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Fast, transient and specific intracellular ROS changesin living root hair cells responding to Nod factors (NFs)
Luis Cardenas*, Adan Martınez, Federico Sanchez and Carmen Quinto
Departamento de Biologıa Molecular de Plantas, Instituto de Biotecnologıa, Universidad Nacional Autonoma de Mexico,
UNAM, Apartado Postal 510-3, Cuernavaca, Morelos 62271, Mexico
Received 11 April 2008; revised 23 June 2008; accepted 21 July 2008; published online 27 August 2008.*For correspondence (fax 52 + 777 3136600; e-mail [email protected]).
Summary
The role of reactive oxygen species (ROS) in root-nodule development and metabolism has been extensively
studied. However, there is limited evidence showing ROS changes during the earliest stages of the interaction
between legumes and rhizobia. Herein, using ratio-imaging analysis, increasing and transient ROS levels were
detected at the tips of actively growing root hair cells within seconds after addition of Nod factors (NFs). This
transient response (which lasted up to 3 min) was Nod-factor-specific, as chitin oligomers (pentamers) failed
to induce a similar response. When chitosan, a fungal elicitor, or ATP was used instead, a sustained increasing
signal was observed. As ROS levels are transiently elevated after the perception of NFs, we propose that this
ROS response is characteristic of the symbiotic interaction. Furthermore, we discuss the remarkable spatial
and temporal coincidences between ROS and transiently increased calcium levels observed in root hair cells
immediately after the detection of NFs.
Keywords: reactive oxygen species, polar growth, root hairs, Nod factors, nodulation.
Introduction
Legumes can acquire nitrogen through a symbiotic inter-
action with rhizobial bacteria. This process involves a
molecular dialogue between the two partners, in which
legume roots exude flavonoids that induce the expression of
bacterial nodulation genes encoding proteins involved in the
synthesis and secretion of specific lipochitooligosacchar-
ides: the so-called Nod factors (NFs). These NFs signal back
to the plant root, and trigger several responses such as ion
changes (K+, Cl), Ca2+and H+), cytoplasmic alkalinization,
calcium oscillations and gene expression that lead to bac-
terial invasion and nodule formation (Cardenas et al., 2000;
Oldroyd and Downie, 2004).
In plants, reactive oxygen species (ROS) modulate
numerous biological processes such as growth, cell cycle,
programmed cell death, plant defense, hormone signaling,
biotic and abiotic stress responses and development. ROS
have also been found to play a key role in regulating polar
growth in root hair cells, fucus zygotes and pollen tubes
through their ability to regulate calcium channels, which are
involved in maintaining the apical calcium gradient (Coelho
et al., 2008; Foreman et al., 2003; Jones et al., 2007; Potocky
et al., 2007). On the other hand, ATP has also emerged as an
important modulator of NADPH oxidases in plant cells (Kim
et al., 2006; Song et al., 2006). In fact, extracellular ATP has
been found to modulate intracellular calcium and the levels
of ROS in root hair cells (Jeter et al., 2004; Kim et al., 2006;
Song et al., 2006).
Whereas compelling evidence indicates that NFs are
signal molecules secreted by bacteria that induce various
plant cellular responses, it remains unknown whether such
rhizobial signal molecules may also elicit pathogen-like
responses. It has been proposed that plant pathogenesis
and symbiosis are variations on a common theme (Baron
and Zambryski, 1995). In this regard, previous results
indicate that rhizobia might be initially recognized as
intruders that somehow evade or overcome the plant
defense response. Indeed, several plant defense responses
are induced during root nodule ontogeny (Gamas et al.,
1998; Parniske et al., 1990; Vasse et al., 1993). In alfalfa, not
all infection threads culminate in successful infection; many
abort even compatible symbiotic interactions because of the
hypersensitive response triggered in the root cortex (Vasse
802 ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd
The Plant Journal (2008) 56, 802–813 doi: 10.1111/j.1365-313X.2008.03644.x
et al., 1993). In peas, the plant defense response has been
proven to be far more critical for arresting the advancement
of rhizobial infection during incompatible interactions
(Perotto et al., 1994). Wisniewski et al. (2000) proposed that
diamine oxidase (DAO) could be a potential source for
hydrogen peroxide (H2O2), which might be used by cell wall
peroxidase (POD) for hardening the glycoprotein matrix
(MGP). Together, these data indicate the importance of ROS
metabolism during symbiotic interactions (Wisniewski
et al., 2000).
Additional evidence for the role of ROS signaling during
rhizobia–legume interactions has been described in Medi-
cago truncatula, where a peroxidase gene (rip1) is induced in
the presence of NFs from Sinorhizobium meliloti (Cook
et al., 1995). This peroxidase has a cis domain that is ROS
sensitive (Ramu et al., 2002). It is interesting that rip1
transcription and ROS production co-localize in the same
root cells (Ramu et al., 2002). In fact, exogenous H2O2 can
induce rip1 expression, suggesting that cis elements (OCS
and OBP) in the rip1 gene are required for induction after
ROS production. Furthermore, it has been demonstrated
that ROS and ethylene are part of the NFs-induced signal
cascade involved in nodule development in Sesbania
rostrata (D’Haeze et al., 2003).
During the early stages of M. truncatula–S. meliloti sym-
biosis, the oxidation of nitroblue tetrazolium (NBT) was
detected within the infection threads, indicating that O2) is
produced during this process (Santos et al., 2001). Further-
more, it is well known that there is an accumulation of H2O2
during the infection process and during nodule senescence
(Rubio et al., 2004). Accordingly, it is plausible that rhizobia
should have a mechanism to respond against ROS accumu-
lation in plants. In this regard, bacterial ROS scavenging
enzymes such as superoxide dismutase, glutathione-
S-transferase and catalase seem to play a protective role in
the legume–rhizobia interaction (Jamet et al., 2003; Ramu
et al., 2002; Santos et al., 2000; Sigaud et al., 1999). The
increased activity of these ROS scavenging enzymes in
S. meliloti appears to be essential for the regulation of
intracellular ROS production during the establishment and
maintenance of symbiosis with the plant host (Jamet et al.,
2003).
Paradoxically, decreased ROS production in response to
treatment with specific NFs has been also reported in
M. truncatula (Lohar et al., 2007; Shaw and Long, 2003b).
However, these results were obtained several minutes after
the addition of NF, and ROS levels were measured not from
a single cell, but from whole sectioned roots. These
apparently contradictory results prompted us to analyze
ROS responses at the subcellular level using single living
root hair cells from the responsive root region. In addition,
improved cell imaging methodology was used to measure
ROS levels within seconds after the addition of NFs. Herein,
we used a semi-quantitative ratio-imaging approach to
show that intracellular ROS levels transiently increased in
single living root hair cells within a few seconds after
treatment with NFs. This response was specific for NFs, and
was different from that induced by chitosan, a fungal elicitor,
ATP or chitin pentamers that constitute the non-active
backbone of the NFs.
Results
Growing root hairs exhibit a tip-localized ROS distribution
Single growing root hair cells were loaded with different
concentrations of an ROS-sensitive fluorescent dye (CM-
H2DCFDA) in order to achieve optimal loading conditions
that did not alter growth and root hair morphology. Root hair
cells imaged under these conditions presented a tip-loca-
lized ROS signal. Figure 1 (inset) shows the co-localization of
differential interference contrast (DIC), and the fluorescent
image indicates where the ROS distribution extends to in the
subapical region. The location of this signal is similar to that
previously described in root hairs from Arabidopsis thaliana
(Foreman et al., 2003), and hence we considered this to be a
typical ROS distribution for an actively growing root hair
cell. Furthermore, time-lapse imaging microscopy demon-
strated that ROS levels in growing root hair cells remained
unaltered in time, with only discrete fluctuations (Figure 1).
In contrast, when root hair cells entered the mature stage,
the ROS levels were notably decreased and were completely
absent in non-growing cells (data not shown).
NFs induce a rapid and specific transient increase
in intracellular ROS levels
Actively growing Phaseolus vulgaris root hair cells from root
zone II (Heidstra et al., 1994) were analyzed after loading the
roots with the ROS-sensitive dye, under conditions pre-
viously described. After root hair cells showed a typical ROS
distribution (Figure 2a, left-hand image), they were treated
with Rhizobium etli NFs (10)9M). Rapid intracellular ROS
elevation at the apical region of the cell was observed; ROS
levels started to increase 15 s after the addition of NFs to the
growth medium, and reached a maximum level after 1 min
(Figure 2a, middle image; Figure S1). Thereafter, the signal
decreased to basal levels (Figure 2a, right-hand image).
Similar results were obtained when 15 independent root hair
cells were analyzed (Figure 2b). ROS elevation occurred
transiently within the first 3 min, and subsequently declined
to basal intracellular levels that were finally attained
approximately 4 min after treatment with NFs (Figure 2b).
The ROS signal decreased to below the basal level by 10 min
after addition; this coincided with the arrest of root hair
growth, and with the typical swelling response observed at
the apical dome (data not shown). ROS signals could not be
detected in young (emerging) root hair cells from root zone I
ROS changes in root hairs responding to NFs 803
ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd, The Plant Journal, (2008), 56, 802–813
Figure 1. Intracellular reactive oxygen species
(ROS) levels observed in growing Phaseolus
vulgaris root hairs.
Inset: an overlay of a DIC and the corresponding
fluorescent image from a root hair cell; the tip-
localized intracellular ROS distribution was
revealed using an ROS-sensitive dye (CM-
H2DCFDA). The drawing indicates the region of
interest (ROI) where the measurement was
performed. Red and blue colors indicate high
and low intensities, respectively. Scale bar:
15 lm. The graph illustrates the relative ROS
values pooled from 15 different individual root
hair cells, and shows that the fluorescent signal
remained invariable over time.
(b)
(a) Figure 2. Intracellular reactive oxygen species
(ROS) changes in living Phaseolus vulgaris root
hairs after treatment with Nod factors (NFs).
(a) The left-hand image shows a growing root
hair cell loaded with CM-H2DCFDA dye and
presenting a tip-localized ROS signal (t = 0).
The middle image depicts the same root hair cell
treated with Rhizobium etli NFs (t = 1 min): the
intracellular ROS levels rapidly increased within
the first 10–15 s, and peaked after 1 min; there-
after, basal ROS levels were achieved after 3 min,
as observed in the right-hand image. Red and
blue colors indicate high and low ROS concen-
tration levels, respectively. Scale bar: 15 lm.
(b) Time course analysis of ROS production in
root hair cells treated with growth medium
containing NFs (10)9M) or chitin oligomers
(10)9M); a control with only growth medium
was also included. Images were analyzed for
relative intensity values at the tip of each root
hair cell. Pooled data from 15 different cells are
shown.
804 Luis Cardenas et al.
ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd, The Plant Journal, (2008), 56, 802–813
(data not shown), because this root region has particularly
elevated ROS levels (Shin et al., 2005) that mask single-cell
measurements.
The observed transient ROS responses were specifically
induced by NFs, as the addition of growth medium alone or
growth medium containing chitin oligomers (pentamers)
did not induce any response (Figure 2b). Accordingly, chitin
oligomers were used as a negative control for the rest of
the study.
H2O2 and UV radiation induced similarly increased ROS
levels in root hair cells
In order to test if intracellular ROS levels could be artificially
increased in root hairs, exogenous hydrogen peroxide
(50 lM) was added to the growth medium. Under these
conditions, a sustained increase in intracellular ROS levels
was observed after 3 min (Figure 3). Intracellular ROS levels
were also artificially increased in root hair cells after a 5-s
pulse of UV light (340 nm), as previously reported (Dixit and
Cyr, 2003; Mackerness et al., 2001) (Figure 3). This con-
tinuously increasing ROS signal was similar to that observed
after the addition of H2O2. Apparently, root hair cells could
only overcome UV and H2O2 treatment within the first 3 min;
after this time there was a dramatic increase in intracellular
ROS levels (Figure 3).
In contrast, the transient ROS response induced in root
hairs after treatment with NFs (Figure 2) was different from
that observed with exogenously applied H2O2, or after UV
irradiation (Figure 3). A sustained and increasing ROS signal
that eventually saturated the probe was observed instead
(Figure 3), suggesting that these cells were dying. At the
cellular level, root hair cells treated in this way became
vacuolated, and a swelling response was usually observed
(data not shown). Collectively, these data confirm that the
conditions and the fluorescent dye concentration used
adequately probed the levels of intracellular H2O2 and free
radicals in living root hair cells under different conditions.
Chitosan induced sustained increases in intracellular
ROS levels
In order to assess whether the ROS levels observed in root
hairs after treatment with NFs were specific for the symbiotic
interaction, a fungal elicitor was added instead. Chitosan,
which is widely used to induce a hypersensitive response in
plants, was added to root hair cells that were previously
treated with the ROS-sensitive dye (Figure 4, left-hand
image), and ROS levels were analyzed under the aforemen-
tioned conditions. ROS levels were dramatically increased
(Figure 4, middle image) by 5 min after treatment with chit-
osan, and reached their highest level by 9 min (Figure 4,
right-hand image). This sustained and increased response
was similar to that induced by UV light radiation and H2O2
treatments (Figure 3). It is worth mentioning that besides
causing a dramatic increase in intracellular ROS levels, chit-
osan also markedly reduced cytoplasmic streaming by
10 min after its addition (data not shown). Intracellular ROS
levels in root hair cells were entirely different when com-
paring transient increases after NF treatment (Figure 4b) with
sustained increases after elicitor treatment (Figure 4a,b).
Ratio-imaging of intracellular ROS levels reveals a
tip-focused signal that responds to treatment with NFs,
and is inhibited by diphenylene iodonium (DPI)
The ROS-sensitive dye (CM-H2DCFDA) used in the experi-
ments previously described is a single-wavelength dye that
Figure 3. Reactive oxygen species (ROS)
changes in response to hydrogen peroxide
(H2O2) and UV radiation.
Root hair cells loaded with CM-H2DCFDA dye
and treated with 50 lM exogenously applied
H2O2 (black squares) or for 5 s with UV radiation
at 340 nm (grey circles) were immediately im-
aged after treatment. These cells responded with
sustained increased ROS levels, and both treat-
ments induced similar responses.
ROS changes in root hairs responding to NFs 805
ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd, The Plant Journal, (2008), 56, 802–813
does not allow ratio-imaging. In order to account for the
variably accessible cytoplasmic volume of root hair cells, we
introduced a reference dye (see Experimental procedures for
the pseudo-ratio-imaging analysis. This approach was used
to depict, in a semi-quantitative way, the subcellular ROS
distribution in growing root hair cells. We found that in-
tracellular ROS levels were indeed focused to the apical
dome (Figure 5, inset, left-hand image), and were drastically
increased in response to NFs with a transient pattern that
peaked after 1 min (Figure 5, inset middle image; Figure S2).
This response resembled that obtained previously with the
non-ratio-imaging approach (Figure 2, middle image), and
was very consistent in 10 of 12 cells; moreover, this ratio
analysis allowed the visualization of the subcellular dis-
tribution before and after treatment with NFs. It is interesting
that at the end of the transient response, the intracellular
ROS levels remained higher than the initial values observed
before treatment with NFs (Figure 5).
DPI is an inhibitor of NADPH oxidases and flavin-contain-
ing enzymes, and has been widely used to reduce intracel-
lular levels of ROS in plant cells (Foreman et al., 2003; Lohar
et al., 2007; Shaw and Long, 2003b). Growing root hair cells
have constant intracellular levels of ROS that did not change
when chitin pentamers were used as a control (Figure 6).
However, with DPI treatment, the intracellular levels of ROS
were drastically reduced after 4 min, although they did not
completely disappear, and remained at the basal level after
10 min of treatment with DPI (Figure 6). When root hairs
(a)
(b)
Figure 4. Differential intracellular reactive oxy-
gen sepcies (ROS) responses obtained with
treatment with chitosan and Nod factors (NFs).
(a) The left-hand image depicts a growing root
hair cell loaded with CM-H2DCFDA and showing
the typical tip ROS distribution (t = 0). The
middle image represents the same root hair cell
after treatment with chitosan: the cell presented
increased ROS levels. The right-hand image
illustrates elevated ROS levels observed after
9 min of chitosan treatment. The red color
indicates high levels of ROS. Scale bar: 15 lm.
(b) Graph showing that treatment with chitosan
induced a continuous increase in intracellular
ROS. The ROS level did not return to the initial
values (red squares). Conversely, the addition of
NFs induced transient ROS induction (black
diamonds). Chitosan or NFs were added at the
beginning of the series (t = 0).
806 Luis Cardenas et al.
ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd, The Plant Journal, (2008), 56, 802–813
showed basal levels of ROS (after 10 min of treatment with
DPI) they were challenged with NFs, but specific transient
changes in ROS were not observed (Figure 5). The absence
of transient ROS induction after treatment with NFs in root
hairs previously treated with DPI suggests that the activation
of NADPH oxidases is closely linked to the perception and
signaling of NFs.
Root hair cells treated with DPI showed arrested growth
and, eventually, root hair swelling (data not shown). As
organelles such as chloroplasts and mitochondria with
highly oxidizing metabolic activity or high electron flow
are also important sources of ROS production in plant cells,
we explored the subcellular distribution of mitochondria
in growing root hair cells using a mitochondria-specific
fluorescent probe (Mitotracker Green). Mitochondria were
distributed throughout the cell, but were more abundantly
localized at the apical region of the root hair cells (Figure 6,
see inset), which coincides with the region in which the ROS
signal was observed. Thus, we propose that these mito-
chondria could partially contribute to ROS production in this
region, including basal production observed after DPI
treatment.
Extracellular ATP modulates intracellular levels of ROS
Extracellular ATP has been described as inducing changes in
intracellular levels of ROS (Song et al., 2006); however, the
subcellular distribution of these ROS have not been
described. Root hair cells previously loaded with ROS-sen-
sitive and reference dyes were challenged with 10 mM ATP.
Under these conditions a continuous increase of apical ROS
levels was observed (Figure 7), which was eventually
Figure 5. Root hairs pre-treated with dipheny-
lene iodonium (DPI) did not display the transient
intracellular reactive oxygen species (ROS)
response.
Root hair cells were treated with a reference dye
(Cell Tracker Red) and ROS-sensitive dye (CM-
H2DCFDA) for ratio-imaging of the spatial dis-
tribution of ROS. Root hair cells that were
preliminarily treated with DPI and then chal-
lenged with Nod factors (NFs) did not show the
transient ROS response (gray trace). Root hair
cells under the same conditions without DPI
showed the typical transient response after
treatment with NFs. This transient response
was observed in 10 of 12 cells. The inset shows
the typical subcellular distribution before treat-
ment with NFs (left image), at the peak of the
response (middle image) and after the transient
response (right-hand image). Note that the
intracellular ROS levels remained slightly ele-
vated at the end of the experiment. Scale
bar: 15 lm.
Figure 6. Diphenylene iodonium (DPI) gradually
reduced the levels of intracellular reactive oxy-
gen species (ROS).
Root hair cells previously treated with DPI were
closely monitored for production of intracellular
ROS after 4 min (we did not observe a change
prior to that time); as depicted, DPI treatment
resulted in gradually decreased levels of cyto-
plasmic ROS after 4 min, but ROS production
was not abolished the (black circles). Root hairs
treated with pentamers as a control did not show
any response (gray diamonds). Inset, a DIC
image of a living root hair cell (left-hand image)
treated with Mitotracker Green to follow the
mitochondrial distribution (right-hand image).
Note that the apical region is enriched with
mitochondria. Scale bar: 15 lm.
ROS changes in root hairs responding to NFs 807
ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd, The Plant Journal, (2008), 56, 802–813
accompanied by a higher cytoplasmic accumulation at the
tip region that sometimes resulted in cell bursting (data not
shown). Furthermore, repeated local delivery of 5 mM ATP in
the vicinity of the root hair cell using a blunt needle resulted
in transient increases in the intracellular levels of ROS
(Figure 7).
Discussion
In the present study, the production and distribution of
intracellular ROS, as well as the specific response to NFs,
were analyzed in growing P. vulgaris root hair cells. Inter-
estingly, ROS levels were dramatically and transiently
increased within a few seconds after treatment with NFs.
The response was specific for NFs, and was clearly different
to that observed after the addition of H2O2, ATP or chitosan,
or after exposure to UV radiation.
As ROS can be used as intracellular signals, all organisms
have developed several ways to counteract their deleterious
effects (Mittler, 2002; Neill et al., 2002; Vieira Dos Santos and
Rey, 2006). The ability of cells to suppress ROS toxicity, and
to decode the strength and amplitude of the signal, requires
many genes involved in regulating the ROS homeostatic
response (Mittler et al., 2004). The functions of ROS signal-
ing in eukaryotic cells include the regulation of cell
migration, growth modulation, opening and closing of ion
channels, gene expression, development and programmed
cell death (Foreman et al., 2003; Mittler et al., 2004; Ushio-
Fukai, 2006). As ROS easily diffuse across the plasma
membrane, and have a short half-life, rapid localization at
the subcellular level is crucial for understanding the nature
of the signaling events after a given stimulus. As the ROS-
sensitive dye (CM-H2DCFDA) is a non-ratiometric and single-
wavelength dye, it was necessary to use an additional dye as
a reference for ratio-imaging. Using this approach, we were
able to register transient ROS changes induced by NFs in a
semi-quantitative way. In this work, we showed that normal
root hair cells from P. vulgaris present a tip-localized ROS
signal when analyzed with a pseudo-ratio-imaging app-
roach. These ROS changes transiently occurred within a few
seconds, and lasted up to 3 min, on average, after root hairs
were challenged with NFs. In addition, we found that this
response was localized to the tip of the growing cell. This
apical response suggests an important role for ROS during
the perception of NFs, probably in regulating polar growth,
as reported in Arabidopsis, pollen tubes and focus zygotes
(Cardenas et al., 2006; Coelho et al., 2008; Foreman et al.,
2003; Potocky et al., 2007; Takeda et al., 2008). Transient
ROS changes might participate in decoding the rhizobial
signal as a part of symbiosis. Although this idea has been
previously proposed (Ramu et al., 2002), responses at the
subcellular level have not been observed. By using a
pseudo-ratiometric approach, it was possible to subcellu-
larly visualize transiently increased ROS levels in root hair
cells responding to NFs. Interestingly, intracellular ROS
levels remained higher than the initial values. This suggests
that increased ROS levels could be necessary for inducing
expression of some early nodulins, as previously suggested
(Ramu et al., 2002). Early nodulin expression could be
involved in morphological changes that anticipate infection
thread formation, or in the regulation of infection thread
number, thereby allowing bacteria to enter root hair cells
when they are able to circumvent the high basal levels
of ROS.
Multiple sources for ROS production inside cells (Ushio-
Fukai, 2006) have been described. In particular, it is known
that mitochondria and chloroplasts are major sources
for generation of ROS as a result of intense membrane
Figure 7. ATP induced an increase in the levels
of intracellular reactive oxygen species (ROS).
Root hair cells loaded with the ROS-sensitive dye
and the reference dye were exposed to 10 mM
ATP; intracellular ROS increased constantly until
reaching a constant value (black circles). Root
hair cells under the same conditions, but
exposed to rapid 5 mM ATP perfusion (3 s)
showed transiently increased ROS levels (gray
diamonds). This response was reproduced when
cells were perfused again with 5 mM ATP.
Arrows indicate when ATP was added.
808 Luis Cardenas et al.
ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd, The Plant Journal, (2008), 56, 802–813
electron flow (Mittler et al., 2004). Plant NADPH oxidases
have been shown to be the main source of ROS during
pathogen attack and UV irradiation (Rao et al., 1996; Sagi
and Fluhr, 2001, 2006; Torres et al., 2005). In this work, we
showed that root hairs from P. vulgaris showed decreased
intracellular ROS levels when previously treated with DPI
(Figure 6, black trace). However, a basal level is main-
tained, indicating that other sources such as plant cell wall
diamine oxidase and mitochondria could engage in
cytoplasmic production of ROS (Wisniewski et al., 2000).
In fact, we observed that mitochondria were located more
abundantly at the tip region of the root hair (Figure 6,
inset), and might potentially contribute to generation of
ROS in the apical zone. Further analysis revealed that root
hair cells previously treated with DPI and subsequently
challenged with NFs failed to respond with transient
increases in intracellular levels of ROS (this work). This
result suggests that NADPH oxidases are most likely to be
the main source of intracellular ROS. The evidence above,
in addition to previous reports (D’Haeze et al., 2003; Ramu
et al., 2002), suggest that ROS production is intimately
related with the NFs perception pathway. Although it has
been shown recently that phosphatidyl inositol 3-Kinase
(PI3K) and phosphatidyl inositol-specific phospholipase C
(PI-PLC) inhibitors suppress ROS production, a clear
analysis of subcellular ROS distribution has not yet been
provided (Peleg-Grossman et al., 2007). Furthermore, it is
not known how early ROS homeostasis is executed at the
subcellular level, or what the differences are between
symbiotic and pathogenic responses (Levine et al., 1994).
As the ROS response was transiently observed after
treatment with NFs, root hair cells must not only have a
mechanism to increase the production of ROS, but must
also have a mechanism to efficiently remove or neutralize
them. ROS homeostasis can be achieved by scavenging
intracellular ROS or inhibiting their production. The
present finding of increased ROS production only seconds
after exposure to NFs seems to contradict the findings of
Lohar et al. (2007) recently reported in M. truncatula, at 1 h
after treatment with NFs. That study found decreased
expression of NADPH oxidase genes, which could account
for the reduced levels of ROS observed after 1 h (Lohar
et al., 2007; Shaw and Long, 2003b). However, it should be
noted that the previous experiments were started several
minutes after exposure to NFs, and did not explore the
immediate response. This consideration leads us to
suggest that NFs may both positively and negatively
modulate the intracellular levels of ROS. According to our
results, NFs might rapidly stimulate NADPH oxidase either
directly or indirectly in the early stages. This could be
followed later by inhibition, as demonstrated by Lohar
et al. (2007). It has been reported that DPI reduces
intracellular levels of ROS, and mimics the swelling
response induced by NFs (Lohar et al., 2007). It is possible
that decreased ROS levels are required later on during the
swelling response, but that higher concentrations might be
required during the very early stages of the symbiotic
process.
It has been reported that an Arabidopsis NADPH oxidase
(RBOH) has EF-hand motifs that are involved in calcium
binding (Keller et al., 1998; Sagi and Fluhr, 2001), and that
ROS can activate calcium channels (Foreman et al., 2003;
Mori and Schroeder, 2004). Furthermore, it has been
reported that the oscillating growth pattern of root hair cells
is coupled to extracellular pH and changes in ROS (Mon-
shausen et al., 2007): this suggests that ROS could be
involved in cell wall property changes that allow polarized
growth. The observed ROS gradient (this work) in the apical
region spatially correlates with the recently described
localization of NADPH oxidase at the apical plasma mem-
brane of root hair cells (Takeda et al., 2008). These data
support the idea that ROS and calcium are two key
interacting signaling elements required to modulate polar-
ized tip growth. It is plausible that the previously reported
elevated calcium influx observed after treatment with NFs
(Cardenas et al., 1999; Shaw and Long, 2003a) could be
involved in the transient increases in ROS observed in the
present study. In general, the EF-hand and calmodulin
binding domains in some NADPH oxidases are thought to
be well suited for this kind of regulation (Banfi et al., 2004;
Tirone and Cox, 2007). In fact, some calmodulins have been
shown to be differentially expressed in response to NFs
(Camas et al., 2002). However, there may be other mechan-
isms responsible for downregulating their function, as
NADPH oxidases, which are upregulated during a pathogen
attack, are modulated by different kinases, acting in a
sequential or parallel manner (Benschop et al., 2007). It will
be interesting to determine how this fine regulation is
accomplished, and whether ROS changes activate calcium
responses or vice versa. In this scenario, calcium and ROS
play synergistic key roles in modulating the early stages of
the symbiotic interaction.
That the signal of the ROS-sensitive dye (CM-H2DCFDA)
was decreased, even though it is irreversibly photooxidized,
might be the result of at least two factors. Firstly, the ROS-
generating mechanism is tip localized, which means that it
occurs in a very limited region of the root hair cells, and
could be downregulated after the transient response to NFs,
as suggested above, with the consequence that there is a
reduction in the generation of ROS. Secondly, the limited
region with increased ROS levels could be rapidly dissipated
by the strong cytoplasmic streaming and diffusion.
In animal cells, ATP induces ROS production by activating
NADPH oxidase (Dichmann et al., 2000; Pines et al., 2005). A
regulatory role for extracellular ATP in modulating cellular
ROS levels via activation of NADPH oxidases has been
recently suggested to occur in plant cells (Roux and
Steinebrunner, 2007), including root hair cells (Kim et al.,
ROS changes in root hairs responding to NFs 809
ª 2008 Universidad Nacional Autonoma de MexicoJournal compilation ª 2008 Blackwell Publishing Ltd, The Plant Journal, (2008), 56, 802–813
2006; Song et al., 2006). Our results add weight to the idea
that ATP induces changes in intracellular ROS levels in root
hair cells, as previously suggested (Song et al., 2006), and
thus also favors the idea that ATP could be involved in polar
growth, as it can increase intracellular levels of ROS. Analysis
of the spatiotemporal correlation between extracellular ATP,
calcium and ROS changes in the early stages of symbiosis,
and also during pathogen attack, will help in the under-
standing of the signal pathways involved in each response.
Based on the findings of the present study, we propose that
the early production and distribution of ROS are closely
related to ATP and calcium signaling in legume root hair cells.
Indeed, increased levels of ROS (this work) and calcium
spatially and temporally coincide after treatment of root hair
cells with NFs (Cardenas et al., 1999; Shaw and Long, 2003a).
Pathogenesis and symbiosis have many common fea-
tures (Baron and Zambryski, 1995). The precise regulation of
ROS production seems to play a key role in successful
Rhizobium–legume interaction (Perotto et al., 1994; Santos
et al., 2001; Vasse et al., 1993). It is possible that by
regulating ROS production to occur at the right time and
place, rhizobia are allowed to enter the host plant without
triggering a hypersensitive response. A failure to control
ROS elevation might provoke an infection thread abortion
(Vasse et al., 1993). The response of root hair cells to NFs
with a transient ROS signature signal different from that
observed after treatment with chitosan, UV and H2O2
suggests that these cells can differentiate symbiotic from
pathogenic signals within seconds. The inability of intracel-
lular ROS to reach initial basal levels after the transient
response suggests that increased ROS levels could play a
role in the cellular responses. This idea is supported by
experiments involving treatment with DPI that showed an
inhibition of root hair curling and infection thread formation
(Peleg-Grossman et al., 2007).
Using a semiquantitative ratiometric approach in living
root hair cells, we established that specific transient
elevations in ROS occur at the tip within seconds of
treatment with NFs. This transient ROS signature could be
the earliest downstream signal after a symbiotic or patho-
genic molecular stimulus is perceived by the plant. It is
important to unravel the mechanisms underlying ROS
signaling during the early symbiotic interaction, in addition
to the intimate connections between calcium signaling,
extracellular ATP, cell wall peroxidase activities and poten-
tial cytoskeleton rearrangements triggered by transient
Ca2+ elevation, and ROS production.
Experimental procedures
Seed germination
Phaseolus vulgaris cv. Negro Jamapa seeds were surface-sterilizedwith sodium hypochlorite for 5 min, followed by five rinses with
sterile water, subsequent treatment with pure ethanol for 1 min andfive more rinses with water, as described in Cardenas et al. (1995).Sterile bean seeds were transferred to special plates with wet papertowels, covered with foil and then transferred to a growth chamberat 27�C. After 48 h, seeds were germinated and ready to use in ourexperiments.
Mounting the living root hairs
The 2-day-old seedlings were placed in liquid Fahreus medium atpH 6.0. After 8 h root hairs were usually well adapted to the med-ium. Intact seedlings containing the growing root hairs weremounted in chambers constructed from large Petri dishes. Thesewere perforated in the center, and the hole was covered with a largeglass cover slip glued with silicon. Seedlings were visualized undera Diaphot 300 (Nikon, http://www.nikon.com) inverted microscopewith an 40·/1 NA water immersion lens (Nikon). The chambercontained a layer of solid Fahreus medium (phytagel 0.8%), and theseedlings were set over this layer. At this point, growth medium wascontinuously perfused with a peristaltic pump at 0.2 ml min)1 (Bio-Rad, http://www.bio-rad.com). The total volume in the chamber wasmaintained in 2.5–3 ml, on average, and the root region wascovered with cellophane paper. The solid Fahreus medium andthe cellophane paper helped to prevent root movement.
Treatment of root hair cells with an ROS-sensitive
(CM-H2DCFDA) and reference dye (CMTPX)
In brief, the ROS-sensitive probe CM-H2DCFDA [5-(and-6)-chlor-omethyl-2¢,7¢-dichlorodihydrofluorescein diacetate, acetyl ester](Molecular Probes, http://probes.invitrogen.com) was dissolved inDMSO (Sigma-Aldrich, http://www.sigmaaldrich.com) and cen-trifuged for 2 min at 8000 g to remove non-dissolved particles.Then, the dye solution was diluted with Fahreus medium at a finalconcentration of 30–50 lM and then added to the plate, replacing theoriginal medium. After 15 min, the medium was replaced with freedye and measurements were performed. This procedure was car-ried out carefully to avoid any mechanical stress to cells. Whenperforming ratio-imaging, the reference dye Cell tracker� redCMTPX (Invitrogen, http://www.invitrogen.com) was dissolved inDMSO as a stock solution of 30 lM. Special plates containing theseedlings with the growing root hair cells were treated with theCMTPX dye for 2–3 h. After this time, the dyes were clearly locatedin the cytoplasm, and were excluded from the vacuoles (Figure S3).Then, the ROS-sensitive dye was added and observed 60 min laterunder the fluorescence microscope.
Treatment of root hair cells with DPI, H2O2, chitosan,
UV and ATP
Root hairs were treated with DPI (Sigma-Aldrich), which is an in-hibitor of NADPH oxidase and other flavin-containing enzymes. DPIwas dissolved in DMSO and used at 40 lM. H2O2 (Sigma-Aldrich)was freshly prepared each time and used at a concentration of50 lM. Chitosan (Sigma-Aldrich) was prepared according to themethod of Hadwiger and Beckman (1980), dissolved in water andthen cleaved by exposure to glacial acetic acid for more than 12 h.Then, the fragments were neutralized by adjusting the pH to 6.0(Hadwiger and Beckman, 1980). The resulting mixture was used at afinal concentration of 100 mg L)1 by diluting the stock solution withFahreus medium. Treatment with UV was automatically performedas follows: the UV light source was set to open for 5 s, and then the
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shutter was closed so that we could open the path for excitation at485 nm, take an image and visualize the intracellular ROS level ateach point. ATP was prepared as a 0.1 M stock solution in Tris bufferat 180 nM as follows: 45 ll of 1 M Tris base plus 205 ll of dH2O weremixed carefully and then transferred to an Eppendorf tube con-taining 14 mg of ATP with shaking for 30 s until all of the ATP wasdissolved; aliquots were stored at )80�C.
Incubation of root hairs with NFs
Rhizobium etli NFs were purified by HPLC and applied to plant rootsas previously described (Cardenas et al., 1995). Before treatment,NFs were mixed with 0.5 ml of the same medium that the seedlingshad been growing in, and were then added to the growing root hairswith a peristaltic pump to replace the NF-free medium. As a nega-tive control, 10)8
M penta-N-acetylchitopentaose (Seikagaku, http://www.seikagaku.co.jp) dissolved in CHAPS {non-denaturing, zwit-terionic detergent [3-(3-cholamidopropyl)-dimethylammonio]-1-propane-sulfonate; Sigma-Aldrich} was used.
Image acquisition and processing
All images were acquired with a CCD camera (Sensys; RoperScientific, http://www.roperscientific.com) attached to a NikonTE300 inverted microscope with a 40·/1 NA water immersionobjective lens. Loaded cells were excited using a xenon illumina-tion source (DG-4; Sutter Instruments, http://www.sutter.com),which contained a 175 W ozone-free xenon lamp (330–700 nm) anda galvanometer for a wavelength switch. The ROS-sensitive dyeexcitation was 485 nm and the emission was collected at 535 nm(bandpass: 25 nm). The CMTPX dye was excited at 555 nm and theemission was collected at 605 nm (bandpass: 30 nm). The besttemporal and spatial resolutions were achieved when cells wereexposed for 15–20 ms at a 490-nm excitation wavelength, with a2 · 2 binning of the CCD camera. Images were acquired eachsecond, which was fast enough to detect immediate changes inROS levels. These short exposure times were crucial; otherwisephoto-oxidation would have contributed a continuous signal in-crease (Figure S4). All of the filters used were from ChromaTechnology (http://www.chroma.com), and emission filters werelocated in a filter wheel (Sutter Instruments, http://www.sutter.com). The set-up was automatically controlled by METAMORPH/METAFLUOR software (Universal Imaging, http://www.moleculardevices.com). Finally, images were prepared for publication usingAdobe PHOTOSHOP software (http://www.adobe.com).
Acknowledgements
This work was supported by grants from Direccion General deAsuntos del Personal Academico (DGAPA), Universidad NacionalAutonoma de Mexico, Nos IN228903 (LC) and IN204305 (CQ);CONACyT 58323 (LC), 42560-Q (CQ) and 42562-Q (FS). We thankLiliana Martinez, Maria Luisa Barroso, Olivia Santana and NoreideNava for technical support. We also thank Dr Otto Geiger, ChrisWood and Peter K. Hepler for their critical reading of the manuscript.
Supporting Information
Additional Supporting Information may be found in the onlineversion of this article:Figure S1. A time series of a living root hair cell from Phaseolusvulgaris responding to Nod factors (NFs) from Rhizobium etli.
Figure S2. A time series of a living root hair cell from Phaseolusvulgaris responding to Nod factors (NFs) using a pseudo-ratio-imaging approach.Figure S3. Root hair cells showing the cytoplasmic distribution ofthe reactive oxygen species (ROS)-sensitive (left-hand image) andreference dyes (middle image). The DIC image that depicts thecytoplasm distribution is also included (right-hand image).Figure S4. Effect of exposure time in root hair cells loaded with areactive oxygen species (ROS)-sensitive dye and a reference dye forratiometric imaging of intracellular ROS levels.Please note: Wiley-Blackwell are not responsible for the content orfunctionality of any supporting materials supplied by the authors.Any queries (other than missing material) should be directed to thecorresponding author for the article.
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