Nano Today (2015) 10, 631—655
Available
online at www.sciencedirect.com
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j ournal homepage: www.elsevier.com/locate/nanotoday
REVIEW
RNA as a stable polymer to build
controllable and defined nanostructures for
material and biomedical applications
a a,b c a
Hui Li , Taek Lee , Thomas Dziubla , Fengmei Pi ,
a,d e e a
Sijin Guo , Jing Xu , Chan Li , Farzin Haque ,
e a,∗
Xing-Jie Liang , Peixuan Guo
a
Nanobiotechnology Center, Markey Cancer Center, and Department of Pharmaceutical Sciences,
University of Kentucky, Lexington, KY 40536, USA
b
Department of Chemical and Biomolecular Engineering, Sogang University, Seoul, Republic of Korea
c
Department of Chemical and Materials Engineering, University of Kentucky, Lexington, KY 40506, USA
d
Department of Chemistry, University of Kentucky, Lexington, KY 40506, USA
e
Laboratory of Nanomedicine and Nanosafety, CAS Key Laboratory for Biomedical Effects of Nanomaterials
and Nanosafety, National Center for Nanoscience and Technology of China, Beijing 100190, China
Received 14 July 2015; received in revised form 9 September 2015; accepted 14 September 2015
Available online 26 October 2015
KEYWORDS Summary The value of polymers is manifested in their vital use as building blocks in mate-
Biopolymer; rial and life sciences. Ribonucleic acid (RNA) is a polynucleic acid, but its polymeric nature
in materials and technological applications is often overlooked due to an impression that RNA
RNA nanotechnology;
is seemingly unstable. Recent findings that certain modifications can make RNA resistant to
RNA nanostructure;
RNase degradation while retaining its authentic folding property and biological function, and
RNA therapeutics;
the discovery of ultra-thermostable RNA motifs have adequately addressed the concerns of RNA
phi29 DNA packaging
motor; unstability. RNA can serve as a unique polymeric material to build varieties of nanostructures
pRNA including nanoparticles, polygons, arrays, bundles, membrane, and microsponges that have
potential applications in biomedical and material sciences. Since 2005, more than a thousand
publications on RNA nanostructures have been published in diverse fields, indicating a remark-
able increase of interest in the emerging field of RNA nanotechnology. In this review, we aim
to: delineate the physical and chemical properties of polymers that can be applied to RNA;
introduce the unique properties of RNA as a polymer; review the current methods for the con-
struction of RNA nanostructures; describe its applications in material, biomedical and computer
sciences; and, discuss the challenges and future prospects in this field.
© 2015 The Authors. Published by Elsevier Ltd. This is an open access article under the CC
BY-NC-ND license (http://creativecommons.org/licenses/by-nc-nd/4.0/).
∗
Corresponding author. Tel.: +1 859 218 0128; fax: +1 859 257 1307.
E-mail address: [email protected] (P. Guo).
http://dx.doi.org/10.1016/j.nantod.2015.09.003
1748-0132/© 2015 The Authors. Published by Elsevier Ltd. This is an open access article under the CC BY-NC-ND license (http://creativecommons.org/licenses/by-nc-nd/4.0/).
632 H. Li et al.
Introduction chemical diversity offer a rich repertoire of available prop-
erties from which one can custom-design a polymer for a
desired application.
Polymers have been extensively used by humans since the
Biological macromolecules, as natural building blocks,
earliest recorded history. Tree saps, tar and plant fibers, all
are critical for the functioning of living organisms. RNA is
represent the earliest natural polymeric materials used by
one of the five most important biological macromolecules
humans [1].
in addition to DNA, proteins, lipids and carbohydrates.
Since the 1950s, through continued synthesis and
With some aspects similar to DNA, RNA, composed of four
manufacturing improvements, synthetic polymers have dra-
nucleotides including adenosine (A), cytosine (C), guanosine
matically improved in quality and strength to the point
(G) and uridine (U), is special in its homogeneity. RNA is
where they, in many cases, can have mechanical properties
a homopolymer of nucleotide, but is also a heteropolymer
that better match desired use, as compared to alternative
of A, U, G, and C. Each nucleotide contains a ribose sugar,
natural counterparts. Synthetic polymers have the manufac-
a nucleobase, and a phosphate group. The nucleotides are
turing advantages of rapid production rates and synthetic
covalently linked together through 3 → 5 phosphodiester
simplicity. However, owing to the inherently random nature
bonds between adjacent ribose units, giving the direction-
of most polymerization mechanisms, chain polydispersity
ality to the sugar-phosphate backbone that defines RNA as
and controlled shaping remain two of the key limiting
a polynucleic acid. The phosphate moieties in the backbone
hurdles that have led to increased variable performance
are negatively charged, making RNA a polyanionic macro-
and overall reduced control of the final properties [2—4].
molecule at physiological pH. RNA molecules are typically
As such, there has been much effort towards develop-
single-stranded; however, Watson-Crick (canonical) base-
ing synthetic building blocks and schemes that can create
pair interactions (A:U and G:C), wobble base pairing (such
monodisperse polymer systems [5—7]. These, however, are
as G:U) [24] or other non-canonical base pairing such as
typically very expensive, time consuming and difficult to
control. twelve basic geometric families of edge-to-edge interac-
tion (Watson-Crick, Hoogsteen/CH or sugar edge) with the
As a result of these developments, we are at another
orientation of glycosidic bonds relative to the hydrogen
unique turning point in the evolution and design of polymers.
bonds (cis or trans) [25—28], all together give rise to various
We once again turn towards nature as our inspiration for the
structural conformations exhibiting loops, hairpins, bulges,
development of advanced biomaterials. By applying what we
stems, pseudoknots, junctions, etc., which are essential ele-
have learned about the complexity and versatility of nucleic
ments to guide and drive RNA molecules to assemble into
acid structures, it is now possible to create materials with
desired structures [12,29—31].
revolutionary properties previously considered unattainable
On the contrary, synthetic polymers are usually formed
through synthetic strategies. Recent advances in RNA chem-
via polymerization reaction, a chemical process through
istry, RNA biology and RNA nanotechnology have shown that
which many monomers form covalent bonds between each
RNA as a biopolymer not only shares the common character-
other and finally form a long chain or network, imparting
istics of other polymers, but also possesses a range of unique
them with their desired structural properties.
properties advantageous for applications in nanotechnology
Generally, the properties of polymers are strongly
as well as biomedical and material sciences [8—14].
dependent on their monomer chemistry. Moreover, the
In this review, we will (1) delineate the physiochemical
molecular weight and 2D structure (e.g., linear chain-
properties of polymers that can be applied to RNA, (2) intro-
shaped structure or branch-shaped structure) also play
duce the unique properties of RNA as a polymer, (3) review
important roles in determining the characteristics and
the current methods for constructing RNA nanostructures for
properties of a specific polymer. Important properties of
diverse applications, and (4) discuss the future prospects
chemical polymers include [32]: (1) rheological properties,
including challenges, solutions and new directions of this
(2) solubility, (3) volumetric and viscometric properties,
nascent field.
(4) stress-strain relationships, (5) electrical properties, (6)
thermal properties, (7) optical properties, (8) stiffness, (9)
Physical and chemical properties of polymers
flex life, (10) hardness, (11) chemical resistance, etc. Vari-
in relationship to RNA nanotechnology ous physical or chemical tests can be readily performed to
characterize these properties for RNA polymers.
The word (poly)-(mer) means (many)-(parts) and refers to Traditional synthetic polymers are heterogeneous and
macromolecules consisting of a large number of repeating have typical polydispersity index greater than 1 [33,34].
elementary units covalently joined together. These ‘mers’ In contrast, RNA is synthesized by either in vitro tran-
control the inter-chain interactions, and dictate the final scription or solid phase chemistry. Both approaches are
polymer characteristics. Given the large variations in poly- based on stepwise reactions and will generate RNA poly-
mer morphologies, multiple ways are used to describe mers with defined sequences, structures, and molecular
polymer structure. Polymers can be formed from one type weights. This leads to a polydispersity index of 1 of a specific
of monomer (homopolymers) or of various monomers (het- RNA. Structurally, the average molecular weight deter-
eropolymers). Heteropolymers can be further described mines the mechanical property of the polymer. However,
by the arrangement of the monomers along the back- as polydispersity increases, the increased lower molecu-
bone, including alternating, random, and block formations lar weight chains can act as a lubricating/solvating system,
and also adopt more elaborate structures, including star, reducing its mechanical strength and integrity. As increases
ring, branched, dendrimeric, crosslinked, ladder, and oth- in temperature result in increased molecular motion,
ers [15—23]. These large arrays of potential structures and these weak associations begin to destabilize and reduce
RNA as a stable polymer 633
mechanical integrity. Such polymers are classically referred Thermodynamic stability of RNA
to as thermoplastics [35], as their mechanical strength
weakens with increased temperature. However, this prop- From a thermodynamic point of view, the stability of
erty also means they can be intentionally deformed at higher the double helix of RNA can be evaluated by measur-
0
temperatures and then regain their structural properties ing the Gibbs free energy (G ) required for double
once cooled. Thermodynamically, RNA molecule is relatively helix formation, or conversely, double helix unwinding
0 0 0
more stable at lower temperature and intends to dissoci- −
( G = G helix formation = G helix unwinding). Remarkably, the
ate or misfold at higher temperatures. Thus, RNA displays RNA double helix is more thermodynamically stable than the
0
the typical thermoplasticity of polymers. Boiling-resistant DNA double helix considering G for RNA double helix for-
RNA has been discovered and constructed [36], suggesting a mation is, on the average, −3.6 to −8.5 kJ/mol per base
0
potential application of RNA in molding technology. pair stacked and G for DNA double helix formation is
−
Chemical polymers have a wide range of applications 1.4 kJ/mol per base pair stacked [52]. Moreover, the pres-
in biomedical and material sciences. Specific applications ence of special motifs such as bends, stacks, junctions and
include, but not limited to [1,37—50]: (1) sutures for surgery, loops in the tertiary structure of RNA may also further
(2) dental devices, (3) orthopedic fixation devices, (4) scaf- improve its stability [8]. In addition, various proteins, such
2+
folds for tissue engineering, (5) drug formulation (e.g., as RNA chaperone proteins, and metal ions, such as Mg
controlled release of drugs, excipients for drug stabiliza- may also interact or coordinate with RNA and significantly
tion or solubilization), (6) biodegradable vascular stents, (7) contribute to the stability of RNA [53,54].
biodegradable soft tissue anchors, (8) implantable biomed-
ical devices, (9) flexible transparent displays, (10) field
effect transistors, (11) solar cell panels, (12) printing elec- Enzymatic stability of RNA
tronic circuits, (13) organic light-emitting diodes, (14)
supercapacitors, etc. Usually, an ideal chemical polymer In biological systems, the instability of RNA is mainly the
for biomedical and industrial applications should exhibit result of enzymatic degradation by ribonucleases (RNases).
the majority of the following properties: (1) non-toxic, (2) The presence of RNases in living organisms is universal,
no or low immunogenicity (if applicable, for in vivo use), suggesting that RNase-mediated RNA degradation is a vital
(3) biodegradable and metabolizable, (4) mechanical fea- process for normal biological function. Several important
tures that fit the needs of the specific application, (5) easily roles of RNases have been revealed, including degrading sur-
sterilizable, (6) processability, (7) scalability, (8) electrical plus cellular RNA [55,56], editing messenger RNA, processing
conductivity, and (9) thermostabilty. RNA as a polymer favor- microRNA and other non-coding RNA during their maturation
ably displays many of these properties, as described below. [57,58], defending against the invasion of viral RNA [59],
and providing crucial machinery for RNA interference (RNAi)
[60,61]. RNases can be divided into two major categories: (1)
endo-ribonucleases that cleave phosphodiester bonds within
Unique properties of RNA as a polymer to
the RNA backbone [62]. Examples include RNase A, RNase H,
build nanostructures
RNase I, RNase III, RNase L, RNase P, RNase PhyM, RNase T1,
RNase T2, RNase U2, RNase V, etc.; (2) exo-ribonucleases
The 2 -hydroxyl group makes RNA dramatically
that cleave phosphodiester bonds at either the 5 or the 3
different from DNA
end of an RNA chain [63]. Examples include polynucleotide
phosphorylase (PNPase), RNase PH, RNase II, RNase R, RNase
The characteristic of RNA that defines and differentiates it
D, RNase T, oligoribonuclease, exoribonuclease I, exoribonu-
from DNA is the 2 -hydroxyl on each ribose sugar of the back-
clease II, etc. RNA is indeed very sensitive to degradation by
bone. The 2 -OH group offers RNA a special property, which
RNases, which confers a very short half-life and thus a poor
can be either an advantage or a disadvantage. From a struc-
pharmacokinetic profile to most RNA molecules. This degra-
tural point of view, the advantage of this additional hydroxyl
dation limits the in vivo application of RNA molecules as
group is that it locks the ribose sugar into a 3 -endo chair
therapeutics. However, chemical modifications of RNA can
conformation. As a result, it is structurally favorable for the
overcome this shortcoming. For example, the substitution
RNA double helix to adopt the A-form which is ∼20% shorter
of the 2 hydroxyl group with a Fluorine (2 -F), O-methyl
and wider rather than the B-form that is typically present in
(2 -O-Me) or Amine (2 -NH2) dramatically increases the sta-
the DNA double helix. Moreover, the 2 -OH group in RNA is
bility of RNA in vivo by preventing degradation by RNases
chemically active and is able to initiate a nucleophilic attack
[64—66]. Recent studies also showed that the stability of
on the adjacent 3 phosphodiester bond in an S 2 reaction.
N siRNA in serum is also highly depended on the specific RNA
This cleaves the RNA sugar-phosphate backbone and this
sequences and the degradation of both short and long RNA
chemical mechanism underlies the basis of catalytic self-
duplexes mostly occurred at UA/UA or CA/UG sites [67].
cleavage observed in ribozymes [51]. The disadvantage is
Synthetic polymers always show good stability against
that the 2 -OH group makes the RNA susceptible to nuclease
various enzymes. However, biodegradable polymers that can
digestion since many RNases recognize the structure of RNAs
be degraded by enzymes such as proteases, oxidoreduc-
including the 2 -OH group as specific binding sites. However,
tases and phospholipases are more beneficial for therapeutic
such enzymatic instability has been overcome by applying
applications [68]. The nanocarriers composed of enzyme
chemical modification of the 2 -OH group (see the sections
sensitive polymers can control the site of cellular uptake
Enzymatic stability of RNA and Methodology II: Chemical
of carriers and drug release to improve the drug efficacy
modification of RNA).
[69—71]. Synthetic polymers can also be designed to be
634 H. Li et al.
◦ ◦ ◦
non-degradable or degradable under certain physiological phi29 DNA packaging motor from 60 to 90 to 108 to transit
conditions. For example, Poly(lactic-co-glycolic acid) (PLGA) from triangle, square, and pentagon structures, respectively
(which is generally regarded as safe) is approved by FDA, as [92].
it can be degraded in the body by hydrolysis and has now
been widely used to fabricate nanoparticles for drug deliv-
RNA can form complex 3D structures in nanoscale
ery. Poly (beta-amino ester) is another class of degradable
biomaterial developed by Langer group [72], which can bind
While most biologically active DNAs are double-stranded, in
negatively-charged RNA or DNA and facilitate gene trans-
contrast, most RNAs in living organisms are single-stranded.
fections. Although the biodegradable polymers are highly
However, RNA molecules contain self-complementary
attractive for drug delivery purposes, their degradation
sequences which facilitate the self-folding of these RNAs.
rate is very hard to control and the pharmacokinetics and
In addition to Watson-Crick base paring, non-Watson—Crick
biodistribution profiles of the nanocarriers can be elusive.
base pairs and coaxial stacking of helices also play important
Synthetic polymers usually are composed of repeated same
roles in promoting RNAs folding into complex 3D structures
subunit, while RNA is the repetition of four subunits A, U, G
[12,53]. This remarkable folding capability not only provides
and C in a specific sequence order. Therefore, RNA polymers
the structural basis for the diverse biochemical functions of
might be advantageous concerning controllable biodegrad-
different RNA molecules, but also provides huge opportuni-
ability [73,74] simply by tuning the ratio and location of
ties for designing novel RNA nanostructures. For example,
2 -modified nucleotides in the RNA sequence.
the subdomain IIa-1 RNA of the IRES from HCV has a unique
◦
90 bend L-shaped structure. Molecular modeling using this
L-shaped motif showed that a square shaped nanoparti-
The versatile and plastic properties of RNA
cle can be formed with four repeating L-shaped motifs, as
verified by gel shift assay and FRET assay [93] (Fig. 1I).
The versatility of RNA is highly evident given the diversity
Moreover, it has been found that proteins, small molecule
of structural repertoires available in nature, which include
ligands as well as monovalent and/or divalent metal ions
simple structures such as helical stems and single stranded
are also important mediators of RNA folding, which could
hairpin loops to more complicated structures such as multi-
add another layer of complexity to the assembly of RNA
way junctions and pseudoknots [75—84]. Persistence length
nanostructures [53].
is a basic mechanical property used in polymer science to
measure the flexibility and stiffness of a polymer. If a poly-
mer is shorter than the persistence length, the molecule will Toolkits and methodologies for the
basically be a rigid rod. From a mechanical perspective, the
construction of RNA nanostructures
persistence length of dsRNA (62—63 nm) is slightly longer
than dsDNA (45—50 nm) in an aqueous solution [85,86]. The
The diverse function of RNA molecules in cells such as
stretch modulus of short dsRNA (<150 bp) is ∼100 pN, which
ribozymes, riboswitches, microRNAs, long non-coding RNAs
is 3 times lower than dsDNA of similar length, is based on AFM
and aptamers had attracted increasing attention in the sci-
and tweezer studies [87]. Interestingly, RNA was observed to
entific community. All these properties of RNA originated
shorten upon twisting with two-orders of magnitude slower
from nature that RNA can adapt different structures and
timescale compared to DNA, which in contrast lengthened
spatial conformations. The laws of how nature manipulates
with a faster timescale. More recently, single molecule force
RNA structures can also be explored to construct artificial
spectroscopy were used to study ∼10 nm long dsDNA con-
RNA nanostructures. Besides the template-guided folding of
taining ribonucleoside monophosphates (rNMPs) located at
RNA nanostructures that is similar to the tactics in DNA nano-
specific positions within the DNA strands [88]. The results
technology, self-assembly of RNA building blocks is another
demonstrated that the perturbation of stiffness and the
leading approach for bottom-up RNA nanotechnology. A
plastic properties by rG intrusions is location and sequence
wide variety of RNA nanostructures have been success-
dependent, and can either soften or stiffen the DNA com-
fully constructed based on different assembly principles and
plex. MD simulations indicated that the perturbations are
approaches (Fig. 1). In this section, we will review several
from local structural distortions arising from hydrogen bond-
toolkits and methodologies that have shown great success
ing between the OH group of rG and electronegative sites of
for constructing multifunctional RNA nanostructures.
either the phosphate backbone or vicinal base. However,
many factors such as sequence, local structural environ-
ment, and metal ion concentrations [89,90] can significantly Toolkit I: Hand-in-hand interactions involving RNA
influence RNA versatility, stiffness and plasticity at the loops
molecular level [91]. The balance of the ion-mediated elec-
trostatic force and the non-electrostatic (chemical) forces Taking the construction of a wooden table as an analogy,
determine the equilibrium structure of the RNA. It is com- external dowels are used to link variety of wood blocks into
mon to find that one RNA molecule can exist in more than a structure. One of the unique properties of RNA is its folding
one conformation, and one kind of RNA molecule can dis- into loops and hairpin structures. RNA loops can serve as
play multiple bands in native gel electrophoresis due to the inter-RNA mounting dovetails, thus external dowels are not
redistribution of modular motif and local thermal energy. necessary for self-assembly into unique structure.
The versatile and plastic properties of RNA as polymer have The packaging RNA (pRNA) in phi29 DNA packaging motor
been applied to the construction of RNA polygons by stretch- [94—102] forms a hexameric ring structure through inter-
ing the internal angle of the three-way junction (3WJ) of locking of two looped regions in each pRNA molecule, named
RNA as a stable polymer 635
Figure 1 Design and construction of RNA nanostructures. (A) Phi 29 DNA packaging motor pRNA hexamer [110]. Reprinted with
permission from Ref. [110]. Copyright 1998 Elsevier. (B) pRNA dimer and trimer [106]. Adapted with permission from Ref. [106].
Copyright 2003 American Scientific Publishers. (C) pRNA arrays [112]. Reprinted with permission from Ref. [112]. Copyright 2004
American Chemical Society. (D) RNA tecto squares [116]. Reprinted with permission from Ref. [104]. Copyright 2004 The American
Association for the Advancement of Science. (E) The RNA nanoring [114]. Reprinted with permission from Ref. [114]. Copyright 2007
American Chemical Society. (F) The tRNA-based polyhedron [118]. Reprinted with permission from Ref. [118]. Copyright 2010 Nature
Publishing Group. (G) Cubic RNA-based scaffolds designed in silico [144]. Reprinted with permission from Ref. [144]. Copyright 2010
Nature Publishing Group. (H) Triangular RNA—protein complex [127]. Reprinted with permission from Ref. [127]. Copyright 2011
Nature Publishing Group. (I) The self-assembling RNA square [93]. Reprinted with permission from Ref. [93]. Copyright 2011The
National Academy of Sciences of the United States of America. (J) RNA microsponges for siRNA delivery [147]. Reprinted with
permission from Ref. [147]. Copyright 2012 Nature Publishing Group. (K) pRNA nanoparticles fabricated via hand-in-hand and foot-
to-foot tool kits [113]. Reprinted with permission from Ref. [113]. Copyright 2013 RNA Society. (L) pRNA nanoparticles fabricated
via branch extension tool kit [113]. Reprinted with permission from Ref. [113]. Copyright 2013 RNA Society. (M) Single stranded
RNA origami [136]. Reprinted with permission from Ref. [136]. Copyright 2014 The American Association for the Advancement of
Science. (N) Boiling-resistant RNA triangles and the array based on RNA triangles [36]. Reprinted with permission from Ref. [36].
Copyright 2014 American Chemical Society. (O) The self-assembled RNA membrane [152]. Reprinted with permission from Ref. [152].
Copyright 2014 Nature Publishing Group. (P) RNA origami tile and tube [139]. Reprinted with permission from Ref. [139]. Copyright
2014 John Wiley and Sons.
the right- and left-hand loops (Fig. 1A). The left-hand and for constructing stable RNA polygonal nanoparticles. Loop
right-hand were brought together from interlocking inter- extended RNA pairs with confirmed dimer formation capa-
action among four nucleotide sequences in the loops. Single bility were used as building blocks for higher order RNA
pRNA molecule with self-complimentary sequences in the oligomer nanoparticles (Fig. 1B). Using a reengineered loop
loops can be used to construct homodimer nanoparticles, extended pRNA toolkit, pRNA dimer, trimer, tetramer, pen-
or several pRNAs with the right-hand loop matching the tamer, hexamer, and heptamer were constructed with highly
sequence of the left-hand loop in another pRNA can be used efficient self-assembly, as shown by gel shift assays and AFM
to construct heterodimer nanoparticles. Through the inter- imaging [113].
locking loop interactions between different pRNA, dimer, Other loop—loop interactions have also been reported
trimer, and hexamer RNA nanoparticles have been created to build various RNA nanostructures. For example, nonco-
[103—112]. The interlocking loop sequences were further valent loop—loop contacts based on RNAI/IIi kissing-loop
extended to increase the thermodynamic stability of gen- complex have been used to build RNA nanorings which
erated RNA nanoparticles [113]. A toolkit with a set of are thermostable, ribonuclease resistant and capable of
hand-in-hand loop sequences has been designed and tested delivering RNA interference modules [85,114,115] (Fig. 1E).
636 H. Li et al.
Moreover, RNA kiss-loops were also used to build square- able to bind MG to emit fluorescence as shown in the fluores-
shaped tetrameric RNA nanoparticles and three-dimensional cent spectra (Fig. 2A and B). This property makes pRNA 3WJ
polyhedrons based on rationally designed RNAs [116—118] structure an extraordinary nanocarrier for targeted gene
(Fig. 1D and F). In addition, micrometer-scale RNA filaments delivery [123]. Moreover, an X-shaped motif from the cen-
have also been constructed by the rational design of tectoR- tral domain of the pRNA was discovered through extending
NAs incorporating 4-way junction (4WJ) motifs, hairpin loops the right-hand loop with a double-stranded sequence [73].
and their cognate loop—receptors [119,120]. The X-shaped pRNA motif can be self-assembled from four
RNA oligos and it creates a scaffold that allows for the
conjugation of four RNA functional moieties at the same
Toolkit II: Foot-to-foot interactions involving
time. Functional RNA modules such as survivin siRNA pre-
palindrome sequence and sticky ends
served their target gene knock-down effect after being fused
to the X-shaped structure (Fig. 2C). Branched hexavalent
pRNA nanoparticles can also be constructed through the foot
RNA nanoparticles were further constructed from three 3WJ
to foot interaction between pRNA monomers. While hand-in-
motifs, integrated by one 3WJ core motif structure or by
hand interaction involve ‘‘left’’ and ‘‘right’’ hand and the
palindrome sequence mediated linking of two pRNA-X cores
interaction is ‘‘multiple’’ and ‘‘inter’’ heterosexual, foot-
[113].
to-foot interaction includes only one foot that is the one
Recently, Khisamutdinov et al. reported using RNA as
unique palindrome sequence by self-homosexual interaction
an anionic polymer to build programmable self-assembling
of the identical RNA molecule. The foot domain is located in
boiling-resistant RNA nanostructures based on pRNA-3WJ
the helical 5 /3 open region of pRNA. Extending this region
[36] (Fig. 1N). A triangular shaped RNA nanoparticle was
with helical sequences does not compromise the entire pRNA
designed and prepared by carefully joining extended helices
molecule folding. A palindrome sequence reads the same
to the thermodynamically stable pRNA-3WJ motif of the
→
whether from 5 3 direction on one strand or from 5 → 3
bacteriophage phi29 DNA packaging motor. The step-wise
direction on the complementary strand. Extending the 3 end
self-assembly of the triangle RNA nanoparticles was con-
of pRNA monomer with a palindrome sequence can serve
firmed by native PAGE analysis, and AFM imaging revealed
as a sticky end for linking two pRNA monomers, and is
the triangular shape of the nanoparticles as expected.
denoted as a foot-to-foot interaction [112]. The foot-to-foot
The constructed nanoparticles are thermodynamically ultra-
interaction by palindrome sequences can also be utilized to
stable and robust. Functional motifs including siRNA,
bridge RNA nanostructures, motifs, or scaffolds for construc-
ribozyme, folate and fluorogenic RNA aptamers retained
ting RNA hexamers, octamers, decamers, and dodecamers
their activities after conjugation to the RNA nanoparticles.
(Fig. 1K). A pRNA array was constructed by combining
Moreover, these RNA triangles could be used as building
hand in hand-loop-interactions and foot-to-foot palindrome
blocks to construct supramolecular complexes such as RNA
sequence interactions [112] (Fig. 1C). Recently, strategies
hexagons and patterned hexagonal arrays. The pRNA-3WJ
involving both loop—loop interaction and sticky-end cohe-
is also highly tunable [92], the naturally preserved angle
sion were also reported to assemble three-dimensional and ◦
between the helices H1 and H2 of pRNA-3WJ is ∼60 and
structurally well-defined RNA nanoprisms by re-engineering ◦
this angle can be stretched to form square-shaped (90
pRNA [121]. ◦
angle) and pentagonal shape (108 angle) nanoparticles
with pre-designed sequences (Fig. 3A). The polygons formed
Toolkit III: Grafts of motifs from naturally-occurring by one-step self-assembly manner with efficiency >90%, as
RNA molecules demonstrated by gel shift assays. The different sizes and
shapes of the polygons were also confirmed by dynamic
Synthetic RNA nanoarchitectures can be designed with the light scattering (DLS) and AFM. The equilibrium dissocia-
known naturally-occurring three-dimensional RNA motifs. tion constants (KD) for triangle, square and pentagon are
◦
Particularly, some RNA motifs in nature exhibit extraordi- 18.8 nM, 20.3 nM and 22.5 nM, and the Tm values are 56 C,
◦ ◦
nary stability, for example, phi29 motor pRNA [54,110,122], 53 C and 50 C, respectively, revealing structure and shape-
tRNA [118], 5S RNA[123], and others [115]. These motifs dependent thermodynamic features. In a recent paper by
have been used to create synthetic RNA nanostructures Jasinski et al, the authors showed that square-shaped RNA
[36,93,118,124,125]. The central domain of the pRNA nanoparticles with fluorogenic and ribozymatic properties as
molecule contains a three way junction (3WJ) core struc- well as different sizes can be successfully constructed by uti-
ture [54]. This 3WJ can be assembled from three individual lizing the pRNA-3WJ at each corner and different length RNA
RNA fragments with high efficiency in the absence of metal duplexes at each edge of the square RNA nanoparticles [125]
ions [123]. The 3WJ motif itself creates a branched structure (Fig. 3B). DLS and AFM determined the sizes of the small,
that allows for constructing multifunctional RNA nanoparti- medium, and large square RNA nanoparticles are 4.0, 11.2,
cles with different functional moieties at each end of the and 24.9 nm, respectively. The physiochemical properties of
branches. RNA nanoparticles can also be designed and fab- the nanoparticles can be easily tuned, as the utilization of
ricated via branch extension tool kit [113] based on the 3WJ 2 -F RNA as the core strand significantly increased the melt-
motif (Fig. 1L). 3WJ core retained its original folding and the ing temperature as well as the nanoparticle’s resistance to
conjugated RNA module on the branches can fold into their serum-mediated degradation.
authentic structure and remain functional [123,126]. For Naturally occurring stable RNA-protein complexes were
example, after incorporated into 3WJ motif, HBV ribozyme also explored as building blocks for nanostructures. For
retain its capacity to cleave its RNA substrate and generate example, the assembly of archaeal box C/D sRNPs com-
smaller cleavage products, and MG binding aptamer was also prising the L7Ae protein from Archaeoglobus fulgidus and
RNA as a stable polymer 637
Figure 2 Construction and functional assays of thermodynamically stable pRNA-(three-way junction) 3WJ or pRNA-X nanoparticles.
(A and B) HBV ribozyme assay and MG aptamer assay of pRNA-3WJ nanoparticles [123]. Adapted with permission from Ref. [123].
Copyright 2011 Nature Publishing Group. (C) Survivin gene knock-down assay of pRNA-X nanoparticles [73]. Reprinted with permission
from Ref. [73]. Copyright 2012 Elsevier.
a box C/D RNA has been utilized to build an equilateral tri- [114], and the tetraloops GNRA and UNCG [138] were used to
angle shaped synthetic RNA protein complex [127] (Fig. 1H). mediate internal RNA tertiary interactions, resulting in orga-
The construction relies on the interaction between ribo- nized and scalable RNA crossover tiles. The designed RNA
somal protein L7Ae and the Kink-turn motif in box C/D origami nanostructures are also robust, which could form
RNA. L7Ae can bind to the box C/D K-turn motif through by either annealing or co-transcription on mica. In contrast
hydrogen bonding with high specificity and affinity [128]. to DNA origami, this RNA origami approach does not need
It was reported that using RNA-protein complex (RNP) as short staple strands to facilitate the folding of the origami
building block for nanostructures enhanced its stability in structure, but using RNA modules such as kissing loops to
serum comparing to pure unmodified RNA based nanopar- replace the role of staple strands. Interestingly, a differ-
ticles [129]. The RNP nanostructure could be served as a ent RNA origami approach which is a direct extension of
scaffold for protein or RNA functionalities. For example, an the DNA origami to RNA was also reported in 2014 [139]
affibody peptide, which can recognize HER2 receptor, was (Fig. 1P). In this study, a single-stranded RNA scaffold and
connected to RNP triangle through fusing to L7Ae protein, multiple staple RNA strands were used to assemble defined
and the functionality of affibody peptide was still retained. RNA nanostructures including a 7-helix bundled RNA tile and
siRNA targeting to GFP gene can be conjugated to the RNP a 6-helix bundled RNA tube. The authors also showed that
triangle through extending the RNA strand and the GFP siRNA functional modules such as biotin could be introduced into
on RNP nanoparticles still can be processed by dicer and the RNA origami structures by chemical modifications of the
knock down GFP expression in cells. scaffold strands.
Toolkit IV: RNA origami Toolkit V: RNA/DNA hybrid nanostructures
DNA origami, which involves the folding of a long template RNA/DNA hybrids can also be used to construct func-
single stranded DNA aided by multiple short staple DNA tional nanoarchitectures. Similar to split-protein systems,
strands, was reported in 2006 [130]. A wide range of 2D RNA/DNA hybrids can be computationally designed for acti-
and 3D nanostructures have been successfully constructed vating different split functionalities in the presence of
using the DNA origami technique [131—135]. In 2014, a sim- respective equivalent strands [140—143] (Fig. 5A). Toe-
ilar approach for RNA origami was reported to fold single hold interactions were used to trigger disassociation of
stranded RNA into RNA tiles and further assembled into RNA/DNA hybrids and re-association of the double-stranded
hexagonal lattices [136] (Fig. 1M). A variety of RNA tertiary RNA and DNA. The thermodynamics and kinetics of the
◦
motifs, including the 180 kissing loop motif of the HIV-1 DIS toehold interactions can be tuned to control the dissocia-
◦
[137], the 120 loop—loop complex of RNA i/ii inverse loop tion and re-association processes. RNA interference modules
638 H. Li et al.
Figure 3 Construction of RNA polygons based on pRNA-3WJ. (A) Construction of RNA triangle, square and pentagon by tuning the
interior pRNA-3WJ angle [92]. Reprinted with permission from Ref. [92]. Copyright 2014 Oxford University Press. (B) Construction
of RNA squares with tunable sizes [125]. Reprinted with permission from Ref. [125]. Copyright 2014 American Chemical Society.
as well as other functionalities such as fluorophores and more enzymatically stable than RNA, this approach has the
RNA aptamers can be successfully triggered inside mam- potential to improve the pharmacological profiles of RNA-
malian cells. This RNA/DNA hybrids concept has also been based nanoparticles. Moreover, controlled release of the
applied to other nanostructures such as nanorings and cubes split functionalities opens a new avenue for the develop-
[114,115,144—146], and the spilt functionalities still retain ment of nucleic acid-based switches to modulate cellular
their authentic functionalities. Because RNA/DNA hybrid is functions in vivo.
RNA as a stable polymer 639
Methodology I: Rolling circle transcription large-area of RNA membrane. After the cRCT process, the
water in the RNA membrane was evaporated and the dried
Typically, the design and production of RNA nanoparticles RNA membrane was concentrated by EISA process. The self-
have relied on the production of discrete RNA strands that assembled RNA membrane was fabricated densely on the
can be assembled in a controlled and predictive fashion to tube wall during the evaporation process. The durability
generate nanoparticles with a defined structure and stoi- of the fabricated RNA membrane was tested under various
chiometry. Hammond and colleagues have departed from harsh conditions, including RNase and DNase-rich environ-
this approach with an innovative strategy that generates ments. In addition, they confirmed the application of the
monodisperse spherulitic RNA particles from extremely high RNA membrane as an enzyme-responsive drug-release sys-
molecular weight RNA strands by using a rolling circle tran- tem with doxorubicin and siRNA. The results showed that
scription (RCT) approach [147,148] (Fig. 1J). They created the RNA membrane can provide a high drug-loading effi-
a circular DNA construct containing a siRNA gene without ciency and can be a great candidate for future membrane
any terminator sequences and proceeded by a T7 pro- industry.
moter. As a result, T7 RNA polymerase can continuously
transcribe the circular DNA hundreds of times to gener-
ate a tremendous number of copies of the tandem RNA Methodology II: Chemical modification of RNA
unit. As the continuous RNA strand is transcribed, magne-
sium pyrophosphate crystals are simultaneously generated, A great deal of work on chemical modifications aiming to
and the RNA strands attach to the crystallite surfaces to improve the chemical stability and in vivo properties of RNA
form composite structures; each structure grows in length have been reported [153—156]. Common chemical modi-
to become fiber-like, then, forms sheet-like lamellae. The fications of RNA can be categorized into five classes: (1)
lamellae, typically ∼10 nm thick, finally condense into Modification of inter-nucleotide phosphodiester backbone.
spherulites with diameters varying from a few micrometers This type of modification is the most classic and simplest
to hundreds of micrometers, referred by the author as RNAi method to improve the performance of RNA in the biological
microsponges. To achieve efficient cellular uptake, PEI was environment. For example, creation of a phosphorothioate
introduced to condense the RNAi-microsponge from 2 m to (PS) linkage by replacing one non-bridging oxygen atom on
200 nm, and to protect the RNA from degradation by RNase. the phosphate backbone with a sulfur atom substantially
The PEI introduced a positively charged outer layer to the increases the stability of RNA in vitro and in vivo [157]. Other
microsponges to facilitate cell binding and entry. It was backbone modifications such as boranophosphate, phospho-
also demonstrated that the spherulitic RNAi-microsponges ramidate and methylphosphonate have also been explored
produced ∼21 nt siRNA fragments after incubation with to enhance the resistance to nuclease-mediated degrada-
Dicer and could transfect a cancer cell line and silence tion [158—160]. However, cytotoxic side-effects were also
firefly luciferase expression. Gene expression knockdown observed if extensive modifications were applied [161].
in vivo by intratumoral injection of the PEI-condensed RNAi- (2) Substitution of 2 -OH group. This is the most widely
microsponges was also reported. This innovative approach used approach since it is well-tolerated, and can enhance
opens new directions to RNA nanoparticle self-assembly nuclease resistance as well as reduce immunogenicity.
and siRNA delivery. However, the therapeutic potential and For example, the naturally occurring 2 -O-methyl (OMe)
in vivo safety of this approach requires further evaluation, modification is nontoxic and able to prevent immune acti-
as PEI has been shown to cause well-known adverse side vation while conferring biological stability simultaneously
effects, such as high cytotoxicity [149,150]. In addition, fur- [161,162]. Guo’s lab also reported that incorporation of
ther reduction of the size of the particles is recommended 2 -Fluoro nucleotides to pRNA scaffold allows the creation
to avoid non-specific healthy organ accumulation. of stable and RNase-resistant RNA nanoparticles with cor-
In material sciences, polymeric membranes are at rect folding and authentic biological activities. The melting
the forefront in the chemical and biotechnology indus- temperature of 2 -F RNA was further enhanced compared
try because of their versatile applications such as water to unmodified RNA [163]. The chemically modified pRNA-
purification, dehydrogenation of natural gas, dialysis of based nanoparticles have shown promising applications in
blood, removal of cell particles, and others [151]. Recently, cancer therapy [36,66,164—167]. Recent study also showed
Lee’s group demonstrated rolling circle transcription can that 2 -F modified pRNA nanoparticles are resistant to I-125
also be applied to the synthesis of macroscopic RNA mem- and Cs-131 radiation with clinically relevant doses, which
branes that has the potential as a controlled drug-release is a required property for applying these RNA nanopar-
system [152] (Fig. 1O). The RNA membrane was fabri- ticles as delivery vehicles for targeted radiation therapy

cated by T7 RNA polymerase transcription system with a [168]. Other options for 2 -modification like 2 -fluoro- -D-
combination of complementary rolling circle transcription arabinonucleotide (FANA) have also shown promise in gene
(cRCT) and evaporation-induced self-assembly (EISA). The silencing applications [169]. (3) Locked nucleic acids (LNA)
circular DNA template and complementary circular DNA and unlocked nucleic acid (UNA). LNA is another class of
template were prepared with long linear DNA and the pro- 2 -modification in which 2 -O and 4 -C is linked via a methy-
moter DNA for starting the RCT, respectively. Upon addition lene bridge. This locked linkage constrains the ribose ring
of T7 polymerase to these two circular DNA templates, into C3 -endo conformation which confers both significant
thousands of copies of single stranded RNA and single increase in thermostability and enhancement in nuclease
stranded complementary RNA were continuously generated. resistance [170]. Successful applications of LNA such as 2 -
The two complementary RNA strands hybridized to each amino-LNA have been studied by Astakhova et al. to show
other thereby forming the double stranded RNA for the great promise in the development of biosensor, aptamer
640 H. Li et al.
and other nanomaterials [171]. Antisense oligonucleotides provides useful RNA structures for designing RNA nanostruc-
(ASO) containing LNA also has been reported to have higher tures [185].
potency and specificity [172,173], but would also cause
liver toxicity in mouse models if LNAs were extensively
incorporated into the sequence[174]. In the other hand, Application of RNA as a polymer in biomedical
UNA is an acyclic and structurally flexible-RNA analogue in
sciences
which the C2 —C3 bond is absent. As a result, the bind-
ing affinity of UNA towards its complementary strand is
RNA as a natural and biocompatible polymer has many
decreased [175]. (4) Modification of ribonucleotide base.
advantages for biomedical applications. It carries a neg-
This approach is less commonly used than other modifica-
ative charge at physiological conditions, which disallows
tion approaches described thus far. However, recently RNA
nonspecific passing through negatively charged cell mem-
tube nanostructures have been reported to be constructed
brane. With the conjugation of chemical ligands and/or
successfully by using RNA scaffolds with 5-biotinylated mod-
RNA aptamers, RNA nanoparticles can be designed for spe-
ified and 5-aminoallyl modified uracil [139]. Other common
cific cell targeting. It is less toxic compared with protein
modified bases such as 2-thio-, 4-thio, 5-iodo-, 5-bromo-,
based nanoparticles since it can avoid antibody induction
dihydro-, pseudo-uracil and diamino-purine also have been
(protein-free nanoparticle), allowing repeated treatment
demonstrated to confer enhancement in stability as well
of chronic diseases. It also does not induce an interferon
as specificity of base-pairing interactions [155,176,177].
response nor cytokine production [92,186]. RNA nanoparti-
(5) Modification of ribose moiety. This modification strat-
cles designed with a size range 10—40 nm display favorable
egy, for example, altritol nucleic acid (ANA) and hexitol
pharmacokinetic properties [186], such as extended half-
nucleic acid (HNA), is mainly applied in siRNA design to
life in vivo (5—12 h compared to 0.25—0.75 h for siRNA),
enhance potency and nuclease resistance [178]. Besides
clearance: < 0.13 L/kg/h, volume of distribution: 1.2 L/kg.
these classes, other novel methods such as photocaging
Furthermore, RNA nanoparticles are classified as chemical
modification have been used to control RNAi induction [179].
drugs rather than biological entities. This classification will
The particular effect of various chemical modifications on
facilitate drug approval.
RNA are summarized in Table 1. It is expected that the ratio-
As a building block for nanoparticles, RNA can be synthe-
nal choice of precise chemical modifications will greatly
sized with defined structure and stoichiometry. Multivalent
contribute to the development of RNA nanostructures for
RNA nanoparticles can be constructed using special RNA
applications in biomedical sciences and materials sciences.
motifs as building blocks that combine therapy, targeting,
Moreover, the strategy of combining different modification
and detection, all functionalities in one particle.
approaches also has the potential to improve the properties
of RNA more dramatically.
RNA as a biocompatible nanomaterial for tissue
Methodology III: Computational approach engineering
Tissue engineering is a new area with lots of active research
The first step in RNA nanoparticle construction is the
and some recent success. Biocompatible nanomaterials are
consideration of the blueprint [180]. This requires an under-
needed for various applications in tissue engineering, such
standing of the assembly and folding mechanism in the
as scaffolds or arrays that can function as temporary matri-
bottom-up assembly. Designing the sequence of the building
ces and/or niches for the controlled deposition, infiltration,
block is critical for successful RNA nanostructure assembly,
proliferation, and differentiation of cells. It would also be
which can be achieved by experience and brainstorming
advantageous if these nanomaterials could be highly bio-
taking into consideration of RNA folding, complementa-
compatible and mimic the natural tissue microenvironment
tion, hand-in-hand interaction, foot-to-foot interaction, and
in vivo.
the use of thermostable motifs, kissing loops, sticky ends,
Shu et al. reported that nanometer scale 3D RNA arrays
helices, stem loops, etc. All RNA nanoparticles constructed
can be assembled by using pRNA as building blocks [112]
based on phi29 motor pRNA was achieved via experience and
(Fig. 1C). By rational design, the authors incorporated
brainstorming without computer algorithm besides the tra-
palindrome sequences (nucleotide sequences that read the
ditional RNA folding program developed by Zuker 30 years
same 5 → 3 on one strand and 3 → 5 on the complemen-
ago [181]. It is expected that computer algorithms will facil-
tary strand) into the 3 -end of the pRNA. The palindrome
itate RNA nanoparticle construction. A variety of computer
sequences served as links for bridging two pRNAs via foot-on-
programs such as NanoFolder, NanoTiler and RNA2D3D are
foot interactions. Loop—loop interactions were further used
available to facilitate the in silico design of RNA sequences
to link pRNA molecules into a chain. The formation of pRNA
(these sequences may contain inter-strand and intra-strand
arrays was confirmed with both polyacrylamide gel elec-
pseudoknot-like interactions) capable of self-assembly into
trophoresis (PAGE) and AFM. These RNA arrays are unusually
multi-sequence RNA nanostructures and the 3D modeling
stable and resistant to a wide range of temperatures, salt
of such structures [182—184]. For example, by utilizing
concentrations, and pH environments. The microstructures
computational modeling and sequence optimization, three-
of the RNA assays are also tailorable by changing the
dimensional cubic RNA-based scaffolds can be successfully
RNA nucleotide sequences. Since RNA molecules are highly
designed and engineered with precise control over their
biocompatible and not toxic, these RNA arrays have the
shape, size and composition [144]. Moreover, online RNA
potential to be good tissue engineering scaffolds.
structure databases such as RNAJunction database also
RNA as a stable polymer 641
Table 1 Summary of chemical modifications of RNA.
Chemical modifications Advantages Disadvantages References
Phosphate backbone
• •
Phosphorothioate (PS) • Improve nuclease resistance Destabilize siRNA duplexes [157—162]
• • ◦
Boranophosphate (BO) Combine with other (e.g. decreases Tm by 0.5 C
•
Phosphonoacetate (PACE) modifications to dramatically per PS linkage)
• •
Phosphoramidate improve RNA property Extensive modification causes
•
Methylphosphonate cytotoxic effect
2 -OH group
•
Small 2 -substituents (e.g. • Significantly improve • Extensive or full modification [36,66,161—169,
2 -O-methyl (2 -OMe), nuclease resistance will reduce or fully deactivate 173]
•
2 -fluoro (2 -F), Greatly thermo-stabilizes siRNA potency
•
2 -aminoethyl, 2 -deoxy-2 - dsRNA duplex (e.g. increase Tm Bulky 2 -modifications are
◦ ◦
fluoroarabinonu-cleic acid 0.5—0.7 C per 2 -OMe and 1 C only tolerated at limited
(2 -F-ANA)) per 2 -F) position owing to their
• •
Bulky 2 -modifications (e.g. Particularly, 2 -OMe is distortion of RNA helix
2 -O-MOE, 2 -O-allyl) nontoxic and prevents immune structure activation
•
Bulky 2 -modifications can
modulate thermo-stability and
duplex asymmetry, and also
give higher binding affinity
Locked nucleic acid (LNA) • LNA enhances the • LNA would probably cause [170—175]
Unlock nucleic acid (UNA) complementary binding affinity liver toxicity
•
and greatly improves Extensive modification with
◦
thermostability by 2—10 C per LNA and UNA generally results
incorporation, as well as in decreased activity of siRNA
improves nuclease resistance and failure in annealing of
and reduces RNA dsRNA, respectively immunogenicity
•
Each UNA destabilizes duplex
◦
by 5—8 C to improve local
destabilization of siRNA
duplex, and enhance
biostability in vivo
Ribose moiety
•
Altritol nucleic acid (ANA) • Enhance thermostability (e.g. • Modification at seed region [178]
•
Hexitol nucleic acid (HNA) 2 -F-ANA increases Tm of RNA would slightly reduce siRNA
• ◦
2 -deoxy-2 -fluoroarabino- duplex by 0.5—0.8 C per potency
nucleic acid (2 -F-ANA) modification)
• •
Cyclohexenyl nucleic acid Improve nuclease resistance
Ribonucleotide base
•
(5-bromo-, 5-iodo-, 2-thio-, Stabilize base-pairing and to • Some base modifications (e.g. [139,177]
4-thio-uracil, dihydro-, enhance binding specificity 5-bromo- and 5-iodo-uracil)
•
pseudo, 5-biotinylated, Particularly, 2-thio- and will affect siRNA potency
5-aminoallyl-uracil, pseudo-uracil reduce cellular
diamino-purine) immune response
RNA nanoparticles for targeted therapeutic system. In 2003, Hoeprich et al. constructed a pRNA-based
delivery carrier to deliver hammerhead ribozymes [187]. Upon conju-
gation to the pRNA 5 /3 ends, the HBV ribozymes were able
to fold correctly and almost completely cleaved the polyA
Targeted delivery is a major challenge that nucleic acid ther-
signal of HBV mRNA in vitro. Targeted therapeutics delivery
apeutics is facing. RNA nanoparticles with chemical ligand
to specific cancer cells can be achieved by using ligand-
and nucleic acid aptamers have shown great promise in this
conjugated RNA nanoparticles as carriers. Furthermore,
regard. The utilization of RNA nanostructures as a platform
the cargo in vivo release profile from RNA nanoparticles
for targeted therapeutics delivery has been successfully
can also be controlled through the rational design of RNA
demonstrated by a series of studies using the phi29 pRNA
642 H. Li et al.
nanoparticles. In 2005, Guo et al. reported the construction effects [186]. The regression of gastric cancer and breast
of chimeric pRNA dimer with one subunit harboring folate cancer by RNA nanoparticles harboring siRNA [73,123,167]
and the other subunit harboring a gene silencing siRNA tar- or anti-miRNA [173] has also been reported recently.
geting surviving [108]. Incubation of these pRNA dimers with A recent paper also reported the development of novel
cancer cells resulted in receptor-mediated binding and entry immunomodulators by engineering rationally designed RNA
to cells and induced efficient gene silencing. Animal trials polygonal nanoparticles [92]. When immunological adju-
showed that ex vivo delivery of the pRNA dimer harboring vants CpG DNA were incorporated into the RNA polygons,
both folate and survivin siRNA could suppress tumor develop- potent immunostimulation (cytokine TNF-␣ and IL-6 induc-
ment. Khaled et al. studied the fabrication of a protein-free tion) was observed both in vitro and in vivo, compared to
20—40 nm pRNA trimer which could harbor three functional controls. Moreover, the RNA nanoparticles could deliver CpG
modules including siRNA, CD4 aptamer or folate ligands DNA to macrophages specifically and the degree of immuno-
and a fluorescent dye per nanoparticle [111]. They showed stimulation significantly depended on the size, shape, and
that the pRNA trimer could also bind and enter into cells the number of payload per RNA nanoparticle. This finding
and modulate gene expression and apoptosis both in vitro demonstrates that RNA nanotechnology, such as developing
and in vivo. In 2006, Guo et al., reported incorporating a RNA nanoparticles based on pRNA, has great potential to
folate-AMP into the 5 -end of phi29 pRNA and showed that develop novel immunomodulators.
folate conjugated pRNA dimer nanoparticles were able to
deliver survivin siRNA into nasopharyngeal epidermal car-
RNA nanoparticles for controlled drug delivery
cinoma cells and silence the target gene [188]. The pRNA
system can also be used to deliver anti-virus siRNAs. Zhang
Many pre-clinical studies are evaluating RNAi as novel thera-
et al., developed a folate-linked pRNA conjugated with the
peutics for different diseases. However, one concern is that
siRNA targeting the Coxsackievirus B3 (CVB3) protease 2A
single gene targeted therapy might eventually fail due to
(siRNA/2A) [189]. They observed that the modified pRNA
mutations over time or development of alternative signaling
could achieve a similar antiviral effect to that of siRNA/2A
cascades or escape pathways. Multivalent RNA nanoparti-
alone and also strongly inhibited CVB3 replication.
cles can be a very promising vehicle for delivery of multiple
The latest advance in the utilization of phi29 pRNA
siRNAs to suppress multiple genes simultaneously. A recent
for therapeutics delivery is the discovery of a phi29 pRNA
publication by Afonin et al. showed that several RNA and
three-way junction (3WJ) motif with unusual thermody-
RNA/DNA nanocubes could be functioned with multiple dou-
namic stability. The slope of the melting temperature curve
◦ ble stranded RNAs and the siRNAs can be conditionally
of the three-fragment RNA complex is close to 90 , indicat-
released through ssDNA toehold-mediated interactions. Fur-
ing extremely low G of the phi29 pRNA-3WJ complex [123].
thermore the RNA nanocubes can be tracked intracellularly
The pRNA 3WJ motif was used as a RNA scaffold to construct
through FRET (Förster resonance energy transfer) stud-
bi-, tri-, and tetra-valent RNA nanoparticles with very high
ies using fluorophores [190]. In addition, spherical nucleic
chemical and thermodynamic stability [73,123,180]. The
acid (SNA) nanoparticle conjugates developed by Mirkin
resulting RNA nanoparticles are resistant to denaturation
group have also shown promise for systemic siRNA deliv-
in 8 M urea and do not dissociate at ultra-low concen-
ery for treating diseases such as glioblastoma [191,192]
trations both in vitro and in vivo. Each arm of the 3WJ
(Fig. 5D). In vivo studies on glioma-bearing mice showed
or X-motif can harbor one siRNA, ribozyme, miRNA, or
that SNA nanoparticle conjugates targeting the oncoprotein
aptamer without affecting the folding of the central core,
Bcl2Like12 effectively increased intratumoral apoptosis,
and each daughter RNA molecule within the nanoparticle
and reduced tumor burden and progression without adverse
folds into respective correct structure with authentic bio-
side effects [192].
logical function. The effects of gene silencing progressively
DNA origamis have been exploited as a carrier for chem-
increased with increasing number of siRNA modules in the
ical drug doxorubicin through noncovalent intercalation
RNA nanoparticle. More importantly, systemic delivery of
interactions. The DNA origami/doxorubicin nanoparticles
targeting ligand containing RNA nanoparticles into tumor-
were able to enter into doxorubicin-resistant cancer cells
bearing mice revealed that the RNA nanoparticles remained
and circumvent their drug resistance [193]. Furthermore,
intact in vivo without showing any sign of dissociation or
the DNA origami/doxorubicin nanoparticles showed a slow
degradation. These RNA nanoparticles can specifically tar-
drug release profile at pH 7.4 under physiological condi-
get subcutaneous tumor xenografts [73,123,167], as well
tions but showed enhanced release capability in pH 5.5
as orthotopic breast cancer [173] and intracranial glioma
corresponding to tumor subcellular organelles [194]. As
tumors [164] without detectable accumulation in liver, lung
we discussed in previous section, RNA origami structures
or other healthy organs or tissues (Fig. 4A—C). A recent
have been reported [136]. With favorable thermodynamic
study also showed that the pRNA-3WJ nanoparticle conju-
stability and excellent serum stability after chemical modi-
gated with folate can specifically target colorectal cancer
fications, RNA origami is expected to be more favorable than
metastasis in the liver, lungs and lymph node simulta-
its counterpart DNA origami as a drug carrier for achieving
neously in vivo, without accumulation in normal liver or
controlled drug release.
lung parenchyma [165] (Fig. 4D). Pharmacological analy-
sis in mice indicated that the pRNA nanoparticles display
favorable pharmacokinetic (PK) and pharmacodynamic (PD) RNA nanoparticles for vascular targeting
profiles, with in vivo half-life extended 10-fold compared to
siRNA alone and did not induce adverse immune response A critical feature to drug delivery is the transportation of
including cytokine, interferon, antibody, and other toxic therapeutics to their intended target sites. Arguably, as
RNA as a stable polymer 643
Figure 4 pRNA nanoparticles for cancer targeting. (A) pRNA-3WJ nanoparticles target folate-receptor positive tumor xenografts
[123]. Reprinted with permission from Ref. [123]. Copyright 2011 Nature Publishing Group. (B) pRNA-3WJ nanoparticles target glioma
[164]. Reprinted with permission from Ref. [164]. Copyright 2015 Impact Journals, LLC. (C) pRNA-X nanoparticles target folate-
receptor positive tumor xenografts [73]. Reprinted with permission from Ref. [73]. Copyright 2012 Elsevier. (D) pRNA nanoparticles
targeting colorectal cancer metastases [165]. Reprinted with permission from Ref. [165]. Copyright 2015 American Chemical Society.
∼
almost all cells in the body are within 100 m of the vas- [197,198], inflammatory markers (ICAM-1, VCAM-1)
culature, and by way a vascular endothelial cell, it stands to [199—204], and thrombomodulin [205]. Targeting of
reason that the vascular delivery route represents the most CD31, ICAM1 and VCAM represents a unique opportunity
promising mean of any site specific delivery strategy [195]. as their binding of nanoparticles to their sites highlights
Owing to the significant heterogeneity in endothelial cells, a novel endocytic mechanism, CAM mediated endocytosis
both temporally and regionally, it has been observed that [198,206]. The use of antibodies as targeting agents is
the vascular endothelium has unique expression of surface technically challenging owing to their size, cost of produc-
markers that are highly regionally variant. In other words, it tion and potential immune responses. RNA aptamers have
is potentially possible to target unique endothelial zip codes already shown exciting advantages in vasculature targeting.
to locally accumulate nanocarriers [196]. High affinity aptamers (56 pM) against P-selectin have been
Current strategies for vascular targeting of nanocarriers developed [207]. Microbubbles coated with a low density
2
have primarily focused on antibody and peptide based (1000 copie/m ) of P-selectin aptamers demonstrated high
strategies, targeting to surface markers CD31 (PECAM-1) adhesion even under shear rates as high as 1700 L/s. The
644 H. Li et al.
Figure 5 Functional RNA nanostructures for therapeutics delivery and medical detection. (A) Triggered siRNA delivery based on
RNA/DNA hybrid nanostructures [140]. Reprinted with permission from Ref. [140]. Copyright 2013 Nature Publishing Group. (B)
QD-aptamer-doxorubicin conjugate nanoparticles as a cancer-targeted imaging, sensing and treatment platform [210]. Reprinted
with permission from Ref. [210]. Copyright 2007 American Chemical Society. (C) PSMA aptamer-conjugated gold nanoparticles for
targeted molecular CT imaging and therapy of prostate cancer [213]. Reprinted with permission from Ref. [213]. Copyright 2010
American Chemical Society. (D) Spherical nucleic acids scaffold for loading RNA therapeutics [191]. Reprinted with permission from
Ref. [191]. Copyright 2014 American Chemical Society.
real promise of vascular-targeted RNA nanoparticles comes RNA, RNA molecules with high binding affinity to their tar-
from the combination of the high binding affinity to carrier gets hold great potential as a platform to construct imaging
sizes below 70 nm. The capillary bed represents the greatest probes which can specifically detect their targets in vitro
promise of vascular targeting, where there already exists a and in vivo.
highly active transcytosis mechanism, with approximately Fluorescent RNA nanoparticles conjugated with aptamer
ten thousand times more caveolae than other endothelial have been widely explored for cancer detection. For
cells [208]. These 70 nm endocytic vesicles are an exciting example, Bagalkot et al. [210] developed a QD-aptamer-
target for drug delivery [209] yet require a carrier system doxorubicin conjugate nanoparticle as a cancer-targeted
like RNA nanoparticles that are simultaneously small and imaging, sensing and treatment platform (Fig. 5B). A10
have high affinity to permit transcytosis and tissue bed RNA aptamer, which specifically binds to the extracellular
delivery. domain of the prostate specific membrane antigen (PSMA),
was conjugated to the surface of fluorescent quantum
dots and the anticancer drug doxorubicin was intercalated
RNA nanoparticles as non-invasive medical into the double-stranded stem of the A10 aptamer. In the
detection reagents conjugate nanoparticle, fluorescence of doxorubicin was
quenched by the aptamer through donor-quencher FRET,
Functional RNA structures such as aptamers can be used and the fluorescence of QD was quenched by DOX through
for developing non-invasive molecular and cellular imaging donor-acceptor FRET mechanism. When the nanoparticle
reagents which may have applications in the diagnosis of enters the prostate cancer cell and doxorubicin is released,
various diseases including cancer, cardiovascular diseases, the fluorescence of QD and DOX is re-activated. Other RNA
and infectious diseases. Considering it is relatively easy to aptamers conjugated with fluorescent dye chemicals have
conjugate a fluorophore, radionuclide, quantum dot (QD), also been utilized for breast cancer diagnosis, such as EpCAM
gold nanoparticle, or other imaging functional groups to aptamer labeled with DY647, TYE665 or FITC [211].
RNA as a stable polymer 645
Conjugating RNA aptamer with radioactive material can this novel design, the authors determined the half-life (t1/2)
also be applied as diagnostic radiopharmaceuticals to detect of the MG aptamer containing pRNA-3WJ inside living cells
cancer cell markers. In a recent study reported by Gomes to be ∼4.3 h.
et al. [212] a 36 nucleotide long truncated RNA aptamer
with 2 F pyrimidine and 2 -O-methyl purine modification was
constructed for targeting to the human matrix metallopro- RNA as a polymer for biosensor systems
tease 9 (hMMP-9), which promotes tumor metastasis and The biomolecular-based detection system has been widely
is an important marker of malignant tumors. The 5 -end investigated in many applications including clinical diag-
amine modified RNA aptamer was conjugated to MAG3-NHS, nosis, food industry, environmental monitoring industry,
99m
which served as a chelator for Technetium-99m ( Tc). The and security industry [217,218]. Conventionally, biosensors
99m
Tc labeled modified RNA aptamer was able to specifically can detect proteins, nucleic acids such as DNA or RNA
detect its target in human brain tumors with autoradiogra- sequences, small organic molecules, and others [218—220].
phy. RNA molecules are well suited to serve as detection tools
With the conjugation of the PSMA RNA aptamer to the for small molecules, for example, antibiotics, peptides,
surface of gold nanoparticles (GNPs) [213], a targeted metal ions, ligands, etc. [221,222] because of their unique
computed tomography (CT) imaging and therapy system folding structures, functional conformation, predictable
for prostate cancer can also be established (Fig. 5C). base-pairing, and high fidelity. These characteristics of RNA
The CT imaging study revealed that the PSMA aptamer- allow for the development of ribozyme or aptamer, and
conjugated GNPs could generate more than four-fold greater aptazyme-based biosensors [223—225]. Also, as the target,
CT intensity for a PSMA-expressing cell line than a non-PSMA- RNA can be used to develop the biosensor for the detection
expressing cell line, suggesting good specificity in detection of messenger RNA or micro RNA [226—229]. Various detec-
of the targeted cancer cells. tion methods of RNA-based biosensors were proposed such as
electrochemical type, fluorescence type, optical type, and
electrical type. Also, there are various detection platforms
RNA nanoparticles for intracellular imaging and for RNA-based biosensors (Fig. 7) [230—235]. In this section,
detection we briefly introduce RNA-based biosensors for biomedical
and environmental monitoring applications.
An interesting example of applying RNA in intracellular The first proof of concept of using RNA in a biosen-
imaging is the Spinach RNA aptamer, which is the RNA sor was developed by Breaker Group [221]. Self-cleaving
mimic of Green fluorescent protein (GFP). GFP has been hammerhead-ribozymes were created with seven differ-
extensively utilized as a reporter protein in cell and molec- ent RNA switches and these immobilized each pixel that
2+
ular biology. Similarly, the RNA mimics of GFP should also responded allosterically to six types of analytes (Co ,
have remarkable applications in biomedical research, espe- cGMP, cCMP, cAMP, FMN and theophylline). The platform
cially for intracellular imaging of RNA. By using the method of biosensor array was prepared on a polystyrene cell cul-
of systematic evolution of ligands by exponential enrich- ture plate which was coated with gold by physical vapor
ment (SELEX), Paige et al. developed a novel class of RNA deposition. The ribozyme was immobilized onto gold sur-
aptamers, termed Spinach that bind to fluorophores resem- face via a 5 -thiotriphosphate-terminated RNA moiety. Then,
bling the fluorophore in GFP [214] (Fig. 6A). Upon binding each hammerhead ribozymes cleaved off their 3 frag-
of the targeted fluorophores, these RNA aptamers were ment according to addtion of individual analytes. They also
capable of emitting tunable fluorescence with comparable showed the quantitave and qualitive measurement of cAMP
brightness to enhanced GFP (EGFP) and many other fluo- in culture media from E. coli strand.
rescent proteins. Moreover, the RNA-fluorophore complex is RNA can also serve as the detection analytes to detect
resistant to photobleaching. Interestingly, the Spinach RNA viable E. coli as an indicator organism in drinking water,
aptamer can be expressed in vivo by fusing to other cellular which was proposed by Baeumner group [228,229]. This
RNAs, for example, 5S RNA, to enable live-cell imaging and RNA-based biosensor was generated with the extraction and
monitoring of these cellular RNAs. Furthermore, fluorescent amplification of mRNA molecules from E. coli in 20 min.
sensors for detecting a variety of small molecules and cel- Viable E. coli in the water were identified and quantified
lular metabolites, including adenosine 5 -diphosphate (ADP) using a 200 nt target sequence from mRNA. The detec-
and S-adenosylmethionine (SAM), in vitro and in living cells tion limit of the biosensor system could detect around
could also be generated by combining the Spinach aptamer, 40 viable E. coli in water (5 fmol per sample) using the
a transducer, and a target-binding aptamer [215] (Fig. 6B). electrochemiluminescence (ECL) detection method. They
Reif et al. [216] recently reported another novel method introduced the isothermal amplification technique, a nucleic
to enable real-time monitoring of RNA folding and degra- acid sequence-based amplification (NASBA) for mRNA ampli-
dation in living cells based on the pRNA-3WJ. The authors fication.
designed and constructed RNA nanoparticles by incorporat- RNA was also applied to develop medical diagnosis
ing an RNA aptamer capable of binding to malachite green biosensors. Theophylline (1,3-dimethylxanthine) is a com-
(MG), the hepatitis B virus ribozyme and the luciferase siRNA mon agent in the bronchodilators and used for acute
into the pRNA 3WJ. When MG aptamer binds to MG dye, it and chronic asthma. Gothelf group developed a RNA-
will emit fluorescent light only if the aptamer folds correctly. based electrochemical biosensor for theophylline in serum
The MG aptamer system can then be used to monitor the with a ferrocence (Fc) redox probe [225,233]. In this
degradation of the constructed RNA nanoparticles by fluo- study, the thiol group-modified and amino group-modified
rescent microscopy and fluorescence spectroscopy. By using RNA aptamer was immobilized onto gold substrate via
646 H. Li et al.
Figure 6 Spinach RNA aptamer for intracellular imaging and sensing. (A) Live-cell imaging of Spinach-tagged 5S RNA[214].
Reprinted with permission from Ref. [214]. Copyright 2011 The American Association for the Advancement of Science. (B) Imaging
cellular metabolites in E. coli with sensor RNA[215]. The sensor RNA comprises Spinach (black), a transducer (orange), and a target-
binding aptamer (blue). Reprinted with permission from Ref. [215]. Copyright 2012 The American Association for the Advancement
of Science.
Figure 7 The basic constitution of RNA-based biosensor.
covalent bonding between thiol group and gold substrate. the theophylline added to RNA apatmer-modified electrode,
Then, the Fc redox probe was covalently attached to the the aptamer folds into the conformationally restricted hair-
3 -amino group of RNA aptamer through Fc-caroxylic acid pin strucutre. As a result, this phenomenon changed the
NHS reaction. Usually, the RNA aptamer stays on the open electron transfer that was monitored by cyclic and differ-
conformation in absence of theophylline. However, when ential pulse voltammetry. Moreover, specific recognition of
RNA as a stable polymer 647
Table 2 Classification of RNA polymer-based bioelectronics.
RNA-based bioelectronics References
Biocomputation devices Biologic gate [238,243]
Biomemory [238,243,266]
Bioinformation processor [242,243,245,247,248,250]
Biosensors Biomedical Sensor [215,217,221,222,225—227]
Environmental sensor [228,229]
dopamine by the RNA aptamer allows selective amperomet- [237—239]. As a result, the field of bioelectronics has
ric detection of dopamine from 100 nM to 5 M range in the been created [240,241]. Bioelectronics has led to the
presence of competitive neurotransmitters such as catechol, development of the nanoscale biochip, biosensor, and bio-
epinephrine, norepinephrine, and others [232]. computation devices such as information storage devices,
In an alternative approach, Hammond group used a RNA- logic gates, field-effect transistors and computation sys-
based fluorescent biosensors for detecting the cyclic di-GMP tems (Table 2) [242—245]. Typically, bioelectronic devices
and cyclic AMP-GMP [226]. The c-di-GMP was generated are composed of a biological actuation portion, and an
by a GEMM-I riboswitch aptamer and the riboswitch ligand electronic signal transduction portion. So far, the biologi-
mutation can recognize the c-AMP-GMP, c-di-GMP. The flu- cal component is usually composed of biomolecules, such
orescence turn-on was activated by the DFHBI fluorescent as protein and DNA [239,242,244]. Recently, some pioneer-
molecule for cell imaging. This system provided selective ing groups have suggested that the RNA-based bioelectronic
and sensitive detection for each cyclic dinucleotide. Thus, devices also exhibited the logic gate behavior, processing
there are many examples demostrating that RNA molecules functions, and biocomputations [180,246—250]. The advan-
are promising candidates for biosensor applications. tages of RNA-based computation are summarized in Fig. 8.
Biocomputation approaches for information control, stor-
age, and processing using RNA-based devices brings new
Application of RNA as a polymer in material
possibilities that embody multiple functions in biological sys-
sciences tems. The development of biological computers composed
of artificial RNA molecules to operate inside living cells
or tissues would provide a new avenue. A combination of
RNA as a polymer for biocomputation systems
these results will pave the way to develop the new-concept
of biocomputer development in the future such as tissue-
Silicon-based computer systems are ubiquitous [236] but
mimicked computations.
new processors to implement computation, communication,
and controls are needed to meet the demands of vari-
ous applications. Gordon Moore’s Law suggested that due
to the increasing demand of the memory, computer elec- RNA as a polymer for logic gates
tronic devices on the microprocessor will be doubled every
18 months. Scientists and engineers are wondering whether In computer science, the ‘logic’ term is defined as cir-
current computer technology growth can be continued in the cuits which gives an output corresponding to a set of two
next ten years. They raised the concern that silicon micro- input values (True ‘1’, High voltage and False ‘0’, Low volt-
processor speed and miniaturization will eventually reach age). The logic gate is required to have two input values
limits by current technology. Thus, molecular-scale com- for performing Boolean function [241]. Thereby, it gives
puting has been explored since 1994 due to the predictable the logical output to perform the next function. Usually,
ending of Moore’s Law for silicon-based computer devices. man-made computers consist of millions of combinational
In the last few decades, biotechnology has been inte- logic gates. Thus, logic gates are essential components of
grated with nanotechnology and electrical engineering the computer. As aforementioned, in the last few decades,
Figure 8 Advantages of RNA-based biocomputation.
648 H. Li et al.
the concept of a biomolecule-based computation system information processing devices that operate logic gates, sig-
has been proposed or explored to solve the current lim- nal filtering, and cooperativity functions have been reported
itation of silicon-based computations [246,251—255]. The [250,259,265]. RNA devices composed of ribozymes and RNA
first attempt of molecular-scale computation was devel- aptamers received, processed and transmitted the molecu-
oped by Adleman’s group in 1994 [251]. They introduced lar inputs to express the green fluorescent protein as output.
the encoded DNA molecule to solve the Hamiltonian path As a sensor part, the RNA aptamer was introduced and a
problem. This research established a milestone for the hammerhead ribozyme was used to process the cleaving of
field of biomolecule-based computations. Since then, sev- the aptamer. Also, the transmitter part was composed of
eral groups proposed the DNA polymer-based logic systems sequences that bind to the aptamer and ribozymes. It was
[252,254,255]. The basic operation mechanism of DNA-based suggested that the RNA aptamer and ribozyme combina-
logic gate is combinational DNA hybridization that undergoes tion can be used as actuating elements for multi-functional
conformational change or chemical reaction and includes information processor development [250,265].
pH, temperature, light, electrical, or electrochemical sig- An intracellular RNA computation device in a single mam-
nals [251—255]. The function of logic gate gives the discrete malian cell has also been reported [259]. Trigger-controlled
state change such as structure, fluorescence, absorbance, transcription factors were used to regulate the gene expres-
and electrochemical or electrical current as the output. sion individually and the RNA-binding protein was used to
Like this, the various types of DNA-based computations have inhibit the translation of transcripts on target RNA motifs.
been proposed. DNA, however, is hard to use to perform the This computation biosynthetic circuit can provide the NOT,
complex functions because of its simple functionality. To AND, NAND, and N-IMPLY expression functions in individual
develop the new-concept of biocomputation systems, RNA cells. Moreover, two N-IMPLY expression functions can com-
is a candidate owing to its intriguing characteristics. The bine with other cells to operate XOR gate functions and three
folding and assembly of RNA molecules drive themselves logic gates can perform the half-adder and half-subtractor
into secondary and tertiary structures using the formation of functions for arithmetic calculation.
hairpin loops, dovetails, bulges, and internal loops, etc [10].
Thereby, RNA has functionality such as aptamer, ribozyme,
RNA as a polymer for resistive biomolecular
siRNA, non-coding RNA, circular RNA, etc. [180] These var-
ious functional groups can be easily applied to the new memory
concept of logic gate behavior, information storage, infor-
mation processing, and computations as the novel elements RNA can also provide several advantages such as ease of
[256—264]. construction, well defined structure and thermodynamic
An autonomous biomolecular-based computer has been stability for the development of biomolecular memory
proposed to regulate the gene expression ‘‘logically’’ [248]. devices. Based on the discovery of the ultra-high ther-
The basic computation rule is governed by ‘diagnostic rule’ mostable pRNA-3WJ, a pRNA-3WJ/QD hybrid nanoparticle
for prostate cancer state detection. If the specific genes for resistive biomolecular memory application has been con-
relating to prostate cancer are overexpressed, then ssDNA structed [266]. The QD was used as a semiconducting part for
will bind to their mRNA and inhibits the protein synthesis. storage of the electrons and pRNA-3WJ was used as an insu-
The level of specific RNA and the concentration of spe- lating part and serves as the bridge between QD and metal
cific molecule which regulates the point mutations were substrate. The electrical measurement (I—V) was conducted
regarded as an input. The release of short ssDNA modu- to this hybrid structure for resistive memory performances.
lated the levels of gene expression for anticancer activity, This study showed the RNA polymer conjugates can be used
as the output logically. The computation module has two directly for molecular memory device fabrication.
states, ‘‘positive’’ and ‘‘negative’’, in response to the level
of specific gene expression. This biocomputation concept is
Hybrid RNA polymers as semiconductors
related with the identification of mRNAs of disease-related
genes. Thereby, it can be applied to cancer diagnosis systems
based on logic analysis. Biomolecular hybrids of a conducting polymer [poly(O-
A RNAi-based logic evaluator has also been reported to methoxy aniline) (POMA)] and dsRNA have been reported
perform Boolean logic corresponding to input molecules in as semiconductors [267]. Fourier transform infrared spec-
the human kidney cells [249]. The reported biological circuit troscopy (FTIR) indicated that these hybrid polymers are
is composed of several mRNA species that encode the same held together by electrostatic, H-bonding, and pi—pi inter-
protein but have different non-coding regions. This protein actions. The circular dichroism spectra of the hybrid
served as the output. As an input, siRNAs were used to con- polymers indicated that the dsRNA underwent a small dis-
trol the degradation of the target mRNA and the expression tortion in conformation from the canonical A-form towards
of the output protein. Expressions with up to five logic vari- the B-form during the formation of the hybrid polymers. TEM
ables were directly evaluated by this system. micrographs revealed that these polymers create a fibrillar
network structure. The conductivity values of the POMA-RNA
hybrids were three orders of magnitude higher than that of
RNA as a polymer for information processor RNA alone. The I—V curves of the POMA-RNA hybrid poly-
mers also demostrated a semiconducting nature. Based on
these physical characteristics, the POMA-RNA hybrids have
In computer sciences, the information processor is a unit
the potential to be candidates for fabricating biosensors for
that receives the input information and processes it into
other applications.
another form based on programmed functions. RNA-based
RNA as a stable polymer 649
Conjugation of RNA to graphene polymeric building block [36] into a new horizon. The con-
cern of yield and production costs has been and will be
Graphene is a one-atom thick, two-dimensional honeycomb addressed continually by industry scale production and fer-
2
lattice composed of sp -bonded carbon atoms. It can be mentation. It is expected that applications of RNA as a
used as a fundamental building block for constructing other polymer and as building blocks will appear more and more
graphite-based structures such as fullerenes and nanotubes in therapeutics, detection, sensing, nanoelectronic devices,
[268,269]. This newly discovered carbon-based material has and other polymer industries. The anion nature, the thermo-
been a popular subject in material science and nanotechnol- dynamic stability, the insulating property, the self-assembly
ogy. It has been used for the sensing of a toxin Microcystin-LR capability and other novel features such as versatility,
in water [270—273]. RNA aptamer have been covalently molecular-level plasticity, as well as the potential semicon-
immobilized on graphene oxide and a polydispersed sta- ductor behavior will make RNA unique for exploring new
ble RNA-graphene oxide nanosheet have been constructed scientific territories. RNA has been shown to be major com-
[274]. The RNA attached to these nanosheets was resistant ponents of cells and leading functionality of life, and it is
to nuclease degradation and the nanosheets competitively expected that RNA will also be the momentous material of
absorbed trace amounts of the peptide toxin microcystin- daily life in the future.
LR from drinking water. PEI-grafted graphene oxide was also
used to deliver short interfering RNA (siRNA) as well as anti- Acknowledgements
cancer drug doxorubicin to cancer cells [275]. RNA has also
been used as a surfactant to exfoliate flakes of graphene
This work was supported by grants EB019036, EB003730,
from nanocrystalline graphite to produce transparent and
EB012135 from NIH/NIBIB and CA151648 from NIH/NCI to
conducting RNA-graphene-based thin films [276], which has
P.G., Leading Foreign Research Institute Recruitment Pro-
a potential for a variety of electronic applications. Further
gram through the National Research Foundation of Korea
research in RNA-graphene nanocomposites may open a new
(NRF) funded by the Ministry of Science, ICT & Future
avenue towards many applications of graphene-based con-
Planning (MSIP) (2013K1A4A3055268) to T.L., National Dis-
ductive materials.
tinguished Young Scholars grant (NSFC No: 31225009) and
the ‘‘Strategic Priority Research Program’’ of the Chinese
Conjugation of RNA with other nanoparticles Academy of Sciences Grant no. XDA09030301 to X.L. The
funding to P.G.’s Endowed Chair in Nanobiotechnology posi-
The conjugation of a RNA with nanoparticles such as quan- tion is from the William Fairish Endowment Fund. P.G. is
tum dot, iron oxide nanoparticle or gold nanoparticle has the cofounder of Biomotor and RNA Nanotechnology Devel-
been successfully demonstrated by a series of studies for opment Corp. Ltd. We would like to thank Dr. Richard N.
nanosized imaging, therapy and diagnosis [277—282]. For Greenberg, Dr. Daniel W. Pack, Dr. Yi Shu and Dr. Ashwani
example, siRNA and tumor-homing peptides (F3) were conju- Sharma for their constructive comments.
gated to the PEGylated QD core as a scaffold [278,279]. The
complex was efficiently delivered to HeLa cells, released
References
from the endosomal compartment, and triggered knockdown
of EGFP signal. This leads to dual purpose of treatment
[1] C.E. Carraher, Carraher’s Polymer Chemistry, ninth ed., CRC
and imaging. In another case, siRNA was also conjugated
Press, FL, 2013.
to the iron oxide nanoparticle [280,282] for dual purpose:
[2] C. Tsenoglou, Macromolecules 24 (1991) 1762—1767.
(1) in vivo transfer of siRNA and (2) imaging the accumula-
[3] P. Cassagnau, J.P. Montfort, G. Marin, P. Monge, Rheol. Acta
tion of siRNA in tumor through magnetic resonance imaging
32 (1993) 156—167.
(MRI) and near-infrared in vivo optical imaging (NIRF) using
[4] N. Badi, J.F. Lutz, Chem. Soc. Rev. 38 (2009) 3383—3390.
near-infrared Cy5.5 dye. Another report showed that the [5] J.M. Lehn, Polym. Int. 51 (2002) 825—839.
conjugation of gold nanoparticle and RNA also increased the [6] D.A. Tomalia, Prog. Polym. Sci. 30 (2005) 294—324.
availability of the tethered RNA splicing enhancer [283]. [7] J.F. Lutz, Polym. Chem. 1 (2010) 55—62.
In 2007, the pRNA of the phage phi29 DNA-packaging [8] E. Westhof, B. Masquida, L. Jaeger, Fold Des. 1 (1996)
R78—R88.
motor was conjugated to the gold nanoparticles via a
[9] F.J. Isaacs, Nat. Chem. Biol. 8 (2012) 413—415.
thiol group for single particle quantification in bacterial
[10] L. Jaeger, A. Chworos, Curr. Opin. Struct. Biol. 16 (2006)
virus assembly [281]. The pRNA-gold nanoparticle conju-
531—543.
gates were bound to procapsid by in vitro phage assembly.
[11] N.B. Leontis, A. Lescoute, E. Westhof, Curr. Opin. Struct. Biol.
The results demonstrated the feasibility in using RNA-gold
16 (2006) 279—287.
nanoparticle for single molecule imaging and counting of
[12] A. Lescoute, E. Westhof, Nucleic Acids Res. 34 (2006)
biological machines. 6587—6604.
[13] A. Lescoute, E. Westhof, RNA 12 (2006) 83—93.
Prospects [14] W.W. Grabow, L. Jaeger, Acc. Chem. Res. 47 (2014)
1871—1880.
[15] G. Widawski, M. Rawiso, B. Francois, Nature 369 (1994)
RNA is a polymer by nature. Recent technological advances 387—389.
to make RNA chemically and enzymatically stable [65,66] [16] J. Roovers, P.M. Toporowski, Macromolecules 16 (1983)
and the discovery of unusual thermostability of some 843—849.
RNA motifs, as well as important biomedical applications [17] S.G. Gaynor, S. Edelman, K. Matyjaszewski, Macromolecules
29 (1996) 1079—1081.
[123—126,284] have propelled the concept of RNA as a
650 H. Li et al.
[18] K. Inoue, Prog. Polym. Sci. 25 (2000) 453—571. [55] R. Parker, H.W. Song, Nat. Struct. Mol. Biol. 11 (2004)
[19] C.C. Lee, J.A. MacKay, J.M. Frechet, F.C. Szoka, Nat. Bio- 121—127.
technol. 23 (2005) 1517—1526. [56] C.A. Beelman, R. Parker, Cell 81 (1995) 179—183.
[20] K.L. Wooley, J. Polym. Sci., A: Polym. Chem. 38 (2000) [57] M. Ha, V.N. Kim, Nat. Rev. Mol. Cell. Biol. 15 (2014) 509—524.
1397—1407. [58] J. Krol, I. Loedige, W. Filipowicz, Nat Rev. Genet. 11 (2010)
[21] A.D. Schluter, M. Loffler, V. Enkelmann, Nature 368 (1994) 597—610.
831—834. [59] E. Abernathy, B. Glaunsinger, Virology 479-480 (2015)
[22] J.M.J. Frechet, Science 263 (1994) 1710—1715. 600—608.
[23] L.Y. Qiu, Y.H. Bae, Pharm. Res. 23 (2006) 1—30. [60] M.A. Carmell, G.J. Hannon, Nat. Struct. Mol. Biol. 11 (2004)
[24] G. Varani, W.H. McClain, EMBO Rep. 1 (2000) 18—23. 214—218.
[25] U. Nagaswamy, M. Larios-Sanz, J. Hury, S. Collins, Z. Zhang, [61] D. Yang, F. Buchholz, Z. Huang, A. Goga, C.Y. Chen, F.M.
Q. Zhao, G.E. Fox, Nucleic Acids Res. 30 (2002) 395—397. Brodsky, J.M. Bishop, Proc. Natl. Acad. Sci. U.S.A. 99 (2002)
[26] S. Lemieux, F. Major, Nucleic Acids Res. 30 (2002) 4250—4263. 9942—9947.
[27] N.B. Leontis, J. Stombaugh, E. Westhof, Nucleic Acids Res. 30 [62] W.M. Li, T. Barnes, C.H. Lee, FEBS J. 277 (2010) 627—641.
(2002) 3497—3531. [63] Y. Zuo, M.P. Deutscher, Nucleic Acids Res. 29 (2001)
[28] H. Yang, F. Jossinet, N. Leontis, L. Chen, J. Westbrook, H. 1017—1026.
Berman, E. Westhof, Nucleic Acids Res. 31 (2003) 3450—3460. [64] W.A. Pieken, D.B. Olsen, F. Benseler, H. Aurup, F. Eckstein,
[29] Y. Xin, C. Laing, N.B. Leontis, T. Schlick, RNA 14 (2008) Science 253 (1991) 314—317.
2465—2477. [65] A.M. Kawasaki, M.D. Casper, S.M. Freier, E.A. Lesnik, M.C.
[30] C. Laing, S. Jung, N. Kim, S. Elmetwaly, M. Zahran, T. Schlick, Zounes, L.L. Cummins, C. Gonzalez, P.D. Cook, J. Med. Chem.
PLoS ONE 8 (2013) e71947. 36 (1993) 831—841.
[31] C. Laing, D. Wen, J.T. Wang, T. Schlick, Nucleic Acids Res. 40 [66] J. Liu, S. Guo, M. Cinier, L.S. Shlyakhtenko, Y. Shu, C. Chen,
(2012) 487—498. G. Shen, P. Guo, ACS Nano 5 (2011) 237—246.
[32] N. Salim, R. Lamichhane, R. Zhao, T. Banerjee, J. Philip, D. [67] J. Hong, Y. Huang, J. Li, F. Yi, J. Zheng, H. Huang, N. Wei, Y.
Rueda, A.L. Feig, Biophys. J. 102 (2012) 1097—1107. Shan, M. An, H. Zhang, FASEB J. 24 (2010) 4844—4855.
[33] R.G. Gilbert, M. Hess, A.D. Jenkins, R.G. Jones, R. Kratochvil, [68] J. Hu, G. Zhang, S. Liu, Chem. Soc. Rev. 41 (2012)
R.F.T. Stepto, Pure Appl. Chem. 81 (2009) 779. 5933—5949.
[34] M. Rogosic, H.J. Mencer, Z. Gomzi, Eur. Polym. J. 32 (1996) [69] Q. Hu, P.S. Katti, Z. Gu, Nanoscale 6 (2014) 12273—12286.
1337—1344. [70] C. Zhang, D. Pan, K. Luo, W. She, C. Guo, Y. Yang, Z. Gu, Adv.
[35] J.M. Margolis, Engineering Thermoplastics: Properties and Healthcare Mater. 3 (2014) 1299—1308.
Applications, Marcel Dekker, Inc, New York, NY, 1985. [71] A.J. Harnoy, I. Rosenbaum, E. Tirosh, Y. Ebenstein, R. Sha-
[36] E.F. Khisamutdinov, D.L. Jasinski, P. Guo, ACS Nano 8 (2014) harabani, R. Beck, R.J. Amir, J. Am. Chem. Soc. 136 (2014)
4771—4781. 7531—7534.
[37] J.C. Middleton, A.J. Tipton, Biomaterials 21 (2000) [72] D.G. Anderson, A. Akinc, N. Hossain, R. Langer, Mol. Ther. 11
2335—2346. (2005) 426—434.
[38] S. Ramakrishna, J. Mayer, E. Wintermantel, K.W. Leong, Com- [73] F. Haque, D. Shu, Y. Shu, L. Shlyakhtenko, P. Rychahou, M.
pos. Sci. Technol. 61 (2001) 1189—1224. Evers, P. Guo, Nano Today 7 (2012) 245—257.
[39] Y. Ikada, Biomaterials 15 (1994) 725—736. [74] Y. Shu, F. Pi, A. Sharma, M. Rajabi, F. Haque, D. Shu, M. Leggas,
[40] J. Jagur-Grodzinski, Polym. Adv. Technol. 17 (2006) 395—418. B.M. Evers, P. Guo, Adv. Drug Delivery Rev. 66C (2014) 74—89.
[41] F. Hussain, M. Hojjati, M. Okamoto, R.E. Gorga, J. Compos. [75] S.E. Butcher, A.M. Pyle, Acc. Chem. Res. 44 (2011)
Mater. 40 (2006) 1511—1575. 1302—1311.
[42] Y.J. Liu, H.B. Lv, X. Lan, J.S. Leng, S.Y. Du, Compos. Sci. [76] C. Laing, T. Schlick, J. Mol. Biol. 390 (2009) 547—559.
Technol. 69 (2009) 2064—2068. [77] D.M. Lilley, Q. Rev. Biophys. 33 (2000) 109—159.
[43] M. Shahinpoor, K.J. Kim, Smart Mater. Struct. 14 (2005) [78] D. Klostermeier, D.P. Millar, Biochemistry 39 (2000)
197—214. 12970—12978.
[44] W.U. Huynh, J.J. Dittmer, A.P. Alivisatos, Science 295 (2002) [79] C. Altona, J. Mol. Biol. 263 (1996) 568—581.
2425—2427. [80] D.R. Duckett, A.I. Murchie, D.M. Lilley, Cell 83 (1995)
[45] G. Dennler, M.C. Scharber, C.J. Brabec, Adv. Mater. 21 (2009) 1027—1036.
1323—1338. [81] A. Lamiable, D. Barth, A. Denise, F. Quessette, S. Vial, E.
[46] K. Bock, Proc. IEEE 93 (2005) 1400—1406. Westhof, Comput. Biol. Chem. 37 (2012) 1—5.
[47] J.J. Wang, L. Sun, K. Mpoukouvalas, K. Lienkamp, I. Lieber- [82] I. Besseova, K. Reblova, N.B. Leontis, J. Sponer, Nucleic Acids
wirth, B. Fassbender, E. Bonaccurso, G. Brunklaus, A. Res. 38 (2010) 6247—6264.
Muehlebach, T. Beierlein, R. Tilch, H.J. Butt, G. Wegner, Adv. [83] D.H. Mathews, D.H. Turner, Biochemistry 41 (2002) 869—880.
Mater. 21 (2009) 1137—1141. [84] J.M. Diamond, D.H. Turner, D.H. Mathews, Biochemistry 40
[48] I.D.W. Samuel, Philos. Trans. R. Soc. London, Ser. A—–Math. (2001) 6971—6981.
Phys. Eng. Sci. 358 (2000) 193—210. [85] J.A. Abels, F. Moreno-Herrero, T. van der Heijden, C.F. Dekker,
[49] A. Dodabalapur, Mater. Today 9 (2006) 24—30. N.H. Dekker, Biophys J. 88 (2005) 2737—2744.
[50] W. Clemens, I. Fix, J. Ficker, A. Knobloch, A. Ullmann, J. [86] C. Bustamante, S.B. Smith, J. Liphardt, D. Smith, Curr. Opin.
Mater. Res. 19 (2004) 1963—1973. Struct. Biol. 10 (2000) 279—285.
[51] D.M. Lilley, Trends Biochem. Sci. 28 (2003) 495—501. [87] J. Lipfert, G.M. Skinner, J.M. Keegstra, T. Hensgens, T. Jager,
[52] N. Sugimoto, S. Nakano, M. Katoh, A. Matsumura, H. Naka- D. Dulin, M. Kober, Z. Yu, S.P. Donkers, F.C. Chou, R. Das, N.H.
muta, T. Ohmichi, M. Yoneyama, M. Sasaki, Biochemistry 34 Dekker, Proc. Natl. Acad. Sci. U.S.A. 111 (2014) 15408—15413.
(1995) 11211—11216. [88] H.C. Chiu, K. Koh, M. Evich, A. Lesiak, Nanoscale 6 (2014)
[53] R. Schroeder, A. Barta, K. Semrad, Nat. Rev. Mol. Cell Biol. 5 10009—10017.
(2004) 908—919. [89] H.M. Al-Hashimi, S.W. Pitt, A. Majumdar, W.J. Xu, D.J. Patel,
[54] H. Zhang, J.A. Endrizzi, Y. Shu, F. Haque, C. Sauter, L.S. J. Mol. Biol. 329 (2003) 867—873.
Shlyakhtenko, Y. Lyubchenko, P. Guo, Y.I. Chi, RNA 19 (2013) [90] A. Mustoe, C. Brooks, H.M. Al-Hashimi, Ann. Rev. Biochem. 83
1226—1237. (2014) 441—466.
RNA as a stable polymer 651
[91] H. Chen, S.P. Meisburger, S.A. Pabit, J.L. Sutton, W.W. [127] H. Ohno, T. Kobayashi, R. Kabata, K. Endo, T. Iwasa, S.H.
Webb, L. Pollack, Proc. Natl. Acad. Sci. U.S.A. 109 (2012) Yoshimura, K. Takeyasu, T. Inoue, H. Saito, Nat. Nanotechnol.
799—804. 6 (2011) 116—120.
[92] E. Khisamutdinov, H. Li, D. Jasinski, J. Chen, J. Fu, P. Guo, [128] T. Moore, Y. Zhang, M.O. Fenley, H. Li, Structure 12 (2004)
Nucleic Acids Res. 42 (2014) 9996—10004. 807—818.
[93] S.M. Dibrov, J. McLean, J. Parsons, T. Hermann, Proc. Natl. [129] E. Osada, Y. Suzuki, K. Hidaka, H. Ohno, H. Sugiyama, M.
Acad. Sci. U.S.A. 108 (2011) 6405—6408. Endo, H. Saito, ACS Nano 8 (2014) 8130—8140.
[94] C. Schwartz, G.M. De Donatis, H. Zhang, H. Fang, P. Guo, [130] P.W.K. Rothemund, Nature 440 (2006) 297—302.
Virology 443 (2013) 28—39. [131] F.A. Aldaye, A.L. Palmer, H.F. Sleiman, Science 321 (2008)
[95] C. Schwartz, G.M. De Donatis, H. Fang, P. Guo, Virology 443 1795—1799.
(2013) 20—27. [132] N.C. Seeman, Annu. Rev. Biochem. 79 (2010) 65—87.
[96] Z. Zhao, E. Khisamutdinov, C. Schwartz, P. Guo, ACS Nano 7 [133] F. Zhang, J. Nangreave, Y. Liu, H. Yan, J. Am. Chem. Soc. 136
(2013) 4082—4092. (2014) 11198—11211.
[97] P. Guo, C. Schwartz, J. Haak, Z. Zhao, Virology 446 (2013) [134] M.R. Jones, N.C. Seeman, C.A. Mirkin, Science 347 (2015)
133—143. 1260901.
[98] P. Guo, Biophys. J. 106 (2014) 1837—1838. [135] Y.R. Yang, Y. Liu, H. Yan, Bioconjug. Chem. 26 (2015)
[99] G. De-Donatis, Z. Zhao, S. Wang, P.L. Huang, C. Schwartz, V.O. 1381—1395.
Tsodikov, H. Zhang, F. Haque, P. Guo, Cell Biosci. 4 (2014) 30. [136] C. Geary, P. W. Rothemund, E.S. Andersen, Science 345 (2014)
[100] P. Guo, Z. Zhao, J. Haak, S. Wang, D. Wu, B. Meng, T. Weitao, 799—804.
Biotechnol. Adv. 32 (2014) 853—872. [137] C. Lorenz, N. Piganeau, R. Schroeder, Nucleic Acids Res. 34
[101] S. Wang, F. Haque, P.G. Rychahou, B.M. Evers, P. Guo, ACS (2006) 334—342.
Nano 7 (2013) 9814—9822. [138] N. Leulliot, V. Baumruk, M. Abdelkafi, P. Y. Turpin, A. Namane,
[102] D. Shu, F. Pi, C. Wang, P. Zhang, P. Guo, Nanomedicine 10 C. Gouyette, T. Huynh-Dinh, M. Ghomi, Nucleic Acids Res. 27
(2015) 1881—1897. (1999) 1398—1404.
[103] Y. Mat-Arip, K. Garver, C. Chen, S. Sheng, Z. Shao, P. Guo, J. [139] M. Endo, Y. Takeuchi, T. Emura, K. Hidaka, H. Sugiyama,
Biol. Chem. 276 (2001) 32575—32584. Chem.-Eur. J. 20 (2014) 15330—15333.
[104] M. Trottier, Y. Mat-Arip, C. Zhang, C. Chen, S. Sheng, Z. Shao, [140] K.A. Afonin, M. Viard, A.N. Martins, S.J. Lockett, A.E. Maciag,
P. Guo, RNA 6 (2000) 1257—1266. E.O. Freed, E. Heldman, L. Jaeger, R. Blumenthal, B.A.
[105] C. Chen, S. Sheng, Z. Shao, P. Guo, J. Biol. Chem. 275 (23) Shapiro, Nat. Nanotechnol. 8 (2013) 296—304.
(2000) 17510—17516. [141] K.A. Afonin, R. Desai, M. Viard, M.L. Kireeva, E.
[106] D. Shu, L. Huang, S. Hoeprich, P. Guo, J. Nanosci. Nanotech- Bindewald, C.L. Case, A.E. Maciag, W.K. Kasprzak, T.
nol. 3 (2003) 295—302. Kim, A. Sappe, M. Stepler, V.N. Kewalramani, M. Kashlev,
[107] C. Chen, C. Zhang, P. Guo, RNA 5 (1999) 805—818. R. Blumenthal, B.A. Shapiro, Nucleic Acids Res. 42 (2014)
[108] S. Guo, N. Tschammer, S. Mohammed, P. Guo, Hum. Gene 2085—2097.
Ther. 16 (2005) 1097—1109. [142] K.A. Afonin, E. Bindewald, M. Kireeva, B.A. Shapiro, Methods
[109] Y. Shu, M. Cinier, D. Shu, P. Guo, Methods 54 (2011) 204—214. Enzymol. 553 (2015) 313—334.
[110] P. Guo, C. Zhang, C. Chen, M. Trottier, K. Garver, Mol. Cell 2 [143] K.A. Afonin, W.K. Kasprzak, E. Bindewald, M. Kireeva, M.
(1998) 149—155. Viard, M. Kashlev, B.A. Shapiro, Acc. Chem. Res. 47 (2014)
[111] A. Khaled, S. Guo, F. Li, P. Guo, Nano Lett. 5 (2005) 1731—1741.
1797—1808. [144] K.A. Afonin, E. Bindewald, A.J. Yaghoubian, N. Voss, E. Jacov-
[112] D. Shu, W.D. Moll, Z. Deng, C. Mao, P. Guo, Nano Lett. 4 (2004) etty, B.A. Shapiro, L. Jaeger, Nat. Nanotechnol. 5 (2010)
1717—1723. 676—682.
[113] Y. Shu, F. Haque, D. Shu, W. Li, Z. Zhu, M. Kotb, Y. Lyubchenko, [145] K.A. Afonin, W.W. Grabow, F.M. Walker, E. Bindewald, M.A.
P. Guo, RNA 19 (2013) 766—777. Dobrovolskaia, B.A. Shapiro, L. Jaeger, Nat. Protoc. 6 (2011)
[114] Y.G. Yingling, B.A. Shapiro, Nano Lett. 7 (2007) 2328—2334. 2022—2034.
[115] W.W. Grabow, P. Zakrevsky, K.A. Afonin, A. Chworos, B.A. [146] K.A. Afonin, M. Viard, A.Y. Koyfman, A.N. Martins, W.K.
Shapiro, L. Jaeger, Nano Lett. 11 (2011) 878—887. Kasprzak, M. Panigaj, R. Desai, A. Santhanam, W.W. Grabow,
[116] A. Chworos, I. Severcan, A.Y. Koyfman, P. Weinkam, E. Oroud- L. Jaeger, E. Heldman, J. Reiser, W. Chiu, E.O. Freed, B.A.
jev, H.G. Hansma, L. Jaeger, Science 306 (2004) 2068—2072. Shapiro, Nano Lett. 14 (2014) 5662—5671.
[117] I. Severcan, C.V.E.C.A. Geary, L. Jaeger, Nano Lett. 9 (2009) [147] J.B. Lee, J. Hong, D.K. Bonner, Z. Poon, P. T. Hammond, Nat.
1270—1277. Mater. 11 (2012) 316—322.
[118] I. Severcan, C. Geary, A. Chworos, N. Voss, E. Jacovetty, L. [148] K.E. Shopsowitz, Y.H. Roh, Z.J. Deng, S.W. Morton, P. T. Ham-
Jaeger, Nat. Chem. 2 (2010) 772—779. mond, Small 10 (2014) 1623—1633.
[119] L. Jaeger, N.B. Leontis, Angew. Chem Int. Ed. Engl. 39 (2000) [149] S.M. Moghimi, P. Symonds, J.C. Murray, A.C. Hunter, G. Deb-
2521—2524. ska, A. Szewczyk, Mol. Ther. 11 (2005) 990—995.
[120] L. Nasalean, S. Baudrey, N.B. Leontis, L. Jaeger, Nucleic Acids [150] A. Beyerle, M. Irmler, J. Beckers, T. Kissel, T. Stoeger, Mol.
Res. 34 (2006) 1381—1392. Pharm. 7 (2010) 727—737.
[121] C. Hao, X. Li, C. Tian, W. Jiang, G. Wang, C. Mao, Nat. Com- [151] M. Ulbricht, Polymer 47 (2006) 2217—2262.
mun. 5 (2014) 3890. [152] D. Han, Y. Park, H. Kim, J.B. Lee, Nat. Commun. 5 (2014)
[122] P. Guo, S. Erickson, D. Anderson, Science 236 (1987) 690—694. 4367.
[123] D. Shu, Y. Shu, F. Haque, S. Abdelmawla, P. Guo, Nat. Nan- [153] D.R. Corey, J. Clin. Invest. 117 (2007) 3615—3622.
otechnol. 6 (2011) 658—667. [154] M.A. Behlke, Oligonucleotides 18 (2008) 305—319.
[124] Y. Shu, D. Shu, F. Haque, P. Guo, Nat. Protoc. 8 (2013) [155] J.B. Bramsen, J. Kjems, Front. Genet. 3 (2012) 154.
1635—1659. [156] L. Zangi, K.O. Lui, G.A. von, Q. Ma, W. Ebina, L.M. Ptaszek,
[125] D. Jasinski, E.F. Khisamutdinov, Y.L. Lyubchenko, P. Guo, ACS D. Spater, H. Xu, M. Tabebordbar, R. Gorbatov, B. Sena,
Nano 8 (2014) 7620—7629. M. Nahrendorf, D.M. Briscoe, R.A. Li, A.J. Wagers, D.J.
[126] D. Shu, L. Zhang, E. Khisamutdinov, P. Guo, Nucleic Acids Res. Rossi, W.T. Pu, K.R. Chien, Nat. Biotechnol. 31 (2013)
42 (2013) e10. 898—907.
652 H. Li et al.
[157] D.A. Braasch, Z. Paroo, A. Constantinescu, G. Ren, O.K. Oz, [187] S. Hoeprich, Q. ZHou, S. Guo, G. Qi, Y. Wang, P. Guo, Gene
R.P. Mason, D.R. Corey, Bioorg. Med. Chem. Lett. 14 (2004) Ther. 10 (2003) 1258—1267.
1139—1143. [188] S. Guo, F. Huang, P. Guo, Gene Ther. 13 (2006) 814—820.
[158] A.H. Hall, J. Wan, E.E. Shaughnessy, S.B. Ramsay, K.A. Alexan- [189] H.M. Zhang, Y. Su, S. Guo, J. Yuan, T. Lim, J. Liu, P. Guo, D.
der, Nucleic Acids Res. 32 (2004) 5991—6000. Yang, Antiviral Res. 83 (2009) 307—316.
[159] A.M. Awad, M. Sobkowski, H. Seliger, Nucleosides Nucleotides [190] K.A. Afonin, M. Viard, I. Kagiampakis, C.L. Case, M.A. Dobro-
Nucleic Acids 23 (2004) 777—787. volskaia, J. Hofmann, A. Vrzak, M. Kireeva, W.K. Kasprzak,
[160] M.A. Reynolds, R.I. Hogrefe, J.A. Jaeger, D.A. Schwartz, T.A. V.N. KewalRamani, ACS Nano 9 (2015) 251—259.
Riley, W.B. Marvin, W.J. Daily, M.M. Vaghefi, T.A. Beck, S.K. [191] J.L. Rouge, L.L. Hao, X.C.A. Wu, W.E. Briley, C.A. Mirkin, ACS
Knowles, R.E. Klem, L.J. Arnold Jr., Nucleic Acids Res. 24 Nano 8 (2014) 8837—8843.
(1996) 4584—4591. [192] S.A. Jensen, E.S. Day, C.H. Ko, L.A. Hurley, J.P. Luciano, F.M.
[161] M. Amarzguioui, T. Holen, E. Babaie, H. Prydz, Nucleic Acids Kouri, T.J. Merkel, A.J. Luthi, P.C. Patel, J.I. Cutler, W.L.
Res. 31 (2003) 589—595. Daniel, A.W. Scott, M.W. Rotz, T.J. Meade, D.A. Giljohann,
[162] S. Choung, Y.J. Kim, S. Kim, H.O. Park, Y.C. Choi, Biochem. C.A. Mirkin, A.H. Stegh, Sci. Transl. Med. 5 (2013) 209ra152.
Biophys. Res. Commun. 342 (2006) 919—927. [193] Q. Jiang, C. Song, J. Nangreave, X. Liu, L. Lin, D. Qiu, Z.G.
[163] D.W. Binzel, E.F. Khisamutdinov, P. Guo, Biochemistry 53 Wang, G. Zou, X. Liang, H. Yan, J. Am. Chem. Soc. 134 (2012)
(2014) 2221—2231. 13396—13403.
[164] T.J. Lee, F. Haque, D. Shu, J.Y. Yoo, H. Li, R.A. Yokel, C. [194] Q. Zhang, Q. Jiang, N. Li, L. Dai, Q. Liu, L. Song, J. Wang, Y.
Horbinski, T.H. Kim, S.-H. Kim, I. Nakano, B. Kaur, C.M. Croce, Li, J. Tian, B. Ding, ACS Nano 8 (2014) 6633—6643.
P. Guo, Oncotarget 6 (2015) 14766—14776. [195] E. Hood, E. Simone, P. Wattamwar, T. Dziubla, V. Muzykantov,
[165] P. Rychahou, F. Haque, Y. Shu, Y. Zaytseva, H.L. Weiss, E.Y. Nanomedicine (Lond) 6 (2011) 1257—1272.
Lee, W. Mustain, J. Valentino, P. Guo, B.M. Evers, ACS Nano 9 [196] T. Teesalu, K.N. Sugahara, E. Ruoslahti, Methods Enzymol. 503
(2015) 1108—1116. (2012) 35.
[166] T.J. Lee, F. Haque, M. Vieweger, J.Y. Yoo, B. Kaur, P. Guo, C.M. [197] M. Dan, D.B. Cochran, R.A. Yokel, T.D. Dziubla, PLoS ONE 8
Croce, Methods Mol. Biol. 1297 (2015) 137—152. (2013) e81051.
[167] D. Cui, C. Zhang, B. Liu, Y. Shu, T. Du, D. Shu, K. Wang, F. Dai, [198] S. Muro, R. Wiewrodt, A. Thomas, L. Koniaris, S.M. Albelda,
Y. Liu, C. Li, F. Pan, Y. Yang, J. Ni, H. Li, B. Brand-Saberi, P. V.R. Muzykantov, M. Koval, J. Cell Sci. 116 (2003) 1599—1609.
Guo, Sci. Rep. 5 (2015) 10726. [199] T. Bhowmick, E. Berk, X. Cui, V.R. Muzykantov, S. Muro, J.
[168] H. Li, P.G. Rychahou, Z. Cui, F. Pi, B.M. Evers, D. Shu, P. Guo, Controlled Release 157 (2012) 485—492.
W. Luo, Nucleic Acid Ther. 25 (2015) 188—197. [200] A.J. Calderon, T. Bhowmick, J. Leferovich, B. Burman, B.
[169] J.K. Watts, N. Choubdar, K. Sadalapure, F. Robert, A.S. Pichette, V. Muzykantov, D.M. Eckmann, S. Muro, J. Controlled
Wahba, J. Pelletier, B.M. Pinto, M.J. Damha, Nucleic Acids Release 150 (2011) 37—44.
Res. 35 (2007) 1441—1451. [201] S. Muro, T. Dziubla, W. Qiu, J. Leferovich, X. Cui, E.
[170] M. Petersen, J. Wengel, Trends Biotechnol. 21 (2003) 74—81. Berk, V.R. Muzykantov, J. Pharmacol. Exp. Ther. 317 (2006)
[171] I.K. Astakhova, J. Wengel, Acc. Chem. Res. 47 (2014) 1161—1169.
1768—1777. [202] M.D. Howard, E.D. Hood, C.F. Greineder, I.S. Alferiev,
[172] J. Elmen, H. Thonberg, K. Ljungberg, M. Frieden, M. West- M. Chorny, V. Muzykantov, Mol. Pharmaceutics 11 (2014)
ergaard, Y. Xu, B. Wahren, Z. Liang, H. Orum, T. Koch, C. 2262—2270.
Wahlestedt, Nucleic Acids Res. 33 (2005) 439—447. [203] M.A. McAteer, N.R. Sibson, C. von zur Muhlen, J.E. Schnei-
[173] D. Shu, H. Li, Y. Shu, G. Xiong, W.E. Carson, R. Xu, F. der, A.S. Lowe, N. Warrick, K.M. Channon, D.C. Anthony, R.P.
Haque, P. Guo, ACS Nano (2015), http://dx.doi.org/10.1021/ Choudhury, Nat. Med. 13 (2007) 1253—1258.
acsnano.5b02471 (Accepted). [204] H. Yang, F. Zhao, Y. Li, M. Xu, L. Li, C. Wu, H. Miyoshi, Y. Liu,
[174] E.E. Swayze, A.M. Siwkowski, E.V. Wancewicz, M.T. Migawa, Int. J. Nanomed. 8 (2013) 1897.
T.K. Wyrzykiewicz, G. Hung, B.P. Monia, C.F. Bennett, Nucleic [205] M. Christofidou-Solomidou, S. Kennel, A. Scherpereel, R.
Acids Res. 35 (2007) 687—700. Wiewrodt, C.C. Solomides, G.G. Pietra, J.C. Murciano, S.A.
[175] N. Langkjar, A. Pasternak, J. Wengel, Bioorg. Med. Chem. 17 Shah, H. Ischiropoulos, S.M. Albelda, Am. J. Pathol. 160 (2002)
(2009) 5420—5425. 1155—1169.
[176] J.K. Watts, G.F. Deleavey, M.J. Damha, Drug Discovery Today [206] C. Garnacho, R. Dhami, E. Simone, T. Dziubla, J. Leferovich,
13 (2008) 842—855. E.H. Schuchman, V. Muzykantov, S. Muro, J. Pharmacol. Exp.
[177] H. Peacock, A. Kannan, P.A. Beal, C.J. Burrows, J. Org. Chem. Ther. 325 (2008) 400—408.
76 (2011) 7295—7300. [207] T.M. Maul, D.D. Dudgeon, M.T. Beste, D.A. Hammer, J.S. Lazo,
[178] M. Fisher, M. Abramov, A.A. Van, J. Rozenski, V. Dixit, R.L. F.S. Villanueva, W.R. Wagner, Biotechnol. Bioeng. 107 (2010)
Juliano, P. Herdewijn, Eur. J. Pharmacol. 606 (2009) 38—44. 854—864.
[179] S. Shah, S. Rangarajan, S.H. Friedman, Angew. Chem. Int. Ed. [208] W.C. Aird, Crit. Care Med. 31 (2003) S221—S230.
Engl. 44 (2005) 1328—1332. [209] J. Voigt, J. Christensen, V. P. Shastri, Proc. Natl. Acad. Sci.
[180] P. Guo, Nat. Nanotechnol. 5 (2010) 833—842. U.S.A. 111 (2014) 2942—2947.
[181] M. Zuker, P. Stiegler, Nucleic Acids Res. 9 (1981) 133—148. [210] V. Bagalkot, L. Zhang, E. Levy-Nissenbaum, S. Jon, P. W.
[182] E. Bindewald, K. Afonin, L. Jaeger, B.A. Shapiro, ACS Nano 5 Kantoff, R. Langer, O.C. Farokhzad, Nano Lett. 7 (2007)
(2011) 9542—9551. 3065—3070.
[183] E. Bindewald, C. Grunewald, B. Boyle, M. O’Connor, B.A. [211] S. Shigdar, L. Qiao, S.F. Zhou, D. Xiang, T. Wang, Y. Li, L.Y.
Shapiro, J. Mol. Graphics Modell. 27 (2008) 299—308. Lim, L. Kong, L. Li, W. Duan, Cancer Lett. 330 (2013) 84—95.
[184] H.M. Martinez, J.V. Maizel, B.A. Shapiro, J. Biomol. Struct. [212] S. Da Rocha Gomes, J. Miguel, L. Azéma, S. Eimer, C. Ries,
Dyn. 25 (2008) 669—683. E. Dausse, H. Loiseau, M. Allard, J.J. Toulmé, Bioconjugate
[185] E. Bindewald, R. Hayes, Y.G. Yingling, W. Kasprzak, B.A. Chem. 23 (2012) 2192—2200.
Shapiro, Nucleic Acids Res. 36 (2008) D392—D397. [213] D. Kim, Y. Y. Jeong, S. Jon, ACS Nano 4 (2010) 3689—3696.
[186] S. Abdelmawla, S. Guo, L. Zhang, S. Pulukuri, P. Patankar, [214] J.S. Paige, K.Y. Wu, S.R. Jaffrey, Science 333 (2011) 642—646.
P. Conley, J. Trebley, P. Guo, Q.X. Li, Mol. Ther. 19 (2011) [215] J.S. Paige, T. Nguyen-Duc, W. Song, S.R. Jaffrey, Science 335
1312—1322. (2012) 1194.
RNA as a stable polymer 653
[216] R. Reif, F. Haque, P. Guo, Nucleic Acid Ther. 22 (6) (2013) [251] L.M. Adleman, Science 266 (1994) 1021—1024.
428—437. [252] G.P. Archer, S. Bone, R. Pethig, J. Mol. Electron. 6 (1990)
[217] S. Muller, D. Strohbach, J. Wolf, Nanobiotechnol., IEE Proc. 199—207.
153 (2006) 31—40. [253] A. Okamoto, K. Tanaka, I. Saito, J. Am. Chem. Soc. 126 (2004)
[218] H. Pei, X. Zuo, D. Pan, J. Shi, Q. Huang, C. Fan, NPG Asia 9458—9463.
Mater. 5 (2013) e51. [254] D.Y. Zhang, A.J. Turberfield, B. Yurke, E. Winfree, Science 318
[219] K. Maehashi, T. Katsura, K. Kerman, Y. Takamura, K. Mat- (2007) 1121—1125.
sumoto, E. Tamiya, Anal. Chem. 79 (2007) 782—787. [255] B.K. Nanjwade, H.M. Bechra, G.K. Derkar, F. V. Manvi, V.K.
[220] I. Willner, E. Katz, Angew. Chem. Int. Ed. 39 (2000) Nanjwade, Eur. J. Pharm. Sci. 38 (2009) 185—196.
1180—1218. [256] S.E. Lee, D.Y. Sasaki, Y. Park, R. Xu, J.S. Brennan, M.J. Bissell,
[221] S. Seetharaman, M. Zivarts, N. Sudarsan, R.R. Breaker, Nat. L.P. Lee, ACS Nano 6 (2012) 7770—7780.
Biotechnol. 19 (2001) 336—341. [257] W. Weber, J. Stelling, M. Rimann, B. Keller, M. oud-El Baba,
[222] J.R. Hesselberth, M.P. Robertson, S.M. Knudsen, A.D. Elling- C.C. Weber, D. Aubel, M. Fussenegger, Proc. Natl. Acad. Sci.
ton, Anal. Biochem. 312 (2003) 106—112. U.S.A. 104 (2007) 2643—2648.
[223] S. Song, L. Wang, J. Li, C. Fan, J. Zhao, TrAC, Trends Anal. [258] W. Weber, R. Schoenmakers, B. Keller, M. Gitzinger, T. Grau,
Chem. 27 (2008) 108—117. M. oud-El Baba, P. Sander, M. Fussenegger, Proc. Natl. Acad.
[224] C. Furutani, K. Shinomiya, Y. Aoyama, K. Yamada, S. Sando, Sci. U.S.A. 105 (2008) 9994—9998.
Mol. Biosyst. 6 (2010) 1569—1571. [259] S. Auslander, D. Auslander, M. Muller, M. Wieland, M.
[225] E.E. Ferapontova, E.M. Olsen, K.V. Gothelf, J. Am. Chem. Soc. Fussenegger, Nature 487 (2012) 123—127.
4260
130 (2008) 4256— . [260] Y. Benenson, Nat. Rev. Genet. 13 (2012) 455—468.
[226] C.A. Kellenberger, S.C. Wilson, J. Sales-Lee, M.C. Hammond, [261] Z. Xie, S.J. Liu, L. Bleris, Y. Benenson, Nucleic Acids Res. 38
J. Am. Chem. Soc. 135 (2013) 4906—4909. (2010) 2692—2701.
[227] H. Deng, W. Shen, Y. Ren, Z. Gao, Biosensors and Bioelectron- [262] Z. Xie, L. Wroblewska, L. Prochazka, R. Weiss, Y. Benenson,
ics 60 (2014) 195—200. Science 333 (2011) 1307—1311.
[228] J. Min, A.J. Baeumner, Analyt Biochem 303 (2002) 186—193. [263] C. Lou, X. Liu, M. Ni, Y. Huang, Q. Huang, L. Huang, L.
[229] A.J. Baeumner, R.N. Cohen, V. Miksic, J. Min, Biosens. Bio- Jiang, D. Lu, M. Wang, C. Liu, D. Chen, C. Chen, X. Chen,
electron. 18 (2003) 405—413. L. Yang, H. Ma, J. Chen, Q. Ouyang, Mol. Syst. Biol. 6 (2010)
[230] M. Wang, H. Yin, N. Shen, Z. Xu, B. Sun, S. Ai, Biosens. Bio- 350.
electron. 53 (2014) 232—237. [264] Y. Benenson, Curr. Opin. Biotechnol. 20 (2009) 471—478.
[231] A. Qureshi, Y. Gurbuz, S. Kallempudi, J.H. Niazi, Phys. Chem. [265] M.N. Win, C.D. Smolke, Proc. Natl. Acad. Sci. U.S.A. 104
Chem. Phys. 12 (2010) 9176—9182. (2007) 14283—14288.
[232] L. Zhai, T. Wang, K. Kang, Y. Zhao, P. Shrotriya, M. Nilsen- [266] T. Lee, A.K. Yagati, F. Pi, A. Sharma, J.-W. Choi, P. Guo, ACS
Hamilton, Anal. Chem. 84 (2012) 8763—8770. Nano 9 (2015) 6675—6682.
[233] E.E. Ferapontova, K.V. Gothelf, Electroanalysis 21 (2009) [267] P. Routh, P. Mukherjee, A. Dawn, A.K. Nandi, Biophys. Chem.
1261—1266. 143 (2009) 145—153.
[234] J.A. Sioss, R.B. Bhiladvala, W. Pan, M. Li, S. Patrick, P. Xin, [268] A.K. Geim, K.S. Novoselov, Nat. Mater. 6 (2007)
S.L. Dean, C.D. Keating, T.S. Mayer, G.A. Clawson, Nanomed.: 183—191.
Nanotechnol. Biol. Med. 8 (2012) 1017—1025. [269] A.K. Geim, Science 324 (2009) 1530—1534.
[235] E. Farjami, R. Campos, J.S. Nielsen, K.V. Gothelf, J. Kjems, [270] A. Sinha, N.R. Jana, ACS Appl. Mater. Interfaces 7 (2015)
E.E. Ferapontova, Anal. Chem. 85 (2012) 121—128. 9911—9919.
[236] M. Qiu, E.H.M. Sha, ACM Trans. Des. Autom. Electron. Syst. [271] S. Eissa, A. Ng, M. Siaj, M. Zourob, Anal. Chem. 86 (2014)
14 (2009) 1—30. 7551—7557.
[237] A. Noy, Adv. Mater. 23 (2011) 807—820. [272] R.Y. Li, Q.F. Xia, Z.J. Li, X.L. Sun, J.K. Liu, Biosens. Bioelec-
[238] W. Lu, C.M. Lieber, Nat. Mater. 6 (2007) 841—850. tron. 44 (2013) 235—240.
[239] I. Willner, E. Katz, Bioelectronics: From Theory to Applica- [273] H.M. Zhao, J.P. Tian, X. Quan, Colloids Surf., B: Biointerfaces
tions, John Wiley & Sons, New York, 2005. 103 (2013) 38—44.
[240] A.P. De Silva, S. Uchiyama, Nat. Nanotechnol. 2 (2007) [274] X. Hu, L. Mu, J. Wen, Q. Zhou, J. Hazard. Mater. 213 (2012)
399—410. 387—392.
[241] J.R. Heath, M.A. Ratner, Phys. Today 56 (2003) 43—49. [275] L. Zhang, Z. Lu, Q. Zhao, J. Huang, H. Shen, Z. Zhang, Small
[242] R. Di Felice, Nanobioelectronics-for Electronics, Biology and 7 (2011) 460—464.
Medicine, Springer, New York, 2009, pp. 43—79. [276] F. Sharifi, R. Bauld, M.S. Ahmed, G. Fanchini, Small 8 (2012)
[243] Y.S. Chen, M.Y. Hong, G.S. Huang, Nat. Nanotechnol. 7 (2012) 699—706.
197—203. [277] J.H. Jeong, H. Mok, Y.K. Oh, T.G. Park, Bioconjugate Chem.
[244] R. Baron, O. Lioubashevski, E. Katz, T. Niazov, I. Willner, 20 (2008) 5—14.
Angew. Chem. Int. Ed. 45 (2006) 1572—1576. [278] A.M. Derfus, A.A. Chen, D.H. Min, E. Ruoslahti, S.N. Bhatia,
[245] K. Fujibayashi, R. Hariadi, S.H. Park, E. Winfree, S. Murata, Bioconjugate Chem. 18 (2007) 1391—1396.
Nano Lett. 8 (2007) 1791—1797. [279] N. Singh, A. Agrawal, A.K. Leung, P.A. Sharp, S.N. Bhatia, J.
[246] M. Qiu, E. Khisamutdinov, Z. Zhao, C. Pan, J. Choi, N. Leontis, Am. Chem. Soc. 132 (2010) 8241—8243.
P. Guo, Philos. Trans. R. Soc. A 371 (2013) 20120310. [280] Z. Medarova, W. Pham, C. Farrar, V. Petkova, A. Moore, Nat.
[247] D. Faulhammer, A.R. Cukras, R.J. Lipton, L.F. Landweber, Med. 13 (2007) 372—377.
Proc. Natl. Acad. Sci. U.S.A. 97 (2000) 1385—1389. [281] D. Moll, P. Guo, J. Nanosci. Nanotechnol. (JNN) 7 (2007)
[248] Y. Benenson, B. Gil, U. Ben-Dor, R. Adar, E. Shapiro, Nature 3257—3267.
429 (2004) 423—429. [282] A.K. Gupta, M. Gupta, Biomaterials 26 (2005) 3995—4021.
[249] K. Rinaudo, L. Bleris, R. Maddamsetti, S. Subrama- [283] A.J. Perrett, R.L. Dickinson, Z.ˇ Krpeti´c, M. Brust, H.
nian, R. Weiss, Y. Benenson, Nat. Biotechnol. 25 (2007) Lewis, I.C. Eperon, G.A. Burley, Chem. Sci. 4 (2013)
795—801. 257—265.
[250] M.N. Win, C.D. Smolke, Science 322 (2008) 456—460. [284] N. Bourassa, F. Major, Biochimie 84 (2002) 945—951.
654 H. Li et al.
Hui Li, M.S., is currently a Ph.D. candidate Sijin Guo, B.S., received his B.S. in chem-
in College of Pharmacy, University of Ken- istry from Wuhan University, China in 2014.
tucky. He graduated from Shanghai Jiao Tong He is currently a Ph.D. candidate in Prof.
University in 2011 with a M.S. degree in phar- Peixuan Guo’s lab at University of Kentucky.
maceutical sciences and then joined in Prof. His research interests include the study of
Peixuan Guo’s lab in 2012 spring. He has a function, mechanism and application of bac-
broad training in pharmaceutics, molecular teriophage phi29 DNA-packaging nanomotor
biology, cancer biology and nanobiotechnol- as well as applications of RNA nanoparticles
ogy. His current research is focusing on RNA derived from phi29 packaging RNA (pRNA) in
nanotechnology and the development of new therapeutics delivery, targeting and disease
therapeutics and drug delivery systems based treatment (RNA nanotechnology).
on RNA.
Dr. Taek Lee, Ph.D., is currently a post-
doctoral fellow at College of Pharmacy,
Dr. Jing Xu, Ph.D., is an associate professor
University of Kentucky. He obtained her B.S.
at the National Center for Nanoscience and
from Sogang University, Department of Chem-
Technology, Beijing, China. She received her
ical and Biomolecular Engineering, South
B.S. in Chemistry in 2004 and M.S. in Polymer
Korea (2008), and Ph.D. from Department
Science in 2007 from Nankai University, Tian-
of Chemical and Biomolecular Engineering,
jin, China. In 2012, she received her Ph.D. in
Sogang University (2013). He has a broad
Chemistry from the University of North Car-
training in chemical engineering, biology, and
olina at Chapel Hill with Professor Joseph M.
nanobiotechnology. Dr. Lee’s scholarly inter-
DeSimone. Her work focuses on development
est broadly focuses on bioelectronics, biochip
of drug delivery systems for treatment of can-
and medicine. These include, RNA nanoparticle construction and
cers and prevention of infectious diseases.
conjugation for bioelectronics application, therapeutic and diag-
nostic applications.
Dr. Thomas Dziubla, Ph.D., is the Asso-
Dr. Chan Li, Ph.D., is currently an assistant
ciate Gill Professor and Director of Graduate
professor in CAS Key Laboratory for Biomedi-
Studies in the Department of Chemical and
cal Effects of Nanomaterials and Nanosafety,
Materials Engineering at the University of
National Center for Nanoscience and Tech-
Kentucky. He received his B.S. and Ph.D
nology of China. She received her Ph.D.
in Chemical Engineering from Purdue Uni-
degree in chemistry from University of Sci-
versity (1998) and Drexel University (2002),
ence and Technology of China in 2012. She
respectively. In 2002—2004, he was an NRSA
worked as a postdoc at Osaka University
postdoctoral fellow in the Institute for Envi-
in Japan before joining National Center for
ronmental Medicine at the University of
Nanoscience and Technology of China in
Pennsylvania School of Medicine under the
2014. Dr. Li’s research is focused on ligand-
guidance of Dr. Vladimir Muzykantov, where he worked on the
modified nanocarrier loading anticancer drugs to circumvent drug
design of degradable polymeric nanocarriers for the delivery of
resistance, and the formulation and process development of
antioxidants. His research group is interested in the design of new
nanomedicines.
functional polymeric biomaterials which can actively control local
cellular oxidative stress for improved biomaterial integration and
disease treatment. He holds 8 patents, has authored over 50 peer
reviewed publications and has started several companies that are
currently commercializing technologies that have originated from Dr. Farzin Haque, Ph.D., is a Research Assis-
his laboratory. tant Professor in the University of Kentucky
College of Pharmacy, Department of Pharma-
Fengmei Pi, M.S., is currently a Ph.D. can- ceutical Sciences. He received his B.A. degree
didate at College of Pharmacy, University of in Biochemistry and Mathematics (2004) from
Kentucky. She obtained her B.S. and M.S. Lawrence University and a Ph.D. degree in
from China Pharmaceutical University (2007). Chemistry (2008) from Purdue University. He
She worked as a research scientist at Dea- held a postdoctoral appointment (2009—2011)
woong Pharmaceuticals Co. Korea; and senior at the University of Cincinnati, with Pro-
formulation scientist in China GSK Consumer fessor Peixuan Guo. Dr. Haque’s scholarly
Healthcare before joining the University of interest broadly focuses on Nanoscience and
Kentucky (2012). She has broad training and Nanotechnology in Biology and Medicine. These include, nanopore-
working experience in pharmaceutical sci- based technology for single molecule detection and sensing of
ence. Her recent research focused on RNA chemicals and biopolymers; and RNA Nanotechnology - con-
nanotechnology, developing RNA nanoparticles based aptamers for struction of RNA nanoparticles for therapeutic and diagnostic
targeted drug delivery and cancer therapy. applications.
RNA as a stable polymer 655
Dr. Xing-Jie Liang, Ph.D., got his Ph.D. Dr. Peixuan Guo, Ph.D., is William Farish
at National Key Laboratory of Biomacro- Endowed Chair in Nanobiotechnology, direc-
molecules, Institute of Biophysics at CAS. tor of University of Kentucky Nanobiotechnol-
He finished his postdoc at Center for Can- ogy Center and director of NIH/NCI Cancer
cer Research, NCI, NIH, and worked as a Nanotechnology Platform Partnership Pro-
Research Fellow at Surgical Neurology Branch, gram: ‘‘RNA Nanotechnology for Cancer
NINDS. He worked on Molecular imaging Therapy’’. He obtained his Ph.D from Univer-
at School of Medicine, Howard University sity of Minnesota, and postdoctoral training
before he became deputy director of CAS at NIH, joined Purdue University in 1990,
Key Laboratory for Biomedical Effects of was tenured in 1993, became a full Profes-
Nanomaterials and Nanosafety, National Cen- sor in 1997, and was honored as a Purdue
ter for Nanoscience and Technology of China. He is a founder Faculty Scholar in 1998. He constructed phi29 DNA-packaging
member of International Society of Nanomedicine, member of motor, discovered phi29 motor pRNA, pioneered RNA nanotechnol-
American Association for Cancer Research, and member of Amer- ogy, incorporated phi29 motor channel into lipid membranes for
ican Society of Cell Biology. He is current Associate Editors of single-molecule sensing with potential for high-throughput dsDNA
‘Biomaterials’ and ‘Biophysics Report’; Advisory editorial board sequencing. He is a member of two prominent national nanotech
member of ‘ACS Nano’; Editorial member of ‘Advances in Nano initiatives sponsored by NIH, NSF, NIST, and National Council of
Research’, ‘Current Nanoscience’, ‘Biomaterials Research’, ‘Ther- Nanotechnology, director of one NIH Nanomedicine Development
anostics’ and guest editor of ‘Biotechnology Advances’. Developing Center from 2006—2011. His work was featured hundreds of times
drug delivery strategies for prevention/treatment of AIDS and can- over radio, TV such as ABC, NBC, newsletters NIH, NSF, MSNBC, NCI,
cers are current program ongoing in Dr. Liang’s lab based on and ScienceNow. He was a member of NIH/NCI intramural site-visit
understanding of basic physiochemical and biological processes of Review Panel at 2010 and 2014, and a member of the Examina-
nanomedicine. tion and Review Panel (Oversea Expert) of the Chinese Academy of
Sciences since 2014.