|
|
|
|
|
|
|
|
|||||
| Home Help Feedback Subscriptions Archive Search Table of Contents | |||||
First published online 11 November 2008
doi: 10.1242/jcs.036400
| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
Research Article |
1 Institute of Reproductive and Developmental Biology, Imperial College London, Hammersmith Hospital, Du Cane Road, London W12 0NN, UK
2 Department of Histopathology, Charing Cross Hospital, Fulham Palace Road, London W6 8RF, UK
3 Department of Mathematics and Centre for Integrative Systems Biology at Imperial College (CISBIC), Imperial College London, London SW7 2AZ, UK
* Author for correspondence (e-mail: k.hardy{at}imperial.ac.uk)
Accepted 20 August 2008
 |
Summary |
|---|
 Top Summary IntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
Key words: Basal lamina, Cell division, Cell shape, Granulosa cells, Multilayering, Ovary, Theca cells
|
Introduction |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
|
). Furthermore, the transition from quiescence to growth is crucial and must have a role in defining the reproductive lifespan of the female; too few growing follicles could result in anovulatory cycles, whereas too many could result in premature ovarian failure. Increased understanding of the cellular events that occur during initiation of follicle growth will help to determine how they are regulated.
Initiation of follicle growth is associated with oocyte growth, division of the epithelial granulosa cells (GCs) and a dramatic transformation of GC morphology from flattened to cuboidal (Fig. 1A) (Hirshfield, 1991; Picton, 2001). However, these cellular events have not been well characterised, nor is it clear how they are related. In other tissues and cell types, in vitro studies have demonstrated that modulating cell shape affects cell proliferation, and that flattened non-transformed cells divide more than round cells (Chen et al., 1997; Folkman and Moscona, 1978). Paradoxically, in the ovary, descriptive studies suggest that the opposite is true, with cuboidal cells dividing more than flat cells (Gougeon and Busso, 2000; Lundy et al., 1999; Wandji et al., 1997; Wandji et al., 1996), confirmed in a recent quantitative study using human ovary (Stubbs et al., 2007).
As the GCs cuboidalise, a glycoprotein layer – the zona pellucida – forms between the GCs and the oocyte, which maintain extensive contact with each other via transzonal processes (TZPs); the latter emanate from the GCs and traverse the zona (Albertini et al., 2001). When the oocyte is surrounded by a complete layer of cuboidal GCs, it is termed a primary follicle. GC proliferation continues and multiple layers of GCs form (Fig. 1B,C). At the primary stage, a layer of flattened cells, the theca-cell layer, is recruited from the stromal cells to envelop the basement membrane (Fig. 1C).
A unique microenvironment in the follicle is maintained by the follicular basal lamina which completely encloses the GCs, expanding as the follicle grows and separating the oocyte and surrounding GCs from adjacent theca, stromal and interstitial cells. The basal lamina excludes blood vessels and nerves from the GC-oocyte unit until after ovulation and, unlike the zona pellucida, is not traversed by any cells or cell processes (Rodgers et al., 2003). In a wide variety of tissues, basal laminae provide support and anchorage for polarised epithelial cells and also regulate their behaviour (cell shape, proliferation, apoptosis, differentiation and migration) (Berkholtz et al., 2006b; Monniaux et al., 2006). A direct transmembrane link between the ECM and the actin cytoskeleton is provided by integrins, which are expressed in the ovary and have a significant role in the regulation of cell behaviour in a wide range of tissues (Burns et al., 2002; Monniaux et al., 2006). Furthermore, basal laminae can act both as a sieve, selectively regulating passage of large macromolecules, and as a reservoir, binding certain growth factors (LeBleu et al., 2007; Rodgers et al., 2003).
In this study, using detailed morphometry and immunohistochemistry for the cell-cycle protein Ki67 in mouse ovary, we have carried out a quantitative analysis of GC proliferation during initiation of follicle growth and the development of the second and third layers of GCs. We compared GC proliferation, the growth trajectory of oocytes and change in GC cell shape on day 12 post partum (pp) (in the presence of only preantral follicles) with that on day 21 pp (in the presence of a wider range of follicle stages including preantral and antral follicles). We examined how changes in GC shape and oocyte growth relate to GC proliferation. Finally, we investigated how the packing density of GCs on the basal lamina induces the formation of multiple layers of GCs by regulating the orientation of the axis of mitosis, and examined how the position of GCs relative to the basal lamina regulates proliferation.
|
Results |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
|
|
There was significant oocyte growth from the primordial stage onwards (Fig. 3A). The mean oocyte diameter in primordial follicles on day 12 was significantly greater than that on day 21. On day 21, oocytes in follicles which were developing multiple layers of GCs were significantly larger than those on day 12 (Fig. 3A). Oocytes and follicles with more than two layers of GCs are likely not to have had sufficient time by day 12 to grow as much as similar follicles on day 21. The number of GCs increased significantly as follicle development progressed (Fig. 3B). During the early stages of follicle development, the number of GCs was remarkably similar on days 12 and 21. However, on day 21 there were significantly more GCs as the third layer of GCs developed, compared to day 12 (Fig. 3B). It is most probable that follicles on day 12 had only just reached the stage of forming a third layer and, therefore, had fewer GCs than similar, well-established follicles on day 21. GC height increased approximately sixfold from the primordial stage to the stage when a few cells were starting to appear in the second layer (Fig. 3C).
|
Ki67 immunolabelling and follicle stage
The prevalence of Ki67 immunolabelling of GCs was low in the cortex, where the majority of primordial follicles are located, and increased in larger follicles towards the medulla of the ovary (Fig. 4A). Quantitative analysis demonstrated Ki67 labelling in a small proportion of primordial follicles, and a larger proportion of transitional follicles. All follicles from the primary stage onwards contained Ki67-positive GCs (Fig. 4B). The Ki67 labelling index increased significantly as GCs became cuboidal (primordial to primary stages). As the follicles acquired further layers of GCs, there was no significant change in the labelling index on either day 12 or day 21 (Fig. 4C). The proportion of primordial and transitional follicles containing Ki67-positive GCs and the labelling index throughout early follicle development was significantly lower on day 21 than on day 12 (Fig. 4B,C).
|
). MCM2 is present in nuclei throughout the cell cycle but absent in differentiated or quiescent cells (Laskey, 2005). Double immunofluorescence labelling for Ki67 and MCM2 showed that the majority of cells in primordial follicles (Fig. 4D) and some cells in primary follicles (Fig. 4E) were completely unlabelled, suggesting that they were in G0.
Ki67 immunolabelling and cell shape
The proportion of Ki67-positive flat and cuboidal cells was computed overall, for all follicles analysed (Fig. 5A), and for primordial, transitional and primary follicles separately (Fig. 5B). Whereas the majority of flat cells were Ki67-negative (Fig. 5C), a few Ki67-positive flat cells were observed (Fig. 5D); however, a higher proportion of cuboidal cells were Ki67-positive (Fig. 5E,F). Overall, proliferation was around fivefold higher in cuboidal cells compared with flat cells (Fig. 5A). The proportion of Ki67-positive flat cells was similar in primordial and transitional follicles and significantly lower than the proportion of positive cuboidal cells (Fig. 5B), both on day 12 and day 21. In transitional follicles, on day 12 (but not on day 21), the cuboidal cells were immunolabelled more frequently than the flat cells. At the primary stage over a quarter of the cuboidal GCs were Ki67-positive on day 12 (Fig. 5B).
|
GC shape change, Ki67 immunolabelling and oocyte growth
First we examined whether the change in cell shape or onset of proliferation was associated with oocyte growth. Considering just transitional follicles, containing a mixture of flattened and cuboidal cells, there was no increase in oocyte size with an increasing proportion of cuboidal cells (Fig. 6A), therefore change in GC shape was not associated with oocyte growth. In addition, the onset of proliferation was not associated with oocyte growth. Ki67-positive primordial follicles did not contain significantly larger oocytes than Ki67-negative follicles, on days 12 or 21 (Fig. 6B). Furthermore, Ki67-positive primordial follicles did not have significantly more GCs than negative follicles on either day (Fig. 6C).
|
|
Formation of multiple layers of GCs
During our examination of the follicles it appeared that the GCs became closely packed on the basal lamina when the second layer of GCs was forming. This, coupled with our observations of decreased Ki67 immunolabelling in basal cells, led us to ask whether the basal lamina has a role in regulating the onset of the formation of a second layer of GCs. To give an estimate of packing density, we calculated how `wide', on average, the GCs were on the basal lamina, and compared the packing density of GCs at each developmental stage. For this analysis we subdivided the primary plus category into those follicles which were just starting to develop a second layer (termed `new second layer'), and those with a more extensive second layer (`established second layer'). The mean width of GCs was similar at each stage on day 12 and day 21, therefore the data were amalgamated for further analysis. There was a significant reduction in the mean width of GCs on the basal lamina from the primordial stage to the transitional and primary stages (Fig. 8A). At these earliest stages there was a wide range of GC widths, the variance of which reduced significantly as follicles progressed from primordial to transitional (P<0.0001), and from transitional to primary (P<0.0001) stages. The variance was similar as new layers were added (P=0.66). With the appearance of second and subsequent layers, the GCs attained (and maintained) a maximal packing density on the basal lamina of around one GC per 6 µm of basal lamina (Fig. 8A). As GCs became narrower, they became taller (Fig. 8B).
|
We went on to examine the ultrastructural appearance of the basal lamina at these early stages and to investigate whether it changed during formation of multiple layers (Fig. 8C-G). In unilaminar follicles, the basal lamina was generally straight, with a single layer of lamina densa, although this was not always well defined in follicles at this stage (Fig. 8C,D). Outside the lamina densa, away from the GCs, there were occasional collagen fibrils visible (Fig. 8D), but this layer was not continuous or extensive and, indeed, on day 12 was frequently absent. With the appearance of a second layer of GCs, the lamina densa was either straight or closely followed indentations in the GCs, with occasional extra layers of the lamina densa seen on the theca side (Fig. 8E). In follicles with multiple layers of GCs the layer of collagen fibrils varied from sparse to thick and dense (Fig. 8F,G). Hemidesmosomes were attached to the lamina densa by anchoring fibrils (Fig. 8E, insert).
The appearance of collagen fibrils outside the lamina densa led us to consider whether the surroundings of the follicle have a role in providing a confined area for GCs to become packed upon. This was supported by our observations of strong actin labelling within the theca cells, which appeared to form a mesh around the follicle and was strikingly aligned to the basal lamina (Fig. 8H).
Orientation of GC mitosis
The above described observations prompted us to examine whether the attainment of a maximal packing density on the basal lamina was accompanied by a change in the orientation of mitoses (Fig. 9). Approximately 150 H&E-stained sections of day 12 and day 21 ovaries were examined for mitoses in the GCs, and 
100 mitotic figures with a clear orientation were found (Table 2). No mitotic figures were seen in primordial follicles. All of the five mitoses in transitional follicles were, as expected, oriented parallel to the oocyte surface (Fig. 9Ai; Fig. 9B). As the GCs changed shape a mixture of mitoses that were parallel or perpendicular to the basal lamina and oocyte surface were seen (Fig. 9Aii; Fig. 9C; Table 2). The key observation was in the primary plus follicles, where many columnar GCs are attached at the basal surface to the basal lamina via hemidesmosomes, and at the opposite apical surface to the oocyte via TZP and gap junctions (described as `span basal-lamina-oocyte' in Table 2; Fig. 9Aiii). The vast majority (94%) of the mitotic figures in these cells were perpendicular to the basal lamina (Fig. 9D). This type of perpendicular cell division will result in one daughter cell remaining attached to the basal lamina (Fig. 9Aiv), and the other losing contact and contributing to the new second layer of GCs next to the oocyte (Fig. 9Av). These new inner daughter cells appear to be initially evenly and sparsely scattered around the oocyte (Fig. 2E), with the inner layer becoming more continuous, probably as a result of both inward-oriented division from cells on the basal lamina (Fig. 9Avi; Fig. 9F), and lateral division of new inner cells (Fig. 9G). With the development of more layers of GCs, cells divide perpendicular (Fig. 9F), parallel (Fig. 9G), and obliquely to the basal lamina and/or the oocyte.
|
|
|
Discussion |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
Flat GCs can proliferate but rarely do so, particularly in older mice. Cuboidalisation of cells results in a fivefold increase in proliferation, as demonstrated by an increased Ki67 labelling index and an increase in GC number in transitional and primary follicles. These observations are in contrast to in vitro studies of nontransformed endothelial cells, showing that flattened cells have the greater proliferative capacity, which decreases as the cells become more cuboidal, become confluent and ultimately undergo contact inhibition (Chen et al., 1997; Folkman and Moscona, 1978). However, we also observed a subsequent decline in proliferation as GCs reach a maximal packing density, suggesting that a degree of contact inhibition occurs in GCs on the basal lamina. This has been illustrated by a decline in both Ki67 immunolabelling and in the number of mitotic figures in basal cells; only four (13%) of the 30 mitotic figures observed in follicles with two or more layers were on the basal lamina. A low number of mitotic figures have also been observed in GCs on the basal lamina in bovine antral follicles, with the highest numbers being observed in the middle layers (van Wezel et al., 1999).
The potential for flat GCs to occasionally divide has been described before, although not specifically quantified. Positive immunostaining for PCNA has been observed occasionally in primordial follicles of cow, primate, human and sheep (Gougeon and Busso, 2000; Lundy et al., 1999; Wandji et al., 1997; Wandji et al., 1996) but not rat (Gaytan et al., 1996; Oktay et al., 1995). However, positive labelling of flattened GCs following long term in vivo infusion of rats with [3H]thymidine (Hirshfield, 1989) or BrdU (Meredith et al., 2000) suggested that very low levels of cell division were occurring. It is generally thought that primordial follicles are quiescent, but several studies have challenged this notion (Hirshfield, 1989; Lundy et al., 1999; Stubbs et al., 2007). Our results support the view that not all primordial follicles are entirely `quiescent', and that cuboidalisation of GCs is not an absolute pre-requisite for entry into the cell cycle.
Our observations of GCs that were not labelled when staining for either Ki67 or MCM2 (which labels cells in the cell cycle) in early preantral follicles further demonstrate that not all the GCs remain in the cell cycle, even a prolonged one, and suggests that these cells are in G0. Prolonged persistence of BrdU labelling in transitional rat follicles for more than 150 days supports this suggestion that GCs at these early stages can enter and leave the cell cycle (Meredith et al., 2000).
A decline in GC proliferation with advancing age has previously been reported in mice (Pedersen, 1969), monkeys (Gougeon and Busso, 2000), sheep (Lundy et al., 1999) and rats (Hirshfield, 1985). As the numbers of GCs at successive stages of early follicle development were similar on days 12 and 21, the significantly lower proportion of Ki67-positive GCs on day 21 suggest that follicle development becomes slower as the mice reach adulthood. The lower levels of Ki67 immunolabelling on day 21 might be due to the presence of larger preantral and antral follicles, which are sources of possible inhibitors of growth of smaller follicles, such as anti-Müllerian hormone (Durlinger et al., 2002) or activin (Mizunuma et al., 1999). Alternatively, it is possible that increased GC proliferation is due to increased levels of plasma follicle stimulating hormone (FSH) that is seen in prepubertal mice and peaks between days 10 and 16 (Dullaart et al., 1975; Halpin et al., 1986; Stiff et al., 1974), before declining to adult levels. This is feasible, because FSH-receptor mRNA is present in GCs from just after birth in mice (O'Shaughnessy et al., 1996), with levels peaking on day 10 pp (O'Shaughnessy et al., 1997), and FSH has been directly shown to stimulate GC proliferation in preantral follicles (Kreeger et al., 2005; Roy and Greenwald, 1989).
It is clear that bi-directional communication between the oocyte and the surrounding GCs is crucial for successful follicle development (Eppig, 2001; Gilchrist et al., 2004a; Matzuk et al., 2002). However, it is significant that the oocytes in Ki67-negative and -positive primordial follicles are similar in size, indicating that the onset of GC division (as measured by Ki67 immunolabelling) is not directly associated with the onset of oocyte growth. This is consistent with the reported lack of association between PCNA labelling and oocyte size in sheep primordial follicles (Lundy et al., 1999). Furthermore, to our surprise, we saw no increase in oocyte size as the proportion of cuboidal cells increased in transitional follicles. These observations suggest that early events in the oocyte and GCs could be occurring independently, but in parallel.
It is interesting that the relationship between GC proliferation and oocyte growth changed with the development of the second layer of GCs. In the unilaminar follicle, all the GCs are in contact with the basal lamina on one side and the oocyte on the other. With the onset of GC multilayering, two new populations of GCs develop; one in contact with the oocyte, the other with the basal lamina. Subsequent inner layers will be in contact with neither. The observation of a higher Ki67 labelling index in inner cells suggests that cells that have lost contact with the basal lamina divide more frequently, with the removal of the physical and signalling constraints imposed by contact with this ECM. Alternatively, the oocyte might be producing a factor that stimulates proliferation. It is notable that follicles in mice that lack the oocyte-specific growth factor Gdf9 fail to develop a second layer of GCs and have lower levels of GC proliferation, although oocyte growth continues (Dong et al., 1996; Elvin et al., 1999b). It is possible that Gdf9, which first appears at the primary stage (Dong et al., 1996; Elvin et al., 1999a), and increases GC proliferation in vitro (Gilchrist et al., 2004b), is producing a local gradient and stimulating proliferation close to the oocyte. Localised gradients of oocyte-derived BMPs have been observed previously (Hussein et al., 2005).
In follicles that started to develop a second layer, lateral proliferation was not observed in cells contacting both the basal lamina and the oocyte, and the vast majority (94%) of mitoses were oriented perpendicular to the basal lamina. Perpendicular mitoses have been observed in the basal layer of the epidermis and are thought to result both in stratification and asymmetric cell divisions, with one daughter cell losing contact with the basal lamina and therefore losing basal cell characteristics (Lechler and Fuchs, 2005). Furthermore, the orientation of the mitosis is regulated by cell shape, with the axis of the mitosis lying parallel to the long axis of the cell (O'Connell and Wang, 2000). Indeed, it is becoming clear that the cortical landmarks laid down by the distribution of adhesive contacts and external forces have a key role in defining the orientation of the mitotic spindle, and the spindle is aligned along the traction field defined in the preceding interphase (Thery and Bornens, 2006). It is clear from our EM studies, and the work of others, that in unilaminar follicles GCs are tethered at both ends, one end to the lamina densa by anchoring filaments, and the other end to the oocyte via TZPs (Albertini et al., 2001) and adhesive junctions (Fair et al., 1997; Zamboni, 1974). These opposing attachments could produce a traction field along the length of the columnar GC, that would orient the mitotic spindle perpendicular to the basal lamina, producing two asymmetric daughter cells, one basal and one inner. In-situ hybridisation analysis of ovaries from adult mouse chimaeras made by aggregating wild-type and β-globin transgenic eight-cell embryos demonstrated radial proliferation of GC clones across the follicle wall, supporting the idea that mitosis perpendicular to the basal lamina is important in the formation of multiple layers (Boland and Gosden, 1994).
The basal lamina appears to be crucial for normal folliculogenesis and the development of multiple layers. Mice that lack the gene encoding the forkhead transcription factor Foxl2 lack a continuous, regular, basal lamina around follicles and fail to form follicles with multiple layers of GCs (Uda et al., 2004). ECM provides a scaffold for cells, affecting cell behaviour by both its protein composition and physical stiffness or rigidity, and altering cell binding, cortical cues and downstream signalling from the junctions (Berrier and Yamada, 2007; Black et al., 2008). The protein composition of basal lamina changes during folliculogenesis owing to the varying presence and proportions of isoforms of type IV collagen and laminin (Rodgers et al., 2003). In the mouse ovarian follicle, type-IV collagen has been shown to be undetectable by immunohistochemistry in the basal laminae of primordial follicles and to increase as the follicle develops (Berkholtz et al., 2006a). The collagen-laminin composition of the ECM can regulate GC proliferation, with collagen being inhibitory (Huet et al., 2001; Oktay et al., 2000), thus the appearance of collagen IV in the basal lamina might inhibit GC proliferation in adjacent cells.
The physical stiffness of the basal lamina itself and of the surrounding cells might also be involved in constraining lateral cell division in the basal GCs. Mechanical signals can be transmitted bidirectionally between the ECM and the cytoskeleton via transmembrane integrins, resulting in changes in the ECM (rigidity, matrix deposition and remodelling) or the cell (shape, cytoskeletal rigidity, signalling) (Berrier and Yamada, 2007; Ingber, 2004). It has recently been elegantly demonstrated that the stiffness or rigidity of the environment can regulate follicle growth, with isolated mouse follicles cultured in gels of increasing concentrations of alginate (and hence rigidity) exhibiting reduced follicle growth (Xu et al., 2006). Furthermore, we observed collagen fibrils surrounding the basal lamina. These collagen fibrils were similar to those associated with the lamina densa of epithelia in exocrine glands, which contribute to connective tissue and provide mechanical support (Hosoyamada and Sakai, 2003). Collagen is stiff and almost inextensible (Black et al., 2008), so it can be envisaged that collagen fibrils surrounding the follicle could provide mechanical constraint, which could be enhanced by the extensive actin expression observed in the overlying theca layer. The theca-cell layer can expand in a regulated manner, as shown by the presence of mitoses and Ki67-positive cells.
In summary, we have shown that the early ovarian follicle provides a new model for studying the relationship between epithelial cell shape, attachment to the basal lamina and cell behaviour. Oocytes in primordial follicles are enveloped in flat cells that rarely divide. In response to an as yet unknown signal, the GCs cuboidalise and divide more frequently, reaching a maximal packing density on the basal lamina, such that cells are compelled to divide inwards to produce a second layer. We propose that the basal lamina, collagen fibrils and theca-cell layer provide mechanical constraint around the follicle to promote packing of the GCs on the basal lamina and the subsequent formation of multiple layers, while being able to expand in a regulated manner as the follicle grows. Thus, change in cell shape has a key role in initiation of follicle growth.
|
Materials and Methods |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
Ovaries were fixed in 10% buffered formalin (VWR International, Leicestershire, UK) for immunohistochemical or immuofluorescence analysis, or Bouin's fixative (Sigma-Aldrich Ltd., Poole, Dorset, UK) for morphological analysis. All ovaries were dehydrated, processed and embedded in paraffin before being serially sectioned at a thickness of 5 µm. Further ovaries were fixed in 4% paraformaldehyde, infiltrated with 30% sucrose and frozen in optimal cutting temperature (OCT) compound before cryostat sectioning.
Transmission electron microscopy
Ovaries were fixed for 24 hours in 3% v/v glutaraldehyde in 0.1 M cacodylate buffer (pH 7.2), post-fixed in 1% osmium tetroxide in cacodylate buffer for 1 hour and embedded in araldite. Ultrathin sections were stained in a saturated solution of uranyl acetate in 50% ethanol, followed by Reynold's lead citrate, and examined with a Philips CM10 electron microscope.
Immunohistochemistry for Ki67
Immunohistochemistry was performed as described recently (Stubbs et al., 2005), using a rabbit serum block. Sections were incubated with a monoclonal antibody against Ki67 (1:50, DakoCytomation Ltd., Ely, UK; M7249, clone TEC-3) in blocking solution overnight at 4°C, followed by a 1-hour incubation in a secondary biotinylated rabbit anti-rat antibody (1:200, DakoCytomation Ltd; E0468) at room temperature. Labelling was visualised as previously described (Stubbs et al., 2005). As a negative control the primary antibody was omitted.
Immunofluorescence for β-catenin, actin, Ki67 and MCM2
Dehydration and antigen retrieval of formalin-fixed sections were as described previously (Stubbs et al., 2005) before incubation with primary antibodies against either β-catenin (prediluted, Abcam, Cambridge, UK, ab15180) or a cocktail of Ki67 (as above) and MCM2 (1:100, Abcam; ab31159) overnight at 4°C, followed by a 1-hour incubation in a 1:200 dilution of appropriate secondary antibodies conjugated with either Alexa-Fluor-633 (Molecular Probes, Eugene, OR, USA) for detection of β-catenin, or a mixture of Alexa-Fluor-488 and Alexa-Fluor-555 (Molecular Probes) for the detection of Ki-67 and MCM-2, respectively. F-actin was localised in frozen sections by a 90-minute incubation in Alexa-Fluor-555 phalloidin (A34055, Molecular Probes). Following a brief (1-minute) wash in 1 µg/ml DAPI (Sigma-Aldrich) in water, slides were mounted with Prolong Gold antifade reagent with DAPI (Invitrogen, Paisley, UK) and analysed using a confocal laser-scanning microscope (Leica SP2).
Analysis of Ki67 immunolabelling
Slides were examined on an E600 microscope (NikonUK Ltd., Kingston-upon-Thames, UK) and digital images were captured with a DXM 1200 digital camera (Nikon) using the Lucia image analysis program (Nikon). Follicles were scored for developmental stage on the basis of GC shape and the number and completeness of GC layers, as follows: (1) primordial, with one layer of flattened pre-GCs; (2) transitional, where at least one but not all GCs were cuboidal; (3) primary, with one complete layer of cuboidal GCs; (4) primary plus, with an incomplete second layer of GCs; (5) secondary, with two complete layers of GCs and (6) secondary plus, with two complete layers overlying some of the oocyte and three or four layers over the rest (Fig. 1B).
Follicles containing an oocyte with a sharply demarcated nuclear membrane and/or nucleolus were considered to have been sectioned at their largest cross section (LCS) and were analysed in detail. Oocyte and follicle diameters were calculated from the mean of two perpendicular measurements made at the LCS, using Lucia (Nikon). Oocyte diameter excluded the zona pellucida. The boundary of the follicle was defined as the basement membrane, clearly visible as a delineation between the GCs and the surrounding stroma/theca (Fig. 1C).
Unilaminar follicles were scored for GC shape (flattened or cuboidal), number (number of GC nuclei) and Ki67-positivity (moderate or strong brown staining) in follicles at the microscope (x60 objective), while focusing up and down. Follicles with multiple layers of GCs were analysed from digital images. The proportion of Ki67-positive GCs determined the labelling index of the follicle. In a few (seven) follicles, the follicle boundary was not clear for the entire circumference, and in these cases the number of GCs was not counted. To quantify change in GC shape, the average GC height for each follicle was calculated by subtracting the oocyte radius from the follicle radius. GC height, therefore, included developing zona pellucida.
Packing density of GCs on basal lamina
To analyse packing density of GCs on the basal lamina, follicles were categorised as described above, but the primary plus category was subdivided into `new second layer', where follicles had between one and five GCs in the second layer, and `established second layer', where follicles had a second layer of more that five GCs, which was not yet complete. To estimate the packing density of GCs the circumference of the each follicle (which was considered to represent of the amount of basal lamina in the LCS) was calculated from the follicle diameter (
D). The number of GCs in contact with the basal lamina was counted, and the average `width' of GCs calculated (follicle circumference/number of GCs on basal lamina). In addition, the number of Ki67-positive GCs on the basal lamina was counted.
Orientation of mitoses
Bouin's-fixed ovaries were serially sectioned and mounted on slides. Every fifth slide was stained conventionally with haematoxylin and eosin. Every section was examined and digital images captured of follicles with GCs undergoing mitosis (x60 objective). In the majority of follicles, it was possible to classify the orientation of the mitotic spindle relative to the oocyte surface and basal lamina (perpendicular or parallel) from the orientation of either the metaphase plate or spindle itself, or the relative positions of separating chromatids at anaphase or telophase.
Statistical analysis
Statistical analysis of Ki67 staining of GC nuclei was carried out using Stata 10 for Macintosh (Stata Corporation, College Station, TX). The effect of both follicle stage and pup age on oocyte diameters, GC heights and the numbers of GCs in the LCS of follicles was analysed using ordinary regression (regress command), using robust standard errors with clustering by pup. This takes account of possible within-pup correlation in follicle development. Pair-wise comparisons (for example, comparison of oocyte diameter at the primordial stage between day 12 and day 21) were corrected for multiple comparisons by multiplying the P value by the number of comparisons made. A few groups were not normally distributed and significant differences were confirmed using non parametric analysis (Kruskal Wallis for multiple groups; if P<0.05, pair-wise comparisons were performed using the Mann-Whitney U test, again correcting for multiple comparisons).
Mean proportions of both Ki67-positive follicles (with one or more positive GCs) and Ki67-positive GCs at each stage of development and at each age were computed and compared using binomial regression (binreg command). For comparisons between proportions of follicles, confidence intervals and P values in different groups were computed using robust standard errors with clustering by pup. This takes account of possible within-pup correlation in Ki67 staining. For comparisons between proportions of GCs, confidence intervals and P values in different groups were computed using robust standard errors with clustering by follicles, thus taking into account possible within-follicle correlation of dividing cells in those follicles which have initiated growth. P values were corrected for multiple comparisons at each stage of follicle development.
When investigating the density of GCs on the basal lamina, the variance of the width of the GCs lying on the basal lamina was compared at each stage using Levene's robust test statistic for equality of variances (robvar command).
|
Acknowledgments |
|---|
|
Footnotes |
|---|
|
References |
|---|
|
TopSummaryIntroductionResultsDiscussionMaterials and MethodsReferences |
|---|
Albertini, D. F., Combelles, C. M., Benecchi, E. and Carabatsos, M. J. (2001). Cellular basis for paracrine regulation of ovarian follicle development. Reproduction 121, 647-653.[Abstract]
Berkholtz, C. B., Lai, B. E., Woodruff, T. K. and Shea, L. D. (2006a). Distribution of extracellular matrix proteins type I collagen, type IV collagen, fibronectin, and laminin in mouse folliculogenesis. Histochem. Cell Biol. 126, 583-592.[CrossRef][Medline]
Berkholtz, C. B., Shea, L. D. and Woodruff, T. K. (2006b). Extracellular matrix functions in follicle maturation. Semin. Reprod. Med. 24, 262-269.[CrossRef][Medline]
Berrier, A. L. and Yamada, K. M. (2007). Cell-matrix adhesion. J. Cell Physiol. 213, 565-573.[CrossRef][Medline]
Black, L. D., Allen, P. G., Morris, S. M., Stone, P. J. and Suki, B. (2008). Mechanical and failure properties of extracellular matrix sheets as a function of structural protein composition. Biophys. J. 94, 1916-1929.[CrossRef][Medline]
Boland, N. I. and Gosden, R. G. (1994). Clonal analysis of chimaeric mouse ovaries using DNA in situ hybridization. J. Reprod. Fertil. 100, 203-210.
Burns, K. H., Owens, G. E., Fernandez, J. M., Nilson, J. H. and Matzuk, M. M. (2002). Characterization of integrin expression in the mouse ovary. Biol. Reprod. 67, 743-751.
Chen, C. S., Mrksich, M., Huang, S., Whitesides, G. M. and Ingber, D. E. (1997). Geometric control of cell life and death. Science 276, 1425-1428.
Dong, J., Albertini, D. F., Nishimori, K., Kumar, T. R., Lu, N. and Matzuk, M. M. (1996). Growth differentiation factor-9 is required during early ovarian folliculogenesis. Nature 383, 531-535.[CrossRef][Medline]
Dullaart, J., Kent, J. and Ryle, M. (1975). Serum gonadotrophin concentrations in infantile female mice. J. Reprod. Fertil. 43, 189-192.
Durlinger, A. L., Gruijters, M. J., Kramer, P., Karels, B., Ingraham, H. A., Nachtigal, M. W., Uilenbroek, J. T., Grootegoed, J. A. and Themmen, A. P. (2002). Anti-Mullerian hormone inhibits initiation of primordial follicle growth in the mouse ovary. Endocrinology 143, 1076-1084.
Elvin, J. A., Clark, A. T., Wang, P., Wolfman, N. M. and Matzuk, M. M. (1999a). Paracrine actions of growth differentiation factor-9 in the mammalian ovary. Mol. Endocrinol. 13, 1035-1048.
Elvin, J. A., Yan, C., Wang, P., Nishimori, K. and Matzuk, M. M. (1999b). Molecular characterization of the follicle defects in the growth differentiation factor 9-deficient ovary. Mol. Endocrinol. 13, 1018-1034.
Eppig, J. J. (2001). Oocyte control of ovarian follicular development and function in mammals. Reproduction 122, 829-838.[Abstract]
Fair, T., Hulshof, S. C., Hyttel, P., Greve, T. and Boland, M. (1997). Oocyte ultrastructure in bovine primordial to early tertiary follicles. Anat. Embryol. 195, 327-336.[CrossRef][Medline]
Folkman, J. and Moscona, A. (1978). Role of cell shape in growth control. Nature 273, 345-349.[CrossRef][Medline]
Gaytan, F., Morales, C., Bellido, C., Aguilar, E. and Sanchez-Criado, J. E. (1996). Proliferative activity in the different ovarian compartments in cycling rats estimated by the 5-bromodeoxyuridine technique. Biol. Reprod. 54, 1356-1365.[Abstract]
Gilchrist, R. B., Ritter, L. J. and Armstrong, D. T. (2004a). Oocyte-somatic cell interactions during follicle development in mammals. Anim. Reprod. Sci. 82-83, 431-446.
Gilchrist, R. B., Ritter, L. J., Cranfield, M., Jeffery, L. A., Amato, F., Scott, S. J., Myllymaa, S., Kaivo-Oja, N., Lankinen, H., Mottershead, D. G. et al. (2004b). Immunoneutralization of growth differentiation factor 9 reveals it partially accounts for mouse oocyte mitogenic activity. Biol. Reprod. 71, 732-739.
Gougeon, A. and Busso, D. (2000). Morphologic and functional determinants of primordial and primary follicles in the monkey ovary. Mol. Cell. Endocrinol. 163, 33-42.[CrossRef][Medline]
Halpin, D. M., Jones, A., Fink, G. and Charlton, H. M. (1986). Postnatal ovarian follicle development in hypogonadal (hpg) and normal mice and associated changes in the hypothalamic-pituitary ovarian axis. J. Reprod. Fertil. 77, 287-296.
Hirshfield, A. N. (1985). Comparison of granulosa cell proliferation in small follicles of hypophysectomized, prepubertal, and mature rats. Biol. Reprod. 32, 979-987.[Abstract]
Hirshfield, A. N. (1989). Granulosa cell proliferation in very small follicles of cycling rats studied by long-term continuous tritiated-thymidine infusion. Biol. Reprod. 41, 309-316.[Abstract]
Hirshfield, A. N. (1991). Development of follicles in the mammalian ovary. Int. Rev. Cytol. 124, 43-101.[Medline]
Hosoyamada, Y. and Sakai, T. (2003). The ultrastructure of periductal connective tissue and distinctive populations of collagen fibrils associated with ductal epithelia of exocrine glands. Arch. Histol. Cytol. 66, 407-418.[CrossRef][Medline]
Huet, C., Pisselet, C., Mandon-Pepin, B., Monget, P. and Monniaux, D. (2001). Extracellular matrix regulates ovine granulosa cell survival, proliferation and steroidogenesis: relationships between cell shape and function. J. Endocrinol. 169, 347-360.[Abstract]
Hussein, T. S., Froiland, D. A., Amato, F., Thompson, J. G. and Gilchrist, R. B. (2005). Oocytes prevent cumulus cell apoptosis by maintaining a morphogenic paracrine gradient of bone morphogenetic proteins. J. Cell Sci. 118, 5257-5268.
Ingber, D. E. (2004). The mechanochemical basis of cell and tissue regulation. Mech. Chem. Biosyst. 1, 53-68.[Medline]
Kreeger, P. K., Fernandes, N. N., Woodruff, T. K. and Shea, L. D. (2005). Regulation of mouse follicle development by follicle-stimulating hormone in a three-dimensional in vitro culture system is dependent on follicle stage and dose. Biol. Reprod. 73, 942-950.
Laskey, R. (2005). The Croonian Lecture 2001 hunting the antisocial cancer cell: MCM proteins and their exploitation. Philos. Trans. R. Soc. Lond., B, Biol. Sci. 360, 1119-1132.
LeBleu, V. S., Macdonald, B. and Kalluri, R. (2007). Structure and function of basement membranes. Exp. Biol. Med. (Maywood) 232, 1121-1129.
Lechler, T. and Fuchs, E. (2005). Asymmetric cell divisions promote stratification and differentiation of mammalian skin. Nature 437, 275-280.[CrossRef][Medline]
Lundy, T., Smith, P., O'Connell, A., Hudson, N. L. and McNatty, K. P. (1999). Populations of granulosa cells in small follicles of the sheep ovary. J. Reprod. Fertil. 115, 251-262.
Matzuk, M. M. and Lamb, D. J. (2002). Genetic dissection of mammalian fertility pathways. Nat. Cell Biol. 4, S41-S49.[Medline]
Matzuk, M. M., Burns, K. H., Viveiros, M. M. and Eppig, J. J. (2002). Intercellular communication in the mammalian ovary: oocytes carry the conversation. Science 296, 2178-2180.
Meredith, S., Dudenhoeffer, G. and Jackson, K. (2000). Classification of small type B/C follicles as primordial follicles in mature rats. J. Reprod. Fertil. 119, 43-48.[Abstract]
Mizunuma, H., Liu, X., Andoh, K., Abe, Y., Kobayashi, J., Yamada, K., Yokota, H., Ibuki, Y. and Hasegawa, Y. (1999). Activin from secondary follicles causes small preantral follicles to remain dormant at the resting stage. Endocrinology 140, 37-42.
Monniaux, D., Huet-Calderwood, C., Le Bellego, F., Fabre, S., Monget, P. and Calderwood, D. A. (2006). Integrins in the ovary. Semin. Reprod. Med. 24, 251-261.[CrossRef][Medline]
O'Connell, C. B. and Wang, Y. L. (2000). Mammalian spindle orientation and position respond to changes in cell shape in a dynein-dependent fashion. Mol. Biol. Cell 11, 1765-1774.
O'Shaughnessy, P. J., Dudley, K. and Rajapaksha, W. R. (1996). Expression of follicle stimulating hormone-receptor mRNA during gonadal development. Mol. Cell. Endocrinol. 125, 169-175.[CrossRef][Medline]
O'Shaughnessy, P. J., McLelland, D. and McBride, M. W. (1997). Regulation of luteinizing hormone-receptor and follicle-stimulating hormone-receptor messenger ribonucleic acid levels during development in the neonatal mouse ovary. Biol. Reprod. 57, 602-608.[Abstract]
Oktay, K., Schenken, R. S. and Nelson, J. F. (1995). Proliferating cell nuclear antigen marks the initiation of follicular growth in the rat. Biol. Reprod. 53, 295-301.[Abstract]
Oktay, K., Karlikaya, G., Akman, O., Ojakian, G. K. and Oktay, M. (2000). Interaction of extracellular matrix and activin-A in the initiation of follicle growth in the mouse ovary. Biol. Reprod. 63, 457-461.
Pedersen, T. (1969). Follicle growth in the immature mouse ovary. Acta Endocrinol. 62, 117-132.
Picton, H. M. (2001). Activation of follicle development: the primordial follicle. Theriogenology 55, 1193-1210.[CrossRef][Medline]
Rodgers, R. J., Irving-Rodgers, H. F. and Russell, D. L. (2003). Extracellular matrix of the developing ovarian follicle. Reproduction 126, 415-424.[Abstract]
Roy, S. K. and Greenwald, G. S. (1989). Hormonal requirements for the growth and differentiation of hamster preantral follicles in long-term culture. J. Reprod. Fertil. 87, 103-114.
Stiff, M. E., Bronson, F. H. and Stetson, M. H. (1974). Plasma gonadotropins in prenatal and prepubertal female mice: disorganization of pubertal cycles in the absence of a male. Endocrinology 94, 492-496.
Stubbs, S. A., Hardy, K., Da Silva-Buttkus, P., Stark, J., Webber, L. J., Flanagan, A. M., Themmen, A. P., Visser, J. A., Groome, N. P. and Franks, S. (2005). Anti-mullerian hormone protein expression is reduced during the initial stages of follicle development in human polycystic ovaries. J. Clin. Endocrinol. Metab. 90, 5536-5543.
Stubbs, S. A., Stark, J., Dilworth, S. M., Franks, S. and Hardy, K. (2007). Abnormal preantral folliculogenesis in polycystic ovaries is associated with increased granulosa cell division. J. Clin. Endocrinol. Metab. 92, 4418-4426.
Thery, M. and Bornens, M. (2006). Cell shape and cell division. Curr. Opin. Cell Biol. 18, 648-657.[CrossRef][Medline]
Uda, M., Ottolenghi, C., Crisponi, L., Garcia, J. E., Deiana, M., Kimber, W., Forabosco, A., Cao, A., Schlessinger, D. and Pilia, G. (2004). Foxl2 disruption causes mouse ovarian failure by pervasive blockage of follicle development. Hum. Mol. Genet. 13, 1171-1181.
van Wezel, I. L., Krupa, M. and Rodgers, R. J. (1999). Development of the membrana granulosa of bovine antral follicles: structure, location of mitosis and pyknosis, and immunolocalization of involucrin and vimentin. Reprod. Fertil. Dev. 11, 37-48.[CrossRef][Medline]
Wandji, S. A., Srsen, V., Voss, A. K., Eppig, J. J. and Fortune, J. E. (1996). Initiation in vitro of growth of bovine primordial follicles. Biol. Reprod. 55, 942-948.[Abstract]
Wandji, S. A., Srsen, V., Nathanielsz, P. W., Eppig, J. J. and Fortune, J. E. (1997). Initiation of growth of baboon primordial follicles in vitro. Hum. Reprod. 12, 1993-2001.
Xu, M., West, E., Shea, L. D. and Woodruff, T. K. (2006). Identification of a stage-specific permissive in vitro culture environment for follicle growth and oocyte development. Biol. Reprod. 75, 916-923.
Zamboni, L. (1974). Fine morphology of the follicle wall and follicle cell-oocyte association. Biol. Reprod. 10, 125-149.[Abstract]
CiteULike 
Complore 
Connotea 
Del.icio.us 
Digg 
Reddit 
Technorati 
Twitter What's this?
Related articles in JCS:
This article has been cited by other articles:
|
|
 |
|
  P. Da Silva-Buttkus, G. S. Jayasooriya, J. M. Mora, M. Mobberley, T. A. Ryder, M. Baithun, J. Stark, S. Franks, and K. Hardy Effect of cell shape and packing density on granulosa cell proliferation and formation of multiple layers during early follicle development in the ovary Development, December 15, 2008; 135(24): e1 - e1. [Full Text]
|
|
| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
