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Structural biology of DNA photolyases and cryptochromesMarkus Muller and Thomas Carell
Photolyases repair cytotoxic and mutagenic UV-induced
photolesions in DNA by using an amazing light-dependent
repair mechanism. It involves light absorption, electron transfer
from an excited reduced and deprotonated FADH� to the
flipped-out photolesion, followed by the fragmentation of the
photolesions. Cryptochromes are highly related proteins that
no longer repair damaged DNA, but function as
photoreceptors. They feature strikingly similar protein
architectures to photolyases and contain an FAD cofactor as
well. However, cryptochromes possess an additional signal-
transmitting domain, attached either to the N-termini or C-
termini. Recently, the field of photorepair and blue-light
photoperception has experienced significant progress
particularly in structural biology, which is summarized in this
review. Today, crystal structures of many family members are
known and most recently even complexes of photolyases and
DASH-type cryptochrome bound to their DNA substrates
became available providing insight into the critical electron and
energy transfer reactions that enable genome repair.
AddressCenter for Integrated Protein Science CiPSM at the Department of
Chemistry and Biochemistry, Ludwig-Maximilians University Munich,
Butenandtstr. 5-13, D-81377 Munich, Germany
Corresponding author:
Carell, Thomas ([email protected])
Current Opinion in Structural Biology 2009, 19:277–285
This review comes from a themed issue on
Nucleic acids
Edited by Eric Westhof and Dinshaw J Patel
Available online 30th May 2009
0959-440X/$ – see front matter
Published by Elsevier Ltd.
DOI 10.1016/j.sbi.2009.05.003
IntroductionEarly research of DNA repair started with the observation
that bacteria treated with UV-light showed a higher
survival rate after a second irradiation step with blue
light. This enigmatic photoreactivation process was soon
correlated with the function of DNA photolyases [1],
which utilize blue light to clean the bacterial genome
from UV-induced lethal lesions. The field of the photo-
lyase/cryptochrome family has been summarized in a
number of excellent reviews [2��,3]. Here we cover the
most recent advances in the structural biology of photo-
lyases and cryptochromes. Today, DNA photolyases are
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considered to be ancient DNA repair proteins, which
helped already the first living organisms exposed to sun-
light to survive. Upon using a light-induced repair reac-
tion, photolyases revert cyclobutane–pyrimidine-dimers
(CPD) and so-called (6-4) pyrimidine–pyrimidone photo-
lesions inside DNA back into undamaged pyrimidine–pyrimidine dinucleotides. As such they are essential for
genome maintenance in many species. From these photo-
lyases a special class of blue-light photoreceptors evolved,
the so-called cryptochromes. These proteins have lost
their ability to repair photolesions, but act in photoper-
ception and signal transduction of blue light in a broad
range of organisms. In plants, cryptochromes control for
example hypocotyl growth and the transition to flowering
[4]. In mammals, they are central components of the
circadian clock [5]. In birds, cryptochromes are even
supposed to be component of the magnetoperception
system [6,7]. The main difference between photolyases
and cryptochromes is the presence of C-terminal or N-
terminal extensions in cryptochromes that mediate the
signal transduction step. Until today, however, these
extension domains remained inaccessible to structural
analysis so that any information about their mechanism
of function is lacking. Only the short N-terminal exten-
sion of Arabidopsis Cry3 (AtCry3) was structurally charac-
terized, but its function in signal transduction is yet
unknown. However, crystallographic data are available
for the photolyase-like domain of AtCry1.
Evolution of the photolyase/cryptochromefamilyDespite the presence of photolyase and cryptochrome
genes in organisms belonging to all three kingdoms of life
(archaea, bacteria, and eukarya), the evolutionary con-
nections (Figure 1) of the individual members of this
unique protein family are still discussed controversially.
Today, it is widely accepted that the common ancestor
was likely a CPD-photolyase. This protein subdivided
into the today known class I (yellow in Figure 1), class II,
and the recently identified class III subfamilies (not
shown), of which the plant cryptochromes evolved
(green) [8]. The (6-4) photolyases (orange) and the closely
related animal cryptochromes (purple) represent another
distinct branch. In 2003 Brudler et al. [9�] described a new
class of cryptochromes named cryptochrome-DASH
proteins (DASH = Drosophila, Arabidopsis, Synechocys-
tis, Homo, shown in blue). On the basis of sequence
alignment, they grouped these proteins together with
the animal cryptochromes and (6-4) photolyases. How-
ever, Kleine et al. [10] proposed that the plant Cry-DASH
protein named AtCry3 originated from ancient cyanobac-
teria (chloroplasts) while AtCry1/2 were derived from
Current Opinion in Structural Biology 2009, 19:277–285
278 Nucleic acids
Figure 1
Phylogenetic tree of representative members of the cryptochrome/photolyase family, calculated with ClustalX [47]. Organisms with structures available
are listed at their respective position in the tree. The class II and III photolyases were omitted from the tree to provide better clarity. Surrounding:
substrate-bound structures of photolyase/cryptochrome proteins 1TEZ, 2VTB, 3CVU, and 1U3D. The N-terminal extension of AtCry3 is colored in
orange.
a-proteobacteria (mitochondrial). Recent data show now
that the DASH cryptochromes are single-strand-specific
CPD-photolyases [11,12�], which currently shift our per-
ception of these proteins.
Common structural featuresToday, several crystal structures of photolyase and cryp-
tochrome proteins are available. The first crystal struc-
tures obtained in 1995 [13��] and 1997 [14] showed the
CPD-photolyases from Escherichia coli and Anacystis nidu-lans. Both structures revealed the three-dimensional
architecture of these DNA repair proteins in the absence
of the respective DNA substrates. This left the question
of how the electron transfer occurs initially open. How-
ever, the structures showed that the proteins possess a
rather globular structure, uncommon to most DNA bind-
ing proteins. Both structures display the same domain
architecture with an N-terminal a/b domain and a C-
terminal a-helical domain. These photolyases contained
two cofactors. The a-helical domain is harboring the
flavin-adenine-dinucleotide (FAD) cofactor, essential
Current Opinion in Structural Biology 2009, 19:277–285
for catalysis. The second cofactor, which is either an 8-
hydroxy-5-deazariboflavin (8-HDF) or 5,10-methenylte-
trahydrofolate (MTHF), is always bound at the interface
between these two domains, about 9 A away from the
FAD as shown in Figure 2b.
In 2004 the first cocrystal structure of a CPD-photolyase
from A. nidulans in complex with a DNA-duplex contain-
ing a synthetic CPD lesion analog was reported [15��],showing that the protein fold changed only marginally
upon DNA binding. The structure proved that CPD-
photolyase proteins fully open the DNA-duplex structure
at the damaged site and flip the dinucleotide lesion out of
the duplex into the active site. Here the lesion comes in
close contact (3 A) with the active FADH� cofactor. Until
today, photolyases are the only proteins, which are able to
perform such a dramatic dinucleotide flip-out.
The first crystal structures of the photolyase-like domains
of bacterial and plant cryptochromes [9,16,17,18�],reported between 2003 and 2007, revealed a surprising
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DNA photolyases and cryptochromes Muller and Carell 279
Figure 2
(a) Schematic representation of the photoreactivation process. Oxidized FAD is reduced to FADH� in a light-dependent process called photoactivation
that involves electron transfer toward FAD from conserved tryptophane and tyrosine residues. Absorbed light energy is transferred from the accessory
pigments to FADH� by Forster-energy-transfer (FRET), enabling electron transfer and splitting of the CPD-lesion or (6-4)-lesion. (b) Superimposed
electron-transfer and energy-transfer paths in Anacystis nidulans CPD-photolyase (green) and Drosophila melanogaster (6-4) photolyase (red, from
[40]). The numbering is according to Anacystis PHR.
homologous fold topology between all these proteins.
The basic folds of these domains and of CPD-photolyases
are about the same. Most recently, the first crystal struc-
ture of a (6-4) photolyase bound to a DNA-duplex con-
taining a synthetic (6-4) lesion substrate [19�] was
obtained and again the observed protein architecture
was found to be the same. This observation now extends
even to the structure of the Arabidopsis cryptochrome 3 in
complex with a single-stranded DNA strand containing
the same synthetic CPD lesion analog [11]. The structure
of an animal cryptochrome remains yet to be solved but
one can suspect that the structure will be similar as well.
Despite a high level of sequence diversity (41.9% sim-
ilarity, 5.6% identities), the topological similarity be-
tween all photolyase and cryptochrome structures
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known today is one of the most surprising discoveries.
The total rmsd (root mean square deviation) for 9 struc-
tures with varying sequences (Table 1) is only 1.914 A
over 369 residues as calculated with SSM (http://www.e-
bi.ac.uk/msd-srv/ssm) [20]. It seems that all these proteins
utilize similar energy and electron transfer steps which,
owing to the sensitivity of these processes to distance and
orientation changes, force the proteins to keep a common
fold in order to ensure an optimal arrangement of the
essential cofactors [21,22] (Figure 2b).
For photolyases it is known that they utilize the FAD
cofactor in the reduced and deprotonated form (FADH�)
as an electron donating entity (Figure 2a). It is today
believed that the reduction of FAD to FADH� is the first
Current Opinion in Structural Biology 2009, 19:277–285
280 Nucleic acids
Table 1
A list of all to this date available photolyase and cryptochrome structures
Protein Organism PDB-ID Secondary cofactor Substrate Reference
CPD-Phr Escherichia coli 1DNP MTHF None [13��]
CPD-Phr Anacystis nidulans 1QNF 8-HDF None [14]
1TEZ 8-HDF T< >T [15��]
1OWL, 1OWM, 1OWN, 1OWO, 1OWP None None [45]
CPD-Phr Thermus thermophilus 1IQR, 1IQU None Thymine [46]
2J07, 2J08, 2J09 FMN, 8-HDF, 8-IRF None [38]
CPD-Phr Sulfolobus tokodaii 2E0I FAD None [39]
(6-4)-Phr Drosophila melanogaster 3CVU, 3CVY None T(6-4)T [19�]
3CVV, 3CVW, 3CVX 8-HDF, none T(6-4)T [40]
(6-4)-Phr Arabidopsis thaliana 3FY4 None None [37]
Cry1 Arabidopsis thaliana 1U3C, 1U3D None AMP-PNP [18�]
Cry-DASH Synechocystis spp. 1NP7 None None [9�]
Cry3 Arabidopsis thaliana 2IJG MTHF None [17]
2J4D MTHF None [16]
2VTB MTHF T< >T [11]
The rmsd of the nine structures with varying sequences is 1.914 A (1DNP, 1QNF, 1IQR, 2E0I, 3CVU, 3FY4, 1U3C, 1NP4, and 2IJG) as calculated with
SSM [20]. Phr, photolyase (photorepair); MTHF, 5,10-methenyltetrahydrofolate; 8-HDF, 8-hydroxy-5-deazariboflavin; 8-IRF, 8-iodo-8-demethyl-
riboflavin; FMN, flavin-mononucleotide; FAD, flavin-adenine-dinucleotide; T< >T, cyclobutane–pyrimidine-dimer-containing DNA; T(6-4)T, (6-4)
pyrimidine–pyrimidone-dimer containing DNA; AMP-PNP, adenosine 50-(b,g-imido)triphosphate.
required photochemical step (photoactivation). Initial
photoexcitation of FAD is supposed to trigger sequential
electron donations from three conserved tryptophanes
[23] and an additional tyrosine residue in Anacystis photo-
lyase [24], followed by a proton uptake. The tryptophane
cascade needed for FAD reduction is present in all
available photolyase/cryptochrome structures, listed in
Table 1. Next, the repair process involves absorption
of light by the MTHF/8-HDF antenna chromophores,
followed by energy transfer from the excited antenna
pigments to the FADH� and finally electron transfer to
the CPD or (6-4) lesion. The lesion then splits back into a
dipyrimidine dinucleotide as depicted in Figure 2a. The
electron-transport chain of AtCry1, like in Anacystis photo-
lyase, involves a Tyr residue as initial electron donor.
However, the active signaling state of the cryptochromes
was shown to be the semireduced FADH� [25]. Very
recently, comparative redox titrations of photolyase and
Cry1 have shown remarkable differences in the FAD
redox potential, favoring light-induced transitions be-
tween FADox and FADH� in Cry1 as compared to
FADH� to FADH� transitions in photolyase [26]. These
differences were attributed to an asparagine residue (Asn-
386) in the active site of E. coli photolyase, which is
replaced by Asp-396 in Cry1.
DNA bindingAlthough efficient lesion specific but sequence-indepen-
dent DNA binding was early on established for CPD and
(6-4) photolyases, the DNA binding characteristics of
cryptochromes remain to be enigmatic. Photolyases
invade the duplex and flip the lesion out of the duplex
into a rather hydrophobic lesion binding pocket. This
pocket features aromatic Trp residues, which pack
against the lesion holding it in the flipped-out state by
using p–p interactions. A large set of H-bonds established
Current Opinion in Structural Biology 2009, 19:277–285
to the Watson–Crick H-bond donors and acceptors of the
lesions provide additional binding energy to stabilize the
energetically highly unfavored flipped-out state. The gap
created in the duplex after the dinucleotide flip-out is
stabilized by amino acids G397-F406 in Anacystis CPD-
photolyase, which invade the duplex.
The fact that the cryptochrome proteins originate from
DNA repair proteins fueled the idea that they might bind
DNA as well, for example as light-triggered transcription
factors. For Cry-DASH and Arabidopsis Cry3, weak but
unspecific DNA binding was indeed observed [9�,10].
However, for Arabidopsis Cry1, DNA binding could not
be detected. Human Cry2 protein was shown binding to
ssDNA with high affinity (KD �5 � 10�9). Binding to
ssDNA containing a (6-4) photolesion is even better [27�].Yet, the protein is unable to repair the (6-4) lesions, which
is surprising, taking into account that (6-4) photolyases
and mammalian cryptochromes are closely related.
Photolyases exhibit a positively charged surface near the
substrate-binding pocket which promotes interactions
with DNA (Figure 3). All photolyases share these posi-
tively charged DNA binding surfaces. Cry1 from Arabi-dopsis thaliana, which does not bind to DNA, possesses a
strongly reduced surface charge around the FAD binding
pocket. However, Arabidopsis Cry3 features an even
more pronounced positive charge density at the putative
DNA binding site compared to the CPD-photolyase from
E. coli, but it binds DNA only weakly [10]. In addition,
AtCry2, whose modeled surface largely resembles that of
AtCry1, does bind to DNA (Alfred Batschauer, unpub-
lished results [49]). DNA binding was also firmly estab-
lished for AtCry3. Figure 3 shows surface charges
calculated with APBS [28] for several members of the
photolyase/cryptochrome family. The structures of
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DNA photolyases and cryptochromes Muller and Carell 281
Figure 3
Surface-charge representation of various photolyase/cryptochrome proteins calculated with APBS and visualized with PyMOL. All views face the FAD-
binding cavity. The following data-files were used: AtCry1 — 1U3D, AtCry3 — 2VTB, AnCPD-PHR — 1TEZ, Dm(6-4)-PHR — 3CVU. AtCry2 and hCRY1
were modeled in First Approach Mode on the SWISS-MODEL server [29] from 1U3C and 3CVU, respectively.
Arabidopsis Cry2 and human Cry1 were generated in silicoon the Swiss Modeling Server [29] in First Approach modefrom Arabidopsis Cry1 and Drosophila (6-4) photolyase
structures, respectively (rmsd 0.23 A and 0.31 A). In
summary it is now clear that the surface charge alone
is not a sufficient determinant for DNA binding. Huang
et al. [17] proposed that the (di)nucleotide flip-out is the
key step in DNA recognition. They evaluated the
physical properties of residues comprising the putative
substrate binding cavity. While photolyases share a con-
served hydrophobic cavity able to accommodate the
lesions, this cavity contains more charged residues in
Cry3. The authors argue that these charges destabilize
the putative substrate in the ‘flipped-out’ conformation
thus preventing efficient dsDNA binding. These results
were confirmed experimentally by Pokorny et al. [11],
showing that AtCry3 does repair CPDs when the lesion is
located in a preflipped out state such as in bulges of
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dsDNA. Taken together, the data suggest that positive
surface charges promote unspecific DNA binding while
tight binding requires a kind of base flip and nucleotide
binding in a properly hydrophobic/aromatic binding
pocket.
Mechanism of functionThe key element of the photolyase repair mechanism
depicted in Figure 2a is the electron transfer from the
excited FADH� to either the CPD or (6-4) lesion. This
induces in both cases a fragmentation reaction. The active
sites of all crystallized photolyases with their interacting
residues and substrates are shown in Figure 4c–e. For CPD
lesions it is known that the single electron reduced cyclo-
butane ring undergoes a thermally forbidden (Woodward–Hoffmann) [2 + 2] cycloreversion reaction followed by
back transfer of the ‘enabling electron’ to the semireduced
FADH�. In (6-4) photolyases, the fragmentation reaction is
Current Opinion in Structural Biology 2009, 19:277–285
282 Nucleic acids
Figure 4
(a) Proposed reaction mechanism of (6-4) photolyase, based on prerepair and postrepair crystal structures, taken from [19�]. (b) Superposition of
bound substrates in CPD-photolyase (1TEZ, gray) and Arabidopsis Cry1 (1U3D, green). (c) The catalytic site of Anacystis nidulans CPD-PHR, (d)
Drosophila melanogaster (6-4)-PHR and (e) Arabidopsis thaliana Cry3. Interacting residues as calculated with Ligplot [48] are shown in gray, the
photolesion in green and the catalytic FAD in pink. Hydrogen bonds are shown as dashed lines. Note that AtCry3 (e) is shown reversed as compared to
the other structures, for better visibility.
less clear, because repair requires cleavage of one C–C
bond and transfer of a hydroxyl group from the dihydro-
pyrimidine to the pyrimidone ring. Until recently it was
believed that the enzyme stabilizes an oxetane intermedi-
ate, formed after a light-independent reaction of the
C(5)OH group with the acylimine substructure of the
second ring [30]. Two active site histidines were postulated
to promote this reaction [31]. The first was thought to be
involved in deprotonating the hydroxyl group, while the
second was believed to activate the acylimine. This oxe-
tane intermediate was supposed to be cleaved by light-
induced electron injection very similar to the CPD-photo-
lyase catalyzed cycloreversion of a cyclobutane structure.
Two crystal structures of the (6-4) photolyase from Droso-phila bound to lesion containing DNA before and after
repair showed that repair does not involve oxetane for-
mation before light-induced electron transfer. The histi-
dine 369, supposed to activate the acylimine, is in a position
that does not allow efficient proton donation and hence
activation of this substructure [19�] (see Figure 4d). In
addition, Weber and collaborators showed, using ENDOR
Current Opinion in Structural Biology 2009, 19:277–285
spectroscopy, that the second histidine residue originally
believed to deprotonate the lesion’s hydroxyl group is
likely in the protonated state, functioning as a general acid
[32]. In this scenario, His-365 would be unable to depro-
tonate the C5-hydroxyl group. On the basis of these
observations we proposed recently a slightly modified
reaction mechanism, which involves direct electron
donation to the (6-4) lesion followed by cleavage of the
C–OH bond (Figure 4a). Attack of the acylimine is fol-
lowed by the activated OH group to give a radical inter-
mediate, which can rapidly fragment to give the repaired
TT dinucleotide.
In the case of the cryptochromes, the mechanism of action
remains unclear. It was clearly demonstrated that the C-
terminal extensions mediate a constitutive blue-light
response when expressed separatly from the photo-
lyase-like domain [33]. The Sancar group showed that
the mainly disordered C-terminal extension of AtCry1
interacts light-specifically with its photolyase-like domain
[34]. Further, it was demonstrated that AtCry1 undergoes
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DNA photolyases and cryptochromes Muller and Carell 283
autophosphorylation after light absorption [35] and its
crystal structure is showing a bound ATP analog at the
active site [18�]. Together, these observations make a
light-dependent conformational switching mechanism
appear plausible. However, whether or not the AMP-
PNP was bound specifically or represents a crystallo-
graphic artifact is not clear. The nucleoside triphosphate
analog is positioned differently compared to the dimer-
lesion in photolyases, with the ribose ring facing the FAD
binding pocket (Figure 4b). Nevertheless, the position
and function of substrate-contacting residues is similar. It
was hypothesized that binding of ATP blocks access to
the FAD-binding site and thus inhibits electron transfer.
AtCry3 contains all required motifs of a cryptochrome-
signal transducing domain [16,36]. However, the N-term-
inal extension in AtCry3 is positioned so far away from the
active site (Figure 1), hence providing no evidence to
support the theory of a light-dependent conformational
change. The latest addition to the family of photolyase
structures is giving rise to new ideas about the signal
transduction of mammalian cryptochromes. In the struc-
ture of Arabidopsis thaliana (6-4) photolyase, a phosphate
anion was found bound to Glu-243 and Trp-238, close to
FAD. Phosphorylation of a serine found at the same
position in the model of human Cry1 was shown to
modulate its function [37].
The light antennaDespite the overall structural similarity of photolyases
and cryptochromes, a few elements are different. Most
important are different binding-modes of the MTHF in
photolyases and Cry-DASH proteins. Between AtCry3
and E. coli CPD-photolyase, only a single glutamic acid
residue is conserved for MTHF binding [16], but still the
overall structural arrangement is very similar. The photo-
lyase from Thermus thermophilus can bind next to the
natural cofactor 8-HDF also FMN. It is unclear if this
is physiologically relevant. But seemingly, its binding
pocket is more promiscuous than those of other proteins
belonging to this family. Even the synthetic 8-iodoflavin
was found in the photoantenna pocket when crystals were
soaked with this compound [38]. In Sulfolobus tokodaii, a
second FAD molecule was also found in the antenna
pigment binding pocket [39]. The (6-4) photolyase from
Drosophila melanogaster is unexpectedly binding 8-HDF
[40]. As this cofactor was previously believed to occur only
in archaea and cyanobacteria the observation of this
signature molecule for the archaeal world in a eukaryotic
protein came as a surprise. In AtCry1 and SynechocystisCry-DASH, a secondary cofactor was not yet found.
However, biochemical data suggest that MTHF func-
tions in these proteins as the light antenna [41,42].
ConclusionsFifteen years ago CPD-photolyases were considered to be
solitary proteins, which utilize a strange light-dependent
mechanism to clean the genomes of organisms from the
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lesions induced by UV irradiation. In 1958, Claud S.Rupert discovered the first photolyase [1]. In 1993 the
first (6-4) photolyase was found [43] and in the same year
the protein family grew even further by the discovery of
cryptochromes [44]. Cryptochromes and photolyases now
form a family of proteins that absorb blue light to drive
DNA repair and control various biological processes.
Using protein crystallography it was possible to gain
insight into the structures of these proteins and to charac-
terize the DNA binding mode, which revealed for the first
time a dinucleotide flip-out process. Although the mech-
anism of action of CPD and (6-4) photolyases is now well
established, the process allowing cryptochromes to trigger
circadian rhythms and to fuel signaling cascades by blue-
light absorption remains an open question.
AcknowledgementsWe thank the Excellence Cluster CiPSM and the Sonderforschungsbereich749 for generous financial support. Many thanks to Sabine Schneider andAndreas Glas for the help with the figures and critical reading of themanuscript. All structural figures were prepared with PyMol (DeLanoScientific).
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� of special interest
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