Plant Cell, Vol. 10, 5-18, Copyright © 1998, American Society of Plant Physiologists
Genetic Analysis of Female Gametophyte Development and Function
Gary N. Drewsa,
Diana Leea, and
Cory A. Christensena
a Department of Biology, University of Utah, Salt Lake City, Utah 84112
Correspondence to:
Gary N. Drews, drews{at}bioscience.utah.edu (E-mail), 801-581-4668 (fax).
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INTRODUCTION |
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The plant life cycle alternates between a multicellular haploid generation, called the gametophyte, and a multicellular diploid generation, called the sporophyte. In plants, meiosis gives rise to haploid spores, which undergo cell proliferation and differentiation to develop into gametophytes. A major function of the gametophyte generation is to produce haploid gametes. Fusion of the egg cell with the sperm cell gives rise to the sporophyte, thereby completing the life cycle (Raven et al. 1992 
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In many lower plants, gametophytes are the dominant and free-living generation. Angiosperms, by contrast, have dramatically reduced gametophytes, which are comprised of very few cells and are embedded within the sexual organs of the flower (Raven et al. 1992 ). The angiosperm male gametophyte (i.e., the pollen grain or microgametophyte), which develops within the stamen's anther, is a three-celled structure comprised of two sperm cells encased within a vegetative cell (McCormick 1993 ). The female gametophyte is also referred to as the embryo sac or megagametophyte. It develops in the ovule, which is found within the carpel's ovary. The most common female gametophyte form, which is depicted in Figure 1, consists of seven cells and four different cell types: three antipodal cells, two synergid cells, one egg cell, and one central cell (Maheshwari 1950 ; Willemse and Van Went 1984 ; Haig 1990 ; Huang and Russell 1992a ; Reiser and Fischer 1993 ).
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Figure 1.
The Polygonum-Type Female Gametophyte of Arabidopsis.
(A) View in longitudinal section in the context of the ovule.
(B) View perpendicular to that in (A).
The gray areas represent cytoplasm, the white areas represent vacuoles, and the black areas represent nuclei. AC, antipodal cells; CC, central cell; Ch, chalazal region of the ovule; EC, egg cell; F, funiculus; Mp, micropyle; SC, synergid cell; SEN, secondary endosperm nucleus.
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Sexual reproduction in angiosperms is initiated when pollen is transferred from anther to stigma. Shortly thereafter, the male gametophyte germinates a pollen tube and delivers its two sperm cells to the female gametophyte to effect "double" fertilization of the egg cell and the two polar nuclei of the central cell (Maheshwari 1950 ; Russell 1992 ). The female gametophyte plays a critical role at many steps of the reproductive process. For example, as the pollen tube grows, the female gametophyte participates in directing the pollen tube to the ovule (Hulskamp et al. 1995 ; Ray et al. 1997 ), and during fertilization, cytoskeletal components within the female gametophyte direct one sperm cell to the egg cell and the other to the central cell (Russell 1992 , Russell 1993 ; Huang and Russell 1994 ). Upon fertilization, genes expressed in the female gametophyte participate in inducing seed development (Ohad et al. 1996 ; Chaudhury et al. 1997 ) and may continue to play a role in the development of the embryo and the endosperm, which are derived from the egg cell and the central cell, respectively (Ray 1997 ).
Gene products required for female gametophyte development and function could be encoded by genes expressed either within the female gametophyte or in the surrounding sporophytic cells of the ovule. Several sporophytic mutations disrupting ovule development and function have been isolated (Robinson-Beers et al. 1992 ; Lang et al. 1994 ; Leon- Kloosterziel et al. 1994 ; Modrusan et al. 1994 ; Gaiser et al. 1995 ; Elliot et al. 1996 ; Klucher et al. 1996 ; Baker et al. 1997 ; Schneitz et al. 1997 ). In some of these mutants, female gametophyte development is altered (Robinson-Beers et al. 1992 ; Modrusan et al. 1994 ; Elliot et al. 1996 ; Klucher et al. 1996 ; Schneitz et al. 1997 ). However, it is not clear whether these mutations affect female gametophyte development directly or as a secondary consequence of an effect on the ovule's surrounding sporophytic tissue.
Genetic studies also suggest that female gametophyte development depends on the activities of many female gametophyte-expressed genes. For example, studies in maize have shown that most chromosomal deletions are deleterious to the female gametophyte, suggesting that genes essential for embryo sac viability are present throughout the maize genome (Patterson 1978 ; Coe et al. 1988 ; Buckner and Reeves 1994 ; Patterson 1994 ; Vizir et al. 1994 ; Vollbrecht and Hake 1995 ). Moreover, morphological analysis of a battery of embryo sacs harboring a variety of small chromosomal deletions has demonstrated that female gametophyte-expressed genes control fundamental aspects of female gametophyte development, such as nuclear migration, the coordination of developmental events, and the establishment of polarity (Vollbrecht and Hake 1995 ); many of these genes may perform regulatory functions.
The identities and specific functions of the haploid-expressed genes required by the female gametophyte are almost completely unknown. Recently, however, screens for female gametophyte mutants have been initiated in several laboratories, and mutations affecting specific steps of female gametophyte development and function have been identified. In this review, we discuss the approaches that have been used to identify female gametophyte mutants, summarize the cellular processes that are affected in these mutants, and discuss other genetic and molecular approaches that are being used to identify genes required by the female gametophyte. Comprehensive reviews of female gametophyte structure and development have been published previously (Willemse and Van Went 1984 ; Haig 1990 ; Huang and Russell 1992a ; Reiser and Fischer 1993 ); we emphasize recent progress made in Arabidopsis and maize in which genetic analyses of female gametophyte development and function are in progress.
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FEMALE GAMETOPHYTE MUTATIONS |
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Gametophytic Mutations
Not long after the rediscovery of Mendel's laws of heredity in 1900, it was found that some mutations exhibit aberrant segregation patterns (e.g., Correns 1902 ). It was later determined that these mutations affect the gametophytic phase of the plant life cycle (Brink and MacGillivray 1924 ; Jones 1924 ). Over the intervening years, it has become clear that plants contain two broad classes of mutations that exhibit fundamentally different segregation patterns. Sporophytic mutations affect sporophytically expressed genes and generally exhibit Mendelian 3:1 segregation patterns. Gametophytic mutations, by contrast, affect gametophytically expressed genes and are not transmitted through the egg and/or sperm. As a consequence, gametophytic mutations exhibit apparent non-Mendelian segregation patterns and can only be passed from generation to generation as heterozygotes.
Because angiosperms have two gametophytes, three classes of gametophytic mutations exist. The first class affects the female gametophyte but not the male gametophyte, the second class affects the male gametophyte but not the female gametophyte, and the third class affects both gametophytes. We refer to these classes as female gametophyte specific, male gametophyte specific, and general gametophytic, respectively.
The segregation patterns of these mutation classes are summarized in Table 1, which shows that in a self-cross of a heterozygous individual (e.g., genotype A/a), female gametophyte-specific mutations segregate 1:1 for A/A:A/a progeny (Table 1, second row). If a mutation affects both gametophytes and is fully penetrant, it cannot be transmitted to subsequent generations (Table 1, bottom row). However, many gametophytic mutations are partially penetrant (Singleton and Mangelsdorf 1940 ; Nelson and Clary 1952 ; Kermicle 1971 ; Niyogi et al. 1993 ; Kieber and Ecker 1994 ; Springer et al. 1995 ; Chaudhury et al. 1997 ; Feldmann et al. 1997 ) and therefore can be transmitted to subsequent generations.
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Table 1.
Segregation of Sporophytic and Gametophytic Mutations in a Cross of Two Heterozygous Individuals (A/a x A/a)
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Identification of Female Gametophyte Mutations
Mutations affecting the female gametophyte can be identified as lethals in which female gametophytes harboring the mutation either abort development or are nonfunctional. Two basic types of screens, segregation distortion and seed-set screens, have been used to identify female gametophyte mutants.
In segregation distortion screens, the altered segregation of female gametophyte mutants is exploited to identify this mutant class. These screens are facilitated by following the segregation of either linked visible markers (Singleton 1932 ; Rhoades and Rhoades 1939 ; Singleton and Mangelsdorf 1940 ; Redei 1965 ) or linked T-DNAs/transposons (Feldmann et al. 1997 ; Moore et al. 1998 ). For example, in T-DNA-mutagenized lines in which the T-DNA carries a gene conferring Kan resistance, the ratio of Kan-resistant to Kan-sensitive seedlings (KanR:KanS) can be used to identify lines that have a T-DNA insert disrupting a gene required for gametophyte development (Feldmann et al. 1997 ); in the progeny of a plant heterozygous for a female gametophyte-specific mutation, KanR:KanS is 1:1 compared with 3:1 for a sporophytic mutation (Table 1). However, male gametophyte mutations also exhibit segregation distortion (Table 1); thus, additional criteria (e.g., a seed-set screen or reciprocal crosses) are necessary to determine whether a given mutation affects the female or male gametophyte.
Another criterion by which to identify female gametophyte mutants is reduced seed set. This phenotype arises because, on a plant heterozygous for a female gametophyte mutation (e.g., genotype A/a), approximately half of the female gametophytes are mutant and nonfunctional (genotype a) and because an ovule harboring a defective female gametophyte fails to undergo seed development. An ovule that fails to develop into a seed desiccates and forms a small white mass (Meinke and Sussex 1979 ). Thus, one way to identify female gametophyte mutants is to screen for lines with siliques/ears containing 50% normal seeds and 50% desiccated ovules.
In theory, reduced seed set is the only criterion required to identify female gametophyte mutants. However, reduced seed set also can be caused by a variety of other factors, including adverse environmental conditions (e.g., high growth temperature or water stress), chromosomal rearrangements (e.g., reciprocal translocations or large inversions), and sporophytic mutations (e.g., female-sterile mutations with 50% penetrance). Thus, additional experiments (e.g., a segregation distortion screen) are required for the definitive identification of female gametophyte mutants.
The frequency of female gametophyte mutants among mutagenized lines can be estimated from preliminary screening data. In screens currently in progress, ~1% of T-DNA-mutagenized (C.A. Christensen, D. Lee, J. Gold, R. Brown, and G.N. Drews, unpublished data) and transposon-mutagenized (Moore et al. 1998 ) lines exhibit both segregation distortion and reduced seed set. This suggests that female gametophyte mutants occur at high frequency and that in a saturation screen (Waddington 1940 ; Jurgens et al. 1991 ), several hundred embryo sac mutants would be identified.
Female Gametophyte Mutations Fall into Two Classes
The known female gametophyte mutations are listed in Table 2. Many (11/25) of these mutations do not affect the male gametophyte and thus fall into the female gametophyte-specific class (Table 2). Female gametophyte-specific mutations are potentially important for two reasons. First, they are less likely to occur in "housekeeping" genes, because such mutations would be expected to affect the male gametophyte as well as the sporophyte. Second, they may affect female gametophyte-specific processes, such as the establishment of female gametophyte polarity, specification and differentiation of the female gametophyte cells, polar nuclei migration and fusion, antipodal cell death, pollen tube guidance, fertilization, and the induction of seed development (discussed below).
Most (14/25) of the known female gametophyte mutants also affect the male gametophyte and thus fall into the general gametophytic class (Table 2). This class of mutant is also important because many fundamental cellular processes take place during the development of both male and female gametophytes. These include mitosis, vacuole formation, cell expansion, subcellular migration, cellularization, and cell wall formation (discussed below). Furthermore, mutations that affect these critical processes in the gametophyte are unlikely to become homozygous in the sporophyte (Table 1) and can therefore be isolated only in screens for gametophytic mutants.
Phenotypic Analysis of Female Gametophyte Mutants
Phenotypic analysis of female gametophyte mutants in Arabidopsis and maize is facilitated by several factors. First, the Arabidopsis pistil contains 50 to 60 ovules (Christensen et al. 1997 ) and the maize ear contains 400 to 500 ovules (Dumas and Mogensen 1993 ). Second, within an Arabidopsis pistil, female gametophyte development is synchronous (Christensen et al. 1997 ). In maize, each ear contains a gradient of embryo sacs in a developmental series, with adjacent ovules at similar developmental stages (Vollbrecht and Hake 1995 ). Third, within a pistil/ear of a heterozygous female gametophyte mutant, half of the female gametophytes are genotypically wild type and half are genotypically mutant (Table 1); thus, the developmental stage of wild-type female gametophytes can be used to determine the developmental stage of mutant female gametophytes (Christensen et al. 1997 ). Fourth, extensive descriptive studies of female gametophyte structure and development have been conducted in Arabidopsis (Misra 1962 ; Poliakova 1964 ; Webb and Gunning 1990 , Webb and Gunning 1994 ; Mansfield et al. 1991 ; Murgia et al. 1993 ; Schneitz et al. 1995 ; Christensen et al. 1997 ) and maize (Weatherwax 1919 ; Cooper 1937 ; Diboll and Larson 1966 ; Diboll 1968 ; Russell 1979 ; Huang and Sheridan 1994 ; Vollbrecht and Hake 1995 ). These studies, which are summarized in the following section, provide the essential framework upon which mutagenic approaches are based. Finally, confocal laser scanning microscopy (CLSM) procedures have been developed to analyze rapidly female gametophyte development in Arabidopsis (Christensen et al. 1997 ) and maize (Vollbrecht and Hake 1995 ).
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MEGAGAMETOGENESIS |
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Development of the Angiosperm Female Gametophyte
Before one can effectively evaluate the phenotype caused by a gametophyic mutation, it is important to understand how gametophyte development proceeds in the wild type. Over 15 different patterns of female gametophyte development have been described (Maheshwari 1950 ; Willemse and Van Went 1984 ; Haig 1990 ). The developmental pattern exhibited by most species, including Arabidopsis (Misra 1962 ) and maize (Weatherwax 1919 ; Cooper 1937 ), is the "normal type," which is usually referred to as the Polygonum type because it was first described in Polygonum divaricatum (Strasburger 1879 ; Maheshwari 1950 ). The Polygonum-type female gametophyte is found in ~70% of the species that have been examined (Maheshwari 1950 ) and is thought to be the ancestral type (Huang and Russell 1992a ).
Polygonum-type female gametophyte development can be divided into two phases: megasporogenesis and megagametogenesis (Maheshwari 1950 ; Willemse and Van Went 1984 ; Haig 1990 ; Huang and Russell 1992a ; Reiser and Fischer 1993 ). During megasporogenesis, a diploid megaspore mother cell undergoes meiosis to produce four haploid megaspores. The chalazal-most megaspore survives, and the other three undergo cell death. During megagametogenesis, which is depicted in Figure 2, the functional megaspore (Figure 2B) undergoes three rounds of mitosis, producing an eight-nucleate cell (Figure 2C). Two nuclei (the polar nuclei), one from each pole, then migrate toward the center of the cell. In Arabidopsis and other species, the polar nuclei fuse, forming the secondary endosperm nucleus (Figure 2A, bottom, and 2D; Poliakova 1964 ; Newcomb 1973 ; Schulz and Jensen 1973 ; Webb and Gunning 1994 ; Schneitz et al. 1995 ; Christensen et al. 1997 ). By contrast, in maize and other species, the polar nuclei only partially fuse before fertilization (Figure 2A, top; Jensen 1964 ; Diboll 1968 ; Wilms 1981 ; Bedinger and Russell 1994 ; Vollbrecht and Hake 1995 ).
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Figure 2.
Megagametogenesis in Angiosperms.
(A) Depiction of megagametogenesis in maize (top) and Arabidopsis (bottom).
(B) to (D) CLSM images of specific stages in Arabidopsis. (B) One-nucleate stage. This image consists of one 1.5-µm optical section. (C) Mid-eight-nucleate stage. This image is a projection of four 1.5-µm optical sections. (D) Micropylar region of the mature female gametophyte. This image is a projection of four 1.5-µm optical sections.
In the CLSM images, the white spots are nuclei, the gray areas are cytoplasm, and the black areas are vacuoles. AC, antipodal cells; AN, antipodal cell nucleus; CC, central cell; CV, central cell vacuole; DM, degenerate megaspores; EC, egg cell; EN, egg nucleus; EV, egg vacuole; IIn, inner integument; M, megaspore; N, nucleus; OIn, outer integument; PN, polar nuclei; SC, synergid cell; SEN, secondary endosperm nucleus; SN, synergid nucleus; SV, synergid vacuole. Bars = 10 µm.
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During polar nuclei migration, the embryo sac cellularizes to form the seven-celled structure depicted in Figure 1. In some species, this is the final form (Maheshwari 1950 ; Willemse and Van Went 1984 ; Haig 1990 ; Huang and Russell 1992a ). However, in both Arabidopsis and maize, the female gametophyte undergoes additional developmental steps before fertilization. In Arabidopsis, the three antipodal cells degenerate (Figure 2A, bottom; Poliakova 1964 ; Murgia et al. 1993 ; Schneitz et al. 1995 ; Christensen et al. 1997 ). By contrast, in maize, the antipodal cells proliferate into as many as 100 cells in the mature embryo sac (Figure 2A, top; Diboll and Larson 1966 ; Diboll 1968 ; Russell 1979 ; Huang and Sheridan 1994 ; Vollbrecht and Hake 1995 ).
As shown in Figure 1A and Figure 1B, polarity establishment is an important feature of female gametophyte development. The ovule has a distinct axis of polarity. The micropylar pole is the end at which the integuments form a pore, and the chalazal pole is the end that joins the funiculus. The female gametophyte also has a distinct polarity, with the egg and synergid cells at the micropylar pole and the antipodal cells at the chalazal pole.
Thus, to understand how female gametophyte development is regulated, many important questions must be addressed: How is female gametophyte polarity within the ovule established? How is the number of mitoses regulated? Which cytoplasmic elements mediate and control nuclear migration? How is cellularization initiated and controlled? What controls cell specification during megagametogenesis? What factors mediate fusion of the polar nuclei? How are antipodal cell death (in Arabidopsis) and proliferation (in maize) controlled? As discussed below, genetic approaches have begun to identify some of the genes involved in these processes.
Mutations Affecting Specific Steps of Megagametogenesis
It is not known which developmental steps during megagametogenesis are controlled by haploid-expressed genes, nor is it known when these genes are required during megagametogenesis. However, a relatively large number of female gametophyte mutants with defects in megagametogenesis are now available to begin to address these questions. CLSM images and schematics of some of these mutants are shown in Figure 3.
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Figure 3.
Images of Mutants with Defects in Megagametogenesis.
(A) and (B) fem2 mutant phenotype at the terminal developmental stage (compare with Figure 2D). (A) CLSM image consisting of one 1.5-µm optical section. (B) Schematic representation. This mutant does not progress beyond the one-nucleate stage. The fem3, Gf, gfa4, and gfa5 mutants also exhibit this phenotype (Table 2).
(C) and (D) gfa2 mutant phenotype at the terminal developmental stage (compare with Figure 2D). (C) CLSM image consisting of a projection of five 1.5-µm optical sections. (D) Schematic representation. In this mutant, the polar nuclei fail to fuse. The gfa3 and gfa7 mutants also exhibit this phenotype (Table 2).
(E) and (F) fem4 mutant phenotype at the terminal developmental stage (compare with Figure 2D). (E) CLSM image consisting of one 1.5-µm optical section. Only one synergid is shown in this image. (F) Schematic representation. In this mutant, the cell shape and the number, location, or shape of vacuoles are abnormal (Table 2).
In these CLSM images, the white spots are nuclei, the gray areas are cytoplasm, and the black areas are vacuoles. CC, central cell; CV, central cell vacuole; EC, egg cell; EN, egg nucleus; mFG, mutant female gametophyte; N, nucleus; PN, polar nucleus; SC, synergid cell; SEN, secondary endosperm nucleus; SN, synergid nucleus; SV, synergid vacuole. Bars = 10 µm.
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Megagametogenesis is affected in 14 of the female gametophyte mutants listed in Table 2. Some of these mutants (fem2, fem3, Gf, gfa4, and gfa5) are affected at the earliest possible step, the one-nucleate stage (Table 2, and Figure 3A and Figure 3B). In these mutants, it is unclear which cellular processes are affected because developmental arrest at the one-nucleate stage can result from defects in a variety of processes, including mitosis, cell metabolism, and developmental control. Nevertheless, the existence of this mutant class clearly demonstrates that haploid-expressed genes are required very early in megagametogenesis.
Many of the megagametogenesis mutations listed in Table 2 affect steps that follow the one-nucleate stage. The main events that take place subsequent to the one-nucleate stage are nuclear division, polar nuclei migration, polar nuclei fusion, cellularization, and antipodal cell death or proliferation (Figure 2A). Nuclear division is affected in the hdd, ig, lo2, and prl mutants (Table 2). hdd mutant female gametophytes arrest at the two-, four-, or eight-nucleate stage. Some hdd mutant embryo sacs exhibit asynchrony of nuclear divisions at the two poles, suggesting that the HDD gene plays a role in coordinating nuclear division at the micropylar and chalazal poles (Moore et al. 1998 ). ig mutant female gametophytes undergo asynchronous and extra cycles of nuclear division, resulting in excessive numbers of nuclei (Kermicle 1971 ; Lin 1978 , Lin 1981 ; Huang and Sheridan 1996 ). lo2 mutant embryo sacs arrest at the one-, two-, or four-nucleate stage, and in some cases, the nuclei enlarge dramatically (Sheridan and Huang 1997 ). The hdd, ig, and lo2 mutations also cause secondary defects in nuclear migration, nuclear positioning, and/or microtubule organization, suggesting a relationship between nuclear behavior and cytoskeletal organization (Kermicle 1971 ; Lin 1978 , Lin 1981 ; Huang and Sheridan 1996 ; Sheridan and Huang 1997 ; Moore et al. 1998 ). The prl mutation causes developmental arrest, most often at the four-nucleate stage (Springer et al. 1995 ); the PRL gene is related to the yeast MCM2-3-5 genes that are required for initiation of DNA replication (Springer et al. 1995 ).
The remaining megagametogenesis mutations affect steps other than nuclear division. Polar nuclei fusion is affected in the gfa2, gfa3, and gfa7 mutants (Table 2). In these mutants, the polar nuclei migrate appropriately and come to lie side by side but remain unfused (Figure 3C and Figure 3D; C.A. Christensen and G.N. Drews, unpublished data). Cellularization appears to be affected in the fem4 mutant (Table 2). In this mutant, the shapes of the egg cell and synergids are abnormal, and their vacuoles show alterations in number, size, and shape (Figure 3E and Figure 3F; C.A. Christensen and G.N. Drews, unpublished data). Maintenance of the central vacuole may be affected in the fem1 mutant (Table 2). fem1 female gametophytes develop normally until the time of cellularization, upon which the embryo sac disintegrates. In some fem1 mutant embryo sacs, most aspects of morphology are normal except that the central vacuole is not present (S. Subramanian and G.N. Drews, unpublished data).
Thus, mutations affecting specific steps of megagametogenesis have already been identified. With the complement of megagametogenesis mutants already available, molecules mediating some of these steps should soon be identified. For example, isolation of the GFA2, GFA3, and GFA7 genes should identify molecules required for fusion of the polar nuclei.
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POLLEN TUBE GUIDANCE AND FERTILIZATION |
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Fertilization in Angiosperms
Soon after pollination, the male gametophyte forms a pollen tube, which grows great distances through the sporophytic tissue of the carpel to reach its final destination, the female gametophyte (Heslop-Harrison 1987 ; Bedinger et al. 1994 ; Pruitt and Hulskamp 1994 ; Preuss 1995 ; Cheung 1996 ; Smyth 1997 ). The pollen tube enters the female gametophyte by growing through the ovule's micropyle and pushing into one of the synergid cells. The receptive synergid cell undergoes cell death either before or upon pollen tube arrival. In several species, including Arabidopsis, it has been demonstrated that synergid cell death is triggered by pollination or the presence of pollen tubes within the female tissue (Jensen et al. 1983 ; Huang and Russell 1992b ; Christensen et al. 1997 ). During synergid cell death, the synergid cytoskeleton undergoes a reorganization, resulting in the formation of two bands of F-actin (Huang et al. 1993 ; Huang and Russell 1994 ; Huang and Sheridan 1994 ).
After the pollen tube arrives at the synegrid, the contents of the pollen tube, including the two sperm cells, are released into the degenerating synergid cytoplasm. Next, one sperm cell migrates to the egg cell and the other to the central cell, most likely along the F-actin bands (Huang et al. 1993 ; Huang and Russell 1994 ; Huang and Sheridan 1994 ). When the male gametes reach their destinations, their plasma membranes fuse with those of the egg cell and central cell, and the sperm nuclei are transmitted into these cells for karyogamy (Van Went and Willemse 1984 ; Willemse and Van Went 1984 ; Russell 1992 , Russell 1996 ).
This description of the angiosperm fertilization process raises several important questions: How does the pollen tube find its way to the female gametophyte? How does the male gametophyte induce the receptive synergid cell to undergo cell death? What controls reorganization of the synergid cytoskeleton and formation of the F-actin bands? What triggers release of the pollen tube contents into the female gametophyte? How is sperm cell migration along the F-actin bands initiated and controlled? What mediates sperm-egg and sperm-central cell recognition and fusion?
Genetic Analysis of Pollen Tube Guidance
Female gametophyte mutations affecting pollen tube guidance and fertilization have yet to be identified; however, female gametophyte mutations affecting megagametogenesis have been used to establish that the embryo sac plays a role in pollen tube guidance. Descriptive studies of pollen tube growth patterns in many species, including Arabidopsis and maize, suggest that a chemotropic guidance signal directs pollen tube growth to the ovule (Heslop-Harrison 1987 ; Bedinger et al. 1994 ; Pruitt and Hulskamp 1994 ; Preuss 1995 ; Cheung 1996 ; Smyth 1997 ).
A likely source of a chemoattractant is the female gametophyte itself, because this is the pollen tube's ultimate target. Evidence supporting this hypothesis initially came from the analysis of pollen tube growth in Arabidopsis ovule mutants in which female gametophytes do not form. In such mutants, pollen tube growth on the placental surface was random and pollen tubes were rarely found on mutant ovules (Hulskamp et al. 1995 ). However, because the ovule mutants were sporophytic, it could not be ruled out that the loss of pollen tube guidance was due to a defect in the sporophytic tissue. More recently, it has been shown that ovules harboring defective female gametophytes arrested at the one-nucleate stage (because of chromosomal imbalance) fail to receive pollen tubes (Ray et al. 1997 ). Furthermore, we have shown that pollen tube guidance is lost in a battery of Arabidopsis female gametophyte mutants that show no defect in the ovule's sporophytic tissue and in which the embryo sac does not progress beyond the one-nucleate stage (C.A. Christensen and G.N. Drews, unpublished data). Although these data are consistent with the suggestion that the female gametophyte actively attracts pollen tubes, the nature of the proposed chemoattractant(s) and the identity of the female gametophyte cell(s) in which it may be produced remain unclear.
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INDUCTION OF SEED DEVELOPMENT |
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Induction of Seed Development in Angiosperms
During seed development in angiosperms, the fertilized egg cell develops into the embryo, the fertilized central cell gives rise to the endosperm, and the ovule's integuments form the seed coat. During sexual reproduction, these three processes are dependent upon double fertilization of the egg cell and central cell. By contrast, in apomictic species, one or more of these developmental pathways are activated in the absence of fertilization. For example, during diplosporic gametophytic apomixis, an unreduced megaspore mother cell gives rise to a diploid female gametophyte, and embryo development (and sometimes endosperm development) is initiated in the absence of fertilization. Apomixis also may involve activation of embryo development in inappropriate cell types. For example, during sporophytic apomixis (i.e., adventitious embryony), embryo development is activated in somatic cells of the ovule that are external to the female gametophyte (Maheshwari 1950 ; Nogler 1984 ; Koltunow 1993 ; Koltunow et al. 1995 ).
This discussion of sexual and asexual seed development in angiosperms raises several important questions: What controls activation of embryo, endosperm, and seed coat development in response to fertilization? How are embryo and endosperm development induced to undergo seed development in the absence of fertilization in some species? How is embryo development activated in inappropriate cell types in some species? Does the female gametophyte play a role in controlling the induction of seed development, and if so, what is its role?
Mutations Affecting the Induction of Seed Development
To gain insight into the molecular processes controlling the induction of seed development, genetic screens were performed to identify mutants in which seed development occurs in the absence of fertilization. These screens led to the identification of four mutants, fie, fis1, fis2, and fis3, that undergo endosperm and seed coat development in the absence of fertilization (Table 2; Ohad et al. 1996 ; Chaudhury et al. 1997 ). Genetic analysis showed that these four mutants segregate gametophytically and that they fall into the female gametophyte-specific class (Ohad et al. 1996 ; Chaudhury et al. 1997 ). These mutations are either loss-of-function alleles in genes whose normal functions are to prevent seed development before fertilization or gain-of-function alleles in genes that promote seed development (Ohad et al. 1996 ; Chaudhury et al. 1997 ). The phenotypes of the fie and fis mutants suggest that the induction of seed development is controlled by a signal transduction pathway, some components of which are encoded by female gametophyte genes; their isolation provides solid proof that the female gametophyte plays a role in the induction of seed development.
Another mutation that may affect the induction of seed development is ctr1 (Table 2). The ctr1 mutation was first identified as a sporophytic mutation affecting ethylene signal transduction (Kieber et al. 1993 ) and was later shown to exhibit reduced transmission through the female gametophyte (Kieber and Ecker 1994 ). The CTR1 gene encodes a Raf-like Ser/Thr protein kinase that is required for ethylene signal transduction (Kieber et al. 1993 ). The ctr1 phenotype (Table 2) suggests a requirement for CTR1 during female gametophyte function. Pollen tube guidance is normal in this mutant, suggesting that this gene is required for either fertilization or the induction of seed development (C.A. Christensen and G.N. Drews, unpublished results).
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GAMETOPHYTIC MATERNAL CONTROL OF SEED DEVELOPMENT |
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Maternal Control of Seed Development in Angiosperms
In many animal systems, maternal control is a significant factor in embryo development (Gilbert 1994 ). Maternal control is likely to be more complex in plants than it is in animals for two reasons. First, angiosperms undergo double fertilization, which allows for maternal control over both embryo and endosperm development. Second, maternal control can be exerted by either gametophytic (i.e., the female gametophyte) or sporophytic (e.g., ovule cells that surround the female gametophyte; Ray 1997 ) tissue. Because of this complexity, it is important to distinguish between two possible classes of maternal mutations: sporophytic maternal mutations and gametophytic maternal mutations.
For both classes of maternal mutations, defects in embryo and/or endosperm development are not dependent on the genotypes of these two structures. Indeed, in sporophytic maternal mutants such as the Arabidopsis short integument (sin1; Ray et al. 1996 ) and barley shrunken endosperm (seg; Felker et al. 1985 ) mutants, embryo and/or endosperm development is dictated by the genotype of the maternal sporophytic tissue (e.g., the ovule integuments). Similar effects are also caused by FLORAL BINDING PROTEIN7 (FBP7)/FBP11 cosuppression in petunia (Colombo et al. 1997 ). By contrast, embryo and/or endosperm development in gametophytic maternal mutants is dictated by the genotype of the haploid tissue of the female gametophyte.
Gametophytic Maternal Mutations
It should be possible to identify gametophytic maternal mutations in the reduced seed-set and segregation distortion screens described above. However, female gametophyte mutations affecting gametophytic maternal control of embryo development should produce a slightly different seed-set phenotype than those affecting megagametogenesis, pollen tube guidance, fertilization, or the induction of seed development. This is because mutations affecting embryo and/or endosperm development result in defective (white or collapsed) seeds (Meinke and Sussex 1979 ; Clark and Sheridan 1991 ; Miller and Chourey 1992 ). Thus, heterozygous gametophytic maternal mutants should exhibit a 50% defective seeds phenotype compared with the 50% desiccated ovules phenotype exhibited by the other classes of female gametophyte mutants.
The only known mutations that exhibit segregation distortion and cause the 50% defective seeds phenotype are the Arabidopsis fie (Ohad et al. 1996 ), fis (Chaudhury et al. 1997 ), and emb173 (Castle et al. 1993 ) mutations (Table 2). These mutations all cause embryo arrest at the heart or torpedo stage; therefore, it is unlikely that the corresponding genes encode maternal factors required for embryo development. Instead, these mutations could affect gametophytic maternal-effect genes required for endosperm development. Alternatively, these mutations could affect genes required zygotically (i.e., post-fertilization) for endosperm development in at least two wild-type copies; mutations in such genes can also result in a 50% defective seeds phenotype (Castle et al. 1993 ; Ohad et al. 1996 ; Chaudhury et al. 1997 ). Because these two possibilities cannot be distinguished genetically, none of the known female gametophyte mutations clearly falls into the gametophytic maternal class. Thus, the extent to which the maternal gametophytic tissue exerts an influence on embryo and endosperm development in plants remains an important and largely unexplored question.
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IDENTIFICATION OF GENES EXPRESSED IN THE FEMALE GAMETOPHYTE |
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Currently, very few genes expressed in the female gametophyte have been isolated (Springer et al. 1995 ; Kranz and Dresselhaus 1996 ; Nadeau et al. 1996 ; Perry et al. 1996 ). However, several of the female gametophyte mutations listed in Table 2 were created by T-DNA (e.g., the fem and gfa mutations) or transposon (e.g., the hdd mutation) inserts. This will facilitate the rapid cloning of the corresponding genes, which appear to control specific steps of megagametogenesis including cellularization and the fusion of polar nuclei.
Identifying genes expressed in specific cells of the embryo sac has been hampered by difficulties in isolating female gametophytes, which are small and relatively inaccessible. These limitations have also frustrated molecular and biochemical experiments. However, new approaches in maize and Arabidopsis are beginning to overcome these problems.
For example, in maize, procedures for isolating large numbers of viable female gametophytes and egg cells have been developed (Wagner et al. 1988 ; Kranz et al. 1991 ). This advance has allowed the construction of cDNA libraries from unfertilized egg cells (Dresselhaus et al. 1994 ) and the isolation of several clones that appear to be expressed exclusively in the egg cell (Kranz and Dresselhaus 1996 ). These procedures could also be applied to isolate genes expressed specifically in the other female gametophyte cells (Dumas and Mogensen 1993 ).
In Arabidopsis, a large collection of gene-trap and enhancer-trap lines has been generated recently using transposable elements (Sundaresan et al. 1995 ). Among these lines are some that exhibit reporter gene expression in specific female gametophyte cells, including the synergid cells, the antipodal cells, and the central cell (Grossniklaus et al. 1995 ). These lines will be extremely useful as markers for the different female gametophyte cell types. For example, each of these lines could be crossed with the existing group of megagametogenesis mutants to determine whether the mutant phenotypes are associated with inappropriate cell specification. Furthermore, the trapped genes could serve as entry points into the female gametophyte gene regulatory circuitry.
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SUMMARY |
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The female gametophyte is an absolutely essential structure for angiosperm reproduction. It produces the egg cell and central cell (which give rise to the embryo and endosperm, respectively) and mediates several reproductive processes including pollen tube guidance, fertilization, the induction of seed development, and perhaps also maternal control of embryo development. Although much has been learned about these processes at the cytological level, specific molecules mediating and controlling megagametogenesis and female gametophyte function have not been identified.
A genetic approach to the identification of such molecules has been initiated in Arabidopsis and maize. Although genetic analyses are still in their infancy, mutations affecting female gametophyte function and specific steps of megagametogenesis have already been identified. Large-scale genetic screens aimed at identifying mutants affecting every step of megagametogenesis and female gametophyte function are in progress; the characterization of genes identified in these screens should go a long way toward defining the molecules that are required for female gametophyte development and function.
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ACKNOWLEDGMENTS |
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We thank Bob Fischer, Anna Koltunow, Nir Ohad, Crispin Taylor, Ramin Yadegari, and two anonymous reviewers for helpful comments on the manuscript. Our work on female gametophyte development was supported by National Science Foundation Grant No. IBN-9630371.
Received August 8, 1997; accepted November 21, 1997.
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REFERENCES |
|---|
Baker, S.C., Robinson-Beers, K., Villanueva, J.M., Gaiser, J.C., and Gasser, C.S. (1997) Interactions among genes regulating ovule development in Arabidopsis thaliana.. Genetics 145:1109-1124[Abstract]
Bedinger, P., and Russell, S.D. (1994). Gametogenesis in maize. In The Maize Handbook, M. Freeling and V. Walbot, eds (New York: Springer-Verlag), pp. 48-61.
Bedinger, P.A., Hardeman, K.J., and Loukides, C.A. (1994) Traveling in style: The cell biology of pollen. Trends Cell Biol. 4:132-138[CrossRef][Medline]
Brink, R.A., and MacGillivray, J.H. (1924) Segregation for the waxy character in maize pollen and differential development of the male gametophyte. Am. J. Bot. 11:465-469[CrossRef][ISI]
Buckner, B., and Reeves, S.L. (1994) Viability of female gametophytes that possess deficiencies for the region of chromosome 6 containing the Y1 gene. Maydica 39:247-254
Castle, L.A., Errampalli, D., Atherton, T.L., Franzmann, L.H., Yoon, E.S., and Meinke, D.W. (1993) Genetic and molecular characterization of embryonic mutants identified following seed transformation in Arabidopsis.. Mol. Gen. Genet. 241:504-514[CrossRef][ISI][Medline]
Chaudhury, A.M., Ming, L., Miller, C., Craig, S., Dennis, E.S., and Peacock, W.J. (1997) Fertilization-independent seed development in Arabidopsis thaliana.. Proc. Natl. Acad. Sci. USA 94:4223-4228[Abstract/Free Full Text]
Cheung, A.Y. (1996) Pollen-pistil interactions during pollen-tube growth. Trends Plant Sci. 1:45-51[CrossRef]
Christensen, C.A., King, E.J., Jordan, J.R., and Drews, G.N. (1997) Megagametogenesis in Arabidopsis wild type and the Gf mutant. Sex. Plant Reprod. 10:49-64[CrossRef]
Clark, J.K., and Sheridan, W.F. (1991) Isolation and characterization of 51 embryo-specific mutations of maize. Plant Cell 3:935-951[Abstract/Free Full Text]
Coe, E.H., Neuffer, M.G., and Hoisington, D.A. (1988). The genetics of corn. In Corn and Corn Improvement, 3rd ed, G.F. Sprague and J.W. Dudley, eds (Madison, WI: American Society of Agronomy), pp. 81-258.
Colombo, L., Franken, J., Van der Krol, A.R., Wittich, P.E., Dons, H.J.M., and Angenent, G.C. (1997) Downregulation of ovule-specific MADS box genes from petunia results in maternally controlled defects in seed development. Plant Cell 9:703-715[Abstract]
Cooper, D.C. (1937) Macrosporogenesis and embryo-sac development in Euchlaena mexicana and Zea mays.. J. Agric. Res. 55:539-551
Correns, C. (1902) Scheinbare ausnahmen von der Mendel'shen spaltungsregel fur bastarde. Ber. Dtsch. Bot. Ges. 20:159-172
Diboll, A.G. (1968) Fine structural development of the megagametophyte of Zea mays following fertilization. Am. J. Bot. 55:797-806[CrossRef]
Diboll, A.G., and Larson, D.A. (1966) An electron microscopic study of the mature megagametophyte in Zea mays.. Am. J. Bot. 53:391-402
Dresselhaus, T., Lörz, H., and Kranz, E. (1994) Representative cDNA libraries from few plant cells. Plant J. 5:605-610[ISI][Medline]
Dumas, C., and Mogensen, H.L. (1993) Gametes and fertilization: Maize as a model system for experimental embryogenesis in flowering plants. Plant Cell 5:1337-1348[Free Full Text]
Elliot, R.C., Betzner, A.S., Huttner, E., Oakes, M.P., Tucker, W.Q.J., Gerentes, D., Perez, P., and Smyth, D.R. (1996) AINTEGUMENTA, an APETALA2-like gene of Arabidopsis with pleiotropic roles in ovule development and floral organ growth. Plant Cell 8:155-168[Abstract]
Feldmann, K.A., Coury, D.A., and Christianson, M.L. (1997) Exceptional segregation of a selectable marker (KanR) in Arabidopsis identifies genes important for gametophytic growth and development. Genetics 147:1411-1422[Abstract]
Felker, F.C., Peterson, D.M., and Nelson, O.E. (1985) Anatomy of immature grains of eight maternal-effect shrunken endosperm barley mutants. Am. J. Bot. 72:248-256
Gaiser, J.C., Robinson-Beers, K., and Gasser, C.S. (1995) The Arabidopsis SUPERMAN gene mediates asymmetric growth of the outer integument of ovules. Plant Cell 7:333-345[Abstract]
Gilbert, S.F. (1994). Developmental Biology. (Sunderland, MA: Sinauer Associates).
Grossniklaus, U., Moore, J., and Gagliano, W. (1995). Analysis of Arabidopsis ovule development and megagametogenesis using enhancer detection. In Signaling in Plant Development (Cold Spring Harbor, NY: Cold Spring Harbor Laboratory Press), p. 138.
Haig, D. (1990) New perspectives on the angiosperm female gametophyte. Bot. Rev. 56:236-275
Heslop-Harrison, J. (1987) Pollen germination and pollen-tube growth. Int. Rev. Cytol. 107:1-78[ISI]
Huang, B.-Q., and Russell, S.D. (1992a) Female germ unit: Organization, isolation, and function. Int. Rev. Cytol. 140:233-292[ISI]
Huang, B.-Q., and Russell, S.D. (1992b) Synergid degeneration in Nicotiana: A quantitative, fluorochromatic and chlorotetracycline study. Sex. Plant Reprod. 5:151-155
Huang, B.-Q., and Russell, S.D. (1994) Fertilization in Nicotiana tabacum: Cytoskeletal modifications in the embryo sac during synergid degeneration. Planta 194:200-214
Huang, B.-Q., and Sheridan, W.F. (1994) Female gametophyte development in maize: Microtubular organization and embryo sac polarity. Plant Cell 6:845-861[Abstract]
Huang, B.-Q., and Sheridan, W.F. (1996) Embryo sac development in the maize indeterminate gametophyte1 mutant: Abnormal nuclear behavior and defective microtubule organization. Plant Cell 8:1391-1407[Abstract]
Huang, B.-Q., Pierson, E.S., Russell, S.D., Tiezzi, A., and Cresti, M. (1993) Cytoskeletal organization and modification during pollen tube arrival, gamete delivery and fertilization in Plumbago zeylanica.. Zygote 1:143-154[Medline]
Hülskamp, M., Schneitz, K., and Pruitt, R.E. (1995) Genetic evidence for a long-range activity that directs pollen tube guidance in Arabidopsis. Plant Cell 7:57-64[Abstract]
Jensen, W.A. (1964) Observations on the fusion of nuclei in plants. J. Cell Biol. 23:669-672[Free Full Text]
Jensen, W.A., Ashton, M.E., and Beasley, C.A. (1983). Pollen tube -embryo sac interaction in cotton. In Pollen: Biology and Implications for Plant Breeding, D.L. Mulcahy and E. Ottaviano, eds (New York: Elsevier Science Publishing), pp. 67-72.
Jones, D.F. (1924) Selective fertilization among the gametes from the same individuals. Proc. Natl. Acad. Sci. USA 10:218-221[Free Full Text]
Jürgens, G., Mayer, U., Torres-Ruiz, R.A., Berleth, T., and Misera, S. (1991) Genetic analysis of pattern formation in the Arabidopsis embryo. Development (suppl.) 1:27-38
Kermicle, J.L. (1971) Pleiotropic effects on seed development of the indeterminate gametophyte gene in maize. Am. J. Bot. 58:1-7[CrossRef]
Kieber, J.J., and Ecker, J.R. (1994). Molecular and genetic analysis of the constitutive ethylene response mutation ctr1. In Plant Molecular Biology: Molecular Genetic Analysis of Plant Development and Metabolism, G. Coruzzi and P. Puigdomenech, eds (Berlin: Springer-Verlag), pp. 193-201.
Kieber, J.J., Rothenberg, M., Roman, G., Feldmann, K.A., and Ecker, J.R. (1993) CTR1, a negative regulator of the ethylene response pathway in Arabidopsis, encodes a member of the Raf family of protein kinases. Cell 72:427-441[CrossRef][ISI][Medline]
Klucher, K.M., Chow, H., Reiser, L., and Fischer, R.L. (1996) The AINTEGUMENTA gene of Arabidopsis required for ovule and female gametophyte development is related to the floral homeotic gene APETALA2.. Plant Cell 8:137-153[Abstract]
Koltunow, A.M. (1993) Apomixis: Embryo sacs and embryos formed without meiosis or fertilization in ovules. Plant Cell 5:1425-1437[Free Full Text]
Koltunow, A.M., Bicknell, R.A., and Chaudhury, A.M. (1995) Apomixis: Molecular strategies for the generation of genetically identical seeds without fertilization. Plant Physiol. 108:1345-1352[CrossRef][ISI][Medline]
Kranz, E., and Dresselhaus, T. (1996) In vitro fertilization with isolated highe
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INTRODUCTION
FEMALE GAMETOPHYTE MUTATIONS