REVIEW
NPR
Thomas O. Larsen, Jørn Smedsgaard, Kristian F. Nielsen, Michael E. Hansen and
Jens C. Frisvad
Center for Microbial Biotechnology, BioCentrum, Technical University of Denmark, DK-2800,
Kgs. Lyngby, Denmark
www.rsc.org/npr
Phenotypic taxonomy and metabolite profiling in microbial
drug discovery
Received (in Cambridge, UK) 30th September 2005
First published as an Advance Article on the web 7th November 2005
Covering: up to October 2005
Microorganisms and in particular actinomycetes and microfungi are known to produce a vast number of bioactive
secondary metabolites. For industrially important fungal genera such as Penicillium and Aspergillus the production of
these compounds has been demonstrated to be very consistent at the species level. This means that direct metabolite
profiling techniques such as direct injection mass spectrometry or NMR can easily be used for chemotyping/
metabolomics of strains from both culture collections and natural samples using modern informatics tools. In this
review we discuss chemotyping/metabolomics as part of intelligent screening and highlight how it can be used for
identification and classification of filamentous fungi and for the discovery of novel compounds when used in
combination with modern methods for dereplication. In our opinion such approaches will be important for future
effective drug discovery strategies, especially for dereplication of culture collections in order to avoid redundancy in
the selection of species. This will maximize the chemical diversity of the microbial natural product libraries that can
be generated from fungal collections.
1.
1.1
2.
2.1
2.2
2.3
2.4
3.
3.1
3.2
3.3
The potential of microbial natural products in drug
discovery
Antibiotics
Microbial biodiversity
Marine microorganisms
Terrestrial and insecticidal microorganisms
Non-culturable organisms
Molecular genetics and metabolic engineering
Chemotaxonomy and chemo-consistency
Fungal species specific production of profiles of NPs
Chemo-consistency
Phylogeny and classification: is production of natural
products homoplastic?
3.4
4.
5.
6.
Microbial physiology
The chemotaxonomy based drug discovery process
Morphology based strain selection—image analysis
Strategies and methodologies for metabolite profiling
and target analysis
Chemical profiling—TLC
Direct infusion electrospray mass spectrometry
Target analysis and dereplication by MS
Chemical image analysis—UV spectral analysis
Dereplication and partial identification of NPs by
UV-based techniques
Metabolite fingerprinting, profiling and target
analysis by NMR
6.1
6.2
6.3
6.4
6.5
6.6
Thomas O. Larsen was born in Slagelse, Denmark in 1963. He studied chemical engineering at the Technical University of Denmark
(DTU) with focus on organic chemistry and microbiology. After a job at Danisco A/S working on aroma synthesis he returned to DTU
to study fungal volatile production, supervised by Professor Jens C. Frisvad and received his PhD in 1994. After this he joined the Marine
Chemistry Group at the University of Copenhagen, headed by Reader Carsten Christophersen where he was trained as a classical natural
product chemist. In 2001 he stayed for seven months with Dr Nigel Perry, Crop & Food Research, University of Otago, Dunedin, New
Zealand. Currently he holds a position as associate professor at BioCentrum-DTU, at the Center for Microbial Biotechnology (CMB).
DOI: 10.1039/b404943h
Jørn Smedsgaard was born just outside Copenhagen, Denmark, in 1959. He studied at the DTU focusing on analytical chemistry. After
a master’s project focusing on enzyme kinetics studied by NMR in 1986, JS took a detour around a commercial environmental analytical
lab, before he set out to establish a mass spectrometry facility at the Agricultural University as a research assistance. In 1991 he returned
to DTU to set-up a mass spectrometric facility at the Department of Biotechnology (now BioCentrum) and at the same time given the
opportunity to do a PhD study supervised by Professor Jens Frisvad. JS received a PhD degree in 1996 for a chemotaxonomic study of
Penicillium species by direct infusion mass spectrometry. Currently JS holds a position as associate professor at BioCentrum-DTU and
is acting manager for the analytic metabolite profiling facility.
672
Thomas O. Larsen
Nat. Prod. Rep., 2005, 22, 672–695
This journal is
Jørn Smedsgaard
©
The Royal Society of Chemistry 2005
Kristian F. Nielsen was born just outside Copenhagen, Denmark in 1972. He studied chemical and biotech engineering at the DTU with
focus on analytical chemistry and microbiology. In collaboration with the Danish Building Research Institute he studied fungal growth
and mycotoxin production in water damaged buildings, supervised by Ulf Thrane and Suzanne Gravesen and received his PhD in 2001.
In 2004 he was awarded the research price of the Society of Mycotoxin Research for his PhD work. After holding a position as associate
research professor at BioCentrum-DTU, he has just joined Neurosearch A/S.
Michael E. Hansen was born in Nykøbing Falster, Denmark in 1970. He received an MSc degree in engineering from the Department of
Informatics and Mathematical Modelling at DTU, Kgs. Lyngby, in 1998 and a PhD degree in mathematics and statistics from the DTU
in 2004. He then joined CMB as an assistant research professor. His current research interests include developing statistical methods for
the analysis, data mining and data fusion of data extracted from microbiological organisms used within biotechnological applications,
e.g. metabolite profiling, drug discovery and biosystematics.
Jens C. Frisvad was born in Kgs. Lyngby, Denmark in 1952. He studied chemical engineering at the DTU with focus on organic chemistry
and mycology. He received his PhD in 1982 and defended his dr. techn. thesis on “Secondary metabolites and species concepts in
Penicillium and Aspergillus” in 1998. He became a full professor in Industrial Mycology at Biocentrum-DTU in 2001. In 1994 he stayed
for six months with Professor Martha Christensen, Department of Botany, University of Wyoming, Laramie to study Penicillium and
Aspergillus and has been visiting Dr Robert A. Samson, Centraalbureau voor Schimmelcultures, Utrecht, the Netherlands, extensively
to collaborate on mycology and taxonomy.
Kristian F. Nielsen
7.
8.
9.
Michael E. Hansen
Conclusions and future perspectives
Acknowledgements
References
1. The potential of microbial natural products in drug discovery
Microbial natural products (NPs, or secondary metabolites)
have played a pivotal role as sources for drug lead compounds
during the last century. However, in order for natural product
chemistry to continue to be competitive with purely synthetic
based discovery methods, natural product research needs to
continually improve the efficiency of the selection, screening,
dereplication, isolation and structure elucidation processes.1,2
The main intention of this review is to discuss how taxonomy and
information on biodiversity can be used for selection of talented
microbial strains to be included in a screening programme and
how this together with the use of spectroscopic methods in
combination with chemoinformatics can be used as part of an
effective dereplication strategy. In this review we use the terms
natural products or secondary metabolites (but not the terms
specific metabolites or idiolites). We occasionally use the broader
term extrolites, which comprise any metabolite that is outwards
directed in an ecological sense (they could be extracellular or
in the cell wall of the organism). Extrolites can be secondary
metabolites, accumulated acids, extracellular enzymes etc.3
NPs are produced by all organisms but are mostly known
from plants, insects, fungi, algae and prokaryotes. All of
these organisms coexist in ecosystems and interact with each
other in various ways in which chemistry plays a major role.
Williams et al.4 proposed that all secondary metabolites serve
the producing organisms by improving their survival fitness—
“by acting at specific receptors in competing organisms”. On the
contrary to primary metabolites that are common in all living
cells and are involved in the formation of biomass and generation
of energy, secondary metabolites are often only produced by one
or few species.
Many NPs are biologically active and have been used by
man for thousands of years as traditional medicines and as
Jens C. Frisvad
natural poisons. However, it was not until the discovery of
penicillin G 1 from a Penicillium species about 80 years ago
that fungi, actinomycetes and other microorganisms suddenly
became a hunting ground for novel drug leads.5 Hence many
pharmaceutical companies were motivated to start sampling
and screening large collections of microorganisms especially
for antibiotics. About 20 years after the discovery of penicillin
several other antibacterial agents such as cephalosporin C 2,
chlortetracycline 3, chloramphenicol 4, and erythromycin 5
had been discovered.1,6 It has been estimated that drugs that
trace their heritage to secondary metabolites have more than
doubled the lifespan of human beings.7 Apart from the use of
antibiotics to combat bacterial infectious diseases this spans
heterogeneous fields such as the use of fungal NPs as immunosuppressants during organ transplantations (cyclosporine 6), as
aids for neurological diseases (asperlicin), for fungal infections
(semisynthetic lead compounds derived from echinocandin B
9),1 for cardiovascular and metabolic diseases (natural statin
compounds such as lovastatin 7 and pravastatin 8 and synthetic
analogue compounds such as the major selling synthetic statins
crestor 10 and lipitor 11).1
For the past 10–20 years there has been a tendency in drug discovery programmes to favour programmes using combinatorial
chemistry for generation of chemical diversity.1,8,9 The major
reason for this has been the tremendous development of high
throughput screens based on molecular targets in combination
with automated instrument systems, robot technologies etc.
However, apparently there is a growing opinion, at least among
many natural product chemists, that combinatorial chemistry
has failed to supplant NPs as the primary source of broad
chemical diversity.1,8,9 One argument is based on the fact that
the number of new active substances has been declining during
the last 20 years,9 and the fact that a significant number of
the top 35 worldwide selling drugs in the years 2000–2003
are natural product derived compounds (e.g. lipitor and other
synthetic antilipidemic statins).1 On the other hand combinatorial chemistry has achieved significant success in more specific
discovery programs used to generate focused libraries centered
Nat. Prod. Rep., 2005, 22, 672–695
673
on core structures with desired activities, rather than finding
these from an initial lead compound. More attention is now
placed on the quality and diversity of combinatorial libraries,
and provided a starting point, such as a natural product scaffold
is available, it is clear that combinatorial chemistry is sufficiently
advanced to accomplish parallel synthesis.10 A major advantage
of using natural products as drug leads is their often extremely
complex structure, making a total synthesis, and the synthesis of
their analogues, a daunting task, even when cost and yield are
not important.7 Structurally natural products are more likely
to be rich in stereochemistry, concatenated polycyclic rings
and reactive functional groups, than structures generated by
combinatorial chemistry. For example it is doubtful that the
b-lactam ring of the penicillins would have been discovered
by synthetic chemists just making molecules at random.11 In
addition to the great chemical diversity produced in Nature,
there are several other good reasons to choose a natural product
based drug discovery strategy. First of all it makes a lot of sense
to choose NPs since such compounds have “a biological history”
selected by Nature during the evolution to serve a function in
specific biological systems like binding to proteins.8,12 In other
words NPs that are biologically active in assays are generally
small molecules with drug-like properties such as being capable
of being absorbed and metabolised by the human body. At
the same time Nature almost always produces chiral molecules
and with the tendency of shifting towards the patenting and
marketing of chiral drugs, NPs have the natural advantage of
being enantiomeric.6
674
Nat. Prod. Rep., 2005, 22, 672–695
1.1
Antibiotics
Even though more than 30 000 diseases are clinically described
today less than one-third of these can be treated symptomatically
and even a fewer can be cured.13 Hence there is an urgent
need for new therapeutic agents, with infectious disease control
as a striking example. The increasing occurrence of multiresistant pathogenic strains has limited the effect of traditional
antimicrobial treatment, and it has created a global concern
that we may soon be facing a post-antibiotic era with reduced
capabilities to combat microbes.
One very promising new approach for antibiotics is based on
the fact that bacterial colonization and pathogenesis is facilitated
by the ability of the bacteria to communicate and thereby coordinate the behaviour of the entire population. Population activity
such as biofilm formation is coordinated by simple communication systems which in many Gram-negative bacteria is based on
homoserine lactone (HSL) signals, which have been described in
numerous pathogens.14 HSL systems are referred to as quorum
sensing (QS) systems, i.e. they express target genes in relation to
the quorum size (or density) of the population. In most known
cases QS systems control expression of virulence factors such
as biofilm formation by Pseudomonas aeruginosa in the lungs of
cystic fibrosis patients.15 A screening strategy aiming at inhibition of QS is therefore not targeting bacterial growth but instead
at blocking the coordination of bacterial population activity.
This means that a quorum sensing inhibiting (QSI) drug is not
generating a selective pressure on the bacteria, and it is therefore
unlikely that bacteria will develop resistance towards a given QSI
compound. Several natural quorum sensing inhibitors have been
described within the past ca. 10 years some of the latest being the
two well known mycotoxins patulin and penicillic acid.16 Because
the P. aeruginosa genome has now been fully sequenced, DNA
microarray technologies are being used in order to study the
effects of potential new QSI hits at the transcriptional level.16
Altogether the increasing information on microbial pathogen
genomes as well as the completion of the Human Genome
Project will provide thousands of disease related targets to be
used in future screening for novel drug leads.13
2. Microbial biodiversity
A major potential of NPs is the fact that many natural product
resources are largely unexplored, and many environmental
samples for isolation of interesting microorganisms have often
been collected without a defined strategy.17–19 Diverse habitats
are tropical forests soils, the deep sea,20,21 sites of extreme temperature, salinity or pH, since such habitats often generate novel
microorganisms and therefore provide the potential for novel
metabolic pathways and compounds.13 However, at the same
time temperate ecosystems should not be excluded especially
if novel isolation strategies such as metagenome cloning (see
below) is used. Among others the cyclosporins and penicillins
were isolated from fungi collected in temperate regions.13 Even
cold regions can be rich in fungal diversity leading to a high
hit-rate of novel psychrophilic or psychrotolerant species.22,23
A number of these species have recently been investigated and
found to produce several bioactive cyclic peptides.24–26 These
findings support the hypothesis that fungi from colder climates
may be just as chemically prolific (and perhaps just as diverse)
as those from tropical climates, the latter which are much
more often cited as targets for biodiversity sought in screening
programs. In general we find that only relatively few species
appear to be dominant in a certain habitat, leading to the
isolation of high numbers of strains of the same species. For
fungi this is often referred to as the associated funga.27
2.1 Marine microorganisms
With more than 70% of the planet’s surface covered by water
the oceans are probably the most promising habitat to explore
for novel microbial biodiversity. It has been estimated that the
biological diversity in marine ecosystems, such as the deep sea
floor, is higher than in tropical rain forests.17,28–30 Since the
1970’s more than 15 000 NPs have been isolated from marine
microbes, algae and invertebrates. It seems clear that many
microorganisms such as actinomycetes and fungi are washed
from the shore or blown by the air into the sea.31 On the other
hand specific populations of e.g. marine adapted actinomycetes
such as Salinospora and Marinophilus have been discovered
and described recently.31 Many such organisms produce marine
NPs that possess unique structural features as compared to
terrestrial metabolites. Marine NPs often include a myriad
of functional groups, which more than make up for some of
their disadvantages. A major problem is that many promising
bioactive marine compounds can only be isolated in extreme low
yields, because many source organisms are difficult to culture by
standard fermentation procedures. This is because some of these
compounds are only produced as a result of symbiosis between
e.g. an invertebrate and a microorganism.32 The advances in
molecular genetics are expected to have a great impact on marine
natural product chemistry as cloning of polyketides (PKS)
or nonribosomal peptide synthetases from “difficult sources”
into more amendable bacterial hosts potentially can give an
unlimited supply of target compounds.32–34
2.2 Terrestrial and insecticidal microorganisms
Hawksworth35,36 has estimated that approximately 1.5 million
fungal species are present on Earth. Out of this number it is
suggested that around 100 000 valid species have been described
implying that only about 7% of the world’s fungi have been
described today. Hawksworth and Rossman37 speculated where
to find all the undescribed species and suggested that many of
them are likely to be; 1) fungi in tropical forests, and in particular
endophytes that can be isolated in enormous numbers; 2) fungi in
unexplored habitats such as insects; and 3) lost or hidden species,
of which many isolates previously were considered a single
species but when studied by modern molecular or biochemical
methods, prove to comprise several biological species.
Fungi and particularly endophytes indeed are a very promising source of novel biological active compounds as reviewed by
Schulz et al.,38 who found a large hit-rate of novel compounds
among the approx. 6500 endophytic fungi that they screened for
biological activities. The pharmaceutical potential of endophytic
fungi was truly verified with the finding of the taxol 12 producing
endophytic fungus Taxomyces andreanae.39,40
The potential of finding new microorganisms associated with
insects seems to be immense as illustrated by the discovery of
over 200 new species of yeasts from a total of 650 isolates
from the guts of beetles.36 It has been estimated that up to
30 million species of insects exists.41 Fungi have existed and
coevolved with insects some millions of years, and much longer
than with mammals,42,43 so from an evolutionary point of view,
it seems likely that a major part of the fungal biologically active
metabolites are part of the ecological and in particular chemical
defence system directed towards insects.44 Fungi are generally
more nutritious than plant tissue, due to higher levels of proteins,
making them potentially desirable sources of foods for predatory
insects.43 Thus predation has without doubt been one of the
selective forces shaping the chemical defence systems in fungi.44
Evidence for this has been several studies on fungal sclerotium
producing species of Aspergillus which have demonstrated that
these compartments contain a variety of sclerotial compounds
that cause feeding deterrence or have insecticidal effects.45–47
There are many examples of hidden species suddenly being
“discovered” especially within taxonomically well studied genera such as Penicillium, Aspergillus and Fusarium. One recent
example is the description of the two new species P. tulipae and P.
radicicola within the series Corymbifera among the terverticillate
Penicillia. Both these species produce different profiles of
secondary metabolites than the other members of the series:
P. hirsutum, P. albocoremium, P. allii, P. hordei and P. venetum.48
Another important aspect concerning hidden species is the food
safety issue of mycotoxin production. Thus the description of
novel species closely related to already known ones might clarify
inconsistent literature information about mycotoxin production.
This has clearly been the case for P. roqueforti from which
the two new species P. carneum and P. paneum have recently
been described among others based on their ability to produce
secondary metabolites.49–51 Importantly, only the latter two
species can produce the mycotoxin patulin, whereas P. roqueforti,
applied as a starter culture in food production, will not. The issue
of hidden species in combination with the often very difficult task
for mycologists to identify a given fungal culture to the species
level has meant that the literature is full of data on misidentified
species. When chemistry is also reported this leads to erroneous
postulates about metabolite production as described in detail in
Nat. Prod. Rep., 2005, 22, 672–695
675
the next section. Because of these problems many researchers
have, in our opinion, come to the wrong conclusion of rejecting
the usability of metabolites for chemotyping.52
2.3 Non-culturable organisms
The fact that many microorganisms have not been discovered
so far is a major challenge for future research since only little
effort has been addressed to the isolation and cultivation of
organisms difficult to culture. The optimal conditions for growth
and secondary metabolite production vary a lot from species to
species. Beside the general factors such as carbon, nitrogen, trace
metals, temperature, aeration, time of cultivation (see section
3.4), some microorganisms may require stimulation by signal
molecules from other organisms in order to grow even when
provided with the proper nutrients. Thus the addition of factors
such as pyruvate, cyclic AMP and homoserine lactones have
all been demonstrated to increase the generation of greater
numbers of microorganisms.13 A second approach to increase
the diversity is the use of oligotrophic isolation media, such as
the use of seawater based media for marine organisms,31 allowing
only growth of a selected group of strains and at the same time
inhibiting the majority of the natural population.53
An alternative approach to access unculturable organisms,
and in particularly prokaryotic species, is to access their DNA
directly by cloning the metagenome.54–56 Isolated DNA is ligated
into bacterial artificial chromosome (BAC) vectors, which are
low copy plasmids that can contain relatively large DNA inserts.
The BAC vectors are then subsequently transformed into host
microorganisms such as E. coli. The resulting clones can then
be screened for biological activity or alternatively be probed
for sequences of interest. This approach is expected to become a
powerful resource in the future from which new chemical entities
can be accessed for lead discovery.57
2.4 Molecular genetics and metabolic engineering
The genes coding for many natural products and in particular
polyketide synthethase (PKS) genes are modular and produce
multifunctional enzymes. This has lead to new possibilities to
diversify unnatural microbial NPs since it is now possible to
shuffle genes around within these clusters, or even to include
genes from other pathways, thereby generating hybrid enzymes
capable of synthesizing an unlimited set of new molecules
that are difficult to make by traditional chemical methods.58–60
676
Nat. Prod. Rep., 2005, 22, 672–695
Polyketides such as the important compounds erythromycin
and lovastatin have been manipulated with great success.61 In
order to fully explore the potential of genetic engineering for
industrial strain development methods such as comparison
of genomic microarrays, transcription profiles and metabolic
profiles are now being used to guide yield improvement. Genetic
engineering and modification of targeted pathways will without
doubt be very important in future work for construction of
novel pathways and NPs.62–63 Alternatively to directed genetic
modifications novel non-natural products can also be achieved
more randomly from hybrid organisms generated by cell fusion
techniques.64
3.
Chemotaxonomy and chemo-consistency
“The production of antibiotic substances by microorganisms is not
a property characteristic of specific groups of organisms or even
of given species within such groups, but of a few selected strains
within a given species”.65
“Thus, the search for novel secondary metabolites from fungi
belonging to the group Nodulisporium appears to be a random
walk in a random forest, at least once one has covered the more
common metabolites produced by the genus”.66
“Production of similar metabolic products does not provide an
adequate basis for recognition of a new taxon”.67
3.1
Fungal species specific production of profiles of NPs
When reading the three citations above, it seems to be a hopeless
task to use chemotaxonomy in the classification of filamentous
fungi. Opinions on the species specificity of NPs are diverse.
Some biologists claim that metabolite production is strain
specific,65,68 some biologists claim that a few NPs may be species
specific, but that most of them are strain specific,66 and yet other
biologists claim that most if not all NPs are species specific and
even essential features of anyone species.69 However, in plants
NPs appear to be species specific, yet individual NPs often
occur among widely different species that are not phylogenetically related according to DNA sequence data.70 In the fungi
chemotaxonomy based on NPs is an extremely effective and
scientifically well-founded part of fungal taxonomy, even though
it is only used extensively in the Lichens,71 and few selected
fungal genera such as the Penicillium, Aspergillus, and Fusarium
and their perfect states.72–75 The application of chemotaxonomy
based on NPs in other ascomycetous fungal genera such as
Xylaria and Hypoxylon also give very good results,76 and in
general NPs have always clarified and greatly improved fungal
classifications, when included in revisions of species of different
genera in both ascomycetous and basidiomycetous fungi.72
It is important to emphasize that species in Penicillium,
Aspergillus, Fusarium, Xylaria, Hypoxylon etc. are identifiable,
at least for experts, using traditional micromorphological and
macromorphological characters. Species identified based on
such features have later been shown to produce consistent profiles of NPs. The reason for species specificity has occasionally
been questioned and is often based on compilation of both
correctly identified and misidentified producers of particular
compounds. It is well known that species in Penicillium and
Aspergillus may be difficult to identify,77–79 and misidentifications
are unfortunately very common.75,80 One example is cyclopiazonic acid 13, cyclopiamide 14 and cyclopiamine 15, which
were originally reported from (and named after) P. cyclopium.
However, the original producer was actually a P. griseofulvum.80
Another well known example is the producer of viridicatumtoxin
16, which was first identified as P. viridicatum,81 hence the name,
later as P. expansum,82 and finally it was realized that the isolate
was representing a new species P. aethiopicum.75,83 In this case
the misidentification was understandable as the new species was
“hidden” at the time of isolation and structure elucidation of
viridicatumtoxin, but the name of the compound is misleading
now.
In traditional identifications secondary metabolites have only
been used indirectly via the colour of diffusible pigments, odour
of cultures, the KOH test, filter paper methods etc.3,76,78 With the
advent of separation methods such as thin-layer chromatography (TLC), high performance liquid chromatography (HPLC),
and gas chromatography (GC), and advanced detectors it is now
possible to identify the individual NPs (see section 6).
The genus Penicillium has been particularly well studied concerning NPs. This genus contains more than 225 accepted species
of which 166 belong to the ascomycete genus Eupenicillium and
59 belong to the phylogenetically unrelated ascomycete genus
Talaromyces.84 Species of Talaromyces and their anamorphic
states in Penicillium subgenus Biverticillium produce metabolite
biosynthetic families such as mitorubrins 17, rubratoxins 18,
glauconic acids 19, rugulosins 20, luteoskyrins 21, and cyclochlorotines 22 in species specific combinations,85 whereas Eupenicillium species and associated anamorphs in the subgenera
Aspergilloides, Furcatum and Penicillium produce different extrolite families in different species specific combinations.75,83,86,87
In the Penicillium species examined so far all species produced
a large number of already known or not yet structurally characterised NPs.75 The profile of biosynthetic families of NPs is
always species specific, while individual metabolite biosynthetic
families have been found in both phylogenetically closely related
and distantly related species. For example, the series Urticicolae
in Penicillium subgenus Penicilllium section Penicillium contains
three species, all characterized by very short phialides. These
species produce cyclopiazonic acid 13 and patulin 23 in common,
but else they produce different combinations of NPs.
3.2 Chemo-consistency
Usually the rather high number of biosynthetic families of
NPs detectable in each species is sufficient to unequivocally
classify strains into species in Penicillium and Aspergillus, despite
an occasional lack of phenotypical expression of one or two
metabolites. Most often the NPs characteristic of any one
species are consistently expressed. For example of 85 isolates
of Penicillium expansum examined, 83 produced patulin 23,
85 produced chaetoglobosin A 24, 85 produced roquefortine
C 25, 85 produced communesins 26 and 73 produced citrinin
27.88 Likewise a pronounced chemoconsistency was found in P.
crustosum.89 It is important to emphasize that chemotaxonomy
needs to be based on profiles of NPs rather than the individual
NPs, as those individual metabolites may in some cases be
absent because of mutations in regulatory or other important
genes in the gene clusters responsible for their accumulation.90
Some of the early claims that antibiotic production may be
strain specific,65,91–93 were probably based on the use of few or
suboptimal production media and quantitative rather than qualitative differences. At suboptimal conditions, different strains
may produce widely different amounts of NPs, while at optimal
conditions, extrolite production is much more consistent.75,83,94
Of 241 strains of the P. chrysogenum series, 24 did not produce
detectable penicillin G 1.95 Results of Brundidge et al.96 also
indicated that penicillin production may be less than consistent.
However, reexamination of such strains on other media may
show that all strains of P. chrysogenum produce penicillin. In
the closely related species P. nalgiovense, all strains examined
produced penicillin.97 In E. nidulans, most strains produced
penicillin,98,99 but strains of mating type F did not produce
penicillin and the strains apparently lacked the whole penicillin
gene cluster.100 However, these type F strains have never been
examined since, and they may also represent other species in
the genus Emericella, which are not necessarily all producers of
penicillin. Again only examination for the presence of genes of
the penicillin pathway in these non-producing isolates will tell
us if the genes for a whole pathway may be lost completely in
some strains of a species.
Mycophenolic acid 28 was cited as being produced by most
isolates (12/15) of P. brevicompactum by Clutterbuck et al.101
and furthermore the Raistrick phenols (2,4-dihydroxy-6-(2oxopropyl, benzoic acid)) 29 were produced by 14/15 isolates
of strains in the P. brevicompactum series (now series Olsonii in
section Coronata of Penicillium subgenus Penicillium). The one
strain producing neither mycophenolic acid nor the Raistrick
phenols was P. aurantiogriseum var. poznaniense, now regarded
to be a synonym of P. aurantiogriseum in series Viridicata.3
The two strains claimed not to produce mycophenolic acid by
Clutterbuck et al.,101 the ex type cultures of P. stoloniferum (now
P. brevicompactum) and P. biourgeianum (now P. bialowiezense)
have later been shown to produce large amounts of mycophenolic acid.75 Thus in fact the production of mycophenolic acid
and the Raistrick phenols was entirely consistent. Later Frisvad
and Filtenborg examined 124 strains of P. brevicompactum and
Nat. Prod. Rep., 2005, 22, 672–695
677
P. bialowiezense, at that time both included in P. brevicompactum,
and found that all 124 strains produced both mycophenolic
acid and Raistrick phenols.83 It was later realized that while P.
brevicompactum produced brevianamide A 30, P. bialowiezense
never did, but instead produced quinolactacin A 31.75 However,
both species produce mycophenolic acid, the Raistrick phenols
and asperphenamate 32 consistently.75,86
to use many different culture conditions have not resulted in
detection of aflatoxin in any strain of A. oryzae or A. sojae.111
3.3 Phylogeny and classification: is production of natural
products homoplastic?
Several factors may influence the production of NPs by many
strains of a species. 1) All the strains have to be correctly
identified, using other identification features than NPs in order
not to make a circular argument. 2) Some NPs are only produced
under certain environmental conditions and if all trace metals,
phosphate and other medium factors are present in certain
ranges of concentrations, thus several good media need to be
tried out. 3) The seeding medium may influence the production
of NPs in the final production medium (the prehistory of the
inoculum). 4) The strain needs to be in good condition and not
deteriorated because of repeated transfer etc. 5) Accumulation
of carbon dioxide may inhibit metabolite production, 6) The
extraction solvent may also influence the success of detection
of the particular extrolite. 7) An appropriate analytical chemical
method is needed in order ensure that data are correct. However,
genetic factors also play a major role. Often a single point
mutation in a regulatory gene is sufficient to make an isolate
a non-producer of a metabolite, for which it has the remaining
genetic apparatus. In other cases genes may be silent for other
reasons, so the metabolite is not expressed.
The best known examples of non-production of expected NPs
is absence of aflatoxin accumulation in some strains of A. flavus
and absence of ochratoxin A 33 accumulation in some strains
of P. verrucosum and most strains of A. niger (only 6% positive).
While some NPs, such as kojic acid 34 and aspergillic acid 35,
are consistently produced by all strains examined of A. flavus,
aflatoxin B1 36 is only produced by a certain proportion of
all strains. For example the culture ex type of A. flavus does
not produce aflatoxins. On the other hand there have been
indications that in so-called non-aflatoxin producing strains, a
minority of conidia (single spore inoculations) may give rise to
colonies producing aflatoxin anyway.102 It has been shown that
while aflatoxin has never been detected in A. oryzae, which is
the domesticated form of A. flavus, and A. sojae which is the
domesticated form of A. parasiticus, a major part of the genes
needed for aflatoxin production are present in A. oryzae and
A. sojae strains.103–110 So apparently a major part of the genes
required for aflatoxin B1 biosynthesis is present in all strains
of A. flavus, A. parasiticus and their domesticated forms, but
they are not expressed because of silent or defective genes in the
gene cluster responsible for aflatoxin production. The endeavour
678
Nat. Prod. Rep., 2005, 22, 672–695
Results from Frisvad et al.75 show that natural series of species
often contain species that share several NPs, while some others
are only produced by a certain number of the species in the series.
In the series Viridicata of Penicillium subgenus Penicillium series
Viridicata, xanthomegnin 37, viomellein 38, vioxanthin 39 and
other minor compounds of this naphthoquinone biosynthetic
family is produced by five of the nine species known,112 and
could thus either have been lost during evolution in the four
remaining species or gained several times. A search for parts
of the genes or gene cluster in the non-producing strains will
show which hypothesis is correct, but this can only be done
when all the genes involved in xanthomegnin biosynthesis have
been sequenced. However, production of xanthomegnin by some
quite unrelated species of Penicillium from subgenus Furcatum
section Divaricatum series Janthinella such as P. janthinellum
and P. mariaecrucis,87 Aspergillus section Circumdati,73 and
the very distantly related genus Trichophyton shows that these
naphthoquinones have evolved several times.113–115
In a study of species in Aspergillus section Fumigati and the
related teleomorphic genus Neosartorya it was shown that a
phylogeny based on partial b-tubulin and hydrophobin gene
sequences was not at all congruent with phylogenies suggest
by morphology or NPs.116 Thus functional characters such
as profiles of NPs, morphology and physiology are effective
in classifications of fungi, but are maybe less well suited for
phylogenetic analysis because of many homoplasies or even
analogies in such functional characters. Some examples will be
given below.
Griseofulvin 40 was one of the first antifungal NPs found
in filamentous fungi. This chlorine containing polyketide is
produced by several ascomycetous species, some of them closely
related, others very distantly related (Table 1). Griseofulvin production appears to be very consistent in all the species that have
been examined systematically so far.75 According to Table 1, the
griseofulvin biosynthetic capability has been developed at least
13 independent times during evolution. All known species of
Khuskia and its anamorphic state Nigrospora have been reported
to produce griseofulvin, so this is apparently a monophyletic
character of the genus. In contrast griseofulvin production has
been developed 9 independent times in Penicillium, and thus
this character is highly polyphyletic (Table 1). However, it is
not known whether the four species in series Lanosa and the
four species in series Canescentia that produce griseofulvin, are
those that are most closely related according to a single or
multi-gene phylogeny. In Aspergillus, griseofulvin production
appears to be rare, as it has only been reported in A. lanosus,
but in no other species in series Flavi of Aspergillus and its
Petromyces teleomorph.121 The production of griseofulvin by
Memnoniella echinata is also autapomorphic, i.e. not shared
with phylogenetically closely related species, no other species
of Memnoniella or the closely related Stachybotrys produce this
polyketide.134,135 One strain of Phomopsis has also been reported
to produce griseofulvin.120
Mycophenolic acid 28 is a strongly immunosuppressive extrolite and is used for organ transplantations and for treatment of
autoimmune diseases (as the drug formulation mycophenolic
acid mofetil).136 It is also an antibacterial, antifungal and
antiviral compound.136 Mycophenolic acid is produced by five
Penicillia, one Aspergillus, one Byssochlamys and one Septoria
species (Table 2). Mycophenolic acid is thus produced by two
out of three species in series Olsonii, two out of three species
in series Roqueforti, but furthermore by 4 individual species in
different genera (Table 2). According to b-tubulin sequencing
and phylogenetic analysis P. roqueforti and P. carneum, both
producing mycophenolic acid are more closely related to each
other than to P. paneum, the only species in series Roqueforti
not producing mycophenolic acid, and likewise P. bialowiezense
and P. brevicompactum, both producing mycophenolic acid are
more closely related to each other than to P. olsonii, the only
species not producing mycophenolic acid in series Olsonii.137
Despite this concurrence within the two series of Penicillium,
mycophenolic acid biosynthesis seems to have been invented
at least 6 times during evolution (Table 2). Most strains of
Penicillium roqueforti produce mycophenolic acid,137 although
Engel et al. claimed the production of mycophenolic acid
by this species was strain specific.68 However, as mentioned
above P. roqueforti has been shown to be consisting of three
different species P. carneum, P. paneum and P. roqueforti.3,49
P. carneum consistently produces mycophenolic acid,49 whereas
some strains of P. roqueforti may be non-producers. Again this
could be a result of mutations in some of the genes coding for
mycophenolic acid in P. roqueforti or finding an optimal medium
for phenotypic expression of the metabolite.
In some fungal series, such as series Urticicolae in Penicillium,
several NPs are common for all species (Table 3). For example all
known members of this series produce patulin 23, cyclopiazonic
acid 13 and possibly penicillin G 1. On the other hand
griseofulvin 40 has only been found in P. griseofulvum and
P. dipodomyicola, while fulvic acid 41 has been detected in P.
griseofulvum and the new species in the series. In a cladistic
sense griseofulvin and fulvic acid are incongruent. In the series
Viridicata of Penicillium the production of verrucosidin 42,
xanthomegnins 37, viridicatins 43, puberulins 44, terrestric acid
45 is neither consistent with the b-tubulin sequence based phylogeny nor are the many NPs produced congruently. Sequencing
and comparison of the gene and nucleotide sequences of gene
clusters for these NPs will eventually help finding out whether
the genes are inherited, horizontally transferred or have evolved
several times during evolution. In addition P. dipodomyicola
produces four new kinds of alkaloids and four new polyketide
derived extrolite types. The new species in the series produce
Table 1 Taxonomic placement of griseofulvin 40 producers
Species
Subgenus
Section
Series
Order
References
Khuskia oryzae
Khuskia sacchari
Nigrospora musae
Nigrospora sphaerica
Memnoniella echinata
Phomopsis sp.
Aspergillus lanosus
P. nodulum
P. aethiopicum
P. persicinum
P. coprophilum
P. dipodomyicola
P. griseofulvum
P. sclerotigenum
P. jamesonlandense
P. lanosum
P. raistrickii
P. soppii
P. janczewskii
P. murcianum
P. nigricans
P. nodusitatum
P. yarmokense
—
—
—
—
—
—
Circumdati
Aspergilloides
Penicillium
Penicillium
Penicillium
Penicillium
Penicillium
Penicillium
Furcatum
Furcatum
Furcatum
Furcatum
Furcatum
Furcatum
Furcatum
Furcatum
Furcatum
—
—
—
—
—
—
Flavi
Aspergilloides
Chrysogena
Chrysogena
Penicillium
Penicillium
Penicillium
Penicillium
Ramosum
Ramosum
Ramosum
Ramosum
Eladia
Eladia
Eladia
Eladia
Eladia
—
—
—
—
—
—
—
Implicata
Aethiopica
Persicina
Claviformia
Urticicolae
Urticicolae
Expansa
Lanosa
Lanosa
Lanosa
Lanosa
Canescentia
Canescentia
Canescentia
Canescentia
Canescentia
Trichospaerialesa
Trichospaerialesa
Trichospaerialesa
Trichospaerialesa
Sordarialesb
Diaporthalesc
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
Eurotialesd
117,118
118
117
117
119
120
121
This report
83
122
83
83
123,124,125
126
23
87
127,128
129
125,130
This report
124,128,131
This report
This report
a
Sordariaceae, Sordariomycetidae, Ascomycetes. b Chaetosphariaceae, Sordariomycetidae, Ascomycetes. c Valsaceae, Sordariomycetidae, Ascomycetes. d Trichocomaceae, Eurotiomycetidae, Ascomycetes. Unsubstantiated reports, misidentified or reidentified culture: Aspergillus versicolor,132
Penicillium albidum,127 P. brunneostoloniferum (=P. brevicompactum),131 P. concentricum;128 P. kapuscinskii,133 P. melinii,128 P. raciborskii,133 P.
verrucosum var. corymbiferum,128 reidentified to P. aethiopicum,75 P. viridicatum,81 reidentified to P. aethiopicum,80 P. viridicyclopium (=P. cyclopium).131
Nat. Prod. Rep., 2005, 22, 672–695
679
Table 2 Taxonomic placement of mycophenolic acid 28 producers
Aspergillus unilateralis
Byssochlamys nivea
Penicillium bialowiezensc
P. brevicompactumd
P. fagie
P. carneum
P. roqueforti
Septoria nodorum
Subgenus
Section
Series
Order
References
Fumigati
—
Penicillium
Penicillium
Furcatum
Penicillium
Penicillium
—
Fumigati
—
Coronatum
Coronatum
Furcatum
Roqueforti
Roqueforti
—
—
—
Olsonii
Olsonii
—
Roqueforti
Roqueforti
—
Eurotialesa
Eurotialesa
Eurotialesa
Eurotialesa
Eurotialesa
Eurotialesa
Eurotialesa
Mycosphaerellalesb
This report
139
75
140–143
87
83
68,138,144
145
a
Trichocomaceae, Eurotiomycetidae, Ascomycetes. b Mycospaerellaceae, Dothideomycetidae, Ascomycetes. c Including the synonym P. biourgeianum.
Including the synonyms P. hagemii, P. griseo-brunneum, P. patris-mei, P. scabrum, P. stoloniferum. e Including the synonym P. caerulescens.
Unsubstantiated reports or misidentified culture: P. aurantiogriseum,146 P. canescens,146 P. carneolutescens,147 was a P. brevicompactum,80 P. expansum,146
P. meleagrinum,148 P. olivicolor,146 P. paxilli,146 P. rugulosum,146 P. viridicatum.146,149
d
Table 3 Production of NPs by species in Penicillium section Penicillium series Urticicolae
Species
Patulin
Fulvic
acid
Griseofulvin
Cyclopiazonic
acid
Roquefortine
C
Cyclopiamine
Penicillin
Cyclopiamide
P. griseofulvum
P. dipodomyicola
New species
+
+
+
+
−
+
+
+
−
+
+
+
+
−
−
+
−
−
+
?
?
+
−
−
Asteltoxin
−
−
+
15 different groups of chromophore groups, previously seen in
no other or few other Penicillium species. The three species in
Urticicolae also produce many volatile NPs.75,150
Chaetoglobosins are cytotoxic mycotoxins that have also been
considered as drugs.151–153 Chaetoglobosin A 24 is active against
the gastric ulcer involved bacterium Helicobacter pylori and
chaetoglobosin K has been suggested for use in combination
with other drugs in the treatment of RAS-induced cancers.154–156
The chaetoglobosins are both phytotoxic and antifungal.157–160
These very active compounds are produced by an array of very
different species, that are not phylogenetically closely related
(Table 4). The chaetoglobosins thus seem to have evolved at
least 7 independent times.
An overview of Penicillium subgenus Penicillium shows that
all series contain species that have specific profiles of NPs.75
There is a tendency that many NPs are common to several
members of a series, so that each series is polythetic,161 and
in addition have autapomorphic NPs for each species. But
even these autapomorphic NPs in one series may occur as an
autapomorphy in another series. As an example brevianamide
A 30 is produced only by two species in subgenus Penicillium:
P. brevicompactum in series Olsonii and P. viridicatum
Table 4 Taxonomic placement of chaetoglobosin 24 producers
Calonectria morganii
Cylindrocladium floridanum
Chaetomium cochlioides
C. globosum
C. mollipileum
C. rectum
C. subaffine
Diplodia macrospora
Discosia sp.
Phomopsis lepstromiformis
Phomopsis sp.
Penicillium discolor
P. expansum
P. marinum
a
Subgenus
Section
Series
Order
References
—
—
—
—
—
—
—
—
—
—
—
Penicillium
Penicillium
Penicillium
—
—
—
—
—
—
—
—
—
—
—
Viridicata
Penicillium
Penicillium
—
—
—
—
—
—
—
—
—
—
—
Solita
Expansa
Expansa
Hypocrealesa
Hypocrealesa
Sordarialesb
Sordarialesb
Sordarialesb
Sordarialesb
Sordarialesb
Dothidialesc
? (Ascomycetes)
Diaporthalesd
Diaporthalesd
Eurotialese
Eurotialese
Eurotialese
158
157
167
168,169
167,170
167,170
171,172
173
174
175
120
176
83,88,177
75,178,179
Nectriaceae, Sordariomycetidae, Ascomycetes. b Chaetomiaceae, Sordariomycetidae, Ascomycetes. c Botryospaeriaceae, Sordariomycetidae, Ascomycetes. d Valcaceae, Sordariomycetidae, Ascomycetes. e Trichocomaceae, Eurotiomycetidae, Ascomycetes.
680
Nat. Prod. Rep., 2005, 22, 672–695
in the phylogenetically unrelated series Viridicata.75,137
Brevianamide A has not been found in any other microorganism
yet.
The accumulation of this anti-insecticidal extrolite162 in the
conidiophores of P. brevicompactum163,164 has given rise to the hypothesis that brevianamide A may deter fungivorous arthropods
from consuming the penicillus.44 Since brevianamide A is also
accumulated in the conidiophores of P. viridicatum, the same
is probably the case for the latter fungus also. One hypothesis
could be that brevianamide A has evolved twice, even in these
rather closely related species, based on a strong interaction
with the environment, i.e. selection at the species level. An
alternative second hypothesis could be that brevianamide A
genes are present in all 58 species, but have been lost in 56
species, based on loss of genes, gene silencing or mutations in
the biosynthetic genes for brevianamide A. A third hypothesis
could be that the whole gene cluster for brevianamide A has been
horizontally transferred from one species to another. Based on
the distributions of NPs in both phylogenetically closely and
unrelated species, it is most probable that these metabolites have
evolved several times during evolution. The second hypothesis
would require an unrealistically large genome in all fungi, as
most NPs are so widespread in several orders of fungi, that
all fungal species should have all extrolite genes inherited from
their ancestors if the hypothesis was correct. The tryptophan
derived extrolite paxillin 46, for example, is produced via a
gene cluster of 17 genes (ca. 50 000 nucleotides in all),165 and
this gene cluster is not much larger or smaller than other
gene clusters for NPs,166 and with the very large number of
NPs known in Penicillium subgenus Penicillium there is simply
not space for all these gene clusters in any fungal genome.
Horizontal gene transfer of such large gene clusters is also
quite improbable. For present the hypothesis that NPs have been
invented several times during evolution and that ecology has a
major impact on the profiles of NPs seen in filamentous fungi
seems most probable. If this is shown to be true, intelligent
screening for these compounds should be based on ecology
and systematics rather than on phylogeny based on household
genes. Thus it is recommended to emphasize biodiversity at the
species level and explore many different habitats, including a
search for new species. Chemical stimulation by co-occurring
species in the actual habitat is also a natural consequence
of this ecologically based approach. Phylogenetic relatedness
may, or may not, indicate that the same NPs are produced
and will not give any ecological hints on stimulation of NP
production.
3.4 Microbial physiology
It is well known that medium composition and culture conditions have great impact on growth and the production of
secondary metabolites.42,66,94,180,181 The physiology of secondary
metabolism has often been neglected and still few of the regulatory features of secondary metabolism have been elucidated.182
Thus depending on the diversity of the microorganisms to
be studied it may be necessary to use several media and
growth conditions, both during initial morphologically based
investigations and later when “talented” strains are to be
investigated (see Fig. 1) for their full metabolic potential using
a one strain many compounds approach as suggested by Bode
et al.183
Fig. 1 The chemotaxonomy based screening approach. Step 1) Cultures
from either natural samples or in-house collections are cultivated on
a few media used for macro- and micromorphological identification
purposes. Representative strains of the different species are selected
by either experts or by automated image analysis methods.196 Step
2) Extracts are made by micro-extraction of only a few agar plugs
from one fungal culture and all metabolites in the extract are analysed
simultaneously (step 3) using e.g. direct injection mass spectrometry
(DiMS). Mass profiles of the extracts are clustered using chemometric
methods in order to select representative chemotypes.52 Step 4) The
relatively few strains per species that have now been selected are grown
on a larger number of media in order to generate conditions that will
allow the expression of as broad a range of secondary metabolites as
possible for a given strain, according to the one strain many compounds
(OSMAC) philosophy.183 Step 5) Extracts from the best media conditions
can now be separated into microtiter plates generating natural product
compound libraries. At the same time UV and MS data are obtained
allowing compound dereplication of hits from bioassays (step 6) using
comparison of UV and MS spectra with databases. Step 7) Active
compounds are isolated and structure elucidated to generate novel
drug candidates (step 8), altogether at a high-rate, allowing search for
further similar but novel compounds by comparison of spectral data to
information in databases using chemoinformatic tools (see section 6.5).
If possible it is very beneficial to know the genus being
investigated as the general optimal media for good metabolite
production changes.66,184 For example YES and CYA are in
general excellent media for metabolite production for Penicillium
and Aspergillus, whereas they work very poorly for Rhizopus.185
This is also the case for Penicillium sub-genus Biverticillium
(teleomorph Talaromyces), where MEA and OAT give many
more metabolites than other media.181
For initial identification/pre-selection studies solid substrates
in Petri dishes are standard. This ensures easy assessment of
contaminations of what were supposed to be pure cultures,
something which can be difficult to control on media like
rice and maize,186,187 which on the other hand often give
good sporulation and metabolite production. Point inoculated
cultures furthermore have the advantage that mycelia at different
ages are present and thus both intermediates and end-products
can be extracted from the edge and the center respectively using
e.g. the agar-plug-technique.184
Nat. Prod. Rep., 2005, 22, 672–695
681
Different and relatively easy to control conditions to investigate in a discovery programme include growing cultures
at both solid and liquid conditions, incubation at two or
more temperatures, incubation at two or more shaker speeds,
incubation for at least two different time periods, media with
at least two different pH levels, choosing carbon and nitrogen
sources at different concentrations, high- or low phosphate
content, adding trace minerals etc.13 Authors like Hesseltine188–190
Gloer45 and Nielsen et al.181 strongly argue in favour of using
solid substrate fermentations in studies of fungal metabolites
since fungi, unlike other microorganisms, typically grow in
nature on solid substrates such as wood, roots, leaves of plants,
and drier parts of animals such as fecal material that is low in
moisture.
As mentioned earlier others argue that the production of
some metabolites demand very specific “stimuli” e.g. certain
precursors or “triggers” often present in the natural environment
of the given fungus. This comes from the philosophy that most
species are capable of inhabiting several environments as they
would otherwise be too dependent on just one environment, and
that a species will need a certain chemical profile in each of these
environments. This calls for complementing general screening
media with e.g. macerated plant tissue media for plant pathogens
and endophytes as recently illustrated by the stimulation of
some novel fungal phenolic metabolites using plant tissue
media.191,192
Finally, some believe and argue that all metabolites can be
expressed in liquid culture by varying carbohydrate composition, nitrogen source, oxygen tension, pH, redox potential,
water activity, as the right conditions will produce intracellular conditions that will trigger production of a certain
metabolite. Thus liquid conditions have been shown to be
very successful in Fusarium.193 Often metabolites associated
to spore or sclerotia formation are produced under solid
conditions whereas the production of others are enhanced
under liquid conditions. This was demonstrated for P. solitum
where alkaloids such as viridicatol and cyclopenol analogues
where produced in relatively high amounts on semi-solid media
either still or absorbed in lightweight expanded Clay aggregates
(LECA), whereas the often targeted compactin polyketides were
the most dominant compounds produced under submerged
conditions.181
4. The chemotaxonomy based drug discovery process
As argued above the chemical diversity and the resources of
NPs are immense and nowhere near fully exploited. Combined
with the fact that fungi (and probably also other types of
microorganisms) produce very species specific profiles of NP’s
that can be used as efficient tools to select one (or a few)
representative strain(s) for biological testing, and with the
revolution in molecular genomics several new strategies for a
NPs based drug discovery programme are being opened:
-Knowing the biodiversity and ecology;
-Using a metabolite profiling approach;
-Targeting certain ecological niches;
-Using a genome based approach.
There are several other steps to deal with when running a
natural product discovery programme. According to Cordell194
these key steps can be summarized: (i) collection, selection and
cultivation of organisms; (ii) extraction and biological evaluation; (iii) dereplication; (iv) isolation and structure elucidation
of metabolites; (v) biological evaluation; and (vi) information
management.
With the large numbers of already known microbial (approx.
50 000) and plant (approx. 600 000) metabolites,195 one of the
major challenges in modern natural product discovery is to
detect already known and trivial compounds rapidly, a process
known as dereplication. However, in our opinion dereplication
(or avoiding redundancy) can be implemented in several steps of
682
Nat. Prod. Rep., 2005, 22, 672–695
the discovery process. This relies on information management
and data mining of the enormous amounts of biological,
chromatographic and spectroscopic data generated and which
has become a bottleneck in modern drug discovery. To optimize
the drug discovery process dereplication should be implemented
at an early stage, where the cultures of a given microbial
collection (culture collection or natural samples) are selected
for extraction and biological evaluation. Traditionally, microbial
strains have been selected based on morphology, rather than on
more powerful approaches such as automated image analysis of
pure cultures,196 phenotypic characters including production of
secondary metabolite profiles or based on genotyping.13,197 One
reason for the large redundancy in isolation of already known
compounds in screening programs is due to the redundancy in
selection and screening of multiple strains of the same species
already studied by others.
It is therefore very relevant to develop an array of simple
analytical methods and combine these methods with informatics, to select representative and promising strains to screen
rapidly in a bioassay. As will be discussed in detail below, these
methods are based on efficient use of MS, UV and NMR data
in combination with modern informatics tools to characterize
the nature of mixtures of compounds, in crude extracts. When
some representative chemotypic strains have been selected, then
their metabolic potential should be investigated using multiple
growth conditions as discussed in section 3.4 and argued by
Bode et al.183
Having found both some promising strains and their optimal
growth conditions for metabolite production, natural product
compound libraries (NPLs) can be prepared using an integrated
setup for analysis and automated micro-fractionation into e.g.
microtiter plates.16,198 Such NPLs can then be screened in various
bioassays and when hits have been generated these can be correlated to spectroscopic data and again to databases,199 in order
to dereplicate, thus avoiding the finding of trivial compounds as
early as possible. Subsequently, potential novel compounds can
be isolated on a larger scale and their structure elucidated. In
the case of new compounds more analogues can be generated
either by combinatorial or traditional chemistry. Alternatively
an overall screening for new but similar compounds may be
accomplished by an automated UV-guided search discussed in
more detail in section (6).
The overall combined approach using integrated analytical
and informatics techniques were recently presented as an
intelligent screening strategy by Smedsgaard and Nielsen.52 In
this review we also include image analysis of fungal cultures,
other direct profiling techniques and the concept of natural
product libraries (NPLs) as part of a slightly modified intelligent
screening system as illustrated in Fig. 1.
5.
Morphology based strain selection—image analysis
In many cases manual inspection by expert microbiologists
or mycologists of a strain collection could obviously lead to
the dischargement of at least some of these strains based on
high morphological similarities. However, dereplication based
on macromorphological phenotypic characters can also be
automated. Using a special camera system, colours as they
appear from the surface of the fungal cultures, can be mapped
into discrete arrays of pixel values representing a digital image.
Images (micro and/or macro) have to be acquired under totally
standardised conditions with a colour and geometry calibrated
camera set up, so that absolute colour measurements and
comparison can be made. The camera system consists of an
integrating sphere (a so called Ulbricht sphere) combined with a
photometrically calibrated camera system based on the 3-CCD
colour camera. The sphere has a diameter of 36 cm. The inside of
the sphere is covered with a faint titanium dioxide paint to create
optimum light conditions. Light is then brought into the system
through light diodes inside the sphere, giving the sample diffuse
and homogeneous illumination. In a standard camera system the
spectral resolution of an image is normally 8 bits/pixel for each
colour-channel. This camera system is capable of generating
images with a higher spectral resolution for each colour-channel.
The pixel resolution is 32-bit RGB i.e. a bit depth of 232 =
4 294 967 296 per channel and the full pixel resolution is used in
the retrieval process.
Based on the above image acquisition procedure, it has
been shown, that image analysis of fungal cultures can be
used to identify isolates within certain terverticillate Penicillium
species.200 In addition, results from DNA fingerprinting were
recently compared with the results obtained from the image
analysis.196,201 The objective of this study was to investigate if
image analysis could support or maybe serve as a substitute for
subjective phenotyping methods and to substantiate the DNA
fingerprinting of P. commune isolates; one of the most difficult
species to identify within this genus. Fig. 2 illustrates the diversity
of the cultures in appearance.
The figure shows four different clones of the P. commune
after digitization. Although the principles described in Hansen
et al.,196 and Dörge et al.200 were slightly different, the overall
scenario of the methods were the same. First of all the obtained
images contain a large amount of information. To reduce the
computational complexity, the regions of interest (ROI) have
to be detected before further analysis can be done;202 that
is detection of the Petri dish, followed by the colonies and
inoculation points. After having detected the ROI’s, features
can be extracted from the images. The features used are based
on calibrated (RGB) colour measurements extracted from each
of the pixels inside the colonies. Even though colours (colour
intensities) constitute the most important factor for the human
visual system of identification,203 spatial distribution is also
important for the perception and understanding of a scene.
Different isolates may have the same global content of pixels
having certain colours, but the spatial relation of the pixels
determines how we identify them. Therefore textual information
has to be extracted as well.
Based on the colour and textural features, statistical models
can be created for each of the images representing an isolate.201
Using these models distances can be calculated in such a way,
that the distances between visually similar cultures are low,
whereas the distances between visually different cultures are
high. This comparison enables the possibility of making queries
in a database containing visual (phenotypic) information, as
illustrated in Fig. 3. Based on the visual information obtained
from an “unknown” isolate it is possible to calculate distances to
known isolates in the database. Through different classification
methods, such as e.g. the nearest neighbour classification rule, it
is possible to assign species information to the unknown sample.
The studies showed that it was possible to obtain a “leaveone-out” cross-validation identification rate of approximately
93–98% when compared with the identification results based
on DNA fingerprinting. The method described by Hansen and
Carstensen201 has additionally been validated on small-spored
Alternaria species proving to have a good performance when
compared to the traditional identification methods.204
6. Strategies and methodologies for metabolite profiling and
target analysis
Rapid profiling techniques have been desired for many years,
which ultimately may determine all metabolites produced by a
microorganism. In the current age of ‘omics this quest is now a
part of what is known as the metabolomics,205,206 which aims to
detect all small metabolites in a cell or organism. In general
terms these techniques are segregated into: fingerprinting,
footprinting, profiling or target analysis. Fingerprinting aims to
get a “chemical picture” of the sample where the signals cannot
necessarily be used to detect/identify specific metabolites and
depends strongly on the technique used. Profiling techniques
require that signals in the profile (e.g. peaks in a chromatogram)
can be assigned to a specific metabolite whether it is of known
structure or not. Finally, target analysis aims to determine
and quantify specific metabolites. Fingerprinting, profiling or
target analysis can be performed by e.g. TLC screening,184 by
mass-profiling using direct infusion ESI-MS,207 by NMR,208,209
or more by doing elaborate profiling and target analysis,
using hyphenated analytical methodologies e.g. GC-MS(-MS),
Fig. 2 Example of four Petri dishes after digitization. All isolates are different clones of Penicillium commune.
Nat. Prod. Rep., 2005, 22, 672–695
683
Fig. 3 Statistical models are generated based on visual information from the cultures. Using these models distances can be calculated in such a way,
that visually similar cultures have small distances, whereas the visually different cultures have large distances. This comparison enables the possibility
of making queries in a database containing visual (phenotypic) information. Through different classification methods it is possible to assign class
(species, mutant, etc.) information to the unknown sample. Reprinted from Pattern Recognition, 37, Michael Edberg Hansen and Jens Michael
Carstensen, Density-based retrieval from high-similarity image databases, pp. 2155–2164, Copyright (2004), with permission from Elsevier.
LC-UV(spectrometric), LC-MS(-MS), LC-NMR and other
combinations. All these approaches are relevant in NP
discovery.
Most analytical approaches begin with preparation of culture
extracts, which can be anything from simple to daunting.
Screening fungal cultures can be done in a high throughput screening manner by adapting a rapid plug extraction
procedure.210 However, extraction is (like cultivation) not trivial
and consideration should be given to discrimination between
metabolites due to extraction procedure and to ensure that the
sample matrix does not interfere with the subsequent analyses.
The following sections introduce a few of the methodologies
used for metabolite profiling in NP searches in microbes. The
reader is referred to text books and original literature for
detail on how the analytical work and procedures are carried
out.
6.1 Chemical profiling—TLC
The easiest profiling technique to study fungal natural product
in extracts are the agar-plug-TLC technique developed more
than 20 years ago by Filtenborg and Frisvad,211 and Filtenborg
et al.,212 which allow rapid and simple profiling (fingerprinting)
of metabolites almost directly from cultures. By this simple
technique metabolites are extracted “on the fly” by placing a
drop of solvent on the small mycelium plug cut from the culture,
where after the plug is placed on a TLC plate with the wetted
side down for a few seconds and then removed. The plate is
eluted and visualized under UV light by fluorescence or after
selective spraying. While the method may seem primitive, it has
proved efficient for classification, identification and metabolite
detection even under primitive conditions.213 Also, the TLC
technique may be very useful for a first cultural dereplication
method in combination with morphological inspection of cultures on fieldtrips collecting new biodiversity. One standard
TLC plate can accommodate up to 20 extracts/cultures eluted
in two solvent systems, giving a very visual representation
of the chemistry. The information is similar in structure but
not as detailed as obtained from HPLC analysis as discussed
later.
684
Nat. Prod. Rep., 2005, 22, 672–695
6.2
Direct infusion electrospray mass spectrometry
With the arrival of electrospray ionization mass spectrometry
(ESI-MS) and the associated techniques about 15 years ago
the scientific community obtained a marvellous tool for studies
of NPs and other bio-molecules. ESI-MS has the advantage
of being a soft and sensitive ionization technique which can
be optimized to produce mainly protonated or sodiated ions
(assuming positive ESI) from a very broad range of NPs.207 Taking advantage of limited fragmentation in ESI-MS Smedsgaard
and Frisvad207 developed a rapid fingerprinting technique where
mass profiles are determined by infusing crude fungal extract
directly into the electrospray source. Later both Julian et al.214
and Higgs et al.215 used similar approaches as rapid methods to
differentiate and estimate the presence of secondary metabolites
in microbial extracts. The advantages of fingerprinting by
direct infusion mass spectrometry (DiMS) are: fingerprints can
be made within minutes; metabolite and chemical structure
information can be predicted/extracted; data can easily be
stored in databases;216 and data processing is relative easy to
automate.217–218 However, a warning note: infusing complex
samples with many components directly into ESI-MS may lead
to serious discrimination due to what is known as matrix effects.
These matrix effects can discriminate the spectra so that metabolites (or co-extracted media components e.g. PEG and TWEEN)
may “steal” all charges thereby suppressing other metabolites.
Keeping the concentration within a suitable range, using nanoESI techniques and selected solvent compositions can reduce
these effects. As shown in the following examples mass profiles
can, despite these problems, be used through chemometric
methods to classify the samples (fungi) thus grouping the strains
based on their chemical similarities (NP-profile). As fungal
species normally produce stable and often quite unique profiles
of secondary metabolites, as discussed in the previous section,
these mass profiles contain species-specific information.
This was demonstrated almost 10 years ago by Smedsgaard
and Frisvad in a study of a large group of fungal species (43
species on two media, approx. 293 strains).219 They found that
more than 80% of these species could be classified into chemical
classes from the mass profiles which corresponded to species
as determined by classical phenotypic identification. Storing
these spectra in the normal mass spectra library included in
the instrument software many species could be identified semiautomatically.216 These findings have been confirmed in a recent
study now including 57 species and about 500 strains on two
cultivation media.218
Examples of accurate mass profile fingerprints from direct
infusion ESI-MS analyses of extracts from three different, but
related species of Penicillium (associated to dung) are shown in
Fig. 4 (see Smedsgaard et al.218 for experimental details). As can
be seen, they share similarities such as an intense ion at m/z
468.25, as well as differences e.g. only two of the species have
ions at m/z 448.19.
Fig. 4 Mass profile (fingerprint) from direct infusion of crude extract
from three different Penicillium species as described by Smedsgaard
et al.218
These mass profiles contain species specific information
as discussed in the previous sections and can be used for
classification/identification. To illustrate this, 72 DiMS mass
profiles (including the three showed in Fig. 4) from strains of the
8 major Penicillium species associated to dung (from the series
Claviformia and Urticicolae) and two outliers were classified by
cluster analysis as shown by the dendrogram in Fig. 5a. The
classification was done by a binning technique: the ions in each
spectrum were binned into m/z 0.5 wide bins; empty bins are
removed from the analysis. The (bin, ion-count) pairs was sorted
according to the ion count in each (bin, ion-count) and the N = 50
bins with the largest ion count are used to represent each sample.
The bins are given a score according to the ion-count in that bin.
The result is a bin-score vector calculated from each spectrum.
Within each of the class (species) some ions are present in all
the isolates, others may be present in only a few, and therefore
only bins with a score lying within a certain interval are used.
From these selected bins (after they are centered and scaled)
the distances are calculated between all samples and clustered
using WPGMA (weighted average distance) linkage giving the
dendrogram shown in Fig. 5a, a more detailed discussion can be
found in Hansen and Smedsgaard,217 and Smedsgaard et al.218
Fig. 5 Upper (a). Classification of the 7 species in Penicillium series
Claviformia and two outliers (P. formosanum and P. atramentosum) based
on cluster analysis of the raw mass profiles from direct infusion ESI
mass spectrometry of crude extract.218 The DiMS classification point to
the same species groups as classification based on partial beta-tubulin
sequences (lower, b) see Samson et al.137 Strains marked with * are
included in both analyses.
The chemical classification based mass profile fingerprinting
shown in Fig. 5a point to the same groups as cladification based
on partial b-tubulin sequencing.137 These classes have also been
confirmed by classical phenotypic classification by experts.69
This confirms that NPs are closely linked to species, hence
selecting one or a few single isolates within each group rather
Nat. Prod. Rep., 2005, 22, 672–695
685
than all isolates for further studies will give maximal chemical
diversity in a screening programme.
As mentioned above, direct infusion ESI-MS can be optimized
to produce mostly protonated and sodiated molecular ions from
many different chemical compounds. Using the more recent
high resolution and high accuracy mass spectrometers each
ion seen in these spectra is likely to represent one or just a
few metabolites and the chemical structure can with sufficient
accuracy be limited to only a few formulae. However, to obtain
the best possible accuracy an internal mass reference is needed.
Since most dung associated Penicillia will produce roquefortine
C 25 with a [M + H]+ at m/z 390.193, easily seen in positive
mass profiles, the accurate protonated mass of this compound
can be used to correct the mass scale of the bottom spectrum in
Fig. 4 to get the accurate spectrum from P. coprophilum shown
in Fig. 6.
Fig. 6 Mass profile (fingerprint) of P. coprophilum (IBT 21517)
cultivated on YES after the mass scale have been corrected using the
accurate mass of roquefortine C as internal reference. 37 ions above 3%
base peak intensity are listed in Table 5.
Above 3% of the base peak intensity we find 37 ions, of
these 19 correspond to the formula of metabolites known to be
produced by P. coprophilum, most within a few ppm (Table 5).
Five significant unknown ions are included, however these
correspond most likely to three metabolites as the difference
between m/z 417.1798 and 418.1843 ions correspond closely to
the difference between 12 C and 13 C in both mass and intensity.
Looking closer at the griseofulvin group of ions around m/z
350–358, as shown in Fig. 7 bottom spectrum, a series of ion
patterns corresponding to one chlorine atom can be seen. If we
calculate the ion pattern for dehydro-griseofulvin shown at the
top of Fig. 7 and griseofulvin in the middle of Fig. 7 we can see
a good match. However, the intensity of m/z 355.0599 is higher
than expected indicating the presence of another metabolite
in this peak. One could speculate that dihydro-griseofulvin 47
might also be present accounting for the 357 peak.
To validate the findings indicated by the mass profiles in Fig. 7,
the same sample was analyzed by LC-UV-accurate MS and
narrow ion traces were extracted for all these ions shown in
Fig. 7. As the mass spectrometer was overloaded profiles for
both 12 C and 13 C were extracted. Multi-plate channel detectors
(MCP) with time to digital conversion (TDC), a commonly
used detector in a TOF mass spectrometer suffers from dead
time which in case of saturation will give too low mass values,
as seen in the following section. Therefore, the mass traces
shown in Fig. 8 are all made ±0.01 Da e−1 except in case
of serious overload where the trace window is extending to
include lower masses. Looking at the traces corresponding
to the mass of the 13 C isotopes of dehydro-griseofulvin and
griseofulvin, chromatographic peaks about 0.2 minutes apart
can easily be seen in traces from both chlorine isotopes. The area
for the two chlorine traces corresponds nicely to the expected
natural occurrence and there is about three times more dehydrogriseofulvin than griseofulvin. These finding can be confirmed
by looking at the UV spectra.
Table 5 37 ions are found above 3% base peak height in Fig. 5. Of these can 19 ions be assigned to metabolites known to be produced by P.
coprophilum within a few ppm mass accuracy. Roquefortine C was used as natural occurring internal mass reference. Five significant unassigned ions
are included, X1–X5, see text
Metabolite
Formula
Ion
Calculated
Measured
Dehydro-dechloro-griseofulvin
C-dehydro-dechloro-griseofulvin
Dechloro-griseofulvin
Dehydro-dechloro-griseofulvin
Dechloro-griseofulvin
35
Cl-dehydro-griseofulvin
35
Cl–13 C-dehydro-griseofulvin
37
Cl-dehydro-griseofulvin or
35
Cl-griseofulvin
37
Cl-13 C-dehydro-griseofulvin
35
Cl-13 C-griseofulvin
35
Cl-13 C-griseofulvin
37
Cl-13 C-griseofulvin
35
Cl-dehydro-griseofulvin
35
Cl-griseofulvin
X1
Roquefortine C
X2
X3
Meleagrin
Meleagrin
X4
X5
Oxaline
Oxaline
Cyclopiamine
13
C-cyclopiamine
C17 H16 O6
CC16 H16 O6
C17 H18 O6
C17 H16 O6
C17 H18 O6
C17 H15 O6 35 Cl
13
CC16 H15 O6 35 Cl
C17 H15 O6 37 Cl
C17 H17 O6 35 Cl
13
CC16 H15 O6 37 Cl
13
CC16 H17 O6 35 Cl
C17 H17 O6 35 Cl
13
CC16 H17 O6 37 Cl
C17 H15 O6 35 Cl
C17 H17 O6 35 Cl
H+
H+
H+
Na+
Na+
H+
H+
H+
H+
H+
H+
H+
H+
Na+
Na+
317.1025
318.1058
319.1181
339.0845
341.1001
351.0635
352.0669
353.0606
353.0792
354.0639
354.0825
355.0762
356.0796
373.0455
375.0611
317.1021
318.1072
319.1184
339.0846
341.1006
351.0627
352.0667
353.0630
C22 H23 N5 O2
H+
390.1930
C23 H23 N5 O4
CC22 H23 N5 O4
H+
434.1828
435.1862
C24 H25 N5 O4
CC23 H25 N5 O4
H+
H+
H+
H+
448.1985
449.2018
13
686
Nat. Prod. Rep., 2005, 22, 672–695
13
13
13
354.0663
355.0599
356.0634
373.0456
375.0466
389.0195
390.1930
417.1798
418.1843
434.1838
435.1876
436.1991
437.2033
448.1955
449.2027
468.2469
469.2549
section. A similar analysis can be done for the unknown ion pair
X4 and X5 ion pair and m/z 436 and 437 respectively.
6.3
Fig. 7 Prediction of metabolite production from the mass profile of
P. coprophilum (IBT 21517). Shown at the bottom is a small section
of the full mass profile from Fig. 6. The ions found in this part of
the spectrum correspond closely to spectra calculated for protonated
dehydro-griseofulvin and protonated griseofulvin.
The formula of the unknown ions shown in Table 5 can be
predicted under the assumption that only carbon, hydrogen,
oxygen and nitrogen are present and given a mass accuracy. The
mass accuracy can in this case be predicted from the known ions,
in this case about 5 ppm. If we furthermore assume that 417 is
the 12 C isotope and 418 is the 13 C isotope (require that exactly
one 13 C is present) we can calculate all possible formulae. The
results are shown in Table 6. Only two formulae fit within the
limits for both ions: C23 H23 N5 O3 , C25 H25 N2 O4 assuming that
these ions are protonated we need to subtract a proton to get the
real formula. The first of these formulae will then have an even
number of hydrogens which is not possible with an odd number
of nitrogens, hence the second formula is the most likely. Several
databases may help getting a candidate for this formula, see next
Table 6 Calculating the elemental composition of the unknown X2
and X3 ions from Table 5. Mass accuracy 5.0 ppm, double bond
equivalent min = −0.5, max = 50.0 considering both odd and even
electron ions. Search limits 12 C < 500; H < 1000; N < 7; O < 13. First
search X2 of m/z 417.1798 assuming all 12 C carbons: 481 formulae were
evaluated with 3 results within limits. Second search X3 of m/z 418.1843
requiring one 13 C: 4536 formulae were evaluated with 5 results within
limits
Mass
Calc. mass
mDa
ppm
DBE
Formula
417.1798
417.1801
417.1788
417.1814
418.1848
418.1834
418.1853
418.1861
−0.2
1.1
−1.6
−0.5
0.9
−1.0
−1.8
−0.6
2.6
−3.8
−1.1
2.1
−2.3
−4.3
15.0
10.0
14.5
14.5
15.0
2.0
19.5
C23 H23 N5 O3
C22 H27 NO7
C25 H25 N2 O4
13 12
C C24 H25 N2 O4
13 12
C C22 H23 N5 O3
13 12
C C10 H27 N7 O10
13 12
C C25 H21 N6
418.1843
Target analysis and dereplication by MS
Effective dereplication methodologies should aim to ensure that
isolation, structure elucidation and pharmacological investigations are focused on novel compounds. In this scenario, mass
spectrometry and especially high resolution mass spectrometry
is the core technology for dereplication used in combination
with databases such as Antibase, and MarinLit.199,214,220–224 It can
be argued whether dereplication should be done before or after
a bio-assay step (see overview Fig. 1).
The key issue in dereplication is to assign the ions to
chromatographic peaks in the LC-MS spectrum correctly, a task
that can vary from being very easy to impossible. In positive
mode alkaloids usually ionize well and amides reasonably well,
whereas sugars and other polyols ionise very poorly. Carboxylic
acids have a reputation of ionizing poorly in positive mode,
however this is not always the case, although it is certainly
true for phenolics and aromatic carboxylic acids.225 Even small
structural changes between molecules can induce significant
changes in response factors, a good example of this scenario
is the type A and B trichothecenes. The keto group in the
Type B (presumably tautomerisation into a triol), are poorly
detected using ESI+ , however very good ionization is seen
when using ESI− , whereas the opposite is the case for the
type A ones. Therefore it may be advantageous to use online positive/negative ionisation during the chromatographic
run. Ion-traps and quadrupole instruments can easily do this
whereas TOF instruments have problems doing this and still
run in accurate mass mode. Moreover buffering of the solvent
system is even more restricted using polarity switching so for
trace analysis or for very dirty samples it is still advantageous to
run the samples in separate runs with different solvent systems.
It should be noted that the ions formed in both positive
and negative mode are even-electron ions compared to classic
positive electron impact ionization (EI+ ) mass spectrometry
(MS) where odd-electron ions are formed. This means that the
fragmentation mechanisms are fundamentally different.
ESI+ is the most versatile ionization mode and when working
with low resolution data a deconvolution analysis of the data file
is the fastest. However, this is not possible using the full accuracy
of modern TOF instruments as no commercial software can
handle this at the moment. In this case the approach is to: i)
obtain a background subtracted average spectrum of the peak
of interest; ii) deconvolute all the ions from this spectrum to
make sure that they are not coming from co-eluting compounds.
The spectrum is first investigated for the presence of A + 2 and
A + 4 ions, showing chlorine, bromine, and many (>3) sulfur
atoms just as known from classic EI+ mass spectrometry. The
deconvoluted mass spectrum is then assessed for ions seen in
Table 7, this means in practice jumps of 22 (H+ to Na+ ), 5 (NH4 +
to Na+ ), 63 (H+ to Na+ + CH3 CN), 18 (loss of water), 36 (loss
of 2 waters) and other jumps calculated from Table 7. Spectra
should also be examined for dimers [2M + H]+ and [2M + Na]+ ,
which for some compounds can be even more predominant than
the monomeric ions. Acids can exchange H+ to Na+ by a simple
ion exchange mechanism and subsequent adduct formation with
Na+ gives [M–H + 2Na]+ , which very strongly indicates that the
target compound is a carboxylic acid.
Sodium adduct ions are very stable compared with both
protonated and ammoniated ions and we have found that
identification of the sodium adduct ion(s) is very important for
a confident molecular mass determination. To make it easier
to find the sodiated adduct ion(s) it is advantageous to use
ion-source CID fragmentation as pseudo MS/MS, as it will
enhance their abundance along with fragment ions whereas
the relative abundance of the protonated and ammoniated ions
will decrease. This is done by using two “simultaneous” scan
Nat. Prod. Rep., 2005, 22, 672–695
687
Table 7 Common ions observed during LC-MS analyses of small moleculesa
Common adducts
Less common adducts
Common fragments
Less common fragments
Polymeric ions
a
Positive
Negative
[M + H]+ , [M + NH4 ]+ , [M + Na]+ [M + CH3 CN + H]+ , [M +
CH3 CN + Na]+ , [M + K]+
[M–H + 2Na]+
[M − H]− , [M + HCOO]− , [M +
CH3 COO]−
[M − 2H + Na]− , [M + Na − 2H
+ CH3 COOH]−
[M − H − CO2 ]−
[M + H − H2 0]+ , [M + H − 2(H2 O)]+ , [M + H − 3(H2 O)]+ , [M +
H − CO2 ]+
[M + H − CH4 O]+ , [M + H–CH3 COOH]+ , [Fragment + NH3 ]+
[Fragment + CH3 CN]+
[2M + H]+ , [2M + NH4 ]+ , [2M + Na]+
[2M − H]−
(<1500 Da).
Fig. 8 Confirmation of some of the findings shown in Fig. 7 using narrow ion traces (±0.01 Da except in two chromatograms) from accurate LC-MS
analysis of the same sample. The detector was overloaded for some of the ions (the 12 C isotopes of dehydro-griseofulvin and griseofulvin) giving too
low mass values due to the detector dead time error. The two peaks marked with an X are due to the high intensity error.
functions where one is set with a very low potential difference
between the two skimmers in the ion-source and one with a high
potential difference. The deconvoluted mass spectra from the
two scan functions are then compared.
As seen in Table 7 fragment ions with adducts of acetonitrile
and NH3 occasionally occur, however, we have rarely if ever
seen fragments with sodium adducts, although they can be
formed in an ion-trap.226 In ion-source CID, small molecules
are fragmented much more vigorously than larger molecules as
the kinetic energy (potential difference between skimmers) is the
same, meaning that the velocity is proportional to the square
root of the potential difference between the skimmers, e.g. at
m/z 150 Da ion will get double the velocity of a m/z 600 ion
and thus be fragmented much more.
688
Nat. Prod. Rep., 2005, 22, 672–695
Except for scientists working with specific groups of compounds not ionizing very well in positive mode, positive ionization data will usually be available, and ESI− will in many
cases just be used to confirm what is suspected from positive
mode unless “no ionization” was obtained by ESI+ . Nevertheless
it is always safest to have a molecular mass assigned from
analysis using both polarities indicating the same molecular
weight (see for example data for chaetoviridin A 48 in Fig. 9).
Usually ESI− generated spectra are far simpler to analyse than
ESI+ spectra. When using ESI− [M − H]− or an adduct with
formate and/or acetate can be detected, depending on which
of the acids is present in the solvent. These acid adducts can
some times be so predominant that the deprotonated ions are not
detected.
Fig. 9 LC-UV-MS analysis of a Chaetomium globosum extract where chaetoviridin A (C23 H25 ClO6 ) was tentatively identified. A ESI+ time-of-flight
(TOF) MS total ion chromatogram; B ESI+ TOF MS spectrum with annotated peaks; C ESI+ time-of-flight (TOF) MS total ion chromatogram; D
ESI− TOF MS spectrum with annotated peaks; E UV-VIS chromatogram (200–700 nm) from same file as ESI− ; F UV-VIS spectrum of the target
compound. Note that there is a time delay of ca. 0.04 min from the UV-VIS detector to the MS.
However, usually both ions can be detected. If in doubt it may
be necessary to reanalyse the sample using another buffer, e.g.
substitute formate for acetate or vice versa—or mix both to see
two ions with m/z 14 (CH2 ) in-between.
The jump from using nominal mass MS to accurate mass MS
in dereplication when searching databases is very helpful. E.g.
if Antibase 2003 (30 000 compounds) is searched for a nominal
mass in the range 200 to 500 Da, an average of 78 candidates
with even masses is found and 16 with an uneven mass are found.
However, if the accurate mass is known, then for the elemental
composition usually 3–10 candidates are found for an even mass
compound, although there for a few compounds can be up to 40.
For odd mass compounds usually 1 to 5 candidates are found.
However, this demands that the accurate mass is correct and
on QTOF and TOF instrument with TDC detectors this is not
always the case. There are some pitfalls, as also described above,
as the number of ions in a single scan should not exceed a certain
number (usually 50–100 ions), since the mass determination will
else be too low (see also Fig. 8). In such a case the spectra used
for calculating the elementary compositions must be taken in
the front or tail of the chromatographic peak.225
With a mass accuracy of 3 ppm there are usually 2–3
candidates in the 400 to 500 Da region (calculated with max 100
C, 15 O, 8 N, 4 S, 100 H, and 50 DBE), assuming that Cl, Br and
>4 S will be seen by the operator. If the mass accuracy is in the
range of 3 to 6 ppm 4 to 8 candidates are usually found in the
Nat. Prod. Rep., 2005, 22, 672–695
689
400 to 500 Da region. To validate the elemental composition
or narrow down the number of candidates, the elemental
composition should be calculated for all the adducts, dimeric,
and fragment ions which can be unambiguously assigned as
demonstrated by Nielsen and Smedsgaard.225 Subsequently or
integrated in the latter process isotope ratios of A, A + 1, A +
2, A + 3, etc. can be investigated further e.g. eliminating sulfur
and removing candidates where the A and A + 1 ratios does not
support the number of calculated carbon atoms. In this process
it is vital to know if there are interfering co-eluting compounds
which may affect the measured isotope pattern. It is also vital to
know how accurate the MS in use shows the true isotope pattern,
which can easily be checked on some known compounds.
The final step in the dereplication process is to search either
the candidate(s) from the elementary composition calculations
or the molecular mass in appropriate databases, i.e. Antibase,
MARINLIT, NAPRALERT, and Dictionary of Natural Products. The hit(s) from the database search are then matched
against the UV-VIS data from the target peak (see next section),
which usually can eliminate many candidates. After that the
retention on the chromatographic system can be assessed and
usually many very polar/apolar compounds can be eliminated
based on such comparisons. The ionization efficiency in positive
versus negative mode and relative UV-VIS also gives some valid
information. E.g. amines will always ionize well so if a very
small peak is seen in positive mode whereas large peaks are seen
in negative and/or UV then the compound is not an alkaloid.
Finally the fragments obtained by in-source fragmentation
and/or data-depended MS/MS can be evaluated against the
remaining structures.
6.4 Chemical image analysis—UV spectral analysis
With the advancement of HPLC and UPLC as well as much
more stable and better columns for high resolution separation,
combined with fast UV diode array detectors it has become
easy to acquire the UV spectrum of practically every single
component from an extract. Consequently the UV spectrum
has turned into being one of the most readily accessible pieces
of information related to structure of NPs why there is increased
interest in exploiting its usefulness.227
However, the chromatographic data matrix can also be viewed
as a landscape with the retention time being the first dimension,
the spectrum the second, and finally the detected values the third.
These topographic landscapes can be compared automatically
using techniques from image analysis. However, it is crucial
to correct for different artefacts due to differences in the
instrumental acquisition procedure from analysis to analysis.
Some of the most important artefacts include baseline drifts
and shifts in retention time. Baseline correction is done through
subtraction of an estimated baseline, wavelength by wavelength.
The baseline drift can be regarded as a nonlinear function, but
most often segments are detected from which the baseline is
estimated by partially linear interpolation.
In order to compensate for the minor shifts in retention time,
it is necessary to align the chromatograms. All methods are more
or less derivatives of the same basis; to warp the time axis of a
chromatogram in order to obtain the best match to a reference
chromatogram. An early attempt of developing a retention
time warping algorithm was made by Wang and Isenhour.228
Since then, improvements have been made based on different
optimization criteria.229–231 But the probably most efficient way
to do aligning is through the correlation optimized warping
(COW) technique, using all the trace information available.232,233
Although time consuming, COW has proven to be the method
that gives the best results.234 Whereas the aligning algorithms
focus on solving the problem of shifts in the retention time by
optimizing the trace profiles, spectral shape information can
be added to the different aligning concepts.235 In addition, the
similarity between two HPLC matrices Xi and Xj is evaluated
690
Nat. Prod. Rep., 2005, 22, 672–695
in two steps: 1) The similarity between the UV-spectra where Xi
has peaks, and 2) the similarity between the UV-spectra where Xj
has peaks. The peaks were found as the mean absorbance value
from each aligned spectrum, followed by a smothering using a
simple mean filtering over a window of 9 UV-spectra. This was
found to be both fast and sufficient to remove the small spikes
that could be present; however, other filtering techniques could
be applied if needed.236 The principle of the method is based on
evaluating the spectral information present in the HPLC data
matrices, and the algorithm consists of two parts:
1) Calculation of a local similarity, followed by
2) calculation of a global similarity between the HPLC data
matrices.
For two chromatographic data matrices a vector of locally
aligned full spectral similarities is calculated along the retention
time axis. The vector depicts the evaluation of the alikeness
between two fungal extracts based upon eluted compounds
and corresponding UV-absorbance spectra. By comparing coeluting components by their UV-spectra across samples, information about the (dis)similarity between actual compounds
could be examined. The similarity was evaluated as a “distance”
between the observed UV-spectra. Based on these spectra
classification of the samples can be made.204,235
One of the major advantages of applying the method is that
the chemical diversity can be calculated by selecting only a few
input parameters involved in the process. 1) Which part of the
chromatograms and which spectral range to include, 2) perform
a simple baseline correction, 3) align the chromatograms by
warping, 4) scale the chromatograms and finally 5) calculate
the similarity. Therefore, the method removes the bias from
comparisons and makes reproducibility possible between data
files made at different periods. Most algorithms used for warping
mainly rely on chromatographic traces, and problems may occur
when several compounds are eluting within a short period of
time. By using the full UV-spectral information in the aligning,
the algorithm aligns peaks having the same UV-spectrum.
6.5 Dereplication and partial identification of NPs by
UV-based techniques
Apart from exact structural formulae structural databases usually also contain physical chemical data including UV maxima
and minima characteristics of the included compounds. Today
only few organic chemists rely on UV as a primary tool for
structural elucidation, one reason being that the absorption
frequencies of the C–C, C–H and isolated C=C groups cannot
be observed in the easily accessible region of the UV spectrum.
However, many natural products such as polyketides and
alkaloids derived from aromatic amino acids have characteristic
UV spectra (Fig. 10) due to their polyunsaturated nature. In
addition many such NPs often have one or more carbonyl groups
as part of ketone, carboxylic acid, ester or amide functional
groups.
One early report using a UV based library for dereplication
of mycotoxins is the work by Frisvad and Thrane,237 who
used characteristic UV spectra of 187 mycotoxins and other
secondary metabolites for chemotaxonomy and food safety
studies.
Nielsen and Smedsgaard extended this fungal metabolite
database to 474 metabolites now also including MS spectral
data.225 Other research groups have developed similar in-house
HPLC-UV-VIS databases for dereplication purposes.238 Thus
Fiedler et al.239 used their database containing approx. 750 UV
spectra to investigate a set of 600 marine actinomycete strains
for production of both a number of known antibiotics but also
as an approach to discover possible new metabolites. Similarly
Larsen et al. used a knowledge based UV-guided approach
for detection and isolation of novel alkaloid compounds from
fungal extracts.240–242 In order to systematise and keep track
of data and structural knowledge related to UV-spectra of
Fig. 10 Six similar but still slightly different and characteristic UV spectra of fungal alkaloids (anacine 49, verrucine A 50, alantrypinone 51, lapatin
A 52, sclerotigenin 53 and auranthine 54) that can be used for targeting of both known and new (but similar) natural products by X-hitting.235,243
both known and possible new fungal metabolites Hansen et al.
recently developed a new algorithm called X-hitting to be used
in combination with a learning-based database.235 In X-hitting
already known metabolites are tracked by the feature crosshitting, whereas potential new metabolites are indicated by the
new-hitting feature of X-hitting. The algorithm behind X-hitting
compares the shape between two spectra and returns a similarity
index describing how statistically similar the two spectra are. In
order to capture information about the actual shape of each
of the profiles at different scales (coarser or finer details), a
linear combination of the correlation between higher order
derivatives are used. A main criterium being retaining relations
between “neighboring” values in spectra and in addition, that
the algorithm has to be fast to compute. By using derivatives such
relationships can be incorporated by measuring the differences
and the positions of topologies and extreme points. Finally
filtering techniques are applied to the derivatives in order to
reduce the sensitivity to potential noise fragments in the spectra.
Regarding the drug discovery process the great potential of
cross-hitting is its ability to support the choice of the optimal
organism for production of a given natural product. This is
the case both in de-screening of strains producing mycotoxins,
but maybe even more important also for the tracking of new
species producing a desired compound (in this scenario a new
drug lead). In this way cross-hitting of known compounds
can be applied for new-hitting of organisms. Very often a
certain compound is produced as a minor metabolite by one
species (under certain conditions), while it appears as one of
the major metabolites produced by another completely different
species.
The scope of the new-hitting feature of “X-hitting” is in
scenarios where a new lead such as a quinazoline (anacine 49,
verrucine 50, alantrypinone 51, lapatin A 52) or a benzodiazepine (sclerotigenin 53, auranthine 54) (Fig. 10) have already
been discovered by bio-guided screening. Due to the very similar
structure of these two types of compounds (Fig. 10), that both
incorporate anthranilic acid, they have very distinct and similar
chromophore systems, and can easily be tracked down from large
data sets of HPLC Diode array data by X-hitting.235 Thus using
the cross-hitting feature of X-hitting we can easily detect many
of the known quinazolines and benzodiazepines (unpublished
data) produced by Penicillium and Aspergillus.
Nat. Prod. Rep., 2005, 22, 672–695
691
Recently, Larsen et al. demonstrated the potential of newhitting by finding the two novel quinazolines lapatin A (52) and
B.243 Isolation of some new benzodiazepines by our group using
new-hitting is in progress, where the use of sclerotigenin as target
UV-spectrum gives several hits in an extract of Aspergillus janus.
We predict that new-hitting will be a powerful alternative to
finding/generating new leads by traditional organic synthesis or
by combinatorial chemistry methodologies.
6.6 Metabolite fingerprinting, profiling and target analysis by
NMR
Traditionally NMR has been used for structural elucidation of
pure compounds or relatively simple mixtures of compounds
generated from e.g. organic synthesis. The recent combination
of high-performance liquid chromatography interfaced to NMR
has eliminated the need to purify a compound before analysis.
NMR spectra can either be recorded in continuous or stopped
flow. Furthermore the output from an HPLC can be split into
two pathways, one for NMR analysis and the other for MS,
increasing the sensitivity by using a solid phase extraction (SPE)
step between the HPLC column and the NMR spectrometer.209
Thus several papers report the characterisation of numerous
natural products directly from complex mixtures using LCNMR.244–247 When combined with computer assisted software
programs for structural elucidation,248,249 the task of identifying
both known and new NPs by NMR have surely become a much
easier task within the last 5–10 years.
More recently the analysis of complex mixtures and biofluids
with the purpose of categorizing large numbers of individual
spectra by NMR spectroscopy by computational methods has
become an increasing application. This covers areas such as
disease diagnosis, quality control of foods such as citrus juices,
edible/olive oils, wine/beer.208,250,251 Even though it is still a
challenge, metabolite fingerprinting by NMR is considered a
fast, convenient, and effective tool for discriminating between
groups of related samples just based on a comparison on
the distribution of intensity in the NMR rather than on the
assignment of the individual signals.209
To our knowledge no attempts have been made to use e.g.
1
H NMR spectra as part of a microbial drug discovery process
using e.g. 1 H NMR spectra with the purpose of clustering data
of microbial extracts into chemotypes in a similar way as direct
MS profiling has been used.207 On the other hand NMR has
been extensively used in plant metabolomics where some argue
that the metabolome is a fundamentally important biochemical
manifestation of the genome, each extract defining a metabolic
phenotype that forms the basis for discriminating between plants
of different genotypes.209 These are altogether arguments that
are in very good agreement with the major conclusions drawn
in this review. In our opinion the potential for using NMR of
crude extracts as part of a microbial drug discovery process is
largely untapped even though issues such as stringent control of
sample preparation, with precise control of the pH, and precise
temperature control during acquisition need to be addressed.
7. Conclusions and future perspectives
With the genomic revolution the need for new pharmaceutical
leads is enormous. Since there are still many unexplored
resources in Nature, the potential for finding new organisms and
thereby new metabolic pathways is also enormous. Therefore
natural products still have a very important role to play
in the drug discovery process, especially due to their often
very complex and chiral nature. A large proportion of new
leads/scaffolds in the future can therefore be expected to be
NPs and natural product chemistry should therefore not be
considered a competing discipline to combinatorial chemistry.
Instead a combination of the two disciplines seems to be the
right track to follow in the search for valuable new drugs.
692
Nat. Prod. Rep., 2005, 22, 672–695
In this review we have argued that microbial organisms, and
at least eukaryotic filamentous fungi, are very consistent in their
production of secondary metabolites at the species level when
cultured under standardized conditions. In other words strains
of different species represent different chemotypes, whereas
strains of the same species represent the same chemotype. We
have shown that these differences and similarities can easily
be analyzed for using direct analytical profiling techniques
such as DI-HRMS in combination with modern chemoinformatics tools. This might not be the case for other organisms
such as Actinomycetes where horizontal gene transfer could
be a pronounced event leading to potential transferring of
biosynthetic pathways. Recent studies on the new marine genus
Salinospora, however, showed a clear correlation between species
and classes of compounds produced, indicating a large degree
of chemoconsistency also within these types of organisms.31
Additional types of organisms, including several genera and
species need to be studied in order to prove our hypothesis that
secondary metabolites in most cases will be very consistently
produced at the species level also in other microorganisms than
filamentous fungi.
We have argued that instead of including many identical
strains with the same chemotypes in a drug discovery screening process, the effort should instead be addressed on the
investigation of much fewer talented strains under multiple
culture conditions for optimization of secondary metabolite
production in order to fully explore the secondary metabolite
potential of a given organism. Also a combined taxonomic
and thereby ecological knowledge about a given species will
point towards investigation of relevant stimulation studies such
as the stimulation of fungal metabolite production by adding
plant extracts or by co-cultivation of relevant natural co-existing
organisms.
A chemical based drug discovery approach is not only important in the process of dereplicating of culture collections, but
also in the dereplication of single compounds using hyphenated
analytical techniques interphasing LC with MS, NMR and
UV. The importance of high resolution MS in this context
is of course substantial, with the possibility of using accurate
masses for suggesting molecular formulae that can be searched
in various databases. However, the fact that many biological
active NPs contain conjugated systems and thereby more or
less specific UV-chromophores could also be applied as an
important aid not only in the dereplication process both also
for the search and discovery of novel bioactives with similar
structural features as already known bioactives. The different
spectroscopic information that can be gained from MS, NMR
and UV complement each other and are all expected to play and
important role in future chemoinformatics based drug discovery
approaches.
8.
Acknowledgements
The authors wish to acknowledge the support from The Danish
Research Councils for the Program for Predictive Biotechnology
(2000–2004) (Grant No. 9901295) and the IVC Center for
Microbial Biotechnology (2004–2008) (Grant No. 46–00–0005),
during which many of the ideas, methodologies, and results
presented here were generated.
9.
References
1
2
3
4
5
6
7
8
M. S. Butler, J. Nat. Prod., 2004, 67, 2141.
M. S. Butler, Nat. Prod. Rep., 2005, 22, 162.
J. C. Frisvad and R. A. Samson, Stud. Mycol., 2004, 49, 1.
D. H. Williams, M. J. Stone, P. R. Hauck and S. K. Rahman, J. Nat.
Prod., 1989, 52, 1189.
A. L. Demain, Appl. Microbiol. Biotechnol., 1999, 52, 455.
W. R. Strohl, Drug Discovery Today, 2000, 5, 39.
G. L. Verdine, Nature, 1996, 384s, 11.
L. Müller-Kuhrt, Nat. Biotechnol., 2003, 21, 602.
9 D. J. Newman, G. M. Cragg and K. M. Snader, J. Nat. Prod., 2003,
66, 1022.
10 A. Ganesan, Curr. Opin. Biotechnol., 2004, 15, 584.
11 G. A. Petsko, Nature, 1996, 384s, 7.
12 L. J. Nisbet and M. Moore, Curr. Opin. Biotechnol., 1997, 8, 708.
13 V. Knight, J. J. Sanglier, D. DiTullio, S. Braccili, P. Bonner, J. Waters,
D. Hughes and L. Zhang, Appl. Microbiol. Biotechnol., 2003, 62,
446.
14 J. W. Costerton, P. S. Stewart and E. P. Greenberg, Science, 1999,
284, 1318.
15 D. G. Davies, M. R. Parsek, J. P. Pearson, B. H. Iglewski, J. W.
Costerton and E. P. Greenberg, Science, 1998, 280, 295.
16 T. B. Rasmussen, M. E. Skindersø, T. Bjarnsholt, R. K. Phipps, K. B.
Christensen, J. B. Andersen, B. Koch, T. O. Larsen, M. Hentzer, N.
Høiby and M. Givskov, Microbiology, 2005, 151, 1325.
17 A. T. Bull, J. E. M. Stach, A. C. Ward and M. Goodfellow, Antonie
van Leeuwenhoek, 2005, 87, 65.
18 A. T. Bull, A. C. Ward and M. Goodfellow, Microbiol. Mol. Biol.
Rev., 2000, 64, 573.
19 G. M. Müller, G. F. Bills and M. S. Foster, Biodiversity of
Fungi. Inventory and Monitoring Methods, Elsevier Academic Press,
Amsterdam, 2004, 777 pp.
20 M. Jaspars and L. Lawton, Curr. Opin. Drug Discovery Dev., 1998,
1, 77.
21 J. Blunt, B. R. Copp, M. H. G. Munro, P. T. Northcote and M. R.
Prinsep, Nat. Prod. Rep., 2005, 22, 15.
22 J. C. Frisvad, in Innovative Roles of Biological Resource Centers, ed.
M. M. Watanabe, K. Suzuki and T. Seki, Japan Society for Culture
Collections & World Federation for Culture Collections, Tsukuba,
2004, p. 165.
23 J. C. Frisvad, T. O. Larsen, P. W. Dalsgaard, K. A. Seifert, G. LouisSeize, E. K. Lyhne, B. B. Jarvis, J. C. Fettinger and D. P. Overy,
Int. J. Syst. Evol. Microbiol., 2005, in press.
24 P. W. Dalsgaard, T. O. Larsen and C. Christophersen, J. Nat. Prod.,
2004, 67, 878.
25 P. W. Dalsgaard, J. W. Blunt, M. H. G. Munro, T. O. Larsen and C.
Christophersen, J. Nat. Prod., 2004, 67, 1950.
26 P. W. Dalsgaard, T. O. Larsen and C. Christophersen, J. Antibiot.,
2005, 58, 141.
27 O. Filtenborg, J. C. Frisvad and U. Thrane, Int. J. Food Microbiol.,
1996, 33, 85.
28 B. Haefner, Drug Discovery Today, 2003, 8, 536.
29 J. E. M. Stach and A. T. Bull, Antonie van Leeuwenhoek, 2005, 87,
3.
30 U. Höller, A. D. Wright, G. F. Matthée, G. M. Konig, S. Draeger,
H.-J. Aust and B. Schulz, Mycol. Res., 2000, 104, 1354.
31 P. R. Jensen, T. J. Mincer, P. G. Willaims and W. Fenical, Antonie
van Leeuwenhoek, 2005, 87, 43.
32 C. E. Salomon, N. A. Magarey and D. H. Sherman, Nat. Prod. Rep.,
2004, 21, 105.
33 E. W. Schmidt, J. T. Nelson, D. A. Ratsko, S. Sudek, J. A. Eisen,
M. G. Haygood and J. Ravel, Proc. Natl. Acad. Sci. U. S. A., 2005,
102, 7315.
34 P. F. Long, W. C. Dunlap, C. N. Battershill and M. Jaspars,
ChemBioChem, 2005, 6, 1760.
35 D. L. Hawksworth, Mycol. Res., 1991, 95, 641.
36 D. L. Hawksworth, Stud. Mycol., 2004, 50, 9.
37 D. L. Hawksworth and A. Y. Rossman, Phytopathology, 1997, 87,
888.
38 B. Schulz, C. Boyle, S. Draeger, A.-K. Römmert and K. Krohn,
Mycol. Res., 2002, 106, 996.
39 A. Stierle, G. Stobel and D. Stierle, Science, 1993, 260, 214.
40 A. Stierle and G. Stobel, J. Nat. Prod., 1995, 58, 1315.
41 R. Verpoorte, Drug Discovery Today, 1998, 3, 232–238.
42 P. F. Dowd, J. D. Miller and R. Greenhalgh, Mycologia, 1989, 81,
646.
43 P. F. Dowd, in Handbook of Applied Mycology, Vol. 5: Mycotoxins in
Ecological Systems, ed. D. Bhatnagar, E. B. Lillehøj and D. J. Arora,
Marcel Dekker, New York, 1992, p. 333.
44 D. T. Wicklow, in: Coevolution of Fungi with Plants and Animals, ed.
K. A. Pirozynski and D. L. Hawksworth, Academic Press, London,
1998, p. 173.
45 J. Gloer, Can. J. Bot., 1995s1, 73, 1265.
46 Y. Zhang, C. Li, D. C. Swenson, J. B. Gloer, D. T. Wicklow and P. F.
Dowd, Org. Lett., 2003, 5, 773.
47 C. Li, J. B. Gloer, D. T. Wicklow and P. F. Dowd, J. Nat. Prod.,
2005, 68, 319.
48 D. P. Overy and J. C. Frisvad, Syst. Appl. Microbiol., 2003, 26, 631.
49 M. Boysen, P. Skouboe, J. C. Frisvad and L. Rossen, Microbiology,
1996, 142, 541.
50 K. Karlshøj and T. O. Larsen, J. Agric. Food Chem., 2005, 53, 708.
51 K. F. Nielsen, P. W. Dalsgaard, J. Smedsgaard and T. O. Larsen,
J. Agric. Food Chem., 2005, 53, 2908.
52 J. Smedsgaard and J. Nielsen, J. Exp. Bot., 2005, 56, 273.
53 K. Zengler, G. Toledo, M. Rappe, J. Elkins, E. J. Mathur, J. M. Short
and M. Keller, Proc. Natl. Acad. Sci. U. S. A., 2002, 99, 15681.
54 M. S. Osburne, T. H. Grossman, P. R. August and I. A. MacNeil,
Am. Soc. Microbiol. News, 2000, 7, 411.
55 J. Handelsman, M. R. Rondon, S. F. Brady, J. Clardy and R. M.
Goodman, Chem. Biol., 1998, 5, 245.
56 D. Cowan, Q. Meyer, W. Stafford, S. Muyanga, R. Cameron and P.
Wittwer, Trends Biotechnol., 23, 321.
57 N. Peric-Concha and P. F. Long, Drug Discovery Today, 2003, 8,
1078.
58 J. Kennedy and C. R. Hutchinson, Nat. Biotechnol., 1999, 17, 538.
59 B. S. Moore, J. A. Kalaitzis and L. Xiang, Antonie van Leeuwenhoek,
2005, 87, 49.
60 J. Staunton and K. J. Weissman, Nat. Prod. Rep., 2001, 18, 380.
61 B. A. Pfeifer and C. Khosla, Microbiol. Mol. Biol. Rev., 2001, 65,
106.
62 J. Nielsen, Curr. Opin. Microbiol., 1998, 1, 330.
63 J. Nielsen, Appl. Microbiol. Biotechnol., 2001, 55, 263.
64 S. Kosemura, Tetrahedron, 2003, 59, 5055.
65 S. A. Waksman and E. Bugie, Proc. Natl. Acad. Sci. U. S. A., 1943,
29, 282.
66 R. L. Monaghan, J. D. Polishook, V. J. Pecore, G. F. Bills, M. NallinOlmstead and S. L. Streicher, Can. J. Bot., 1995, 73s1, 925, ISBN
87-88584-44-5.
67 A. Ciegler, D. I. Fennell, D. A. Sansing, R. W. Detroy and G. A.
Bennett, Appl. Microbiol., 1973, 26, 271.
68 G. Engel, K. E. von Milczewskii, D. Prokopek and M. Teuber, Appl.
Environ. Microbiol., 1982, 43, 1034.
69 J. C. Frisvad, Dr. Tech. Dissertation, Technical University of
Denmark, 1998.
70 M. Wink, Phytochemistry, 2003, 64, 3.
71 H. T. Lumbsch, in Chemical Fungal Taxonomy, ed. J. C. Frisvad,
P. D. Bridge and D. K. Arora, Marcel Dekker, New York, 1998, p.
345.
72 J. C. Frisvad, U. Thrane and O. Filtenborg, in Chemical Fungal
Taxonomy, ed. J. C. Frisvad, J. C., P. D. Bridge and D. K. Arora,
Marcel Dekker, New York, 1998, p. 289.
73 J. C. Frisvad, J. M. Frank, J. A. M. Houbraken, A. F. A. Kuijpers
and R. A. Samson, Stud. Mycol., 2004, 50, 23.
74 R. A. Samson, J. A. M. Houbraken, A. F. A. Kuijpers, J. M. Frank
and J. C. Frisvad, Stud. Mycol., 2004, 50, 4561.
75 J. C. Frisvad, J. Smedsgard, T. O. Larsen and R. A. Samson, Stud.
Mycol., 2004, 49, 201.
76 V. Hellwig, Y.-M. Ju, J. D. Rogers, Fournier and M. Stadler, Mycol.
Prog., 2005, 4, 39.
77 C. Thom, The Penicillia, Williams and Wilkins, Baltimore, MD,
1930.
78 K. B. Raper and C. Thom, A Manual of the Penicillia, Williams and
Wilkins, Baltimore, MD, 1949.
79 K. B. Raper and D. I. Fennell, The genus Aspergillus, Williams and
Wilkins, Baltimore, MD, 1965.
80 J. C. Frisvad, Arch. Environ. Contam. Toxicol., 1989, 18, 331.
81 R. D. Hutchinson, P. S. Steyn and S. J. van Rensburg, Toxicol. Appl.
Pharmacol., 1973, 24, 507.
82 A. E. de Jesus, W. E. Hull, P. S. Steyn, F. R. van Heerden and R.
Vleggaar, J. Chem. Soc., Chem. Commun., 1982, 16, 902.
83 J. C. Frisvad and O. Filtenborg, Mycologia, 1989, 81, 836.
84 J. I. Pitt, R. A. Samson and J. C. Frisvad, in Integration of Modern
Taxonomic Methods for Penicillium and Aspergillus Classification,
ed. R. A. Samson, and J. I. Pitt, Harwood Academic Publishers,
Amsterdam, 2000, p. 9.
85 J. C. Frisvad, O. Filtenborg, R. A. Samson and A. C. Stolk, Antonie
van Leeuwenhoek, 1990, 57, 179.
86 J. C. Frisvad and O. Filtenborg, in Modern Concepts in Penicillium
and Aspergillus Classification, ed. R. A. Samson, and J. I. Pitt,
Plenum Press, New York, 1990, p. 373.
87 J. C. Frisvad and O. Filtenborg, in Modern Concepts in Penicillium
and Aspergillus Classification, ed. R. A. Samson, and J. I. Pitt,
Plenum Press, New York, 1990, p. 159.
88 B. Andersen, J. Smedsgaard and J. C. Frisvad, J. Agric. Food Chem.,
2004, 52, 2421.
89 S. Sonjak, J. C. Frisvad and N. Gunde-Cimerman, FEMS Microbiol.
Ecol., 2005, 53, 51.
90 J. F. Makins, G. Holt and K. D. MacDonald, J. Gen. Microbiol.,
1983, 116, 3027.
91 S. A. Waksman and E. S. Hornung, Mycologia, 1943, 35, 47–65.
92 S. A. Waksman and A. Schatz, Proc. Natl. Acad. Sci. U. S. A., 1943,
29, 74.
Nat. Prod. Rep., 2005, 22, 672–695
693
93 S. A. Waksman, E. S. Hornung and E. L. Spencer, J. Bacteriol.,
1943, 45, 47.
94 O. Filtenborg, J. C. Frisvad and U. Thrane, in Modern Concepts
in Penicillium and Aspergillus Classification, ed. R. A. Samson and
J. I. Pitt, Plenum Press, New York, 1990, p. 433.
95 K. B. Raper, D. F. Alexander and R. D. Coghill, J. Bacteriol., 1944,
48, 639.
96 S. P. Brundidge, F. C. A. Gaeta, D. J. Hook, C. Jr. Sapino, R. P.
Elander and R. B. Morin, J. Antibiot., 1980, 33, 1348.
97 S. J. Andersen and J. C. Frisvad, Lett. Appl. Microbiol., 1994, 19,
486.
98 E. L. Dulaney, Mycologia, 1947, 39, 570.
99 D. S. Cole, G. Holt and K. D. MacDonald, J. Gen. Microbiol., 1976,
96, 423.
100 A. P. MacCabe, M. B. R. Riach, S. E. Unkles and J. R. Kinghorn,
EMBO J., 1990, 9, 279.
101 P. W. Clutterbuck, A. E. Oxford, H. Raistrick and G. Smith,
Biochem. J., 1932, 24, 1441.
102 J. Jacquet and A. Tantaoui-Eleraki, Ann. Nutr. Aliment., 1977, 31,
563.
103 P.-K. Chang, D. Bhatnagar, T. E. Cleveland and J. W. Bennett, Appl.
Environ. Microbiol., 1995, 61, 40.
104 M. A. Klich, P.-K. Chang, E. J. Mullaney, D. Bhatnagar and T. E.
Cleveland, Appl. Microbiol. Biotechnol., 1995, 44, 439.
105 K. Kusumoto, K. Mori, H. Nogata, H. Ohta and M. Manabe,
J. Ferment. Bioeng., 1996, 82, 161.
106 K. Kusumoto, K. Yabe, Y. Nagata and H. Ohta, FEMS Microbiol.
Lett., 1998, 169, 303.
107 K. Kusumoto, Y. Nogata and H. Ohta, Curr. Genet., 2000, 37, 104.
108 A. J. Watson, L. J. Fuller, D. J. Jeens and D. B. Archer, Appl. Environ.
Microbiol., 1999, 65, 307.
109 K. Matsushima, P.-K. Chang, J. Yu, D. Bhatnagar and T. E.
Cleveland, Appl. Microbiol. Biotechnol., 2001, 55, 585.
110 K. Matsushima, K. Yashiro, Y. Hanya, K. Abe, K. Yabe and T.
Hamasaki, Appl. Microbiol. Biotechnol., 2001, 55, 771.
111 T. Takahashi, P.-K. Chang, K. Matsushima, J. Yu, K. Abe,
D. Bhatnagar, T. E. Cleveland and Y. Koyama, Appl. Environ.
Microbiol., 2002, 68, 3737.
112 F. Lund and J. C. Frisvad, Mycol. Res., 1994, 98, 481.
113 F. Blank, W. C. Day and G. Just, J. Invest. Dermatol., 1963, 40, 133.
114 J. G. Wirth, T. E. Beesley and S. R. Anand, Phytochemistry, 1965,
4, 505.
115 A. S. Ng, G. Just and F. Blank, Can. J. Chem., 1969, 47, 1223.
116 D. A. Geiser, J. C. Frisvad and J. W. Taylor, Mycologia, 1998, 90,
832.
117 K. Furuya, R. Emokita and M. Shirasaka, Ann. Sankyo Res. Lab.,
1967, 19, 91.
118 D. Broadbent, H. G. Hemming and G. McGowern, Trans. Br.
Mycol. Soc., 1974, 62, 625.
119 B. B. Jarvis, W. G. Sorenson, E.-L. Hintikka, M. Nikulin, Y. Zhou,
J. Jiang, S. Wang, S. F. Hinkley, R. A. Etzel and D. G. Dearbom,
Appl. Environ. Microbiol., 1998, 64, 3620.
120 M. Namikoshi, H. Kobayashi, T. Yoshimoto, S. Meguro and K.
Akano, Chem. Pharm. Bull., 2000, 48, 1452.
121 J. C. Frisvad and R. A. Samson, Stud. Mycol., 2000, 45, 201.
122 L. Wang, H.-B. Zhou, J. C. Frisvad and R. A. Samson, Antonie van
Leeuwenhoek, 2004, 86, 173.
123 A. E. Oxford, H. Raistrick and P. Simonart, Biochem. J., 1939, 33,
240.
124 E. G. Jeffreys, P. W. Brian, H. G. Hemming and D. Lowe, J. Gen.
Microbiol., 1953, 9, 314.
125 P. W. Brian, P. J. Curtis and H. G. Hemming, Trans. Br. Mycol. Soc.,
1949, 32, 30.
126 S. M. Clarke and M. McKenzie, Nature, 1967, 213, 504.
127 P. W. Brian, P. J. Curtis and H. G. Hemming, Trans. Br. Mycol. Soc.,
1955, 38, 305.
128 L. Leistner and C. Eckardt, Fleischwirtschaft, 1979, 59, 1892.
129 M. Christensen, J. C. Frisvad and D. I. Tuthill, Mycol. Res., 1998,
103, 527.
130 J. MacMillan, Chem. Ind. (London), 1951, 719.
131 K. Udagawa and S. Abe, J. Antibiot., 1961, 14, 215.
132 D. Kingston, P. Chen and J. R. Vercellotti, Phytochemistry, 1976,
15, 1037.
133 P. W. Brian, Trans. Br. Mycol. Soc., 1960, 43, 1.
134 B. Andersen, K. F. Nielsen and B. B. Jarvis, Mycologia, 2002, 94,
392.
135 B. Andersen, K. F. Nielsen, U. Thrane, T. Szaro, J. W. Taylor and
B. B. Jarvis, Mycologia, 2003, 95, 1227.
136 R. Bentley, Chem. Rev., 2000, 100, 3801.
137 R. A. Samson, K. A. Seifert, A. F. A. Kuijpers, J. A. M. Houbraken
and J. C. Frisvad, Stud. Mycol., 2004, 49, 175.
694
Nat. Prod. Rep., 2005, 22, 672–695
138 P. Lafont, J.-P. Debeaupuis, M. Gaillardin and J. Payen, Appl.
Environ. Microbiol., 1979, 37, 365.
139 O. Puel, S. Tadrist, P. Galtier, I. P. Oswald and M. Delaforgem,
Appl. Environ. Microbiol., 2005, 71, 550.
140 R. Gosio, Rivista Igiene Sanita Publica Ann., 1896, 7, 825.
141 C. L. Alsberg and O. F. Black, U.S. Dept. Agric. Bur. Plant Industry
Bull., 1913, 270, 1.
142 A. E. Oxford and H. Raistrick, Biochem. J., 1933, 27, 1176.
143 A. E. Oxford and H. Raistrick, Biochem. J., 1933, 27, 1473.
144 J. C. Frisvad and O. Filtenborg, Appl. Environ. Microbiol., 1983, 46,
1301.
145 M. Devys, J. F. Bousquet, A. Kollman and M. Barbier, Phytochemistry, 1980, 19, 2221.
146 N. G. Vinokurova, N. E. Ivanushkina, G. A. Kochina, M. U.
Arinbasarov and S. M. Ozerskaya, Appl. Biochem. Microbiol., 2005,
41, 83.
147 Y. Fujimoto, M. Kamiya, H. Tsunoda, K. Ohtsubo and T. Tatsuno,
Chem. Pharm. Bull., 1980, 28, 1062.
148 M. Umeda, T. Yamashita, M. Saito, S. Sekita, C. Takahashi, K.
Yoshihira, S. Natori, H. Kurata and S. Udagawa, Jpn. J. Exp. Med.,
1974, 44, 83.
149 H. S. Burton, Br. J. Exp. Pathol., 1949, 30, 151–158.
150 T. O. Larsen and J. C. Frisvad, Mycol. Res., 1995, 99, 1153.
151 M. Umeda, K. Ohtsubo, M. Saito, S. Sekita, K. Yoshihira, S. Natori,
S. Udagawa, F. Sakabe and H. Kurata, Experientia, 1975, 15, 435.
152 J. P. Springer, J. Clardy, J. M. Wells, R. J. Cole, J. W. Kirksey, R. D.
Macfarlane and D. F. Torgerson, Tetrahedron Lett., 1976, 17, 1355.
153 D. Veselý, D. Veselá and R. Jelı́nek, Mycopathologia, 1995, 132, 31.
154 J. Namgoong, S. Yeon, N. Paak, Y. Kim, C. Kim and K. Kim, Sanop
Misaengmul Hakhoechi, 1998, 26, 137.
155 A. Tikoo, H. Cutler, S. H. Lo, L. B. Chen and H. Maruta, Cancer J.,
1999, 5, 293.
156 A. Tikoo, R. Shakri, L. Conolly, Y. Hirokawa, T. Shishido, B.
Bowers, L. Ye, K. Kohama, R. J. Simpson and H. Maruta, Cancer J.,
2000, 6, 162.
157 A. Ichihara, K. Katayama, H. Teshima, H. Oikawa and S. Sakamura, Biosci., Biotechnol., Biochem., 1996, 60, 360.
158 C. Von Wallbrunn, H. Luftmann, K. Bergander and F. Meinhardt,
J. Gen. Appl. Microbiol., 2001, 47, 33.
159 Y. Amemiya, A. Kondo, K. Hirano, T. Hirukawa and T. Kato, Chiba
Daigaku Engeigakubu Gakujutsu Hokoku, 1994, 48, 13.
160 J. G. Kang, K. K. Kim and K. Y. Kang, Agric. Chem. Biotechnol.
(Engl. Ed.), 1999, 42, 146.
161 P. H. A. Sneath and R. R. Sokal, in Numerical taxonomy,
W. H. Freeman and Co., San Francisco, 1973.
162 R. R. M. Paterson, S. M. J. Simmonds and W. M. Blaney,
J. Invertebr. Path., 1987, 50, 124.
163 B. A. Bird, A. T. Remaley and I. M. Campbell, Appl. Environ.
Microbiol., 1981, 42, 521.
164 B. A. Bird and I. M. Campbell, Appl. Environ. Microbiol., 1982, 43,
345.
165 C. Young, L. McMillan, E. Telfer and B. Scott, Mol. Microbiol.,
2001, 39, 754.
166 N. P. Keller and T. M. Hohn, Fungal Genet. Biol., 1997, 21, 17.
167 S. Udagawa, T. Muroi, H. Kurata, S. Sekita, K. Yoshihira, S. Natori
and M. Umeda, Can. J. Microbiol., 1979, 26, 170.
168 S. Sekita, K. Yoshihira, S. Natori, S. Udagawa, F. Sakabe, H. Kurata
and M. Umeda, Chem. Pharm. Bull., 1982, 30, 1609.
169 S. Sekita, K. Yoshihira, S. Natori and H. Kuwano, Chem. Pharm.
Bull., 1982, 30, 1618.
170 S. Sekita, K. Yoshihira, S. Natori, S. Udagawa, T. Muroi, Y.
Sugiyama, H. Kurata and M. Umeda, Can. J. Microbiol., 1981,
27, 766.
171 H. Oikawa, Y. Murakami and A. Ichihara, Tetrahedron Lett., 1991,
32, 4533.
172 K. Koyoma, K. Takahashi, S. Natori and S. Udagawa, Proc. Jpn.
Assoc. Mycotoxicol., 1991, 33, 40.
173 C. Spöndlin and C. Tamm, Helv. Chim. Acta, 1988, 71, 1881.
174 R. Donoso, A. Rivera-Sagredo, J. A. Hueso-Rodriguez and S. W.
Elson, Nat. Prod. Lett., 1997, 10, 49.
175 O. Convert, A. Jellal, I. Correira, F. Dardoize, L. Menguy and J. C.
Cherton, Analysis, 1994, 22, 217.
176 J. C. Frisvad, R. A. Samson, B. Rassing, M. I. van der Horst, F. T. J.
van Rijn and J. Stark, Antonie van Leeuwenhoek, 1997, 72, 119.
177 T. O. Larsen, J. C. Frisvad, G. Ravn and T. Skaaning, Food Addit.
Contam., 1998, 15, 671.
178 A. Numata, C. Takahashi, Y. Ito, K. Minoura, T. Yamada, C.
Matsusa and K. Nomoto, J. Chem. Soc.,Perkin Trans. 1, 1995, 239.
179 C. Iwamoto, T. Yamada, Y. Ito, K. Monoura and A. Numata,
Tetrahedron, 2001, 57, 2997.
180 G. F. Bills, Can. J. Bot., 1995, 73s1, 33.
181 K. F. Nielsen, T. O. Larsen and J. C. Frisvad, J. Antibiot., 2004, 57,
29.
182 A. L. Demain, Int. Microbiol., 1998, 1, 259.
183 H. B. Bode, B. Bethe, R. Höfs and A. Zeeck, ChemBioChem, 2002,
3, 619.
184 K. F. Nielsen, J. Smedsgaard, T. O. Larsen, F. Lund, U. Thrane
and J. C. Frisvad, in Fungal Biotechnology in Agricultural, Food, and
Environmental Applications, ed. D. K. Arora, New York, Marcel
Dekker, 2003, p. 19.
185 J. Jennessen, K. F. Nielsen, J. Houbraken, J. Schnürer, E. K. Lyhne,
J. C. Frisvad and R. A. Samson, J. Agric. Food Chem., 2005, 53,
1833.
186 D. Wild, G. Toth and H. U. Humpf, J. Agric. Food Chem., 2002, 50,
3999.
187 B. B. Jarvis, in Mycotoxins and Phytoalexins, ed. R. P. Sharma and
D. K. Salunkhe, CRC Press, Boca Raton, 1990, 361.
188 C. W. Hesseltine, Process Biochem. (Oxford, U. K.), 1977, 12, 29.
189 C. W. Hesseltine, Process Biochem. (Oxford, U. K.), 1997, 32, 24.
190 C. W. Hesseltine, J. Ind. Microbiol. Biotechnol., 1999, 22, 482.
191 D. P. Overy and J. W. Blunt, J. Nat. Prod., 2004, 67, 1850.
192 D. P. Overy, C. H. Zidorn, B. O. Petersen, J. Ø. Duus, P. W.
Dalsgaard, T. O. Larsen and R. K. Phipps, Tetrahedron Lett., 2005,
46, 3225.
193 D. R. Lauren, A. Ashley, B. A. Blackwell, R. Greenhalgh, J. D.
Miller and G. A. Neish, J. Agric. Food Chem., 1987, 35, 884.
194 G. A. Cordell, Phytochemistry, 2000, 55, 463.
195 J. Bérdy, J. Antibiot., 2005, 58, 1.
196 M. E. Hansen, F. Lund and J. M. Carstensen, J. Microbiol. Methods,
2003, 52, 221.
197 R. D. Firn and C. G. Jones, Mol. Microbiol., 2000, 37, 989.
198 S. A. S. Mapari, K. F. Nielsen, T. O. Larsen, J. C. Frisvad, A. S.
Meyer and U. Thrane, Curr. Opin. Biotechnol., 2005, 16, 1.
199 G. A. Cordell and Y. G. Shin, Pure Appl. Chem., 1999, 71, 1089.
200 T. Dörge, J. M. Carstensen and J. C. Frisvad, J. Microbiol. Methods,
2000, 41, 121.
201 M. E. Hansen and J. M. Carstensen, Pattern Recognition, 2004, 37,
2155.
202 M. Sonka, V. Hlavac and R. Boyle, in Image Processing, Analysis
and Machine Vision, 2nd ed., Chapman & Hall, California, 1998.
203 M. S. Landy and N. Graham, The Visual Neurosciences, 2004, 1106.
204 B. Andersen, M. E. Hansen and J. Smedsgaard, Phytopathology,
2005, 95, 1021.
205 O. Fiehn, Comp. Funct. Genomics, 2001, 2, 155.
206 L. W. Sumner, P. Mendes and R. A. Dixon, Phytochemistry, 2003,
62, 817.
207 J. Smedsgaard and J. C. Frisvad, J. Microbiol. Methods, 1996, 25, 5.
208 G. P. Pierens, M. E. Palframan, C. J. Tranter and A. R. Carrol,
Magn. Reson. Chem., 2005, 43, 359.
209 P. Krishnan, N. J. Kruger and R. G. Ratcliffe, J. Exp. Bot., 2005,
56, 255.
210 J. Smedsgaard, J. Chromatogr., A, 1997, 760, 264.
211 O. Filtenborg and J. C. Frisvad, Lebensm. Wiss. Technol., 1980, 13,
128.
212 O. Filtenborg, J. C. Frisvad and A. Svendsen, Appl. Environ.
Microbiol., 1983, 45, 581.
213 K. Singh, J. C. Frisvad, U. Thrane and S. B. Mathur, in An Illustrated
Manual on Identification of Some Seed-borne Aspergilli, Fusaria,
Penicillia and their Mycotoxins, Danish Government Institute of
Seed Pathology for The Developing Countries, Denmark, 1991.
214 R. K. Julian, Jr., R. E. Higgs, J. D. Gygi and M. D. Hilton, Anal.
Chem., 1998, 70, 3249.
215 R. E. Higgs, J. A. Zahn, J. D. Gygi and M. D. Hilton, Appl. Environ.
Microbiol., 2001, 67, 371.
216 J. Smedsgaard, Biochem. Syst. Ecol., 1997, 25, 65.
217 M. E. Hansen and J. Smedsgaard, J. Am. Soc. Mass Spectrom.,
2004, 15, 1173.
218 J. Smedsgaard, M. E. Hansen and J. C. Frisvad, Stud. Mycol., 2004,
49, 243.
219 J. Smedsgaard and J. C. Frisvad, Biochem. Syst. Ecol., 1997, 25, 51.
220 H. L. Constant and C. W. Beecher, Nat. Prod. Lett., 1995, 6, 193.
221 D. G. Corley and R. C. Durley, J. Nat. Prod., 1994, 57, 1484.
222 N. Shingematsu, J. Mass Spectrom. Soc. Jpn., 1997, 45, 295.
223 P. Waridel, K. Ndjoko, K. R. Hobby, H. J. Major and K.
Hostettmann, Analysis, 2000, 28, 895.
224 G. R. Eldridge, H. C. Vervoort, C. M. Lee, P. A. Cremin, C. T.
Williams, S. M. Hart, M. G. Goering, M. O’Niel-Johnson and L.
Zeng, Anal. Chem., 2002, 74, 3963.
225 K. F. Nielsen and J. Smedsgaard, J. Chromatogr., A, 2003, 1002,
111.
226 A. Fredenhagen, C. Derrien and E. Gassmann, J. Nat. Prod., 2005,
68, 385.
227 F. VanMiddlesworth and R. J. P. Cannall, in Methods in Biotechnology, Vol 4: Natural Products Isolation, ed. R. J. P. Cannall, Humana
Press Inc., Totowa, NJ, 1998, p. 1.
228 C. P. Wang and T. L. Isenhour, Anal. Chem., 1987, 59, 649.
229 A. J. Round, M. I. Aguilar and T. W. Hearn, J. Chromatogr., A,
1994, 661, 61.
230 D. Bylund, R. Danielsson, G. Malmquist and K. E. Markides,
J. Chromatogr., A., 2002, 961, 237.
231 G. Malmquist and R. Danielsson, J. Chromatogr., A., 1994, 687, 81.
232 N.-P. V. Nielsen, J. M. Carstensen and J. Smedsgaard, J. Chromatogr., A., 1998, 805, 17.
233 N.-P. V. Nielsen, J. Smedsgaard and J. C. Frisvad, Anal. Chem.,
1999, 71, 727.
234 V. Pravdova, B. Walczak and D. L. Massart, Anal. Chim. Acta, 2002,
456, 77.
235 M. E. Hansen, J. Smedsgaard and T. O. Larsen, Anal. Chem., 2005,
77, 6805.
236 P. H. C. Eilers, Anal. Chem., 2003, 75, 3631.
237 J. C. Frisvad and U. Thrane, J. Chromatogr., 1987, 404, 195.
238 H.-P. Fiedler, Nat. Prod. Lett., 1993, 2, 119.
239 H.-P. Fiedler, C. Bruntner, A. T. Bull, A. C. Ward, M. Goodfellow,
O. Potterat, C. Puder and G. Mihm, Antonie van Leeuwenhoek, 2005,
87, 37.
240 T. O. Larsen, K. Frydenvang, J. C. Frisvad and C. Christophersen,
J. Nat. Prod., 1998, 61, 1154.
241 T. O. Larsen, H. Franzyk and S. R. Jensen, J. Nat. Prod., 1999, 62,
1578.
242 T. O. Larsen, K. Frydenvang and J. C. Frisvad, Biochem. Syst. Ecol.,
2000, 28, 881.
243 T. O. Larsen, B. O. Petersen, D. Sørensen, J. Ø. Duus, J. C. Frisvad
and M. E. Hansen, J. Nat. Prod., 2005, 68, 871.
244 S. C. Bobzin, S. Yang and T. P. Kasten, J. Chromatogr., B, 748,
259.
245 O. Corcoran and M. Spraul, Drug Discovery Today, 2003, 8,
624.
246 S. H. Hansen, A. G. Jensen, C. Cornett, I. Bjørnsdottir, S. Taylor,
B. Wright and I. D. Wilson, Anal. Chem., 1999, 71, 5235.
247 L. Wolfender, S. Rodriguez and K. Hostettman, J. Chromatogr., A,
1998, 794, 299.
248 C. Steinbeck, Nat. Prod. Rep., 2004, 21, 512.
249 M. E. Elyashberg, K. A. Blinov, A. J. Williams, E. R. Martirosian
and S. G. Molodtsov, J. Nat. Prod., 2002, 65, 693–703.
250 W. El-Deredy, NMR Biomed., 1997, 10, 99.
251 J. C. Lindon, E. Holmes and J. K. Nicholson, Prog. Nucl. Magn.
Reson. Spectrosc., 2001, 39, 1.
Nat. Prod. Rep., 2005, 22, 672–695
695