Chrysochromulina fragaria sp. nov. (Prymnesiophyceae), a new haptophyte flagellate from Norwegian...
Transcript of Chrysochromulina fragaria sp. nov. (Prymnesiophyceae), a new haptophyte flagellate from Norwegian...
Phycologia (1999) Volume 38 (2), 149-155 Published 16 July 1999
Chrysochromulina fragaria sp. nov. (Prymnesiophyceae), a new haptophyte flagellate from Norwegian waters
WENCHE EIKREM AND BENTE EDV ARDSEN
Section for Marine Botany, Department of Biology, University of Oslo, P. O. Box 1069 Blindem, 0316 Oslo, Norway
W. EIKREM AND B. EDVARDSEN. 1999. Chrysochromulina fragaria sp. nov. (Prymnesiophyceae), a new haptophyte flagellate
from Norwegian waters. Phycologia 38: 149-155.
Chrysochromulina fragaria sp. nov. was one of the dominant species during the 1994 and 1995 Chrysochromulina blooms off the southern coast of Norway. It was isolated by the serial dilution culture method from a surface water sample collected during
the bloom in May-June 1994. The cells are spherical, 4 to 8 f.lm in diameter, and possess a coiling haptonema that is shorter than the two equal to subequal flagella. Each cell contains two chloroplasts, a nucleus, and one mitochondrion, which appears to be
reticulate. The periplast is covered by monomorphic scales (scale faces with identical pattern) of two types arranged in layers. The scale faces have a pattern of radiating ribs arranged in quadrants. One type has inflexed rims, whereas the other lype has erect rims. The first internal transcribed spacer (ITS 1) rONA sequence and scale morphology of C. fragaria are compared with that of Chrysochromulina sp. CCMP 1204. Despite the great similarities in scale morphology, their ITS I rONA regions are very different, indicating that they are different species. Both C. fragaria and Chrysochromulina sp. CCMP 1204 are nontoxic to Artemia franciscana nauplii.
INTRODUCTION
The number of known species in the genus Chrysochromulina
Lackey has increased steadily since the description of the first
marine species by Parke et al. (1955, 1956), and it is now one
of the marine phytoplanktonic genera with the greatest num
ber of species. More than 50 species have been described, and 38 of them have been observed in Scandinavian waters. In
addition, from Scandinavian waters alone we know of 30
forms not described in the literature (Eikrem et al. 1998; Jen
sen 1998) and the number of Chrysochromulina species
worldwide is expected to exceed 100 (Thomsen et al. 1994).
Members of the genus Chrysochromulina are unicellular,
nanoplanktonic, photosynthetic flagellates. Most species are
marine; only a few occur in freshwater (Green & Jordan
1994). They possess two smooth flagella and a haptonema that
is readily recognized with the light microscope. The length of
the haptonema varies greatly from many times the cell di
ameter in some species of Chrysochromulina [e.g. c. 160 fLm
long in C. camella Leadbeater et Manton (Lead beater & Man
ton 1969)] to less than the cell length in others [e.g. c. 5 fLm
in Chrysochromulina spinifera (Fournier) Pienaar et Norris
(Pienaar & Norris 1979)].
Chrysochromulina cells are covered by one to several kinds
of scales arranged in layers. The scales are organic and com
posed mainly of proteins and carbohydrates (Leadbeater 1994). The basic scale is a round or oval plate composed of
micro fibrils, but the variation is great, and many highly sculp
tured and elaborate scale forms are found. The scales of many
species consist of a proximal layer of micro fibrils arranged in
a radial pattern, whereas the pattern of the distal microfibrillar
layer is more variable. Scales may have monomorphic faces (the two scale faces having identical patterns) or dimorphic
faces (the scale faces having different patterns). The cells con
tain two golden-brown chloroplasts, each with a pyrenoid that
may be bulging. The nucleus is posterior or central and the
outer membrane of the nuclear envelope is confluent with the
endoplasmic reticulum enveloping the chloroplast (Hibberd
1980). Located immediately within the cell membrane is a
layer of peripheral endoplasmic reticulum that also extends
into the haptonema (Pienaar 1994). The mitochondrion prob
ably forms a network, as was shown for the coccolithophorid
Pleurochrysis carterae (Braarud et Fagerland) Christensen
(Beech & Wetherbee 1984). The flagellar apparatus consists
of two basal bodies, the haptonematal base, microtubular and
fibrous roots, and accessory and connecting fibers. The mi
crotubular root (R,), which is connected to the mature flagel
lum, may be either simple (a sheet of microtubules) or com
pound (a sheet and a crystalline bundle), and its structure
varies between the species within the genus as presently de
limited. The microtubular root R2 has an origin between the
two basal bodies, is simple, and consists of just a few micro
tubules in the species examined so far. The roots associated
with the right flagellar base contain only a few microtubules (Green & Hori 1994).
With few exceptions, identification of Chrysochromulina
species relies on the examination by electron microscopy of
the organic scales covering the periplast (Lead beater 1994).
We present some morphological and ultrastructural details of
C. fragaria sp. nov., in addition to its sequence of the first
internal transcribed spacer (ITS1) rDNA, and compare it with
that of Chrysochromulina sp. CCMP 1204, which shows a
scale morphology reminiscent of that of C. fragaria sp. nov.
MATERIAL AND METHODS
Cultures
Cultures of Chrysochromulina fragaria were established from
cells isolated by the serial dilution culture method (Throndsen
1978) during a bloom dominated by species of Chrysochrom-
149
150 Phycologia, Vol. 38 (2), 1999
ulina off the southern coast of Norway in May-June 1994.
Strain S19 originated from a surface water sample collected
on 20 May 1994 off FI\'ldevigen (58°25'N, 8°46'E), and strain
U21 was from a surface water sample collected on 2 June
1994 off Grimstad (58°20'N, 8°36'E).
Chrysochromulina sp. strain CCMP 1204, obtained from
the Provasoli-Guillard National Center for Culture of Marine
Phytoplankton (CCMP), was isolated by R. Selvin from a wa
ter sample collected at Baffin Bay, Canada (76°25'N,
82°55'W) on 3 June 1986.
Stock cultures of C. fragaria were grown in filtered sea
water diluted to 30 psu, enriched with nutrients, vitamins, and
trace metals as in IMR 112 medium (Eppley et at. 1967), and
supplemented with 10 nM selenite. The cultures were grown
at 15°C under white fluorescent light with a photon fluence
rate (PFR) of about 50 /-Lmol photons m-2 S-I and a 12:12 h
LD cycle. Stock cultures of strain CCMP 1204 were grown
in K-medium (Keller et at. 1987) at 3°C under similar light
conditions as above. Stock cultures were transferred to new medium every 14 d.
Light microscopy
Living cells of the strains S19 and CCMP 1204 were studied with a Nikon Microphot FX fitted with phase contrast and
differential interference contrast optics and electronic flash.
Strain S19 was photographed using phase contrast and flash.
Electron microscopy
Positively stained whole mounts of strains S19 and CCMP
1204 were prepared according to Moestrup (1984). Some of
the preparations were shadowed with gold-palladium using an
Edward's Speedivac 12 E6 coating unit, c. 30° angle of shadowing.
Thin sections of S19 were prepared according to the fol
lowing protocol. The cells were fixed in 2% glutaraldehyde in
medium for 2 h and rinsed 3 times at 30-min intervals in
medium followed by 2 times at lO-min intervals in 0.1 M Na
cacodylate buffer (pH 8). Postfixation was carried out in 1 %
osmium tetroxide and 1 % ferricyanide in 0.1 M Na cacodylate
buffer for 3 h. The cells were then rinsed 3 times at IS-min
intervals in Na cacodylate buffer and 2 times at lO-min in
tervals in distilled water. The samples were left overnight in
2% aqueous uranyl acetate. Subsequently the cells were rinsed
in distilled water and dehydrated in an ethanol series starting
at 30% and gradually rising to 96%. The dehydration was
concluded with changes in 100% ethanol 4 times at lO-min
intervals and changes in propylene oxide 2 times at lO-min
intervals. The pellets were left overnight in a 1: 1 mixture of
propylene oxide and Epon embedding resin (Burke & Giesel
man 1971). Finally, the cells were changed in Epon 3 times
at I-h intervals before they were polymerized at 50°C for 12
h. The thin sections were stained with lead citrate. Thin sec
tions and whole mounts were viewed in a Jeol 1200ex trans
mission electron microscope.
Artemia bioassay
Toxicity tests were performed using a strain of the crustacean
Artemia franciscana (Creasel, Deinze, Belgium) as previously
described (Edvardsen 1993). Sixty nauplii were exposed to C.
fragaria strain U21 (9 X 108 cells 1-1) and Chrysochromulina
sp. strain CCMP 1204 (3 X 108 cells 1-1), and 30 nauplii were
exposed to C. fragaria strain S 19 for 24 h and 48 h at 25°C
in darkness. Seawater was used as control.
DNA extraction, amplification, and sequencing
DNA was extracted using a 3% CTAB (hexadecyltrimethylam
monium bromide) procedure (Doyle & Doyle 1990). Biotiny
lated and nonbiotinylated primers ITS 1 and ITS2 ( White et at.
1990) were used to amplify the internal transcribed spacer 1
(ITS 1) region. Polymerase chain reaction (PCR) amplifications
were performed in a Techne Genius using the following am
plification profile: 95°C for 5 min, 30 cycles at 50°C for 1 min,
72°C for 1 min and 95°C for 1 min, and a final extension at
noc for 7 min. The PCR reaction mixtures (50 /-Ll) contained
1 U Taq DNA polymerase (Advanced Biotechnologies, UK),
50 ng DNA, 0.5 /-LM of each primer, 200 /-LM dNTp, 2.5 mM
MgCI2, 5 /-Ll lOX reaction buffer, and 5% acetamide. Single
stranded DNA, obtained from the PCR products by using M-
280 streptavidine-coated magnetic Dynabeads (Dynal AS, Nor
way), were sequenced directly with the use of the Sequenace
version 2.0 DNA Sequencing Kit (United States Biochemical)
according to the manufacturer's protocol and were run manually
on 6% acrylamide gels (Sambrook et al. 1989). DNA sequenc
es have been submitted to GenBank: C. fragaria S 19,
AJ238708, Chrysochromulina sp. CCMP 1204, AJ238709.
The alignment was performed automatically using Clustal
W in the GCG package. The distance value was estimated by
Kimura two-parameter analysis (Kimura 1980) using PHYLIP
(Felsenstein 1995).
OBSERVATIONS
Description of the new species
Chrysochromnlina fragaria Eikrem et Edvardsen sp. nov.
Figs 1-16
DIAGNOSIS: Cellulae sphaericae-subsphaericae 4-S JJ.m, appendices in tenuem depressionem apical iter insertae. Haptonema (3-9 JJ.m) ftagellis plerumque aequalibus (10-16 JJ.m) brevius. Periplastus squamis duarum formarum tectus. Squamae aut marginibus inftexis (50-100 nm) ovales vel orbiculares 0.35-0.75 X 0.45-0.S JJ.m, aut marginibus erectis (150-200 nm) orbicularis vel ovales 0.5-0.S X
0.5-0.S JJ.m. Facies proximales et distales utriusque formae squamarum striis radiantibus in quattuor quadrantes dispositis instructae.
Cells spherical to subspherical measuring 4-8 /-Lm, append
ages inserted apically in a slight depression. Haptonema (3-9
/-Lm) shorter than the usually equal flagella (10-16 /-Lm). Peri
plast covered with scales of two types. Scales with inflexed
rims (50-100 nm) oval to round 0.35-0.75 by 0.45-0.8 /-Lm
and scales with erect rims (150-200 nm) round to oval 0.5-
0.8 by 0.5-0.8 /-Lm. Proximal and distal faces of both scale
types with radiating ribs arranged in four quadrants.
HOLOTYPE: Figures 1-9.
ETYMOLOGY: Latin fragaria (strawberry). The organism
gives the impression of the shape of a squat strawberry in the
light microscope.
Eikrem & Edvardsen: A new species of Chrysochromulina 151
".
0.5 Jlm
Figs 1-7. Chrysochromulina fragaria sp. nov. Figs 1, 2. Light micrographs (phase contrast) of living cells. Figs 3-5. Shadow-cast whole mounts of scales. Distal scale faces (arrows). proximal scale faces (arrowheads). Outer layer scales (white arrow, white arrowhead), inner layer scales (black arrows, black arrowheads). Figs 6, 7. Thin sections of scales.
Fig. 6. Cross section showing scales with inflexed rims (arrow) and scales with upright rims (arrowhead). Fig. 7. Tangential section of scales.
Microscopic observations of Chrysochromulina fragaria
sp. nov. strain 819
The spherical to subspherical cells (4-8 J-Lm) bear a hapto
nema (3-8 J-Lm) that is shorter than the two equal or subequal
flagella (10-14 J-Lm) and is capable of coiling. The appendages
are inserted in a slight apical depression (Figs 1,2). Two types
of scales cover the periplast. We have not been able to produce
sections of cells with intact scale investments, but we assume
that the scales are arranged in two layers, with the scales having the tall, erect rims forming the outer layer. We also assume that the rims are on the distal face of the scales, which is
usually the case in Chrysochromulina species (Lead beater 1994). The inner layer consists of round to oval plate scales (0.35-0.75 by 0.45-0.8 J-Lm) with an inflexed rim (50-100
nm) with concentric fibers. Both scale faces have radiating ribs (c. 65-90) extending from center to edge (proximal face) or rim (distal face). The round scales of the outer layer (0.5-
152 Phycoiogia, Vol. 38 (2), 1999
8 9
0.5 J.Lm
12
•
Figs 8-16. Thin sections showing ultrastructural features of Chrysochromulina Jragaria sp. nov.; b, basal body; c, chloroplast; f, flagellum; h, haptonema; m. mitochondrion; n, nucleus; p, pyrenoid.
Fig. 8. Longitudinal section of cell with posterior nucleus, two chloroplasts, a pyrenoid with part of a traversing thylakoid (arrowhead), mitochondrial profile, flagellum, and a Golgi apparatus (arrow). Fig. 9. Cross section through cell showing the 'peculiar' dilations of the Golgi apparatus (arrow). Figs 10, 11. Scales are produced in the Golgi apparatus, which is in the anterior part of the cell. The scales are released near the base of the appendages. Figs 12-14. The flagellar transition zone. Proximal band (arrow), distal band (arrowhead). Fig. 15. Section through the flagellar apparatus showing flagellum, part of the haptonema, and the basal body. Fig. 16. Section through the haptonema showing the seven microtubules.
Eikrem & Edvardsen: A new species of Chrysochromulina 153
Figs 17, 18. Whole mounts of Chrysochromulina sp. CCMP 1204. Fig. 17. Whole cell with detached scales. Stained with uranyl ace-tate. Fig. 18. Details of scales. Shadow-cast preparation showing the two scale types (arrow, arrowhead).
0.8 by 0.5-0.8 fLm) have tall erect rims (150-200 nm) with
no obvious pattern, and the radiating ribs (c. 75-90) extend
from the center to the rim on the distal face and from center
to edge on the proximal face (Figs 3-7). The pattern created
by the radiating ribs divides the scales into four distinct quad
rants (Fig. 7) in both scale types.
The cells contain two golden-brown, parietal chloroplasts,
each with an immersed pyrenoid that may be bulging and may
be traversed by thylakoids, a posterior nucleus, a mitochon
drion, and a Golgi body where the scales are produced (Figs
8-11).
The flagellar apparatus (Fig. 15) has not been studied in
detail, but some features have been revealed. The flagella have
a proximal band consisting of a tripartite plate and a distal
band with a transitional plate (Figs 12-14). The extended part
of the haptonema contains seven microtubules (Fig. 16).
To allow a comparison between the scales of C. fragaria
sp. nov. and those of Chrysochromulina sp. CCMP 1204, we
have included electron micrographs (Figs 17, 18) of a whole
cell and detached scales. Under the light microscope the cells
appear spherical to pear shaped (8-14 by 6-10 fLm). The cells
may be strongly compressed dorsoventrally. The haptonema
(12-20 fLm) is slightly shorter than the flagella (14-24 fLm).
The scales are of two types: one type has an erect rim (85-
100 nm) and measures 0.7-0.9 by 0.8- l .0 fLm; the rim of the
other type appears inflexed (35-50 nm) and it measures 0.5-
0.8 by 0.6-0.9 fLm. All scale faces have radiating ribs (c. 75-
85).
Artemia bioassay
Strains of C. fragaria (S19 and U21) and Chrysochromulina
sp. CCMP 1204 that were grown in complete medium were
nontoxic to Artemia nauplii (all 60/30 nauplii survived in each
test) when exposed for 24 and 48 h under the conditions used.
ITS! nucleotide sequences
Nucleotide sequences of ITS 1 rDNA and flanking stretches of
18S and 5.8S rDNA regions were determined for C. fragaria
strain S19 and Chrysochromulina sp. strain CCMP 1204 (Fig.
19). Terminals of the 18S rRNA coding region and starting
positions of the 5.8S region were determined by comparison
with other haptophytes (Larsen & Medlin 1997; Edvardsen &
Medlin 1998). The length of the ITS1 region was 326 base
pairs (bp) in C. fragaria and 381 bp in Chrysochromulina sp.
strain CCMP 1204. The G/C content of ITS 1 was much higher
in C. fragaria (71%) than in CCMP 1204 (58%). Pairwise
comparisons, including gaps of strain S19 and CCMP 1204,
revealed a distance value of approximately 0.61 (Kimura two
parameter) for the ITS 1 region.
DISCUSSION
Of the species of Chrysochromulina already described, there
are several that resemble C. fragaria when examined by light
microscopy. For instance, C. minor Parke et Manton, C. kappa
Parke et Manton, C. brevifilum Parke et Manton, and C. ad
riatica Leadbeater have the same general appearance as C.
fragaria and are in the same size range. Also, species that are
typically oblong or pear shaped may produce cells that are
round (e.g. C. polylepis Parke et Manton) and may then be
confused with C. fragaria at the light microscope level.
Despite the similarities in cell and scale morphology, ITS 1
data show that Chrysochromulina sp. CCMP 1204 should be
considered a separate species from C. fragaria. The scales of
C. fragaria are in the same size range as the scales of Chrys
ochromulina sp. CCMP 1204 and the number of radiating ribs
overlap. The height of the upright rims and the width of the inflexed rims in C. fragaria are greater than the corresponding
rims in Chrysochromulina sp. CCMP 1204. Length of hap
tonema and flagella and cell size are somewhat overlapping
in the two species, but Chrysochromulina sp. CCMP 1204
tend to be larger with longer appendages. Another distinguish
ing character at the light microscope level is the pronounced
dorsoventral compression of many cells in the Chrys
ochromulina sp. CCMP 1204 cultures; this has not been ob
served in cultures of C. fragaria sp. nov.
The scales of both C. fragaria and Chrysochromulina sp.
CCMP 1204 closely resemble the scales of what once was be
lieved to be a mutant of C. chiton Parke et Manton (Manton
1966, 1967a, 1967b). In the light of recent research on C. pol
ylepis (Edvardsen & Paasche 1992; Edvardsen & Medlin 1998)
one may speculate that C. chiton has two distinct flagellate
forms. In the original culture, C. chiton (Parke et al. 1958)
possessed two types of scales with dimorphic scale faces. After
some time in the history of the culture a flagellate covered with
two types of scales with monomorphic scale faces turned up
(Manton 1966, 1967a, 1967b). According to a hypothesis based
on the morphology of underlayer scales in coccolithophorids,
scales having dimorphic scale faces represent the haploid gen
eration and scales with monomorphic scale faces the dipl0id
generation (Billard 1994). Applying this hypothesis to the case
154 Phycologia, Vol. 38 (2), 1999
_____________________________ 18S __________________________ _
C. fragaria
CCMP 1204
????????? ?????????? ?????????? ?????????? ?????????? ???????TGCG
CAAGATATC CATCGACAAG AGTTGTGTGT TTGTTGGTTC TTGAGAGGCT ACGCAAG AAA.
18S __ ITS1
C. fragaria
CCMP 1204
GAAGGATCA -TTACCAGGT CTTTCCACCC GCACCCTTGC GTACCGTTTC CGTCTTCCGGG
......... A .... C-... .......... .... GTA ... .... A .. CAA T-.G.A .. CCT
C. fragaria
CCMP 1204
CGCGCACCGT TTCATTATCG GAGCGCGTCC TCTGCGCGTC -GGCGTC-CG CCTCCGTGCG
G. G. GGT .. G C .. GAG. GG. CC. GT . -. .. . ... T . TC.. T ...... A.. GG ....... T
C. fragaria
CCMP 1204
TG-------G CGTCGTCGC- ------GCAG GCACTGCT-G GCTCGTCCGG CAGCCGTCTG
C.CATTGGC . ........ GT ATCTTTTTT . . T.TC.T.C. T.GT ... GT. AG.G .. G.CT
C. fragaria
CCMP 1204
GCCGCCTCGG C-.-TCCCCGC CGTAGCGTGC --------CC CCCGCTGGAG CGCCG--T-
.GG .. G .... GCA.A.AG .. AC.G.A.A .. AGAAGGTG.G .T .. T ... TT TT.T.TT.TC
C. fragaria
CCMP 1204
------GCC- GCGCGCGTCC GCGTCGTGCG CGTCGCGTG- G-------CC CTT----GCC
AGAAGC ... T ... T.T .. GG T.T.T ..... . CAGC .... C .TTGAGTT.T ... ATGG.AG
C. fragaria
CCMP 1204
CT----GTCT CCA GGGTGCG GTCCTCGCGT GC-GTCTCGC GCGTCGCGCC CGTCC GGCCT
.. TAGC .. GC .. TT .. A .. T TAG .. G.A.A .GT.C .. TTA A .. GG ... TT TT .. TT .. G.
ITS1 __ S.8S __________________ __
C. fragaria
CCMP 1204
--CCACTCGA GTTGTCACAA -CACACAACT CTTGTCGATG GATATCTTGG CTCTCRCATC
AG .. T ... A . . AACCA .... A ........ . ??????????
Fig. 19. Sequence alignment of ITSI rDNA and flanking stretches of l 8S and 5.8S rDNA of Chrysochromulina fragaria strain SI9 and Chrysochromulina sp. strain CCMP 1204 done in Clustal W.
of C. chiton would imply that the 'mutant' is the diploid gen
eration and the flagellate originally described as C. chiton rep
resents the haploid generation. Considering the large number
of species in the genus, it is tempting to speculate that mor
phologically distinct flagellate stages occur in more species, but
for the 18 species of Chrysochromulina in which the 18S rRNA
gene has been analyzed, it has been shown to be the case only
in Chrysochromulina polylepis. The others appear to be sepa
rate species (Edvardsen, unpublished observations).
The saddle-shaped C. parva Lackey is the type species of
the genus Chrysochromulina. The fact that C. fragaria sp. nov.
and several other Chrysochromulina species differ from the
saddle-shaped species with respect to morphology, ultrastruc
ture, and I8S rRNA signatures (e.g. Green & Hori 1994; Green
& Jordan 1994; Birkhead & Pienaar 1995; Medlin et al. 1997;
Eikrem & Moestrup 1998; Edvardsen, Eikrem, Green, Medlin,
and Moestrup, unpublished observations) may eventually lead
to the erection of a new genus that will include C. fragaria sp.
nov. Molecular data have shown that Chrysochromulina is not
a monophyletic group, and according to 18S rRNA data, C.
fragaria is more closely related to, for example, C. polylepis,
C. chiton, C. kappa, Prymnesium parvum (N. Carter) Green et
al., P. patelliferum Green et aI., and P. calathiferum Chang et
Ryan than to the saddle-shaped species of Chrysochromulina
(Medlin et al. 1997; Simon et al. 1997). Further studies should
include detailed examination of the flagellar apparatus of C.
jragaria, which should be compared with that of genetically
related species.
The Chrysochromulina bloom in May 1994 off the south
coast of Norway was dominated by C. fragaria, c. polylepis,
C. acantha, and C. brevifilum. In 1995, C. fragaria and C.
polylepis occurred in high concentrations in the same area
(Dahl et aI. 1998). Thus, C. fragaria can be a quantitatively
important species in Scandinavian waters. Scales that may be
assigned to C. fragaria have also been observed in the Baltic
(Hajdu et at. 1996) and in Danish waters (Jensen 1998).
ACKNOWLEDGMENTS
We thank Sissel Brubak and Lisbeth Haukrough for excellent
technical assistance and Bjl1lrg Tosterud for preparing the Latin diagnosis. Dag Klaveness and E. Paasche kindly read the man
uscript. Electron microscopy was carried out at the laboratories
for Biosciences, Department of Biology, University of Oslo.
REFERENCES
BEECH PL. & W ETHERBEE R. 1984. Serial reconstruction of the mi
tochondrial reticulum in the coccolithophorid Pleurochrysis carter
ae (Prymnesiophyceae). Protoplasma 123: 226-229.
BILLARD C. 1994. Life cycles. In: The Haptophyte Algae (Ed. by J.e.
Green & B.S.e. Leadbeater), pp. 167-186. Clarendon Press, Oxford.
BIRKHEAD M. & PIENAAR R.N. 1995. The taxonomy and ultrastructure of Chrysochromulina simplex (Prymnesiophyceae). Phycologia 34: 145-156.
BURKE e.N. & GIESELMAN C.W. 1971. Exact anhydride epoxy per
centages for electron microscopy embedding (Epon). Journal of ULtrastructure Research 36: 119-126.
DAHL E., EDVARDSEN B. & EIKREM W. 1998. Chrysochromulina
blooms in the Skagerrak after 1988. In: Harmful Algae = Algas
Nocivas. Proceedings of the 8th International Conference on Harm-
Eikrem & Edvardsen: A new species of Chrysochromulina 155
ful Algae. Vigo, Spain, 1997 (Ed. by B. Reguera, J. Blanco, M.-L.
Fernandez & T Wyatt), pp. 104-105. International Oceanographic
Commission, UNESCO, Vigo, Spain. DOYLE J.J & DOYLE J.L. 1990. Isolation of plant DNA from fresh
tissue. Focus 12:13-15.
EDVARDSEN B. 1993. Toxicity of Chrysochromulina species (Prymnesiophyceae) to the brine shrimp, Artemia salina. In: Toxic Phy
toplankton Blooms in the Sea (Ed. by T.J. Smayda & Y. Shimizu), pp. 681-686. Elsevier, Amsterdam.
EDVARDSEN B. & MEDLIN L. 1998. Genetic analyses of authentic and alternate forms of Chrysochromulina polylepis (Haptophyta). Phy
cologia 37: 275-283.
EDVARDSEN B. & PAASCHE E. 1992. Two motile stages of Chryso
chromulina polylepis (Prymnesiophyceae): morphology, growth,
and toxicity. Journal of Phycology 28: 104-114.
EIKREM W., JENSEN M.0., MOESTRUP 0. & THRONDSEN J. 1998. An
illustrated key to the unmineralized prymnesiophyceaen flagellates
of Scandinavian marine waters with special reference to the genus
Chrysochromulina. In: The Genus Chrysochromulina (Prymnesio
phyceae) in Scandinavian Coastal Waters-Diversity, Abundance
and Ecology, pt. 5 (By M.0. Jensen), pp. 1-36. PhD Thesis, University of Copenhagen.
EIKREM W. & MOESTRUP 0. 1998. Structural analysis of the flagellar
apparatus and the scaly periplast in Chrysochromulina scutellum sp.
nov. (Prymnesiophyceae, Haptophyta) from the Skagerrak and the
Baltic. Phycologia 37: 132-153.
EpPLEY R.W., HOLMES R.W. & STRICKLAND J.D.H. 1967. Sinking rates
of marine phytoplankton measured with a fluorometer. Journal of
Experimental Marine Biology and Ecology. 1: 191-208. FELSENSTEIN J. 1995. PHYLIP (Phylogeny Inference Package) version
3.57c. Distributed by the author. Department of Genetics, University
of Washington, Seattle.
GREEN J.e. & HORI T 1994. Flagella and flagellar roots. In: The Hap
tophyte Algae (Ed. by J.C. Green & B.S.e. Leadbeater), pp. 47-71.
Clarendon Press, Oxford.
GREEN J.e. & JORDAN R.W. 1994. Systematic history and taxonomy.
In: The Haptophyte Algae (Ed. by J.e. Green & B.S.e. Leadbeater),
pp. 1-21. Clarendon Press, Oxford. HAJDU S., LARSSON U. & MOESTRUP 0. 1996. Seasonal dynamics of
Chrysochromulina species (Prymnesiophyceae) in a coastal area
and a nutrient-enriched inlet of the Northern Baltic proper. Botanica
Marina 39: 281-295.
HIBBERD DJ. 1980. Prymnesiophytes (= Haptophytes). In: Phytofia
gellates (Ed. by E.R. Cox), pp. 273-317. ElsevierlNorth Holland,
New York.
JENSEN M.0. 1998. Seasonal dynamics of Chrysochromulina species
(Prymnesiophyceae, Haptophyta) in Danish coastal waters: diver
sity, abundance and ecology. In: The Genus Chrysochromulina
(Prymnesiophyceae) in Scandinavian Coastal Waters-Diversity,
Abundance and Ecology, pt. 4 (By M.0. Jensen), pp. 1-38. PhD
Thesis, University of Copenhagen.
KIMURA M. 1980. A simple method for estimating evolutionary rates
of base substitutions through comparative studies of nucleotide se
quences. Journal of Molecular Evolution 16: 111-120.
KELLER M.D., SELVIN R.C., CLAUS W. & GUILLARD R.R.L. 1987. Me
dia for the culture of oceanic ultraphytoplankton. Journal of Phy
cology 23: 633-638. LARSEN A. & MEDLIN L.K. 1997. Inter- and intraspecific genetic var
iation in twelve Prymnesium (Haptophyceae) clones. Journal of
Phycology 33: 1007-1015. LEADBEATER B.S.e. 1994. Cell coverings. In: The Haptophyte Algae
(Ed. by J.e. Green & B.S.e. Leadbeater), pp. 23-46. Clarendon
Press, Oxford. LEADBEATER B.S.C. & MANTON I. 1969. Chrysochromulina camella
sp. nov. and C. cymbium sp. nov., two new relatives of C. strobilus
Parke and Manton. Archiv fUr Mikrobiologie 68: 116-132.
MANTON I. 1966. Further observations on the fine structure of Chrys
ochromulina chiton, with special reference to the pyrenoid. Journal
of Cell Science 1: 187-192.
MANTON I. 1967a. Further observations on scale formation in Chrys
ochromulina chiton. Journal of Cell Science 2: 411-418. MANTON I. 1967b. Further observations on the fine structure of Chrys
ochromulina chiton with special reference to the haptonema, "peculiar" Golgi structure and scale production. Journal of Cell Sci
ence 2: 265-272. MEDLIN L.K., KOOISTRA W.H.e.F., POTTER D., SAUNDERS G.W. & AN
DERSEN R.A. 1997. Phylogenetic relationships of the "golden algae" (haptophytes, heterokont chromophytes) and their plastids. In: The
Origins of Algae and Their Plastids (Ed. by D. Bhattacharya), pp.
187-219. Springer-Verlag, Vienna. MOESTRUP 0. 1984. Further studies on Nephroselmis and its allies
(Prasinophyceae). II. Mamiella gen. nov. Mamiellaceae fam. nov. Mamiellales ord. nov. Nordic Journal of Botany 4: 109-121.
PARKE M., MANTON I. & CLARKE B. 1955. Studies on marine flagellates II. Three new species of Chrysochromulina. Journal of the
Marine Biological Association of the United Kingdom 34: 579-609. PARKE M., MANTON I. & CLARKE B. 1956. Studies on marine flagel
lates III. Three further species of Chrysochromulina. Journal of the
Marine Biological Association of the United Kingdom 35: 387-414.
PARKE M., MANTON I. & CLARKE B. 1958. Studies on marine flagel
lates IV. Morphology and microanatomy of a new species of Chrys
ochromulina. Journal of the Marine Biological Association of the
United Kingdom 37: 209-228. PIENAAR R.N. 1994. Ultrastructure and calcification of coccolitho
phores. In: Coccolithophores (Ed. by A. W inter & W.G. Siesser), pp. 13-37. Cambridge University Press, Cambridge.
PIENAAR R.N. & NORRIS R.E. 1979. The ultrastructure of the flagellate Chrysochromulina spinifera (Fournier) comb. nov. (Prymnesiophyceae) with special reference to scale production. Phycologia 18: 99-108.
SAMBROOK J., FRITSCH E.F. & MANIATIS T. 1989. Molecular Cloning:
A Laboratory Manual, 2nd ed., 3 vols. Cold Spring Harbor Laboratory Press, New York.
SIMON N., BRENNER J., EDVARDSEN B. & MEDLIN L.K. 1997. The identification of Chrysochromulina and Prymnesium species (Haptophyta, Prymnesiophyceae) using fluorescent or chemiluminescent oligonucleotide probes: a means for improving studies on toxic algae. European Journal of Phycology 32: 393-401.
THOMSEN H.A., BUCK K.R. & CHAVEZ F.P. 1994. Haptophytes as components of marine phytoplankton. In: The Haptophyte Algae (Ed. by J.e. Green & B.S.e. Leadbeater), pp. 187-208. Clarendon Press, Oxford.
THRONDSEN J. 1978. The dilution culture method. In: Phytoplankton
Manual (Ed. by A. Sournia), pp. 218-224. Monographs on Oceanographic Methodology 6, UNESCO, Paris.
W HITE TJ., BRUNS T, LEE S. & TAYLOR J. 1990. Amplification and direct sequencing of fungal ribosomal RNA genes for phylogenet
ics. In: PCR Protocols: A Guide to Methods and Applications (Ed. by M.A. Innis, D.H. Gelfand, J.J. Sninsky & TJ. W hite), pp. 315-322. Academic Press, San Diego.
Accepted 24 March 1999