/s00299-011-1061-7

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

González-Melendi, P., Ramírez, C., Testillano, P. S., Kumlehn, J., and Risueño, M. C. (2005). Three-dimensional confocal and electron microscopy imaging define the dynamics and mechanisms of diploidisation at early stages of barley microspore-derived embryogenesis. Planta 222, 47–57. doi: 10.1007/s00425-005-1515-7

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Hu, T. C., and Kasha, K. J. (1999). A cytological study of pretreatments used to improve isolated microspore cultures of wheat (Triticum aestivum L.) cv. Chris. Genome 42, 432–441. doi: 10.1139/gen-42-3-432

CrossRef Full Text | Google Scholar

Indrianto, A., Barinova, I., Touraev, A., and Heberle-Bors, E. (2001). Tracking individual wheat microspores in vitro: identification of embryogenic microspores and body axis formation in the embryo. Planta 212, 163–174. doi: 10.1007/s004250000375

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Jähne, A., and Lörz, H. (1995). Cereal microspore culture. Plant Sci. 109, 1–12. doi: 10.1016/0168-9452(95)04149-O

CrossRef Full Text | Google Scholar

Jensen, C. J. (1974). “Chromosome doubling techniques in haploids,” in Haploids in Higher Plants: Advances and Potential, ed K. J. Kasha (Guelph, ON: University of Guelph), 153–190.

Kasha, K. J., Hu, T. C., Oro, R., Simion, E., and Shim, Y. S. (2001). Nuclear fusion leads to chromosome doubling during mannitol pretreatment of barley (Hordeum vulgare L.) microspores. J. Exp. Bot. 52, 1227–1238. doi: 10.1093/jexbot/52.359.1227

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Kasha, K. J. (2005). “Chromosome doubling and recovery of doubled haploid plants,” in Haploids in Crop Improvement II, eds C. E. Palmer, W. A. Keller, and K. J. Kasha (Berlin; Heidelberg: Springer-Verlag), 123–152. doi: 10.1007/3-540-26889-8_7

CrossRef Full Text

Kasha, K. J. (2007). “Barley,” in Transgenic Crops IV, Biotechnology in Agriculture and Forestry, Vol. 59, eds E.C. Pua and M. R. Davey (Berlin; Heidelberg; New York: Springer-Verlag), 129–150.

Komari, T., Hiei, Y., Saito, Y., Murai, N., and Kumashiro, T. (1996). Vectors carrying two separate T-DNAs for co-transformation of higher plants mediated by Agrobacterium tumefaciens and segregation of transformants free from selection markers. Plant J. 10, 165–174. doi: 10.1046/j.1365-313X.1996.10010165.x

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Kumlehn, J., and Lörz, H. (1999). “Monitoring sporophytic development of individual microspores of barley (Hordeum vulgare L.). In Anther and Pollen,” in Biology to Biotechnology, eds C. Clement, E. Pacini, and J.-C. Audran (Berlin; Heidelberg; New York: Springer), 183–190.

Kumlehn, J., Lörz, H., and Kranz, E. (1999). Monitoring individual development of isolated wheat zygotes: a novel approach to study early embryogenesis. Protoplasma 208, 156–162. doi: 10.1007/BF01279086

CrossRef Full Text | Google Scholar

Kumlehn, J., Serazetdinova, L., Hensel, G., Becker, D., and Lörz, H. (2006). Genetic transformation of barley (Hordeum vulgare L.) via infection of androgenetic pollen cultures with Agrobacterium tumefaciens. Plant Biotechnol. J. 4, 251–261. doi: 10.1111/j.1467-7652.2005.00178.x

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Lee, F., and Chen, C. (1987). Nuclear fusion in cultured microspores of barley. Plant Cell Rep. 6, 191–193. doi: 10.1007/BF00268476

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Maraschin, S. F., de Priester, W., Spaink, H. P., and Wang, M. (2005). Androgenic switch: an example of plant embryogenesis from the male gametophyte perspective. J. Exp. Bot. 56, 1711–1726. doi: 10.1093/jxb/eri190

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

McKone, M. J., and Halpern, S. L. (2003). The evolution of androgenesis. Am. Nat. 161, 641–656. doi: 10.1086/368291

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Murovec, J., and Bohanec, B. (2012). “Haploids and doubled haploids in plant breeding,” in Plant Breeding, ed I. Abdurakhmonov (InTech). ISBN: 978-953-307-932-5. Available online at: www.intechopen.com/books/plant-breeding/haploids-and-doubled-haploids-in-plant-breeding

Nishihama, R., Ishikawa, M., Araki, S., Soyano, T., Asada, T., and Machida, Y. (2001). The NPK1 mitogen-activated protein kinase kinase kinase is a regulator of cell-plate formation in plant cytokinesis. Genes Dev. 15, 352–363. doi: 10.1101/gad.863701

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Olsen, O. A. (2004). Nuclear endosperm development in cereals and Arabidopsis thaliana. Plant Cell 16, S214–S227. doi: 10.1105/tpc.017111

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Pallotta, M. A., Graham, R. D., Langridge, P., Sparrow, D. H. B., and Barker, S. J. (2000). RFLP mapping of manganese efficiency in barley. Theor. Appl. Genet. 101, 1100–1108. doi: 10.1007/s001220051585

CrossRef Full Text | Google Scholar

Park, S. K., and Twell, D. (2001). Novel patterns of ectopic cell plate growth and lipid body distribution in the Arabidopsis gemini pollen1 mutant. Plant Physiol. 126, 899–909. doi: 10.1104/pp.126.2.899

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Ravi, M., and Chan, S. W. L. (2010). Haploid plants produced by centromere-mediated genome elimination. Nature 464, 615–618. doi: 10.1038/nature08842

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Risueño, M. C., Gimenez-Martin, G., and López-Sáez, J. F. (1968). Experimental analysis of plant cytokinesis. Exp. Cell Res. 49, 136–147.

Pubmed Abstract | Pubmed Full Text | Google Scholar

Seguí-Simarro, J. M., and Nuez, F. (2007). Embryogenesis induction, callogenesis, and plant regeneration by in vitro culture of tomato isolated microspores and whole anthers. J. Exp. Bot. 58, 1119–1132. doi: 10.1093/jxb/erl271

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Seguí-Simarro, J. M., and Nuez, F. (2008). Pathways to doubled haploidy: chromosome doubling during androgenesis. Cytogenet. Genome Res. 120, 358–369. doi: 10.1159/000121085

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text

Sunderland, N., Collins, G. B., and Dunwell, J. M. (1974). Role of nuclear fusion in pollen embryogenesis of Datura innoxia Mill. Planta 117, 227–241. doi: 10.1007/BF00388396

Pubmed Abstract | Pubmed Full Text | CrossRef Full Text | Google Scholar

Sunderland, N., and Evans, L. J. (1980). Multicellular pollen formation in cultured barley anthers: II. The A, B and C pathways. J. Exp. Bot. 31, 501–514. doi: 10.1093/jxb/31.2.501

CrossRef Full Text | Google Scholar

Takamura, T., and Miyajima, I. (1996). Colchicine induced tetraploids in yellow-flowered cyclamens and their characteristics. Sci. Hortic. 65, 305–312. doi: 10.1016/0304-4238(96)00896-5

CrossRef Full Text | Google Scholar

Touraev, A., Vicente, O., and Heberle-Bors, E. (1997). Initiation of microspore embryogenesis by stress. Trends Plant Sci. 2, 297–302. doi: 10.1016/S1360-1385(97)89951-7

CrossRef Full Text | Google Scholar

Keywords: barley, pollen, embryogenesis, live-cell, imaging

Citation: Daghma DS, Hensel G, Rutten T, Melzer M and Kumlehn J (2014) Cellular dynamics during early barley pollen embryogenesis revealed by time-lapse imaging. Front. Plant Sci. 5:675. doi: 10.3389/fpls.2014.00675

Received: 12 September 2014; Accepted: 12 November 2014;
Published online: 08 December 2014.

Edited by:

Jose M. Segui-Simarro, Universitat Politècnica de València, Spain

Reviewed by:

Byung-Ho Kang, University of Florida, USA
Jose M. Segui-Simarro, Universitat Politècnica de València, Spain
Danny Geelen, Ghent University, Belgium

Copyright © 2014 Daghma, Hensel, Rutten, Melzer and Kumlehn. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.

*Correspondence: Jochen Kumlehn, Department of Physiology and Cell Biology, Leibniz Institute of Plant Genetics and Crop Plant Research, Correnstr 3, Gatersleben 06466, Germany e-mail: kumlehn@ipk-gatersleben.de

Present address: Laboratory of Biochemistry, Wageningen University, Wageningen, Netherlands

These authors have contributed equally to this work.