university of groningen regulation of polarity …hepatocyte polarity development, we employed the...
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University of Groningen
Regulation of polarity development in hepatocytesWouden, Johanna Margaretha van der
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CHAPTER 3
Cell polarity development is controlled by sphinganine turnover, which modulates
membrane traffic via the cell-cycle regulatory p27kip1/CDK complex
Johanna M. van der Wouden1, Sven C.D. van IJzendoorn1, Delphine Théard and Dick
Hoekstra
Department of Membrane Cell Biology, Faculty of Medical Sciences,
University of Groningen, Groningen, the Netherlands
1These authors contributed equally to this work
part of this work has been submitted
Chapter 3
78
Abstract The molecular mechanisms that coordinate cell cycle control and cell
polarization are largely unknown. Sphingolipids play a crucial role in
both cell proliferation and polarization. Here, we demonstrate that
polarity-stimulating signaling cascades target dihydroceramide synthase
to reduce the level of free sphinganine. Sphinganine turnover, in turn,
modulates polarized endosomal membrane traffic via p27Kip1 and cyclin-
dependent kinase to control cell polarity development. Our data reveal a
novel mechanism that couples polarized membrane traffic and the
biogenesis of apical plasma membrane domains to the regulation of cell
cycle proteins in response to signaling-modulated sphingolipid
metabolism.
Chapter 3
79
Introduction Epithelial cell polarity depends on the structural asymmetry of apical and
basolateral membrane domains. Its establishment and maintenance
requires a careful orchestration of extra- and intracellular signals,
triggering crucial organelle- and membrane traffic-linked machineries, as
partly elucidated in systems as diverse as yeast, Drosophila and
mammalian cells. Impairment of these events may cause a loss of apical-
basolateral asymmetry and lead to deranged cell growth (Bilder et al.,
2000). Epithelial polarisation preferentially occurs during G1/G0 cell
cycle arrest. However, intracellular signal cascades that control
polarisation in response to cell cycle regulation are unknown.
Hepatocytes, like all epithelia, display distinct apical, bile canalicular (BC)
and basolateral, sinusoidal plasma membrane (PM) domains. Some of the
intracellular sites and molecular components of the mechanisms that
contribute to apical BC biogenesis in hepatocytes have been clarified.
These include E-cadherin (Matsui et al., 2002), protein kinase PK)A and
PKC activities (Zegers et al., 1998), and the sorting of specific
sphingolipids and proteins, mediated by the Golgi and endosomal
recycling system (Maier et la., 2002; Aït Slimane et al., 2002; Zegers and
Hoekstra, 1997). In particular the subapical compartment (SAC), the
hepatocyte equivalent of the common endosome in other epithelia, plays a
central role in polarized lipid and protein trafficking (van IJzendoorn et
al., 1998; Rahner et al., 2002; Wustner et al., 2001), and appears a target
for signals that promote apical-basolateral asymmetry (van IJzendoorn
and Hoekstra, 1999; van IJzendoorn et al., 2000).
Sphingolipids, together with cholesterol, cluster to form particularly
ordered membrane environments or rafts, in which apical proteins
and/or signal transduction molecules are co-assembled (Ait Slimane et
al., 2003; Simons and Ikonen, 1997). Therefore, the lateral dynamics and
organization of sphingolipids may play a prominent role in the regulation
of signalling cascades and cell polarity (Holthuis et al., 2001). Indeed, the
sphingoid base backbones of sphingolipids, i.e. sphingosine and
Chapter 3
80
sphinganine (dihydro-sphingosine), appear highly bioactive compounds
that may function as signalling molecules in the regulation of cell
proliferation, apoptosis, differentiation and membrane traffic (Shayman,
2000; Hannun et al., 2001; Friant et al., 2001). Not surprisingly,
alterations in the cellular levels of free sphingoid bases have been
implicated in various diseases, including hepatocellular carcinogenesis
(Spiegel and Merrill, 1996), which arises from dedifferentiation of mature
hepatocytes (Bralet et al., 2002; Gournay et al., 2002). However, no data
are available as to the involvement of free sphingoid bases in cell
polarisation. Here, we demonstrate for the first time that the sphingolipid
metabolite sphinganine controls membrane polarity development by
interfering with the regulation of cell cycle control via the cyclin-
dependent kinase inhibitor p27kip1.
Results Sphinganine Accumulation Blocks Polarity Development
To examine the involvement of sphingolipid metabolites in the process of
hepatocyte polarity development, we employed the mycotoxin fumonisin
B1 (FB1), which specifically inhibits dihydroceramide (DHC) synthase
activity in the sphingolipid biosynthetic pathway (Fig. 1a). As anticipated,
treatment of well-differentiated hepatoma HepG2 cells with FB1 resulted
in decreased levels of ceramides and complex sphingolipids and,
consequently, increased levels of the sphingoid bases sphinganine (SA)
and phyto-SA (Fig. 1b; Merrill, 1996). In order to examine potential
consequences on HepG2 cell polarity development, i.e. the biogenesis of
apical BC, cells were plated on coverslips in the presence of 0-30 µM FB1.
Each day a coverslip was taken and the ratio BC/100 cells was
determined as a measure for cell polarity (van IJzendoorn and Hoekstra,
2000). Control HepG2 cells rapidly acquired polarity reaching a
maximum ratio BC/100 cells 2 days after plating (Fig. 1c). By contrast,
cells grown in the presence of FB1 showed a dramatic inhibition of the
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Figure 1: Accummulation of SA inhibits HepG2 cell polarity development. (a) Scheme of the sphingolipid metabolic pathway and sites of action of distinct
sphingolipid synthesis inhibitors. (b) Effect of FB1 on sphingolipid profiles. Note
the decrease in ceramides and glycosphingolipids (circles) and the appearance of
free sphingoid bases (arrows) in FB1-treated cells. (c-f) Effect of 0-30 µM FB1
(c), 30 µM FB1 + 10 µM C6-DHC (e), or 0.5-2.0 µM SA (f) on cell polarity
development. (d) Fluorescence microscopical evaluation of cell polarity in control
or FB1-treated cells (nuclei in blue and BC in red). Note the absence of BC in
FB1-treated cultures. Bars 5 µm; * p<0.05 (student t-test).
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82
formation of BC in a dose-dependent manner, resulting in a reduction of
the number of polarised cells by ~75 % 2 d after plating (Fig. 1c,d).With
the concentrations of FB1 used, we did not observe significant effects on
cell viability (trypan blue exclusion; not shown), or overall morphology,
including cell attachment and spreading. Importantly, polarity
development was not restored when FB1-treated cells were replenished
with 10 µM C6-DHC (Fig. 1e) or short-chain ceramide (not shown). This
suggests that the accumulation of SA, rather than the inhibition of de
novo synthesis of ceramides and/or complex sphingolipids, was
responsible for the observed impediment of cell polarity development.
Indeed, the addition of 0.5-2.0 µM SA upon plating the cells inhibited
HepG2 cell polarity development in a dose-dependent manner (Fig. 1f),
thereby closely mimicking the effect of FB1 (Fig. 1c). Taken together, the
data suggest that SA accumulation inhibits the establishment of HepG2
cell polarity.
Sphinganine Turnover Promotes Polarity Development
To obtain further support for a direct correlation between SA level and
cell polarisation, we next investigated whether decreased levels of this
sphingolipid metabolite also affect cell polarity development. A specific
inhibitor of serine palmitoyltransferase, L-cycloserine (LCS) inhibits SA
biosynthesis (Fig. 1a). Treatment of HepG2 cells with 250 µM LCS, similar
to FB1, resulted in decreased levels of ceramides and complex
sphingolipids but, unlike FB1 (cf. Fig.1b), did not give rise to increased
levels of sphingoid bases (Fig. 2a). Rather, it is fair to conclude that the
amount of free sphingoid bases was also reduced, albeit below our
detection level. Interestingly however, in striking contrast to the effect of
FB1, LCS enhanced cell polarity development, in terms of both kinetics
and maximum polarity, evidenced by the steep increase of the number
(Fig. 2b), as well as the size (Fig. 2c) of the BCs. Similar results were
obtained with another specific inhibitor of serine palmitoyltransferase,
ISP-1/myriocin (unpublished data). The opposing effects of LCS and FB1
on polarity development, under the experimental conditions used, point
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Figure 2: LCS promotes HepG2 cell polarity development. (a) Effect of LCS
on sphingolipid profiles. Note the decrease in ceramides, glycosphingolipids and
sphingomyelin in LCS-treated cells (circles). (b,d) Effect of 50-250 µM LCS (b),
250 µM LCS + 10 µM C6-DHC (d), or 250 µM LCS + 0.5-2.0 µM SA (d) on cell
polarity development. (c) Fluorescence microscopical evaluation of cell polarity
in control or FB1-treated cells (nuclei in blue and BC in red). Note the increase
in BC circumference in LCS-treated cells. Bars 5 µm; * p<0.05 (student t-test).
to SA turnover, rather than to decreased levels of (dihydro)ceramide
and/or complex sphingolipids as a crucial parameter in polarity
development, a decrease promoting and an increase inhibiting polarity
development. Indeed, the polarity-stimulating effect of LCS treatment was
completely abolished in the presence of increasing concentrations of
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84
exogenous SA (Fig. 2d), whereas exogenous C6-DHC (Fig. 2d) or short-
chain ceramide were without effect (not shown).
Because these data indicate that the establishment of HepG2 cell polarity
is critically dependent on the level of SA, we next investigated whether
DHC synthase, the predominant enzyme in SA turnover, functions as a
target for cellular signals that contribute to polarity development. For
this, we took into account our previous observation that the stable cAMP
analog dibutyryl cAMP (dbcAMP), via activation of PKA, stimulates HepG2
cell polarity development (Zegers and Hoekstra, 1997; van IJzendoorn
and Hoekstra, 2000a, 2000b). Control and dbcAMP-treated HepG2 cells
were broken, and incubated with 3H-SA and stearyl CoA. The activity of
DHC synthase was significantly upregulated in dbcAMP-treated cells
(approx. 1.5-fold), as evidenced by the increased production of
radiolabeled (dihydro)ceramide, whereas treatment with FB1 blocked the
activity of the enzyme (Fig. 3a). Importantly, dbcAMP failed to stimulate
polarity development in DHC synthase-inhibited or SA-treated cells (Fig.
3b). We conclude that alterations in the pool of free SA, regulated by
signal-mediated mediated modulation of acyl CoA-dependent DHC
synthase activity is a crucial parameter in cAMP/PKA-stimulated HepG2
cell polarity development.
Figure 3: (a) dbcAMP stimulates FB1-
sensitive acyl-CoA-dependent DHC
synthase activity. (b) Increased levels of free
SA block dbcAMP-stimulated polarity
development in HepG2 cells.
Chapter 3
85
Sphinganine Interferes with Polarised Membrane Traffic, exiting
from SAC
cAMP/PKA activity is required for HepG2 cell polarity development (van
IJzendoorn and Hoekstra 2000b) and, moreover, mediates the
stimulating effects of interleukin-6 family cytokines on BC biogenesis
(van der Wouden et al., 2002). We previously identified a specific BC
(apical PM)-directed traffic pathway originating from the subapical
compartment (SAC) in HepG2 cells as a primary target for cAMP/PKA
signalling (van IJzendoorn and Hoekstra, 1999; van IJzendoorn et al.,
2000). Thus, cAMP/PKA activates a specific SAC-to-BC vesicular traffic
route, which is followed by distinct, fluorescently labelled lipids including
sphingomyelin (van IJzendoorn and Hoekstra, 1999; van IJzendoorn et
al., 2000) and galactosylceramide (GalCer; Fig. 4). Inhibition of this route
effectively prohibits polarity development (van IJzendoorn and Hoekstra,
2000a). Since the accumulation of SA prevented dbcAMP-stimulated
development of HepG2 cell polarity (Fig. 4b), we next investigated whether
the observed effect was directly correlated with a frustration of
cAMP/PKA signaling to redirect and stimulate SAC-to-BC membrane
trafficking.
To this end, cells were pretreated with FB1, SA or buffer, and SAC was
preloaded with fluorescent GalCer as described in detail elsewhere (van
IJzendoorn and Hoekstra 2000a, 2000b; van der Wouden et al., 2002).
Cells were subsequently treated with dbcAMP or buffer at 4 ºC, warmed
to 37ºC, and lipid flow from SAC to either apical (BC) or basolateral
membrane was followed for 20 min. In control cells, C6NBD-GalCer
disappeared during this time interval from the bile canalicular pole (BCP),
which constitutes SAC (where the lipid is located at t=0) and BC. Indeed,
the percentage of BCP that contained C6NBD-GalCer decreased in time
(Fig. 4a: 1, 2). The relative distribution of the lipid analogue in the
remaining, faintly-labeled C6NBD-GalCer-positive BCP shows that the
probe predominantly resided in SAC and little if any movement from SAC
to BC could be detected (Fig. 4b and c: 1, 2). Rather, these data indicate
Chapter 3
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Figure 4: FB1 interferes with polarized membrane trafficking from SAC. SAC of control (a-c: 1-3) or FB1-treated (a-c: 4, 5) HepG2 cells were preloaded
with C6NBD-GalCer, as described in detail elsewhere (van Ijzendoorn and
Hoekstra, 2000a, 2000b; van der Wouden et al., 2002). Following a subsequent
chase, the percentage of C6NBD-GalCer positive BCP, comprising BC and/or
SAC, was determined (a), as well as the corresponding relative distribution of
the fluorescent probe in the BCP, i.e., in BC, SAC or both (BC+SAC) (b). 1.
Before the chase (t=o); 2. 20 min chase in Hank’s balanced salt solution (HBSS)
(control cells) ; 3. 20 min chase in HBSS + 1 mM dbcAMP (control cells); 4, 20
min chase in HBSS + 1 mM dbcAMP (FB1-treated cells); 5. 20 min chase in
HBSS + 1 mM dbcAMP + 5 µM roscovitine (FB1-treated cells). Data are
expressed as mean +/- SD of at least three independent experiments carried out
in duplicate. (c) Illustrative images showing the distribution of the fluorescent
probe in the BCP (i.e. BC alone, BC+SAC, or SAC alone). Asterisks: BC; arrows:
SAC. Lower panels are phase contrast images to upper panels. Bars 5 µm.
Chapter 3
87
that the probe was transported from SAC to the basolateral domain of the
cells, consistent with previous observations (van IJzendoorn and
Hoekstra, 2000a, 2000b). By contrast, in dbcAMP-treated cells, C6NBD-
GalCer remained associated with the BCP region during the 20 min
chase, as evidenced by the unchanged percentage of BCP that contained
C6NBD-GalCer (Fig. 4a: 1, 3). Analysis of the corresponding relative
distribution of the probe in the BCP reveals a flow of the lipid analogue
from SAC to BC (Fig. 4b and c: 1, 3; cf. van IJzendoorn and Hoekstra,
2000a, 2000b; van der Wouden et al., 2002). In striking contrast,
dbcAMP failed to target C6NBD-GalCer from SAC to BC in cells in which
SA turnover was inhibited (Fig. 4b and c: 1, 4), but not in cells pretreated
with LCS, in which the SA levels are decreased (unpublished data, cf.
fig.4 1 vs 3). Thus, in cells with elevated SA levels, C6NBD-GalCer
remained associated with the BCP during the 20 min chase (Fig. 4a: 1, 4),
and analysis of the relative distribution of the lipid analogue in the
labeled BCP revealed that most C6NBD-GalCer localized to SAC (Fig. 4b
and c: 1, 4), indicating entrapment of the lipid in SAC. These data
strongly suggest that the turnover of SA is a prerequisite for cAMP/PKA
signaling to redirect polarized membrane traffic from SAC and, in this
way, to stimulate polarity development.
Sphinganine Modulates Transport and Polarity Development Via
p27Kip1/CDK
Both cAMP/PKA signaling and sphingoid bases have been implicated in
cell growth control. Indeed, as shown by BrdU incorporation (Fig. 5a), in
time, cell polarity-stimulating (db)cAMP/ PKA signaling delayed G1-S-
phase transition of HepG2 cells. By contrast, the inhibition of SA
turnover stimulated S-phase entry. Entry of cells into S-phase is typically
regulated by the concerted action of cyclin-dependent kinase (CDK) and
its functional inhibitor p27kip1. During the establishment of HepG2 cell
polarity (0-48 h), p27kip1 expression increased, while under dbcAMP/PKA-
mediated polarity promoting conditions its expression was strongly
enhanced (Fig. 5b). It has been reported that elevated p27kip1 levels in
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Figure 5: Effect of dbcAMP and SA on cell cycle. (a) dbcAMP and FB1 inhibit
and advance S-phase entry, as evidenced by the number of cell that had
incorporated BrdU. (b) Time-dependent expression of p27kip1 in control and
dbcAMP-treated cells. (c) Effect of FB1 on p27kip1 expression. (d) Roscovitine
restores the ability of dbcAMP to stimulate polarity development in FB1-treated
cells. Error bars represent SD of at least three independent experiments carried
out in duplicate.
HepG2 cells delay S-phase entry causing cell cycle arrest in G1 (Klausen
et al., 2000), and its role in the differentiation of a variety of epithelial
cells has been proposed (Quaroni et al., 2001; Boriello et al., 2000;
Deschênes et al., 2001). In contrast, reduced p27kip1 levels, which is
accompanied by increased CDK activity (Li et al., 2002), play a critical
role in the pathogenesis of many human cancers, including
hepatocellular carcinogenesis, which arises from dedifferentiation of
hepatocytes. In order to investigate whether the accumulation of free SA
affects these cell cycle regulatory proteins and, hence, their interference
with HepG2 cell polarity development, we first examined the effect of SA
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on the expression of p27kip1. As shown in Fig. 5c, inhibition of SA
turnover dramatically reduced p27kip1 expression by ~75 %, which could
not be restored by the exogenous addition of C6-DHC (unpublished data),
thus implicating a direct role of free sphingoid base accumulation. Note
that the reduced expression of p27kip1 is in agreement with the observed
stimulatory effect of free SA on S-phase entry (c.f. Fig. 5a). In order to
examine the involvement of CDK activity as a downstream effector of
p27kip1, we next tested the effect of roscovitine, a specific CDK inhibitor,
on the ability of dbcAMP/PKA to stimulate apical PM-directed traffic and
polarity development in DHC synthase-inhibited cells. We observed that
direct short-term inhibition of CDK activity in HepG2 cells with
roscovitine, thereby antagonizing the effect of down-regulated p27kip1
levels in FB1-treated cells, restored the ability of dbcAMP/PKA signaling
to reactivate C6NBD-GalCer trafficking from SAC and to promote its
targeting to BC (Fig. 4b and c: 1, 5). Indeed, the percentage of C6NBD-
GalCer-labeled BCP remained constant during the chase (Fig. 4a: 1, 5),
and analysis of the relative distribution of the probe in the labeled BCP
clearly revealed a flow of the lipid analogue from SAC to BC (Fig. 4b and
c: 1, 5). Importantly, short-term inhibition of CDK activity by roscovitine
also restored the ability of dbcAMP to stimulate polarity development,
despite an inhibition of DHC synthase activity (Fig. 4c). Together, these
data indicate that SA-controlled modulation of the expression and activity
of the cell cycle proteins p27kip1 and CDK interferes with the regulation of
apical membrane traffic from SAC and, hence, polarity development.
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Discussion Cell cycle control and cell polarization are key issues in tissue
development, and resolving the mechanism that co-ordinates these
events is a fundamental challenge in developmental and cell biology.
Thus, while epithelial cells preferentially differentiate and acquire a
polarized phenotype during G1 phase arrest, a loss of epithelial
architecture, i.e. PM depolarization, often occurs during carcinogenesis,
when cell cycle progression is deregulated (Bilder and Perrimon, 2000;
Wodarz, 2000). Here, a novel mechanism is described, identifying at the
molecular level a link between the regulation of sphingolipid metabolism,
cell cycle control and cell polarization, as expressed by biogenesis of the
apical membrane domain, triggered by membrane trafficking from the
subapical compartment, SAC (van IJzendoorn and Hoekstra, 1999; van
IJzendoorn et al., 2000). Moreover, the stimulatory effect of the
cAMP/PKA signaling pathway on cell polarity development (Zegers and
Hoekstra, 1997; van IJzendoorn and Hoekstra, 2000b) includes a cell
cycle control modulation, exerted via controlling the turnover of the
sphingolipid metabolite, sphinganine. The inability to maintain high
p27kip1 levels and to suppress CDK activity precludes the establishment
of an epithelial phenotype, which can be attributed to an inhibitory effect
of CDK activity on cAMP/PKA-stimulated, apical PM directed trafficking
from SAC (Fig. 6). These data also support a role for CDK in endosome
dynamics, as previously reported (Vergès et al., 1997; Gaulin et al., 2000;
Tuomikoski et al., 1989).
Intriguingly, also yeast cell polarization is tightly regulated in the cell
cycle and involves CDK (Madden and Snyder, 1998), the activity of which
is linked to Sic1p (yeast counterpart of p27kip1) and Rho1p (Drgonova et
al., 1999). Furthermore CDK activity plays a crucial role in maintaining
the polarized localization of apical components during mitosis in
Drosophila neuroblasts, which is required for asymmetric cell division
(Tio et al., 2001). In fact, a striking parallel exists between the
mechanisms that control asymmetric division in neuroblasts, and
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Figure 6: Working model for the functional integration of cAMP/PKA signalling, sphingolipid metabolism, cell cycle control, membrane traffic and cell polarity. (see text for explanation)
polarity as established in epithelial cells (Wodarz et al., 2001). Given its
functioning in cellular systems ranging from yeast and Drosophila
neuroblasts to polarized hepatocytes, it is tempting to suggest that as a
general molecular principle, CDK and its regulators may link cell cycle
control to the generation and/or maintenance of the asymmetric, apical
localization of molecules.
DHC synthase-controlled SA turnover appears a key event in cAMP/PKA-
modulated expression and activity of p27kip1 and CDK, membrane traffic,
and the establishment of polarity, all of which appear intimately
connected. The molecular mechanism by which cAMP/PKA signaling
increases DHC synthase activity remains to be investigated. Possibly, PKA
directly phosphorylates DHC synthase or, alternatively, may affect its
localization, as demonstrated for other ER/Golgi enzymes, thus affecting
substrate clearance. A diminished DHC synthase activity, as observed in
FB1-treated cells results in a diminished expression of p27kip1. Possibly,
high levels of free SA promote p27kip1 degradation, similar to the protein
degradation-promoting activities of sphingoid bases in yeast (Chung et
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al., 2000). Decreased p27kip1 levels prevent the downregulation of CDK
activity, which leads to G1-phase shortening and S-phase advance,
typically observed in many cancers. It is of interest to note that the
longevity-assurance gene (LAG1) in yeast encodes an essential component
of the acyl-CoA-dependent, FB1-sensitive DHC synthase (Schorling et al.,
2001). Deletion of LAG1 extends life span, i.e. increases the number of
times an individual yeast cell divides before it polarizes to form a bud
(Jazwinski and Conzelmann, 2002). Moreover, overexpression of LAG1
mediates resistance to FB1 and a human homologue of LAG1, LASS2,
inhibits colony formation of human hepatocellular carcinoma cells,
suggesting a role for LAG1/LASS2 in regulating cell growth (Pan et al.,
2001). Our data also support and provide a mechanism for the
observation that FB1 stimulates DNA synthesis, i.e., via accumulation of
sphingoid bases, in this manner displaying mitogenic activity (Schroeder
et al., 1994; Merrill et al., 2001). Moreover, the perturbing effects of SA on
cell cycle proteins such as p27kip1 and CDK and, consequently, on apical
membrane traffic and the establishment of epithelial architecture, as
shown here, provide a molecular mechanism by which the non-genotoxic
mycotoxin FB1 exerts its (pre)neoplastic hepatocarcinogenic effects
(Gelderblom et al., 2001).
Methods De novo sphingolipid biosynthesis
Control, FB1-, or LCS-treated HepG2 cells were labeled with 14C-serine, scraped
and sphingolipid profiles were determined by thin-layer chromotography (TLC)
and autoradiography as described (Veldman et al., 1998).
Determination of HepG2 cell polarity development
HepG2 cell polarity development was determined by fluorescent microscopical
(Olympus AX70) analysis of the ratio BC/100 cells as described (van IJzendoorn
and Hoekstra, 2000a, 2000b). Data are expressed as mean +/- SD of at least
three independent experiments, carried out in duplicate.
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DHC synthase assay
Cells, control and treated with dbcAMP for 30 min, were scraped, and
homogenized in sucrose buffer by sonication. DHC synthase activity was
measured using 3H-SA and stearyl-CoA as substrate in the presence or absence
of FB1. Lipids were extracted with CHCl3/methanol and separated by TLC.
Radiolabeled SA and (dihydro)ceramide were scraped from the TLC plates and
quantified in a liquid scintilation counter (Veldman et al., 1998). Data are
expressed as percentage of control and standardised to protein content.
Determination of p27kip1 expression
Control cells and cells treated with FB1 for 3 days were scraped. Proteins from
whole cell lysates were separated by SDS-PAGE and transferred to PVDF
membranes (van der Wouden et al., 2002). PVDF membranes were probed
sequentially with monoclonal anti-p27kip1 antibodies (Transduction Laboratories)
and HRP-conjugated secondary antibodies (Amersham). p27kip1 was visualised
by ECL and quantified using Scion Image software.
Acknowledgments S.v.IJ. is supported by the Royal Dutch Academy of Sciences (KNAW). We thank Karin
Klappe for help with the DHC synthase assay.
94