Effect of sulphur mustard on human skin cell lines with differential agent sensitivity
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Transcript of Effect of sulphur mustard on human skin cell lines with differential agent sensitivity
SULPHUR MUSTARD EFFECTS ON HUMAN SKIN CELLS 115
© Crown copyright 2005. Reproduced with the permission of HMSO. J. Appl. Toxicol. 2005; 25: 115–128
JOURNAL OF APPLIED TOXICOLOGYJ. Appl. Toxicol. 2005; 25: 115–128Published online 2 March 2005 in Wiley InterScience (www.interscience.wiley.com). DOI: 10.1002/jat.1044
Effect of sulphur mustard on human skin cell lines withdifferential agent sensitivity
Rachel Simpson and Christopher D. Lindsay*
Biomedical Sciences Department, Dstl Porton Down, Salisbury, Wiltshire SP4 0JQ, UK
Received 27 April 2004; Revised 6 September 2004; Accepted 13 September 2004
ABSTRACT: The ability of sulphur mustard (HD) to induce DNA damage places limits on the efficacy of approaches
aimed at protecting human cells from the cytotoxic effects of HD using a variety of protective agents such as thiol-
containing esters and protease inhibitors. In the present study, potential alternative strategies were investigated by examin-
ing the differential effects of HD on G361, SVK14, HaCaT and NCTC 2544 human skin cells.
The G361 cell line was more resistant to the cytotoxic effects of HD than the NCTC, HaCaT and SVK14 cell lines at
HD doses of >>>>>3 and <<<<<100 µµµµµM HD as determined by the MTT assay. At 72 h after exposure to 60 µµµµµM HD there was up
to an 8.8-fold difference (P <<<<< 0.0001) between G361 and SVK14 cell culture viability. Buthionine sulphoximine (BSO)
pretreatment increased the sensitivity of all four cell lines to HD. A substantial proportion of the resistance of G361 cells
to HD was attributable to BSO-mediated effects on antioxidant-mediated metabolism, although G361 cultures still retained
a high degree of viability at 30 µµµµµM HD following BSO pretreatment. Cell cycle analysis confirmed that SVK14 cells were
relatively more sensitive to HD, as shown by the 2.1-fold reduction (P <<<<< 0.0001) in the percentage of cells in G0/G1 phase
24 h after HD exposure compared with control cultures. This compared well with a 1.2-fold increase (P <<<<< 0.05) in the
percentage of G361 cells in G0/G1 phase following HD exposure, suggesting the existence of a more efficient G0/G1 check-
point control mechanism in this cell line. Manipulation of the cell cycle using various modulating agents did not increase
the resistance of cell lines to the cytotoxic effects of HD. © Crown copyright 2005. Reproduced with the permission of Her
Majesty’s Stationery Office Published in 2005 by John Wiley & Sons, Ltd.
KEY WORDS: sulphur mustard; human skin; viability; cell cycle; buthionine sulphoximine
* Correspondence to: C. D. Lindsay, Biomedical Sciences Department, Dstl
Porton Down, Salisbury, Wiltshire SP4 0JQ, UK.
E-mail: [email protected]
© Crown Copyright 2004, Dstl
the alkylating effects of HD on the DNA of skin cells,
metabolic processes and connective tissue components
that are involved in skin regeneration and healing re-
sponses (Rice and Brown, 1999; Naghii, 2002).
The effect of HD on cells that are rapidly dividing is
particularly severe (Maynard, 1987). This may be due to
the formation of irreparable DNA cross-links (Murnane
and Byfield, 1981). According to Erickson et al. (1980),
cells that are highly sensitive to alkylating agents contain
a relatively higher proportion of DNA cross-links than
cells that are less sensitive, suggesting differences in
DNA repair efficiency. The position of a cell in the cell
cycle at the time of exposure to an alkylating agent
also may be important because mitotically active human
epidermal keratinocytes in culture are particularly sensi-
tive when they are in the S-phase of the cell cycle (Smith
et al., 1991).
Previous work suggests that increased resistance to HD
may be associated with elevated levels of proliferating
cell nuclear antigen (PCNA) (Smith et al., 2001), an ac-
cessory factor for DNA polymerase-δ and -ε in DNA
mismatch repair (Wood and Shivjii, 1997). The PCNA
also plays an essential role in nucleotide excision repair
(Miura et al., 1996; Tomkinson and Mackey, 1998).
Nucleotide excision repair is a DNA repair pathway that
utilizes DNA polymerase-δ or -ε to resynthesize bases
removed in the repair of pyrimidine dimers and other
Introduction
The chemical warfare agent sulphur mustard (HD) was
first used as a chemical weapon during World War I at
Ypres in 1917 (Haber, 1986). Sulphur mustard is a potent
vesicant and exposure to this agent may cause temporary
or permanent incapacitation. Within tissues, HD forms
irreversible covalent bonds with a variety of nucleophilic
groups, especially the genetic bases of DNA (Fox and
Scott, 1980; Klassen et al., 1986). The mono- and
bifunctional cross-links that HD forms with DNA results
in mitosis inhibition and death of the cell (Brooks and
Lawley, 1963). Sulphur mustard is bound rapidly by the
skin where it exerts cytotoxic effects predominantly upon
the mitotically active basal keratinocytes (Vogt et al.,
1984). However, the mechanism behind this and subse-
quent vesication is poorly understood. Recent work has
shown that, in vivo, epidermal melanocytes are the most
susceptible cell type in the dermo-epidermal region and
the severity of the lesion is related to skin type (Brown
and Rice, 1997). Sulphur mustard lesions typically take
many weeks or months to heal, and this may be due to
116 R. SIMPSON AND C. D. LINDSAY
Published in 2005 by John Wiley & Sons, Ltd. J. Appl. Toxicol. 2005; 25: 115–128
bulky DNA adducts (Wood and Shivjii, 1997) formed
by benzo[a]pyrene and nitrogen mustards (Smith and
Seo, 2002). According to Sparfel et al. (2002), nucleotide
excision repair is the major pathway for elimination
of DNA adducts formed by chemical carcinogens. This
indicates that it may be important also in the repair of
bulky lesions induced by HD. Previous reports have sug-
gested that the capacity of HD to induce DNA damage
places limits on the efficacy of approaches aimed at pro-
tecting human cells from the cytotoxic effects of HD
using scavenging agents such as hexamethylenetetramine
(Lindsay and Hambrook, 1997; Smith et al., 1997;
Andrew and Lindsay, 1998a), mono-isopropylglutathione
(Lindsay et al., 1997; Andrew and Lindsay, 1998b) and
di-isopropylglutathione (Lindsay and Hambrook, 1998).
In addition, the use of protease inhibitors such as E64
and mafenide hydrochloride (Lindsay et al., 1996) has
been shown to prevent dermo-epidermal separation in
human skin explants exposed to HD but did not prevent
the degradation of basal epidermal keratinocytes.
This report describes the differential effects of HD
on four human skin-derived cell lines: G361 malignant
melanoma cells, SVK14 cells (SV40 virus transformed
keratinocytes) and two spontaneously transformed kerat-
inocyte cell lines HaCaT and NCTC 2544; biochemical
assays were used to assess viability following HD
exposure and the consequences of inhibiting glutathione-
based antioxidant metabolism on sensitivity to HD.
Flow cytometry was used to determine the effect of HD
on cell cycle profiles of two cell lines with differential
sensitivity to HD. The effects of cell cycle inhibitors
on SVK14 and G361 cultures were determined further to
assess the therapeutic potential of modulating the cell
cycle on the cytotoxic effects of HD. The aim of the
present study was to determine if approaches based on
controlling cell cycle processes in human cells had thera-
peutic potential for enhancing the slow healing nature of
HD lesions.
Materials and Methods
Materials
Sulphur mustard was obtained from the Detection Depart-
ment, Dstl, Porton Down. The cell cycle profiles were
determined in cells treated with propidium iodide as
described in the DNA-Prep Coulter Reagents assay
kit (Beckman Coulter UK, High Wycombe). The cell
cycle inhibitors acyclovir, aphidicolin, olomoucine,
rapamycin, staurosporine and trichostatin were obtained
from Calbiochem (Merck Biosciences, Nottingham, UK).
Protein determinations were carried out using the Micro
BCA™ protein assay reagent kit (Pierce, Perbio Science
UK, Cheshire). All other chemicals were supplied by
Sigma-Aldrich (Poole, UK).
Cell Culture
The SVK14 human epidermal keratinocyte cell line (from
Dr Taylor-Papadimitriou, Imperial Cancer Research Fund,
London, UK) and the G361 human melanoma cell line
(European Collection of Cell Cultures, Health Protection
Agency, Porton Down, Salisbury, UK) were used for
these studies. The HaCaT and NCTC 2544 (hereafter
referred to as NCTC) cell lines were supplied by the
Biomedical Research Centre, Dundee, UK. The SVK14
and G361 cell lines were grown in a medium of 82%
(v/v) Dulbecco’s modified Eagle medium (DMEM) and
17% (v/v) foetal calf serum (FCS), containing 80 IU ml−1
penicillin, 80 µg ml−1 streptomycin, 1% non-essential
amino acids and 2 mM glutamine (hereafter referred to as
DMEM medium). The HaCaT cell line was grown in a
medium of DMEM, 10% (v/v) FCS, 100 IU ml−1 penicil-
lin, 100 µg ml−1 streptomycin and 2 mM glutamine (here-
after referred to as HaCaT medium). The NCTC cell
line was grown in a medium comprised of M199
medium and 10% (v/v) FCS, containing the same
antibiotics as for the HaCaT line and 2 mM glutamine
(hereafter referred to as NCTC medium). The cultures
were maintained at 37 °C in a humidified atmosphere
of 5% CO2–95% air.
The cells were grown in 150 cm2 flasks. Prior to
passaging or plating out, the monolayers (at 80–90%
confluency) were removed from the plastic substratum of
the flasks by incubation at 37 °C using a trypsin–EDTA
solution for 5–10 min. Following sedimentation of the
cell pellet by centrifugation at 300 g for 5 min at 4 °C
and resuspension of the pellet in DMEM, HaCaT or
NCTC medium, aliquots (100 µl) of each cell line were
pipetted into 96-well cell culture plates at a density of
50 000 cells per well. The cells were allowed to attach
and grow for 24 h at 37 °C in a humidified atmosphere of
5% CO2–95% air. The cell monolayers were subconfluent
at this time. The cell cycle analysis experiments em-
ployed 25 cm2 flasks containing cells seeded at 0.5 × 106
cells per flask. The SVK14 and G361 cells, once pipetted
into the flasks, were allowed to attach and begin growing
for 24 h at 37 °C in a humidified atmosphere of 5% CO2–
95% air prior to utilization, at which time the cultures
were subconfluent.
The MTT Assay
The cell culture viability assay used was the MTT assay.
The assay was carried out as described by Griffiths et al.
(1994) at various time points after HD exposure. Propan-
2-ol was used to extract the purple formazan product from
the cells. Absorbance of the solubilized formazan product
was measured at 570 nm against a solvent blank of
propan-2-ol using a Titertek Multiskan MCC plate-reader
(Flow Laboratories, Rickmansworth, Hertfordshire, UK).
SULPHUR MUSTARD EFFECTS ON HUMAN SKIN CELLS 117
© Crown copyright 2005. Reproduced with the permission of HMSO. J. Appl. Toxicol. 2005; 25: 115–128
Gentian Violet Assay
Cell culture density was determined by nuclear staining
with 0.1% (w/v) gentian violet (GV). The assay, origin-
ally described by Gillies et al. (1986), was carried out at
various time points after HD exposure. Briefly, cells in
the 96-well plates were stained with GV (100 µl well−1)
for 15 min. The stain was decanted and non-adherent
stain was removed by immersing the plates in running
tapwater for 10 min. The plates were then air-dried. The
dye was solubilized using 200 µl per well of a solvent
comprised of ethanol (50%, v/v) and acetic acid (1%, v/
v). Absorbance of the solubilized GV stain was measured
at 590 nm against the same solvent blank used to
solubilize the GV stain, using a Titertek Multiskan MCC
plate-reader. This assay permits quantification of cell
numbers in cultures because absorbance at 590 nm is
proportional to cell number (Gillies et al., 1986).
Dose–Response Study of the Effects of HD onSVK14, G361, HaCaT and NCTC Cell Viability
A stock solution of HD (50 mM) was prepared in
propan-2-ol. Working dilutions containing 0, 3, 10, 20, 30,
60, 100, 300 and 1000 µM were prepared in phosphate-
buffered saline (PBS, pH 7.4) and pipetted onto SVK14,
G361, HaCaT and NCTC cultures in 96-well plates
(100 µl per well). The HD-containing solutions were made
up and used immediately. The plates were incubated with
these solutions for 1 h at 37 °C in a humidified atmos-
phere of 5% CO2–95% air. The PBS solutions (contain-
ing 0–1000 µM HD) were removed and replaced with the
appropriate medium (100 µl per well) for each cell line.
Vehicle controls of up to 2% (v/v) were used. Cell cul-
ture viability was determined up to 72 h after HD expo-
sure using the MTT and GV assays as described above.
The data are shown as the mean absorbance ± SEM for
groups of eight cultures, expressed as a percentage of the
absorbance of control cultures (0 µM HD-treated).
Photography
Photographs of representative GV-stained cultures were
taken with a Nikon F-301 camera (using Kodak 64T colour
slide film) attached to a Nikon Diaphot phase-contrast
inverted microscope using a magnification of ×100.
Determination of SVK14, G361, HaCaT and NCTCCell Culture Growth Characteristics
To determine the growth rates of the four cell lines over
96 h, SVK14, G361, HaCaT and NCTC cultures were
sown into 96-well cell cultures plates at a seeding density
of 50 000 cells per well as described above. After an
incubation period of 24 h to allow the cells to adhere
(time t = 0 h), cell cultures in the 96-well plates were
fixed with 4% (w/v) formaldehyde in PBS at 4, 24, 48,
72 and 96 h after the initial period allowed for attachment
of cells. The cell density of the cultures was assessed
using the GV assay as described above. The data are
expressed as the mean absorbance (590 nm A) ± SEM for
groups of 24 cultures.
Effects of Depletion of Glutathione AntioxidantStatus on Cellular Sensitivity to HD UsingButhionine Sulphoximine
To determine if a significant element of the greater resist-
ance of G361 cells to HD was attributable to glutathione
(GSH) metabolism, SVK14, G361, HaCaT and NCTC
cells were sown into 96-well plates as noted above at a
density of 50 000 cells per well. After a period of attach-
ment, the cell cultures were exposed for 24 h to either
100 µM buthionine sulphoximine (BSO) (Armstrong
et al., 2002) in 100 µl of medium per well or to medium
only under the conditions noted above. The cultures were
subconfluent at this stage. Cells pretreated to ± BSO then
were exposed to 0, 20, 30 or 60 µM HD in PBS for 1 h
as described above. This was then replaced with medium
and the cultures incubated for a further period of 48 or
72 h. Cell viability was subsequently determined by the
MTT assay. The data are shown as the mean absorbance
(570 nm A) ± SEM for groups of eight cultures, ex-
pressed as a percentage of the absorbance of control cul-
tures (0 µM HD-treated). For comparison purposes, only
the data for the 72 h time point at 30 µM HD is shown.
Cell Cycle Analysis of HD-Exposed Cultures byFlow Cytometry
The effect of a mid-range dose of HD (30 µM) on cell
cycling activity in the most resistant (G361) and most
sensitive (SVK14) cell lines was determined by exposing
cultures to HD followed by flow cytometry analysis of
HD exposed and non-exposed cultures as described below.
A stock solution of HD (50 mM) was prepared in
propan-2-ol. The working dilution (30 µM) was prepared
in PBS. The medium overlying SVK14 and G361 cell
cultures, previously passaged into 25 cm2 flasks as de-
scribed above, was removed and immediately replaced by
5 ml per flask of either PBS or the 30 µM HD working
dilution. The flasks then were incubated for 1 h at 37 °C
in a humidified atmosphere of 5% CO2–95% air, after
which the PBS or HD solution was replaced with DMEM
growth medium (5 ml). The cultures then were incubated
at 37 °C in a humidified atmosphere of 5% CO2–95%
air. Cell cycle analysis was carried out at selected time
118 R. SIMPSON AND C. D. LINDSAY
Published in 2005 by John Wiley & Sons, Ltd. J. Appl. Toxicol. 2005; 25: 115–128
flasks at a density of 0.5 × 106 cells per flask in 5 ml of
DMEM medium. The SVK14 and G361 cells, once
pipetted into the flasks, were allowed to attach for 24 h at
37 °C in a humidified atmosphere of 5% CO2–95% air
prior to utilization. After the cells had adhered to the
plastic substrate of the flasks for 24 h, the medium was
removed and fresh DMEM medium (5 ml) was added.
The cell cycle synchronizing agents were made up in
the manufacturer’s recommended vehicle (refer to Table
1 for details) and 50-µl aliquots of inhibitor were added
to each flask. Vehicle controls were included and all
flasks were incubated at 37 °C in a humidified atmos-
phere of 5% CO2–95% air for 24 h to permit cell cycle
synchronization of the cell cultures. The cultures were
subconfluent prior to the addition of HD or control
buffer.
To determine the effect of 30 µM HD on partially
synchronized cultures of SVK14 and G361 cells after the
24 h incubation period with the cell cycle synchronizing
agent or vehicle control, cell cycle analysis was carried
out on control cultures (not treated with synchronizing
agent; n = 3) and on cultures treated with synchronizing
agent (n = 3). The remaining flasks were exposed to
30 µM HD or PBS for 1 h at 37 °C in a humidified
atmosphere of 5% CO2–95% air. The 30 µM HD or PBS
was removed from each flask and replaced with DMEM
medium; all flasks were returned to the 37 °C incubator
for further incubation periods of 24 or 48 h. Cell cycle
analysis was carried out at 24 and 48 h after HD expo-
sure as described above.
Statistical Analysis
The results were analysed using Welch’s approximate
two-tailed t-test on Instat™ Software (GraphPad Soft-
ware, San Diego, CA).
points (24, 48 and 72 h) after exposure to HD as
described below.
To prepare samples for flow cytometry, the contents
of each 25 cm2 flask was washed in PBS. The PBS was
aspirated and the cells removed from the flask by incuba-
tion at 37 °C with trypsin–EDTA for 5–10 min. The cells
were centrifuged (300 g, 4 °C, 5 min) and resuspended in
0.5 ml of DMEM medium. The DNA-Prep Reagent kit
(Beckman Coulter) was used to prepare SVK14 and
G361 cells for cell cycle analysis. Briefly, 0.1 ml of LPR
(a saponin and formaldehyde containing reagent used to
fix and permeabilize cells) was added to each sample in
DMEM medium. The samples were incubated at room
temperature for 10 min. A 1-ml aliquot of DP stain (the
propidium iodide component of the DNA-Prep kit) was
added to stain cellular DNA. The cell samples were
incubated at room temperature in the dark for 2 h.
Propidium iodide fluorescence (560–680 nm) was meas-
ured using a Beckman-Coulter EPICS® XL-MCL™ four-
colour flow cytometer, following excitation (at 488 nm)
with a 15 mW argon ion laser with the sample flow rate
set to high. EXPO™ 32 software (version 1.2; Beckman-
Coulter) was used to analyse the fluorescence output.
Fluorescence counts were collected over 300 s; the per-
centages of cells in each phase of the cell cycle were
determined by gating the G0/G1, S and G2/M phase cell
populations as described by Ormerod (1996), expressed as
the mean percentage of groups of eight cultures ± SEM.
Screening of Cell Cycle Synchronizing Agents
A series of cell cycle synchronizing agents were identi-
fied in the literature and screened at the concentrations
recommended in the literature (Table 1) for efficacy in
the cell lines used. The SVK14 and G361 cells were pre-
pared as described above by seeding cells into 25 cm2
Table 1. Cell cycle synchronising agent profiles for SVK14 and G361 cells
Inhibitor Classa Concb G361c SVK14c
Acyclovir (Cioe et al., 1992) G0/G1 500 µMD 0 G0/G1
Aphidicolin (Mutomba and Wang, 1996) Early S 0.1 µg ml−1D 0 G0/G1
Hydroxyurea (Lee et al., 1997) G1/S 375 µMW G1/Sd G1/Sd
Hydroxyurea G1/S 1 mMW S G2/M
Indole-3-carbinol (Cover et al., 1998) G0/G1 100 µME G0/G1d 0
Indole-3-carbinol G0/G1 225 µME Toxic Toxic
Indirubin-3-monoxime (Marko et al., 2001) G2/M 2 µMD S 0
Low Temperature (Doyle et al., 1996) G0/G1 4 °C 0 0
Mimosine (Hoffman et al., 1991) G1 300 µMW S/G2/M S
Olomoucine (Schutte et al., 1997) G1 200 µMD 0 G2/M
Rapamycin (Morice et al., 1993) G1 0.1 nmD 0 0
Staurosporine (Zong et al., 1999) G1 20 nmD G0/G1 G0/G1d
Trichostatin (Inkoshi et al., 1999) G1 17 nmD S/G2/M G0/G1
a The published activity for these cell cycle regulators.b The concentrations at which these compounds were used in the present study. The designations D, W and E refer to
the solvent vehicles DMSO, water and ethanol, respectively.c The predominant (although partial) activity found for the given regulators.d These agents were found to be the best at synchronizing the cell cycle at their respective positions (although only
partially) in SVK14, G361 or both cell lines.
SULPHUR MUSTARD EFFECTS ON HUMAN SKIN CELLS 119
© Crown copyright 2005. Reproduced with the permission of HMSO. J. Appl. Toxicol. 2005; 25: 115–128
Results
Dose–Response Study of the Effects of HD inSVK14, G361, HaCaT and NCTC Cells
The SVK14, G361, HaCaT and NCTC cells were
exposed to HD (up to 1000 µM) for 1 h, with viability
being measured at 4, 24, 48 and 72 h time points after the
exposure, using the MTT assay (Fig. 1) and GV assay
(for which similar results were obtained; data not shown).
Vehicle controls for all experiments were run, which
indicated that propan-2-ol had no significant effects on
cell culture viability (data not shown). Initially, at the 4 h
time point, the four cell lines exhibited similar responses
to HD, with viability only decreasing after exposure to
1000 µM HD. At 24 h after exposure, the HaCaT cell line
was found to be the most resistant to HD but only at
concentrations of <100 µM; the G361 cell line appeared
to be the more sensitive cell line at concentrations of
>30 µM HD. At 48 h after HD exposure, the dose–
response profile of G361 cells was largely maintained.
However, the relative viability of the remaining cell lines
was found to decline to a greater extent at HD concentra-
tions of >3 µM, so that at 72 h after HD exposure the
G361 cell line was found to be more resistant to the
cytotoxic effects of HD than the NCTC, HaCaT and
SVK14 cell lines at HD doses of >3 and <100 µM. More
specifically, at 72 h there were 1.3- (P < 0.001), 2.0- (P
< 0.0001), 3.4- (P < 0.0001), 4.7- (P < 0.0001) and 8.8-
fold (P < 0.0001) differences between G361 and SVK14
cell culture viability at 3, 10, 20, 30 and 60 µM HD,
respectively, although this pattern did not extend to
100 µM HD. An intermediate challenge concentration
of 30 µM HD was selected with which to investigate the
effects of HD on morphology, BSO and cell cycling
activity in G361 and SVK14 cells.
Figure 1. Effect of HD on SVK14 (�), G361 (�), HaCat (�) and NCTC (�) cells. Cells were exposed to HD (up to1000 µM) for 1 h. Cell culture viability was determined using the MTT assay at periods of 4 h (a), 24 h (b), 48 h (c)and 72 h (d) after exposure. Data are expressed as the mean percentage viability of control cultures (not exposedto HD) ± SEM (n = 8)
120 R. SIMPSON AND C. D. LINDSAY
Published in 2005 by John Wiley & Sons, Ltd. J. Appl. Toxicol. 2005; 25: 115–128
Growth of SVK14, G361, HaCaT and NCTC CellCultures
The growth characteristics of the four cell lines were
determined over 96 h using the GV assay as an index of
cell density (Fig. 3). It was found that the SVK14 cell
line grew more slowly compared with the other cell lines,
the difference being most apparent at the longer time
points so that at 72 h after t = 0 the order of cell culture
density was HaCaT>NCTC>G361>SVK14. The growth
curves for the cell lines shown were different to each
other, but overall the curves for the G361 cell line
most resembled those of the HaCaT and NCTC cell
lines. The differences in the growth profiles were particu-
larly marked at 72 and 96 h for G361 cultures, whose
density was found to be greater than that of SVK14 cul-
tures by 1.7-fold (P < 0.0001) and 1.4-fold (P < 0.0001),
respectively.
Figure 2. (a) Photomicrograph of a 72-h control culture of G361 cells stained with GV, demonstrating thedendritic morphology associated with this cell line. (b) Photomicrograph of a G361 culture 72 h after exposure to30 µM HD stained with GV, showing a reduction in culture density but maintaining the dendritic morphology seenin the control cultures. (c) Photomicrograph of a 72-h control culture of SVK14 cells stained with GV, demonstrat-ing the epithelial cobblestone morphology seen in this cell line. (d) Photomicrograph of an SVK14 culture 72 h af-ter exposure to 30 µM HD stained with GV, showing a necrotic population characterized by a reduction in cellculture density, loss of cell morphology, cellular fragmentation and nuclear condensation (magnification: ×100)
Photomicrography of HD-exposed G361 andSVK14 Cells
Photomicrographs taken of GV-stained cultures showed
the dendritic morphology of control (non-HD exposed)
G361 cells, with heavy GV staining of the nucleus
and the cytoplasm (Fig. 2a). At 72 h after exposure
to 30 µM HD the number of G361 cells in the culture
was reduced, although the cells had maintained their
morphology (Fig. 2b). The epithelial morphology of
SVK14 cells in control cultures is shown in Fig. 2c,
with dense staining of the nucleus and lighter staining
of the cytoplasm. At 72 h after exposure to 30 µM HD
there was a considerable reduction in the number of
cells, with cytoplasmic swelling and necrosis being
evident (Fig. 2d). This reduction of cell density in HD-
exposed SVK14 cells was greater than that found in
G361 cultures.
SULPHUR MUSTARD EFFECTS ON HUMAN SKIN CELLS 121
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Figure 3. Determination of SVK14 (�), G361 (�),HaCat (�) and NCTC (�) cell culture growth rates. Thegrowth rates of the four cell lines are shown over peri-ods of up to 96 h. The cell density of the cultures wasassessed using the GV assay. The data are expressed asmean absorbance (A590 nm) ± SEM (n = 24)
Figure 4. The effect of BSO pretreatment on thecytotoxicity of HD in SVK14, G361, HaCat and NCTCcells 72 h after exposure to HD (30 µM). Cell cultureswere either exposed to medium only (black bars)or pre-exposed to BSO (100 µM) for 24 h prior to HDexposure (hatched bars). Cell viability was determinedby the MTT assay. The results show that BSO pretreat-ment significantly exacerbates the toxicity of HD. Dataare expressed as the mean percentage viability of con-trol cultures (not exposed to HD) ± SEM (n = 8). * P <0.05; ** P < 0.01; *** P < 0.0001
time point, show that BSO pretreatment in addition to
subsequent HD exposure (30 µM) resulted in a further
reduction in the viability of G361 (P < 0.0001), HaCaT
(P < 0.01), NCTC (P < 0.001) and SVK14 (P < 0.05)
cultures compared with cultures exposed to HD alone.
Vehicle controls showed that propan-2-ol did not contrib-
ute to the toxicity of HD (data not shown). The data
show that a substantial proportion of the resistance of
G361 cells to HD is attributable to BSO-mediated effects
on antioxidant-mediated metabolism, although G361 cul-
tures still retained a substantial degree of viability (43%)
at 30 µM HD following BSO pretreatment. Overall, the
magnitude of the BSO-mediated decrease in viability
in HD-exposed cells (expressed as a ratio relative to the
viability value of cultures exposed only to HD) was
of the order G361 (0.50)>SVK14 (0.58)>NCTC (0.63)>HaCaT (0.81), indicating that BSO pretreatment of G361
cells reduced viability by 50%. The relative similarity of
the level of BSO-induced viability reduction in SVK14
cell cultures (42%) further supported the selection of
G361 and SVK14 cells for further comparative analysis.
Cell Cycle Analysis of HD-exposed G361 andSVK14 Cultures by Flow Cytometry
Flow cytometry was carried out on G361 and SVK14
cells to determine the effect of HD on cell cycling activ-
ity. The flow cytometer output data set shown in Fig. 5
is a set of representative profiles for SVK14 and G361
cell control cultures (not exposed to HD; ‘−HD’ in the
figure), as well as cell cultures exposed to 30 µM HD
(‘+HD’ in the figure). Vehicle controls showed that
propan-2-ol did not affect the viability of the cultures
(data not shown). The data set shows that cell cycling
activity over 72 h in SVK14 cells was more sensitive to
disruption than cell cycling in G361 cells over this
period. This is exemplified by the 24-h data, which show
both a broadening of the G0/G1 peak and a shift to the
right indicating that DNA damage has occurred in
SVK14 cells. In contrast, although the cell cycle profile
for G361 cells retained much of its integrity over the 72-
h period, SVK14 cell counts had degenerated to back-
ground levels by this time. A complete data set (for 24
and 48 h only) is described in Table 2 for both cells lines,
in which the percentage values for the proportion of cells
in various phases of the cell cycle are shown. The table
contains data from cultures at 24 and 48 h after HD
exposure. Tabulated data are not shown for the 72-h time
point because only background counts were measured for
SVK14 cells at this time.
The results shown in Table 2 indicate that at 24 h the
control G361 cell cultures had a greater proportion of
their number in G0/G1 phase (by 1.3-fold; P < 0.001)
compared with control SVK14 cultures. In contrast, the
proportion of cells in S-phase was greater in SVK14
Buthionine Sulphoximine-mediated CellularSensitization to HD
The effects of BSO pretreatment on cellular sensitivity
to HD were determined in G361, SVK14, HaCaT and
NCTC cells. The use of 100 µM BSO in control cultures
showed that BSO did not affect significantly the viab-
ility of any of the four cell lines (data not shown). The
results in Fig. 4, depicting data collected at the 72 h
122 R. SIMPSON AND C. D. LINDSAY
Published in 2005 by John Wiley & Sons, Ltd. J. Appl. Toxicol. 2005; 25: 115–128
With respect to HD-induced effects on the cell cycle,
the data in Table 2 confirmed that at 24 h the SVK14
cells were relatively more sensitive to HD, as shown by
the 2.1-fold reduction (P < 0.0001) in the percentage of
cells in G0/G1 phase after HD exposure compared with
Figure 5. Cell cycle profiles of SVK14 and G361 cells to compare the effects of exposure to 30 µM HD. The cellcycle profiles of the SVK14 and G361 cells not exposed to HD (controls) are indicated by ‘−HD’ at 24, 48 and 72 h.Cell cycle profiles of cultures exposed to HD are denoted by ‘+HD’. The first peak denotes the G0/G1 phase cellpopulation; the smaller peak denotes the G2/M phase cells and S-phase cells are in the trough between the peaks.The x-axis of each graph denotes fluorescence intensity (arbitrary units); the y-axis denotes cell counts measured ateach fluorescence channel. The data are representative flow cytometer profiles for each cell line. The data fromthis experiment are described in Table 2 as relative percentages of cells in each phase of the cell cycle for ± HD-treated SVK14 and G361 cultures
Table 2. The relative proportion of SVK14 and G361 cells in each phase of thecell cycle 24 and 48 h after HD exposure (30 µM)a
Cell line Treatment G0/G1 S G2/M
Data at 24 h
SVK14 −HD 49.0 ± 1.5 11.2 ± 1.5 37.2 ± 2.8
+HD 23.7 ± 2.1 46.9 ± 2.0 26.6 ± 2.8
(P < 0.0001) (P < 0.0001) (P < 0.05)
G361 −HD 61.5 ± 1.8 7.2 ± 1.0 30.2 ± 2.3
+HD 72.8 ± 3.4 4.2 ± 2.6 22.6 ± 1.4
(P < 0.05) (NS) (P < 0.05)
Data at 48 h
SVK14 −HD 47.6 ± 1.1 14.6 ± 1.8 35.1 ± 2.2
+HD 14.9 ± 1.4 38.8 ± 3.1 36.1 ± 3.6
(P < 0.0001) (P < 0.0001) (NS)
G361 −HD 63.0 ± 1.4 9.7 ± 1.7 26.8 ± 1.8
+HD 43.9 ± 3.7 22.9 ± 2.7 32.0 ± 1.7
(P < 0.01) (P < 0.01) (NS)
a Data are presented as the mean percentage of cells in each phase of the cell cycle ± SEM (n = 8). The data
confirm that SVK14 cells are more sensitive to HD than G361 cells, as shown by the significant differences in
the percentage of cells in G0/G1 and S-phase between HD-exposed and control cells. There were differences in
the percentage of cells in each phase of the cell cycle when comparing exposed and control G361 cells, but these
differences were not as large as those measured for SVK14 cells. The HD-exposed SVK14 cells have a lower
percentage of cells in G0/G1 than control cells; the reduced proportion of cells is due to a shift in the G0/G1 peak
to the right, which is indicative of DNA damage.
cultures than in G361 cells (by 1.6-fold; P < 0.05). The
SVK14 cell cultures also had more cells in G2/M phase
than was the case for G361 cultures (by 1.2-fold),
although this was not statistically significant. A similar
overall pattern was found at 48 h.
SULPHUR MUSTARD EFFECTS ON HUMAN SKIN CELLS 123
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control cultures. This compared well with a 1.2-fold
increase (P < 0.05) in the percentage of G361 cells in G0/
G1 phase following HD exposure. A 4.2-fold increase (P
< 0.0001) in the proportion of cells in S-phase was meas-
ured after SVK14 cells were exposed to HD, whereas the
proportion of G361 cells in S-phase fell by 1.7-fold fol-
lowing HD exposure, although this difference was not
significant. Sulphur mustard-induced perturbations in the
G2/M phase cell populations were found also in SVK14
and G361 cell cultures, resulting in 1.4- and 1.3-fold
reductions (P < 0.05 and P < 0.05, respectively) in the
proportion of cells in this phase of the cell cycle. At the
48-h time point, HDinduced disruption of G0/G1 phase in
SVK14 cells increased further, with a 3.2-fold reduction
(P < 0.0001) in the percentage of cells in this phase. This
contrasts with only a 1.4-fold reduction (P < 0.01) in
G361 cells. A 2.7-fold increase (P < 0.0001) in the
proportion of cells in S-phase was found in SVK14 cells
exposed to HD compared with control cultures, whereas
this proportion was lower (2.4-fold; P < 0.01) in G361
cells exposed to HD. No significant difference was found
in the relative proportions of SVK14 or G361 cells in G2/
M phase in HD-exposed and control cultures.
Screening of Cell Cycle Synchronizing Agentsand the Effect of HD (30 µµµµµM) on PartiallySynchronized Cultures of SVK14 and G361 Cells
A series of cell cycle synchronizing agents were screened
to determine if the cell cycle of SVK14 and G361
cultures could be halted reversibly at various stages of
the cell cycle (Table 1). Selected inhibitor treatments
were used to synchronize cultures of SVK14 and G361
cells prior to exposing them to HD, with cell cycle analy-
sis being carried out at 24 and 48 h after HD exposure
to determine if synchronization could modulate the
cytotoxicity of HD.
Some of the cell cycle inhibitor treatments tested
did not have any effect on SVK14 and G361 cells
(rapamycin, low temperature). Of the remainder,
acyclovir, aphidicolin, indole-3-carbinol, indirubin-3-
monoxime, mimosine, olomoucine and trichostatin pro-
duced different effects in SVK14 cells compared with
those obtained in G361 cell cultures; none of these
inhibitors produced completely synchronized cultures
(data not shown). In the case of indole-3-carbinol, a
lower concentration (100 µM) than the published one
(225 µM) had to be used because the higher dose was
found to be cytotoxic. Indole-3-carbinol was found to
have reversible but only partial G0/G1 modulatory effects
in G361 cells at 100 µM (data not shown). Figure 6
shows the effects of staurosporine on SVK14 cells, in
which only partial synchronization of cell cultures in
G0/G1 phase was obtained. At 48 h, it was found that
staurosporine increased the proportion of cells in G0/G1
phase from 51% in control cells to 54.5% for SVK14
cells. This partial synchronization was a pattern that was
found also for hydroxyurea in both cell lines (data not
shown).
It can also be seen from Fig. 6 that staurosporine
pretreatment of SVK14 cells exacerbated the effects of
Figure 6. The effect of 30 µM HD upon SVK14 cells partially synchronized in G0/G1 of the cell cycle with a 24-hstaurosporine pretreatment prior to HD exposure (30 µM). Cell cycle analysis was carried out 24 and 48 h after HDexposure. The cell cycle profiles of the SVK14 cells not exposed to HD (controls) are indicated by ‘−HD’ at 24 and48 h. Cell cycle profiles of cultures exposed to HD are denoted by ‘+HD’. The first peak denotes the G0/G1 phase cellpopulation; the smaller peak denotes the G2/M phase cells and S-phase cells are in the trough between the peaks.The x-axis of each graph denotes fluorescence intensity (arbitrary units); the y-axis denotes cell counts measured ateach fluorescence channel. The data are representative flow cytometer profiles for each cell line. The data from thisexperiment are described in Table 3 as total cell counts for ± staurosporine-pretreated and ± HD-exposed SVK14cultures. Partial synchronization of SVK14 cells with staurosporine was shown to exacerbate the effects of HD
124 R. SIMPSON AND C. D. LINDSAY
Published in 2005 by John Wiley & Sons, Ltd. J. Appl. Toxicol. 2005; 25: 115–128
Table 3. Effects of exposure to HD following pretreatment with/withoutstaurosporine on SVK14 cell cultures: total flow cytometer cell counts are shownat 24 and 48 h as an index of viability for SVK14 cultures given no pretreatmentand no exposure to HD, cultures pretreated with staurosporine only, culturesexposed to HD only and cultures both pretreated with staurosporine and thenexposed to HD as described in the Methods section (data are mean cell countvalues ± SEM; n = 3)
0 µM HD 30 µM HD
24 h 48 h 24 h 48 h
Control 17 100 ± 490 17 900 ± 352 8650 ± 620 1650 ± 150
(−staurosporine)
+Staurosporine 12 100 ± 600 15 000 ± 590 2720 ± 270 390 ± 30
(P < 0.0001) (P < 0.001) (P < 0.0001) (P < 0.0001)
subsequent HD exposure, so that at 48 h after HD expo-
sure the flow cytometer histogram of staurosporine-
pretreated cultures recorded only background counts.
Table 3 shows cell counts from an experiment in which
total cell numbers (counts) were compiled from flow
cytometry histograms from experiments described in
Fig. 6 as an index of culture viability for each treatment.
At the 48-h time point, it was found that cell counts
for cultures treated with staurosporine were 84% of that
of control cultures (where 17 900 counts = 100%, P <0.001; Table 3). At 48 h, the cell counts in cultures
exposed to HD only (30 µM) were 9.2% compared
with control cultures. However, cell counts in cultures
pretreated with staurosporine before HD exposure were
only 2.2% of control counts (P < 0.0001), indicating that
staurosporine pretreatment exacerbated the toxicity of
HD. The reversibility of the effects of staurosporine are
shown in Table 3: the cell counts for the staurosporine-
pretreated cultures at 48 h had increased to 15 000 from
12 100 at 24 h. In contrast, the histogram profile for HD-
treated SVK14 cells shows a characteristically broadened
G0/G1 peak with a lower number of recorded counts.
Hydroxyurea, reported to be a G1/S phase synchronizing
agent (Lee et al., 1997), partially synchronized cultures of
G361 and SVK-14 cells at G1/S phase of the cell cycle
but did not reduce the cytotoxicity of HD in either cell
line (data not shown).
Discussion
In this study, the human skin cell lines SVK14, HaCaT,
NCTC and G361 were used to model the cytotoxicity of
HD to obtain information on the biochemical basis for
differences in sensitivity to HD. Marked biochemical and
morphological differences in the responses of the cell
lines were found over a 72-h period following exposure
to HD. At the 4-h time point, relatively little response to
HD was seen except at the highest concentration of HD
(1000 µM). At the 24-h time point, the G361 cell line
was found to be more sensitive to HD than SVK14,
HaCaT and NCTC cells at 60, 100 and 300 µM HD,
whereas at 48 h the G361 cells became relatively more
resistant to HD, particularly at 10, 20 and 30 µM HD.
At 72 h this pattern became established further at 3–
60 µM HD.
The results confirm previous findings by Smith et al.
(2001), who found that cellular proliferation in G361 cul-
tures could recover following HD exposure, although in
the present study this was not evident at HD doses of
>60 µM. This is suggestive of a limited repair capability
and would explain the markedly greater resistance of
G361 cells at 72 h compared with SVK14 cells, signific-
ant differences in cell culture viability being found at
20, 30 and 60 µM HD. These observations were con-
firmed by photomicrography of control and HD-exposed
cell cultures, which indicated that, at 72 h after exposure
to 30 µM HD, although G361 cultures showed some
reduction in cell density the remaining cells were found
to maintain the dendritic morphology seen in control
cultures. In contrast, the normal epithelial cobblestone
morphology of control SVK14 cells was lost in HD-
treated cultures, with substantial losses in cell culture
density being found. The remaining SVK14 cells showed
a loss of normal cell morphology, as well as cellular frag-
mentation and nuclear condensation.
These findings are consistent with Smith et al. (2001),
who also showed that G361 cells were more resistant
than SVK14 cells to the effects of H2O2 to a similar ex-
tent, alluding to related resistance mechanisms involving
an upregulated DNA repair capacity. In the present study,
differences in cell population growth rates alone could
not account for the greater sensitivity of SVK14 cells to
HD, because despite the known deleterious effects of HD
on rapidly dividing cells (Maynard, 1987) the G361 cell
cultures were found to have a higher growth rate than
SVK14 cell cultures.
Intracellular antioxidant status, specifically the quantity
of intracellular glutathione (GSH) in cell lines, has been
reported to be important in the protection of cells against
SULPHUR MUSTARD EFFECTS ON HUMAN SKIN CELLS 125
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HD toxicity (Gross et al., 1993). Thus, a series of experi-
ments were carried out using BSO to inhibit the activity
of γ-glutamyl cysteine synthetase (Armstrong et al.,
2002), with a view to determining if antioxidant status
was responsible for the relatively higher level of resist-
ance to HD found in G361 cultures. It was found that
although GSH metabolism played a significant part in the
mediation of HD toxicity in all four cell lines, the data
indicated that in G361 cell cultures the pretreatment with
BSO resulted in a relatively greater reduction in viability
compared with non-BSO-pretreated cultures at 30 µM HD
in relation to the other three cell lines investigated. This
implies that a large proportion of the resistance of G361
cultures to HD may be attributable to increased intra-
cellular antioxidant status. Previous studies have shown
that thiol agents such as mono-isopropylglutathione ester
and di-isopropylglutathione ester are capable of confer-
ring protection against HD in vitro (Lindsay et al., 1997;
Andrew and Lindsay, 1998b; Lindsay and Hambrook,
1998). However, other factors cannot be ruled out, be-
cause at 30 µM HD the G361 cultures contained a rela-
tively high proportion of cells that remained viable even
after BSO pretreatment. In order to probe this further, a
comparative analysis on cell cycling activity in SVK14
and G361 cultures was carried out because previous stud-
ies have suggested that G361 cells may have a more
efficient DNA repair capacity, as indicated by elevated
levels of PCNA in this cell line (Smith et al., 2001).
The DNA repair involved may be nucleotide excision
repair, because PCNA is an essential co-factor in this
type of repair (Bootsma, 2001). The SVK14 cells were
employed for comparative cell cycle studies because BSO
increased the toxicity of HD to a similar extent in both
cell lines.
In G361 cells the selected challenge dose of HD
(30 µM) was found to have relatively little effect on
the cell cycle profile at 24, 48 and 72 h post-exposure
compared with SVK14 cells. In particular, G361 cultures
maintained a high proportion of their population in G0/G1
phase even after HD exposure at 24 h. However, cell
cycling activity in the more sensitive SVK14 cell line
was found to be disrupted substantially, with most of the
propidium iodide-stained DNA accumulating in a broad-
ened G0/G1 peak that extended into the S-phase popula-
tion at 24 h after HD exposure. By 48 h the DNA signal
of the SVK14 cell cycle profile had degenerated sub-
stantially, and at 72 h only background noise could be
detected. This marked degeneration of the cell cycle pro-
file occurred in SVK14 cells only, and well before the
MTT assay in the HD titration experiments could detect
significant decreases in viability in this cell line compared
with the G361 cell line. Therefore, HD exposure caused
early damage to the DNA of SVK14 cells 24 h after HD
exposure, but this did not result in substantial loss of
viability (as determined by the MTT and GV assays)
until later time points. This indicates that early nuclear
events may be important in HD cytotoxicity, particularly
in relatively sensitive cell lines.
An increase in the width of the G0/G1 peak and a shift
in measured data counts to the right of the data collection
histogram are characteristic of increasing amounts of
genotoxic damage (Wagner et al., 1998). This can be in-
terpreted also as a reduction in G0/G1 peak counts if, as
was the case in the present study, the flow cytometry data
collection gates for HD-exposed cells are kept the same
as for control (unexposed) cultures. The results from the
cell cycle analysis therefore suggested that G361 cells
were more resistant to DNA damage than SVK14 cells,
even at later time points. One possible mechanism for
this difference in sensitivity is that in SVK14 cell cul-
tures a greater proportion of the cell population was in S-
phase; keratinocytes are known to be especially sensitive
to alkylating agents when in this phase of the cell cycle
(Smith et al., 1991). The finding that G361 cultures
tended to have a lower proportion of their cell population
in S-phase compared with SVK14 cultures may be
significant.
Attempts were made to modulate DNA damage and
concomitant cell cycle disruption by altering the progres-
sion of the cell cycle, because the efficiency of DNA
repair may be a function of the position of the cell in the
cell cycle (Gorczya et al., 1993). Relatively few studies
have assessed the effects of cell cycle regulation on DNA
repair (Smith and Seo, 2002). The G1 phase cell cycle
checkpoint effectively arrests the cell cycle if DNA dam-
age is detected and enables repair before progression to
S-phase (Smith and Seo, 2002). It should be noted that in
the present study the G361 cells were able to retain the
integrity of the cell cycle profile 24 h after HD exposure,
particularly with respect to G0/G1 phase counts, which
increased marginally from 61% of the total cell popula-
tion in control cultures to 73% of the cell population in
HD-exposed cultures. This is suggestive of the existence
of a more efficient G1 phase cell cycle checkpoint in
G361 cells compared with SVK14 cultures; in the latter
case, G0/G1 phase counts decreased substantially from
49% of the total cell population in control cultures to
24% of the cell population in HD-exposed cultures.
Effective repair in G1 phase is essential, because in S-
phase there may be no excision repair (Bell et al., 1999).
The expression of factors associated with nucleotide
excision repair, such as DNA polymerase-δ, has been
reported to be higher at the G1/S junction than elsewhere
in the cell cycle (Wang, 1996), therefore a variety of
cycle synchronizing agents were used to halt or increase
the relative proportion of cells in G0/G1 phase prior to
HD exposure. A major criterion for their use was that
their effects on cell cycle profiles should be reversible.
In the present study, indole-3-carbinol reversibly
but only partially held G361 cells at G0/G1 in the cell
cycle, and had no effect on SVK14 cells. Indole-3-
carbinol treatment has been reported to downregulate
126 R. SIMPSON AND C. D. LINDSAY
Published in 2005 by John Wiley & Sons, Ltd. J. Appl. Toxicol. 2005; 25: 115–128
cyclin-dependent kinase 6 (CDK6) transcription by selec-
tively disrupting the interactions of SP1 (transcription
factors) with a composite DNA-binding site within the
CDK6 promoter, arresting cells in G1 (Cram et al., 2001).
Inhibition of CDK6 correlates with a reduction in endo-
genous retinoblastoma protein (Cover et al., 1998). The
CD6-dependent phosphorylation of retinoblastoma protein
is required for the progression of cells through G0/G1
and into S-phase. Indole-3-carbinol had no beneficial
effect on G361 cells subsequently exposed to HD.
Staurosporine reversibly held SVK14 cells in G0/G1
phase of the cell cycle but the partial synchronization
obtained prior to HD exposure was found to exacerbate
the effects of HD. Staurosporine is reported to be a
broad-spectrum protein kinase inhibitor, examples of
whose targets include protein kinase C (Swe et al., 1996),
protein kinase A (Ruegg & Burgess, 1989), tyrosine pro-
tein kinase and CaM kinase (Yanagihara et al., 1991).
Staurosporine exploits the same potential hydrogen-bond
interactions as ATP (the cofactor for the protein kinases)
in its mechanism of binding (Furet et al., 1995). The
addition of staurosporine prior to HD exposure may
have resulted in the inhibition of these protein kinases
(which are involved in DNA double-strand break repair
mechanisms), possibly increasing the sensitivity of the
cells to the damaging effects of HD (Tuteja and Tuteja,
2001).
Hydroxyurea reversibly (but only partially) held
G361 and SVK14 cells at S-phase in the cell cycle. The
partial synchronization of G361 and SVK14 cells with
hydroxyurea prior to HD exposure was found to exacerb-
ate the effects of HD in both cell lines. Hydroxyurea
has been reported to destroy the tyrosyl free radical at the
active site of the M2 protein subunit of ribonucleotide
reductase, inactivating the enzyme (Yarbro, 1992). This
blocks the de novo synthesis of deoxyribonucleotides
(Hendricks and Matthews, 1998), synchronizing DNA
synthesis in S-phase. If no excision repair occurs in S-
phase (Bell et al., 1999), HD will cause greater damage
to cells synchronized in S-phase because potentially no
DNA repair may occur after the HD exposure until the
cells have completed the cell cycle. This may explain
why 30 µM HD caused cell cycle disruption in G361
cells partially synchronized in S-phase prior to HD expo-
sure, when previously this concentration of HD had pro-
duced only limited cell cycle disruption in non-pretreated
cells. Aphidicolin (an early S-phase inhibitor) also was
used in the present study, although both SVK14 and
G361cell cultures were found to be affected adversely by
treatment with aphidicolin. This may be because DNA
polymerase-δ and -ε associated with nucleotide excision
repair are specifically inhibited by this agent (Wood and
Shivjii, 1997).
In summary, the use of various cell cycle synchroniz-
ing agents was found to produce variable effects in
SVK14 and G361 cells. These agents had either no
protective action or exacerbated the cytotoxicty of
HD. More efficient methods for maintaining cells in
G0/G1 phase will be required to determine if maintaining
a relatively greater proportion of the cell population in
this part of the cell cycle at the time of HD challenge has
potential therapeutic benefit. The finding that, in G361
cells, a larger proportion of the cell population was in
G0/G1 phase at any time (before or after HD exposure)
compared with the more sensitive SVK14 cell line
may be significant in relation to the greater resistance to
HD-induced cell cycle disruption measured in G361 cell
cultures.
The greater resistance of G361 cells to HD may be
related to the role of PCNA, which not only is associated
with nucleotide excision repair but also may have a
role in cell cycle regulation. The PCNA interacts with
cyclin D, a molecular species that regulates cell cycle
progression from G1 phase to S phase (Xu et al., 2001).
Therefore, the basis for the greater resistance of the
G361 cell line to HD could be due to a combination of
greater DNA repair capacity (e.g. through an upregulated
nucleotide excision repair capability) and more efficient
cell cycle control processes that halt the cycle at the
appropriate checkpoints. The failure of mitotically active
cells to halt at the appropriate checkpoints would
result in the cell attempting to replicate codons with
HD-induced monofunctional DNA base alterations and
bifunctional inter- and intra-strand cross-links. This
would have several consequences, such as strand breaks,
mutations, disruption of DNA replication and transcrip-
tion processes and eventually cell death (Wang, 1998).
According to Smith and Seo (2002), p53 mediates the G1
phase checkpoint following DNA damage and it is likely
that it is this action that allows DNA repair to progress
by giving the cell a greater amount of time for DNA
repair to occur (in G1 phase) before the cell enters S-
phase. Further work will investigate the biochemical
basis of increased HD resistance in G361 cells, particu-
larly with respect to p53 activity following DNA damage
and the activation of its associated genes Gadd45 and
p48XPE (Smith and Seo, 2002) to determine if the differ-
ences in susceptibility to HD between SVK14 and G361
cells are attributable to differential expression of selected
components of the nucleotide excision repair pathway.
Acknowledgement—We would like to thank John Hayes for supplyingthe HaCaT and NCTC cells and for helpful technical discussions andadvice.
References
Andrew DJ, Lindsay CD. 1998a. Protection of human upperrespiratory tract cell lines against sulphur mustard toxicity byhexamethylenetetramine (HMT). Hum. Exp. Toxicol. 17: 373–379.
Andrew DJ, Lindsay CD. 1998b. Protection of upper respiratory tractcell lines against sulphur mustard by glutathione esters. Hum. Exp.
Toxicol. 17: 387–395.
SULPHUR MUSTARD EFFECTS ON HUMAN SKIN CELLS 127
© Crown copyright 2005. Reproduced with the permission of HMSO. J. Appl. Toxicol. 2005; 25: 115–128
Armstrong JS, Steinauer KK, Hornung B, Irish JM, Lecane P, BirrellGW, Peehl DM, Know SJ. 2002. Role of glutathione depletion andreactive oxygen species generation in apoptotic signalling in a humanB lymphoma cell line. Cell Death Differ. 9: 252–263.
Bell LM, Lannon CL, Yhap M, Pyesmany AF, Henry M, Laybolt K,Riddell DC, van Velzen D. 1999. Drug resistance in leukemia andlymphoma III. Adv. Exp. Med. Biol. 457: 289–296.
Bootsma D. 2001. The ‘Dutch DNA Repair group’ in retrospect. Mutat.
Res. 485: 37–41.Brooks P, Lawley PD. 1963. Effects of alkylating agents on T2 and T4
bacteriophage. Biochem. J. 89: 138–144.Brown RF, Rice P. 1997. Histopathological changes in yucatan minipig
skin following challenge with sulphur mustard. A sequential study ofthe first 24 h. Int. J. Exp. Pathol. 78: 9–20.
Cioe L, Mukhopadhyay S, Rovera G. 1992. Selective-inhibition ofproliferation in V-ABL-transformed and BCR-ABL-transformed cellsby a nucleoside analogue. J. Biol. Chem. 267: 22178–22182.
Cover CM, Hsieh SJ, Tran SH, Hallden G, Kim GS, Bjeldanes LF,Firestone GL. 1998. Indole-3-carbinol inhibits the expression ofcyclin-dependent kinase-6 and induces a G1 cell cycle arrest ofhuman breast cancer cells independent of estrogen receptor signal-ling. J. Biol. Chem. 273: 3838–3847.
Cram EJ, Liu BD, Bjeldanes LF, Firestone GL. 2001. Indole-3-carbinolinhibits CDK6 expression in human MCF-7 breast cancer cells bydisrupting sp1 transcription factor interactions with a compositeelement in the CDK6 promoter. J. Biol. Chem. 276: 22332–22340.
Doyle A, Griffiths JB, Newell DG. 1996. Cell + Tissue Culture: Labo-
ratory Procedures. John Wiley: Chichester; Section 4E: 3.3.Erickson LC, Laurent G, Sharkey NA, Kohn KW. 1980. DNA cross-
linking and monoadduct repair in nitrosourea-treated human tumourcells. Nature 288: 727–729.
Fox M, Scott M. 1980. The genetic toxicology of nitrogen and sulphurmustard. Mutat. Res. 75: 131–168.
Furet P, Caravatti G, Lydon N, Priestle JP, Sowadski JM, Trinks U,Traxler P. 1995. Modelling study of protein kinase inhibitors: bind-ing mode of staurosporine and origin of the selectivity of CGP52411. J. Comput. Aid. Mol. Des. 9: 465–472.
Gillies RJ, Didier N, Denton M. 1986. Determination of cell number inmonolayer cultures. Anal. Biochem. 159: 109–113
Gorczya W, Gong J, Ardelt B, Traganos F, Darzynkiewicz Z. 1993.The cell-cycle related differences in susceptibility of HL-60 cells toapoptosis induced by various anti-tumour agents. Cancer Res. 53:3186–3192.
Griffiths GD, Lindsay CD, Upshall DG. 1994. Examination of thetoxicity of several protein toxins of plant origin using bovine pulmon-ary endothelial cells. Toxicology 90: 11–27.
Gross CL, Innace JK, Hovatter RC, Meier HL, Smith WJ. 1993. Bio-chemical manipulation of intracellular glutathione levels influencescytotoxicity to isolated human lymphocytes by sulphur mustard. Cell
Biol. Toxicol. 9: 259–268.Haber LF. 1986. The Poisonous Cloud: Chemical Warfare in the First
World War. Oxford University Press: Oxford.Hendricks SP, Matthews CK. 1998. Differential effects of hydroxyurea
upon deoxyribonucleoside triphosphate pools, analyzed with vacciniavirus ribonucleotide reductase. J. Biol. Chem. 273: 29519–29523.
Hoffman BD, Hanauskeabel HM, Flint A, Lalande M. 1991. A newclass of reversible inhibitors. Cytometry 12: 26–32.
Inkoshi J, Katagiri M, Arima S. 1999. Neuronal differentiation of neuro2a cells by inhibitors of cell cycle progression trichostatin A andbutyrolactone. Biochem. Biophys. Res. Commun. 256: 372–376.
Klassen CD, Amdur MO, Doull J. 1986. Casarett and Doull’s Toxicol-
ogy: The Basic Science of Poisons. Macmillan Publishing: New York.Lee SE, Mitchell RA, Cheng A, Hendrickson EA. 1997. Evidence for
DNA-PK-dependent and -independent DNA double-strand breakrepair pathways in mammalian cells as a function of the cell cycle.Mol. Cell Biol. 17: 1425–1433.
Lindsay CD, Hambrook JL. 1997. Protection of A549 cells against thetoxic effects of sulphur mustard by hexamethylenetetramine. Hum.
Exp. Toxicol. 16: 106–114.Lindsay CD, Hambrook JL. 1998. Diisopropylglutathione ester protects
A549 cells from the cytotoxic effects of sulphur mustard. Hum. Exp.
Toxicol. 17: 606–612.Lindsay CD, Hambrook JL, Smith CN, Rice P. 1996. Histological as-
sessment of the effects of percutaneous exposure of sulphur mustardin an in vitro human skin system and the therapeutic properties of
protease inhibitors. Symposium paper, In Medical Defense
Biosciences Review, vol. II. US Army Medical Research and Devel-opment Command: Baltimore; 899–908.
Lindsay CD, Hambrook JL, Lailey AF. 1997. Monoisopropylglutathioneester protects A547 cells from the cytotoxic effects of sulphurmustard. Hum. Exp. Toxicol. 16: 636–644.
Marko D, Schatzle S, Friedel A, Genzlinger A, Zankl H, Meijer L,Eisenbrand G. 2001. Inhibition of cyclin-dependent kinase 1 (CDK1)by indirubin derivatives in human tumour cells. Br. J. Cancer 84:283–289.
Maynard RL. 1987. A medical review of chemical warfare agents.
Technical Paper No. 484. CBDE: Porton Down.Miura M, Sasaki T, Takasaki Y. 1996. Characterization of x-ray-
induced immunostaining of proliferating cell nuclear antigen inhuman diploid fibroblasts. Radiat. Res. 145: 75–80.
Morice WG, Brunn GJ, Wiederrecht G, Siekierka JJ, Abraham RT.1993. Rapamycin-induced inhibition of p34cdc2 kinase activation isassociated with G1/S-phase growth arrest in lymphocytes-T. J. Biol.
Chem. 268: 3734–3738.Murnane JC, Byfield JE. 1981. Irreparable DNA cross-links and
mammalian cell lethality with bifunctional alkylating agents. Chem.
Biol. Interact. 38: 75–86.Mutomba MC, Wang CC. 1996. Effects of aphidicolin and hydroxyurea
on the cell cycle and differentiation of trypanosoma brucei bloodstream forms. Parasitology 80: 89–102.
Naghii MR. 2002. Sulfur mustard intoxication, oxidative stress, andantioxidants. Mil. Med. 167: 573–575.
Ormerod MG. 1996. Analysis of DNA — general methods. In Flow
Cytometry: a Practical Approach, Ormerod MG (ed.). IRL Press:Oxford; 19–135.
Rice P, Brown RFR. 1999. The development of lewisite vapour inducedlesions in the domestic white pig. Int. J. Exp. Pathol. 80: 59–67.
Ruegg UT, Burgess GM. 1989. Staurosporine, K-252 and UCN-01:potent nonspecific inhibitors of protein kinases. Trends Pharmacol.
Sci. 10: 218–220.Schutte B, Nieland L, Engeland MV, Henfling MER, Meijer L,
Ramaekers FCS. 1997. The effect of the cyclin-dependent kinaseinhibitor olomoucine on cell cycle kinetics. Exp. Cell. Res. 236: 4–15.
Smith ML, Seo YR. 2002. p53 regulation of DNA excision repairpathways. Mutagenesis 17: 149–156.
Smith WJ, Sanders KM, Gales YA, Gross CL. 1991. Flow cytometricanalysis by vesicating agents in human cells in vitro. J. Toxicol. Cut.
Ocul. Toxicol. 10: 33–42.Smith CN, Lindsay CD, Upshall DG. 1997. Presence of methenamine/
glutathione mixtures reduces the cytotoxic effect of sulphur mustard.Hum. Exp. Toxicol. 16: 247–253.
Smith CN, Lindsay CD, Hambrook JL. 2001. An in vitro comparisonof the cytotoxicity of sulphur mustard in melanoma and keratinocytecell lines. Hum. Exp. Toxicol. 20: 483–490.
Sparfel L, Langouet S, Fautrel A, Salles B, Guillouzo A. 2002. Invest-igations on the effects of oltipraz on the nucleotide excision repair inthe liver. Biochem. Pharm. 63: 745–749.
Swe M, Bay BH, Sit K. 1996. Interphase and M-phase oral KBcarcinoma cells are targeted in staurosporine-induced apoptosis.Cancer Lett. 104: 145–152.
Tomkinson AE, Mackey ZB. 1998. Structure and function of mamma-lian DNA ligases. Mutat. Res. 407: 1–9.
Tuteja N, Tuteja R. 2001. Unraveling DNA repair in humans: molecularmechanisms and consequences of DNA repair defect. Crit. Rev.
Biochem. Mol. Biol. 36: 261–290.Vogt RF, Dannenberg Jr AM, Schofield BH, Hynes NA, Papirmeister
B. 1984. Pathogenesis of skin lesions caused by sulphur mustard.
Fundam. Appl. Toxicol. 4: S71–S83.Wagner ED, Rayburn AL, Anderson D, Plewa MJ. 1998. Analysis of
mutagens with single cell gel electrophoresis, flow cytometry andforward mutation assays in an isolated clone of chinese hamsterovary cells. Environ. Mol. Mutagen. 32: 360–368.
Wang JYJ. 1998. Cellular responses to DNA damage. Curr. Opin. Cell
Biol. 10: 240–247.Wang T. 1996. Cellular DNA Polymerases. In DNA Replication
in Eukaryotic Cells, DePamphilis, LM (ed.). Cold Spring HarbourLaboratory Press: Cold Spring Harbour; 461–493.
Wood RD, Shivjii MKK. 1997. Which DNA polymerases are used forDNA-repair in eukaryotes? Carcinogenesis 18: 605–610.
128 R. SIMPSON AND C. D. LINDSAY
Published in 2005 by John Wiley & Sons, Ltd. J. Appl. Toxicol. 2005; 25: 115–128
Xu H, Zhang P, Liu L, Lee MYWT. 2001. A novel PCNA-bindingmotif identified by the panning of a random peptide display library.Biochemistry 40: 4512–4520.
Yanagihara N, Tachikawa E, Izumi F, Yasugawa S, Tamamoto H,Miyamotot E. 1991. Staurosporine-An effective inhibitor for Ca2+/calmodulin-independent protein kinase II. J. Neurochem. 56: 294–298.
Yarbro JW. 1992. Mechanism of action of hydroxyurea. Semin. Oncol.
19: 1–10.Zong ZP, Fujikawa-Yamamoto K, Li AL, Yamaguchi N, Chang YG,
Murakami M, Odashima S, Ishikawa Y. 1999. Both low and highconcentrations of staurosporine induce G1 arrest through down-regulation of cyclin E and CDK2 expression. Cell Struct. Funct. 24:457–463.