© 2016. Published by The Company of Biologists Ltd | Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
RESEARCH ARTICLE
FRMD4A–cytohesin signaling modulates the cellular release
of tau
ABSTRACT
One of the defining pathological features of Alzheimer’s disease is
the intraneuronal accumulation of tau (also known as MAPT) protein.
Tau is also secreted from neurons in response to various stimuli and
accumulates in the cerebrospinal fluid of Alzheimer’s disease
patients. Tau pathology might spread from cell to cell through a
mechanism involving secretion and uptake. Here, we developed an
assay to follow cellular release and uptake of tau dimers. Individual
silencing of ten common late-onset Alzheimer’s disease risk genes in
HEK293T cells expressing the tau reporters suggested that FRMD4A
is functionally linked to tau secretion. FRMD4A depletion by using
RNA interference (RNAi) reduced and overexpression increased tau
secretion. The activity of cytohesins, interactors of FRMD4A and
guanine-nucleotide-exchange factors of Arf6, was necessary for
FRMD4A-induced tau secretion. Increased Arf6 and cell polarity
signaling through Par6 and atypical protein kinase Cζ (aPKCζ)
stimulated tau secretion. In mature cortical neurons, FRMD4A RNAi
or inhibition of cytohesins strongly upregulated secretion of
endogenous tau. These results suggest that FRMD4A, a genetic
risk factor for late-onset Alzheimer’s disease, regulates tau secretion
by activating cytohesin–Arf6 signaling. We conclude that genetic risk
factors of Alzheimer’s disease might modulate disease progression
by altering tau secretion.
KEY WORDS: Alzheimer’s disease, Neurodegenerative disease,
Functional genomics, Polarity signaling, Risk gene, PARD6A
INTRODUCTION
Tau (also known as MAPT) is a microtubule-associated protein
normally localized in the cytosol of neurons and other cells
(reviewed by Buée et al., 2000). Intraneuronal accumulation of
hyperphosphorylated and fibrillar aggregated forms of tau results in
the formation of pathological neurofibrillary tangles that characterize
several neurodegenerative diseases, including Alzheimer’s disease
(Ballatore et al., 2007; Morris et al., 2011). In patients suffering from
Alzheimer’s disease, and also other forms of central nervous system
(CNS) injury, increased tau levels are found in the cerebrospinal fluid
(CSF) (Ost et al., 2006; Vigo-Pelfrey et al., 1995). Previously, CSFtau was thought to mostly originate from degenerated axons and dead
neurons (Blennow et al., 1995). However, tau is also found in the CSF
of healthy human subjects (Blennow et al., 1995; Vandermeeren et al.,
1
2
Neuroscience Center, University of Helsinki, FI-00014 Helsinki, Finland. Institute
of Clinical Medicine-Neurology, University of Eastern Finland, FI-70211 Kuopio,
3
Finland. Department of Neurology, Kuopio University Hospital, FI-70029 Kuopio,
4
Finland. Institute of Biomedicine, University of Eastern Finland, FI-70211 Kuopio,
Finland.
1993; Vigo-Pelfrey et al., 1995) and interstitial fluid of healthy wildtype mice (Yamada et al., 2011).
Recent data suggest that misfolded tau can propagate from cell to
cell in a prion-like fashion (Frost et al., 2009; Sanders et al., 2014). Tau
can be released from cells, including neurons, in the absence of disease
or toxicity, and tau release is enhanced by neuronal activity (Pooler
et al., 2013) and modified by changes in the tau protein that are
associated with tauopathies (Karch et al., 2012). Presynaptic glutamate
release is associated with tau secretion (Yamada et al., 2014), and
synaptic contacts enhance cell-to-cell propagation of tau (Calafate
et al., 2015). It has been suggested that full-length non-vesicleassociated tau is released by an unconventional temperature-dependent
secretion process that is not blocked by inhibitors of the conventional
secretory pathway, such as monensin or brefeldin A (Chai et al., 2012).
Tau misfolds into low molecular weight (LMW) oligomers prior
to assembly into fibrils. Tau dimers appear to be a crucial building
block for the formation of tau aggregates, including paired-helical
filaments (PHFs) (Friedhoff et al., 1998). Both extracellular LMW
tau oligomers and short fibrils, but not monomers or long fibrils, can
be taken up by neurons (Wu et al., 2013). Frost et al. have shown that
extracellular tau aggregates, but not tau monomers, are taken up by
cultured cells and can induce fibrillization of intracellular fulllength tau (Frost et al., 2009). Macropinocytosis, an endocytic
process characterized by actin-driven membrane ruffling that allows
internalization of extracellular fluids and macromolecular
structures, has been shown to be involved in cellular uptake of tau
fibrils (Holmes et al., 2013).
The question of how genes associated with late-onset Alzheimer’s
disease (LOAD) confer the risk for sporadic disease is important for
better understanding of the etiology of the disease and for
developing effective therapies. We recently used a proteinfragment complementation assay (PCA)-based in vitro system
combined with individual knockdown of the top ten LOAD risk
genes following RNA interference (RNAi) to study their potential
functional connection to amyloid-beta precursor protein (APP)
metabolism and regulation of tau phosphorylation (Martiskainen
et al., 2015). Here, we developed a sensitive live-cell assay system
for monitoring cellular release and uptake of tau dimers, based on the
PCA principle (Remy and Michnick, 2006). Using a combination of
these assays and small interfering RNAs (siRNAs) against selected
LOAD risk genes, we found that a pathway involving FRMD4A, a
LOAD risk gene (Lambert et al., 2013), together with its partners in
the atypical protein kinase C (aPKC)–Par cell polarity signaling
complex and Arf6, regulate tau secretion.
*Author for correspondence (Henri.Huttunen@helsinki.fi)
RESULTS
A sensitive live-cell assay for monitoring secretion of
tau dimers
Received 18 September 2015; Accepted 24 March 2016
We developed a sensitive live-cell assay system as a quantitative
in vitro model for studying cellular release and uptake of tau dimers.
2003
Journal of Cell Science
Xu Yan1, Niko-Petteri Nykä nen1, Cecilia A. Brunello1, Annakaisa Haapasalo2,3,4, Mikko Hiltunen2,3,4,
Riikka-Liisa Uronen1 and Henri J. Huttunen1,*
RESEARCH ARTICLE
PCA allows detection of interactions of proteins fused with
complementary reporter protein fragments. We have previously
used a PCA based on humanized Gaussia princeps luciferase
(GLuc) (Remy and Michnick, 2006) for studying cellular regulation
of both APP and tau (Martiskainen et al., 2015; Merezhko et al.,
2014; Nykänen et al., 2012). Here, we used a tau dimer PCA
reporter based on the tau 0N4R isoform carrying complementary
GLuc fragments (Fig. 1). Luminescence generated in washed cell
monolayers served as a quantitative measure of the amount of
intracellular tau dimers, whereas the luminescence signal in celland debris-cleared conditioned medium was used as a readout of tau
secretion.
Expression of tau–GLuc reporter proteins was compared to nontagged tau in HEK293T cells (Fig. 2A). Coexpression of tau–
GLuc1 and tau–GLuc2 in HEK293T cells resulted in a high level of
PCA signal. As the highest PCA signals were generated by reporter
constructs that carried the GLuc fragment at the C-termini (Fig. 2B),
we proceeded with assay development based on tau–GLuc1C and
tau–GLuc2C constructs. Expression of tau reporters alone or in
combination with free GLuc fragments did not generate
luminescence signal (Fig. 2C,D). When tau–GLuc1 and tau–
GLuc2 (hereafter tau–GLuc1/2) constructs were expressed together,
there was high luminescence generated by washed cell monolayers
but also a strong luminescence signal present in the cleared culture
medium (Fig. 2D). The signal from the medium was independent of
changes in lactate dehydrogenase (LDH) release, suggesting that the
appearance of tau reporters in media was not due to passive leakage
and disruption of cells (Fig. 2D). Both intracellular and secreted tau
levels correlated with the level of tau–GLuc1/2 reporter gene dose
(Fig. 2E). During a 24-h observation period, tau–GLuc1/2 reporters
accumulated in serum-free culture medium with linear kinetics for
up to 20 h, as shown by a LDH-normalized tau secretion PCA
(Pearson r 2=0.9715; Fig. 2F).
A previous report using the split GFP system to study tau
oligomerization found that aggregation reduced the signalgenerating ability of the tau reporter system (Chun et al., 2007).
Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
Western blot analysis of tau–GLuc species from the cell lysate
showed that monomeric tau–GLuc1/2 reporters migrated at
∼70 kDa and with a minor band at ∼140 kDa representing
dimeric tau, and some lower bands likely representing truncated
tau species (Fig. 2G). Chemical crosslinking (BS3) was used to
preserve higher oligomeric tau species in both the cell lysate and
conditioned medium. In the crosslinked, concentrated medium
sample, there was a weak band corresponding to monomeric tau,
and the rest of the tau immunoreactivity appeared as a high
molecular mass smear (Fig. 2G), similar to previously described
in vitro generated tau fibrils (Wu et al., 2013). In cell lysates, the
monomeric tau band remained strong even after crosslinking, with
some additional dimeric and trimeric and tetrameric bands visible.
When the tau–GLuc1/2 conditioned medium was resolved on a
native gel, a roughly equal ratio of tau–GLuc monomers and dimers
was observed (Fig. 2H). In addition, some tau–GLuc was trapped in
the stacking gel suggesting that some tau–GLuc1/2 in the
conditioned medium was in an aggregated form. These results
show that the majority of the secreted tau–GLuc reporters are in the
form of monomers, dimers and soluble pre-aggregates or fibrils, and
thus the GLuc tag does not interfere with the normal
oligomerization and aggregation behavior of tau.
Next, we studied the reversibility of the tau–GLuc PCA system in
a detergent titration experiment. As expected, addition of SDS to
samples containing either full-length GLuc enzyme or tau–GLuc1/2
reporter complexes completely suppressed all luminescence signal
starting from 0.01% concentration of the detergent (Fig. 2I, left
panel). Addition of Triton X-100, a milder non-ionic detergent
capable of dissociating protein complexes, had no effect on the
activity of the GLuc enzyme even up to 1% concentration, whereas
luminescence derived from tau–GLuc1/2 reporter complexes was
completely suppressed by only 0.1% detergent concentration
(Fig. 2I, middle panel). A similar effect was observed with
saponin, a glucoside with detergent properties (Fig. 2I, right panel).
These data suggest that the majority of tau–GLuc1/2-derived
luminescence signal is generated by tau dimers that are reversibly
Journal of Cell Science
Fig. 1. Experimental design used in this study. GLuc
PCA-based detection of tau dimer release and uptake, and
the screening strategy for studying the effects of LOAD
susceptibility genes on tau release and uptake.
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Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
Fig. 2. See next page for legend.
associated. Moreover, given that it is highly unlikely that the soluble
tau–GLuc aggregates observed in Fig. 2H would be dissolved by
0.1% Triton X-100, it seems that the tau–GLuc in the aggregate
form is not capable of generating luminescence.
Whereas the tau–GLuc reporter dimers accumulated in the culture
medium, a PCA reporter complex consisting of tau and the peptidylprolyl cis-trans-isomerase Pin1 (Nykänen et al., 2012), was not
secreted at high levels (Fig. 2J). Ceramide regulates exocytosis
2005
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RESEARCH ARTICLE
Fig. 2. GLuc PCA-based detection of tau dimer release. (A) Western blot
analysis of tau–GLuc reporter constructs and non-tagged tau in HEK293T
cells. GAPDH was used as loading control. (B) Expression of different
combinations of tau–GLuc reporters carrying the luciferase fragments either at
the N- or C-termini. (C) GLuc fragments expressed alone or with a single
luciferase fragment attached to tau do not generate significant background
signal. (D) The tau–GLuc1C and tau–GLuc2C PCA signal in washed cell
monolayers (left) and in conditioned medium (middle) is shown. Relative LDH
release (right) was used as a release control. (E) The tau PCA signal intensity
in cells and medium is dependent on the reporter gene dosage (reporter
plasmids at 60 ng, 80 ng and 100 ng per well). (F) Tau release kinetics during a
24-h incubation. The tau dimer level in the medium was determined by PCA,
and the PCA signal was normalized to the LDH release. All values are relative
to the 24-h timepoint. (G) Western blot analysis of tau–GLuc reporter
constructs in cell lysates and conditioned medium. Concentration (3×) and
crosslinking was used to facilitate detection of secreted tau–GLuc reporters.
(H) Native PAGE analysis of tau–GLuc1/2 in 100× concentrated conditioned
medium. 100× concentrated medium from mock-transfected cells (–) was used
as a control. (I) The reversibility of the tau–GLuc1/2 interaction (red) in
conditioned medium was studied by titrating with SDS (left panel), Triton X-100
(middle panel) and saponin (right panel). Full-length Gaussia luciferase (blue)
was used as a control. (J) Comparison of cellular and medium PCA signals
from cells expressing tau–GLuc1/2 and Pin1–GLuc1 and tau–GLuc2
reporters. (K) The effect of GW4869 (10 µM, 24 h) on tau–GLuc1/2 reporter
release. RLU, relative light units. Results are mean±s.e.m. from three or four
replicate experiments. *P<0.05, ***P<0.001 (ANOVA).
(Rohrbough et al., 2004) and exosomal secretion (Trajkovic et al.,
2008), and tau might be secreted in association with small vesicles
such as exosomes (Saman et al., 2012) and other microvesicles
(Dujardin et al., 2014). GW4869, an inhibitor of ceramide
generation by neutral sphingomyelinase (nSMase), reduced tau–
GLuc1/2 reporter secretion from HEK293T cells by 32% (Fig. 2K)
suggesting that tau secretion could be linked to sphingomyelin
metabolism and membrane microdomains associated with ceramide
signaling.
The total tau content in the cell lysate and conditioned medium
was determined by enzyme-linked immunosorbent assay (ELISA)
and normalized to the total protein content. Cell lysates contained
on average 16,700±1300 pg of tau per µg of protein whereas
the medium contained 77.6±7.3 pg of tau per µg of protein
(mean±s.e.m.; Fig. 3A). Based on these values, it seems that less
than 0.5% of the cellular tau is released in our HEK293T cell
system. This is comparable to a previous report showing that 0.1–
0.3% of cellular tau is released from transfected HEK293 T-Rex
cells and from human induced neurons (Chai et al., 2012).
It remains currently unclear whether tau is secreted inside or in
association with microvesicles (Dujardin et al., 2014; Saman et al.,
2012; Simón et al., 2012), in vesicle-free form (Chai et al., 2012;
Kim et al., 2010a) or as a mixture of those. In the HEK293T cellbased system, 99.8% of the tau dimer-derived PCA signal was
abolished after addition of 0.005% (v/v) trypsin to the conditioned
medium (Fig. 3B). Addition of 0.005% saponin (v/v) together with
0.005% trypsin resulted in a 99.9% loss of the PCA signal. These
data suggest that the majority of tau dimers are in vesicle-free form,
with less than 0.5% of secreted tau being inside vesicles. tau–
GLuc1/2- conditioned medium was next fractionated into ectosomal
(larger microvesicles), exosomal and vesicle-free fractions
(Fig. 3C), and their tau content was analyzed by western blotting
(Fig. 3D). Owing to the low level of vesicular tau, the unfractionated
and vesicle-free media fractions were further concentrated by
performing an Amicon filter centrifugation before loading onto the
gel. Semi-quantitative analysis of the western blots confirmed that
the majority (99.7%) of tau secreted by HEK293T cells was in
vesicle-free form whereas ectosomal (0.22%) and exosomal
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(0.05%) tau represented a small minority of the extracellular tau
produced by these cells (Fig. 3E). PCA analysis also confirmed that
the vast majority of the tau-dimer-derived PCA signal remained in
the vesicle-free fraction after the ultracentrifugation steps (Fig. 3F).
Taken together, these data characterize a PCA-based assay for
monitoring cellular release of soluble tau dimers.
Studying cellular uptake of tau dimers using the tau–GLuc
PCA
In order to study cellular uptake of our tau reporters, we first
conditioned medium for 24 h with HEK293T cells expressing
tau–GLuc1 and tau–GLuc2. When naïve recipient cells were
exposed to the tau–GLuc1/2-conditioned medium for 4 h, washed
with PBS and immunostained for tau, a punctate intracellular tau
pattern was observed (Fig. 4A, right) suggesting that some of the
tau–GLuc1/2 reporters had been internalized by the cells. Cells
exposed to conditioned medium generated by mock-transfected
cells did not show similar tau-immunoreactive puncta (Fig. 4A,
left).
PCA data further showed that a simple washing step by PBS
abolished >99% of the cell-bound PCA signal (Fig. 4B),
suggesting that although extracellular tau species bind to the cell
surface, the tau uptake process in HEK293T cells is not very rapid
or efficient. Heparan sulfate proteoglycans (HSPGs), which are
ubiquitously expressed on cell surfaces, mediate uptake of tau
assemblies from monomers to oligomers and fibrils (Holmes et al.,
2013; Mirbaha et al., 2015). An additional washing step with
20 µg/ml heparin further reduced the signal. Addition of trypsin to
the cells after these washing steps showed that majority of the cellsurface-bound tau had been removed, suggesting that the
remaining PCA signal represents internalized tau species.
Further addition of saponin, to allow cell-membrane penetration
of trypsin, abolished the remaining cell-bound signal (Fig. 4B).
Thus, a washing procedure including three steps [PBS, heparin
(20 µg/ml in DMEM) and PBS] was used in all subsequent tau
uptake experiments.
As shown in Fig. 4C, the accumulation kinetics of the tau PCA
signal suggest a saturable mechanism, with the uptake rate slowing
down after 4 h. Therefore, an exposure time of 4 h was used in all
subsequent tau uptake experiments. Overall, the internalized tau
PCA signal was low, possibly due to re-secretion of a significant
portion of uptaken tau (data not shown). Addition of GW4869,
previously shown to reduce tau secretion (Fig. 2K), to the cells 16 h
before and during incubation with tau-conditioned medium
significantly increased the tau PCA signal retained by the cells
(by up to 184%; Fig. 4D), supporting the idea of rapid re-secretion
of internalized tau dimers.
RNAi screen of LOAD susceptibility genes
In order to study whether LOAD risk genes are functionally linked
to tau secretion and uptake, we used a panel of siRNAs for knocking
down ApoE, BIN1, CLU, ABCA7, CR1, PICALM, CD33, CD2AP,
FRMD4A and TREM2 expression (Martiskainen et al., 2015)
(Fig. 1). These top ten LOAD risk genes were selected based on
meta-analyses of LOAD genetic association studies (Bertram et al.,
2007), with the addition of two recently identified risk genes
(Guerreiro et al., 2013; Jonsson et al., 2013; Lambert et al., 2013).
MS4A6A and MS4A4E were excluded as they are not expressed in
HEK293T cells. The knockdown efficiencies of the selected
siRNAs were determined by quantitative real-time PCR (qPCR)
in our previous study (Martiskainen et al., 2015). We co-transfected
tau–GLuc1 and tau–GLuc2 PCA reporters with the selected
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Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
Fig. 3. Characterization of the tau–GLuc
reporters in conditioned medium. (A) ELISA
analysis of total tau levels in HEK293T cell lysates
and conditioned medium after transient
transfection with tau–GLuc1/2 reporters.
(B) Addition of 0.005% (v/v) trypsin to the taureporter-conditioned medium shows that the
majority of HEK293T-secreted tau is free-floating
and not protected by vesicle membrane. Addition
of 0.005% (v/v) saponin and trypsin shows that
permeabilization of the vesicle membrane allows
nearly complete degradation of the reporter
proteins in the medium. Results in A and B are
means±s.e.m. (n=3). (C) Schematic presentation
of the conditioned medium fractionation process.
Ectosomal, exosomal and vesicle-free fractions
were separated by sequential centrifugation.
(D) Western blot analysis of tau–GLuc1/2 reporter
proteins in conditioned medium and isolated
media fractions. Vesicle-free, ectosomal,
exosomal and unfractionated full media were
analyzed. Cell lysate served as a positive control
of tau expression. Some samples were
concentrated 100× by filter centrifugation to
facilitate detection of tau. Flotillin-1 was used as a
marker of ectosomes. (E) Optical-density-based
quantification of tau–GLuc1/2 levels (from
experiments as in D). All values are relative to the
tau–GLuc1/2 level in full medium (100%). (F) PCA
analysis of the tau–GLuc1/2 dimer signal in
unfractionated medium and isolated media
fractions. RLU, relative light units. Results in E and
F show the mean from two replicate experiments.
However, in CHME-5 cells transfected with both tau–GLuc1 and
tau–GLuc2 PCA reporters and either TREM2 or CD33 siRNA,
there was no change in either cellular tau dimerization or secreted
tau dimer content (Fig. 5D). This suggests that the effects of
TREM2 and CD33 on tau release seen in HEK293T cells are not
recapitulated in a microglial cell line.
FRMD4A–cytohesin signaling regulates cellular release
of tau
As our previous study has shown that FRMD4A is reduced in the
brain of LOAD patients and functionally linked to tau (Martiskainen
et al., 2015), we wanted to further explore the role of FRMD4A in tau
secretion. For FRMD4A overexpression studies, we first verified that
tagged FRMD4A constructs are properly expressed and localized in
HEK293T cells. Expression of FRMD4A–HA and FRMD4A–GFP
resulted in similar localization patterns, mostly in cytosolic vesiclelike structures (Fig. 6A). Coexpression of FRMD4A–GFP with tau–
GLuc2 did not reveal substantial colocalization of the two proteins.
In HEK293T cells, overexpressed tau was present close to the plasma
membrane, in regions where occasional FRMD4A-positive vesicles
were also observed (Fig. 6B, arrowheads). The FRMD4A–HA
construct was also used to verify the silencing efficiency of the
FRMD4A siRNA at the protein level. Coexpression of the FRMD4A
siRNA with the FRMD4A–HA plasmid resulted in a 39% reduction
2007
Journal of Cell Science
siRNAs in HEK293T cells. Knockdown of any of the LOAD genes
did not result in significant changes in the level of intracellular tau
dimers (Fig. 5A). For assessing tau secretion, conditioned medium
was analyzed for both tau dimer content, by PCA, and LDH release,
as a specificity control. Based on the LDH-normalized tau PCA
signal in the medium, knockdown of CD33, CD2AP, FRMD4A and
TREM2 reduced tau secretion (Fig. 5B). TREM2 knockdown had
the strongest effect (−55%), whereas the effect of CD33, CD2AP
and FRMD4A was between −19% and −27% (mean values from
cells transfected with two independent siRNAs per target gene).
For the tau uptake assay, we transfected recipient cells with
siRNAs against LOAD risk genes, exposed them to tau–GLuc1/2conditioned medium for 4 h, washed them and measured the level
of the internalized tau dimer PCA signal (Fig. 5C). Only ApoE
knockdown caused a significant change in tau uptake (+29%).
TREM2 and CD33 are strongly expressed in myelomonocytic
cells and their expression level in HEK293T cells is low. Next, we
used the tau release PCA assay and siRNA in the CHME-5 cell line,
which is derived from primary cultures of human fetal microglial
cells (Janabi et al., 1995). Because tau accumulates in microglial
cells during aging, overexpression of tau in microglial cells induces
their activation (Wang et al., 2013) and microglia might facilitate
spreading of tau pathology (Asai et al., 2015), the effect of TREM2
and CD33 on tau secretion could be a potentially interesting lead.
Fig. 4. Tau–GLuc1/2 reporter uptake in naïve HEK293T recipient cells.
(A) Immunofluorescence micrographs of tau–GLuc1/2 internalized by naïve
HEK293T cells. After 4 h incubation of naïve recipient cells in the mock- (left) or
tau–Gluc1/2- (right) conditioned medium, cells were washed, fixed and
immunostained with the tau-5 antibody. Nuclei were counterstained with
Hoechst 33342. Scale bar: 10 µm. (B) Comparison of the effects of wash
conditions on cell-bound tau as determined by the PCA. Naïve HEK293T cells
were exposed to tau–GLuc1/2 conditioned medium for 24 h. Before PCA
measurement, conditioned medium was removed from the wells and the cells
were washed as indicated. (C) Tau dimer uptake kinetics over a 24-h period.
Values are relative to maximal uptake at 24 h. (D) Addition of GW4869 to the
conditioned medium enhances the cellular PCA signal, and thus the amount of
internalized tau–GLuc1/2 reporters. Recipient cells were pretreated with
GW4869 or an equal volume of DMSO for 16 h before a medium change and
during the 4-h exposure to tau–GLuc1/2-conditioned medium. Results are
mean±s.e.m. (n=3). **P<0.01 (ANOVA).
of the FRMD4A–HA protein level (Fig. 6C). This is in line with the
reduction of FRMD4A mRNA level (−41%) with this siRNA
(Martiskainen et al., 2015).
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Increasing levels of FRMD4A expression dose-dependently
increased the levels of tau dimer PCA signal in medium (maximum
+146%), whereas the cellular tau dimer PCA level remained almost
unchanged (Fig. 6D). These data, together with that shown in
Figs 5B and 6C, show that the level of FRMD4A expression
correlates with the level of tau release in HEK293T cells. In
epithelial cells, FRMD4A has been shown to act as a scaffolding
protein connecting the cell polarity complex between Par3 and Par6
(PARD3 and PARD6A, respectively) to Arf6 signaling mediated by
cytohesin-1 (Ikenouchi and Umeda, 2010). SecinH3, a smallmolecule antagonist of cytohesin and Sec7 (the yeast cytohesin)
guanine-nucleotide-exchange factor (GEF) activity (Hafner et al.,
2006), suppressed the tau secretion induced by FRMD4A
overexpression while increasing intracellular tau dimer levels
(Fig. 6E). In cells expressing endogenous levels of FRMD4A,
SecinH3 also increased intracellular tau levels but had only a mild
effect on tau secretion (Fig. 6F).
FRMD4A–cytohesin signaling enhances translocation of active
Arf6 to the plasma membrane (Ashery et al., 1999; Hafner et al., 2006;
Ikenouchi and Umeda, 2010). Similar to overexpression of FRMD4A,
overexpression of wild-type Arf6 in HEK293T cells expressing tau–
GLuc1/2 cells strongly enhanced both intracellular tau dimerization
and tau secretion. Overexpression of wild-type Arf6 caused a strong
increase in tau secretion (Fig. 6G), which was almost completely
blocked by coexpression of Arf6 siRNA but was not affected by
SecinH3 treatment. Expression of the dominant-negative mutant Arf6
T27N also mildly increased tau secretion, but, in comparison to wildtype Arf6, the effect was significantly lower (−69%; Fig. 6H). The
constitutively active Arf6 Q79L mutant had the strongest impact on
tau secretion, with a more than 30-fold increase compared to
endogenous Arf6 levels.
aPKC subtype ζ (aPKCζ) is a ceramide-binding protein and, as a
part of the Par polarity signaling complex, regulates several
membrane trafficking events also related to exocytosis (Horikoshi
et al., 2009; Joberty et al., 2000; Wang et al., 2009). Overexpression
of aPKCζ enhanced tau secretion with an effect comparable to
FRMD4A overexpression (Fig. 7A). Expression of the C-terminal
ceramide-binding region of aPKCζ (C20ζ, amino acids 405–592)
(Wang et al., 2009) did not significantly affect basal tau secretion
but coexpression of C20ζ suppressed aPKCζ-overexpressioninduced tau secretion.
Par6 links aPKCζ to Par3 (Joberty et al., 2000), and Par3 has
been shown to activate Arf6 through FRMD4A (Ikenouchi and
Umeda, 2010). Expression of wild-type Par6 resulted in a
sevenfold increase in tau secretion whereas expression of Par6
(S345A), an inactive mutant not phosphorylated by aPKC
(Gunaratne et al., 2013), had little effect (Fig. 7C). SecinH3
treatment had no effect on aPKCζ- or Par6-induced tau secretion,
suggesting that cytohesin GEF activity is not required for this
effect of the aPKC–Par6 complex (Fig. 7B,D). These results show
that tau secretion is regulated by the activity of the FRMD4A–
cytohesin–Arf6 pathway and the associated aPKC–Par6 polarity
complex signaling.
Whereas cytohesins (also known as mSec7 proteins) have a role
in vesicle transport at the presynaptic terminal (Ashery et al., 1999;
Neeb et al., 1999), the role of FRMD4A in neurons remains poorly
understood. We transduced cultures of mouse cortical neurons with
lentivirus expressing FRMD4A short hairpin RNA (shRNA),
resulting in 99% reduction of endogenous FRMD4A mRNA
levels (Fig. 8A). Mature [21 days in vitro (DIV)] cortical neurons
were transduced with a GFP-expressing lentivirus, an FRMD4A
shRNA lentivirus or were left untreated, and medium was
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conditioned for 3 days. A mouse-specific ELISA was used to
measure secretion of endogenous tau. As shown in Fig. 8B,
silencing of FRMD4A expression in neurons significantly
promoted tau secretion (+390%, P=0.046 versus untransduced
control cells). As the effect was opposite to what was observed in
HEK293T cells, we also tested the effect of the cytohesin inhibitor
SecinH3. Compared to vehicle-treated mature neurons, SecinH3
also enhanced tau secretion (Fig. 8C), similar to the FRMD4A
shRNA. The maximum effect was reached at 20 µM (+204%,
P=0.031). These results suggest that altering the activity of
FRMD4A–cytohesin signaling significantly affects tau secretion,
but compared to non-neuronal cells, such as HEK293T, the effect is
unexpectedly in the opposite direction.
DISCUSSION
Here, we report development of a new assay system for monitoring
the cellular release and uptake of soluble tau dimers. Although the
assay was designed to be a minimally invasive live-cell system, there
are two potential caveats: the use of GLuc reporter fusion fragments
at the C-terminus of tau and the requirement of overexpression of
tau–GLuc reporter constructs. However, the C-terminal GLuc fusion
of tau did not interfere with the normal expression, localization
and oligomerization or aggregation behavior of tau. In our transienttransfection-based setup in HEK293T cells, tau reporter expression
was not associated with significant toxicity. LDH release was used
to control for unspecific release of cytosolic proteins.
The PCA signal generated by the secreted tau–GLuc1/2 reporters
appears to be largely derived from tau dimers, which have been
previously shown to be the crucial building blocks for formation of
tau aggregates and PHFs (Friedhoff et al., 1998). Native gel and
western blot analyses suggested that the secreted tau–GLuc
reporters spontaneously assembled into dimers and, to some
degree, into soluble aggregates or fibrils. Importantly, the tau–
GLuc1/2 dimers could be dissociated with low concentrations of
Triton X-100 and saponin suggesting that they are reversibly
associated. The association of GLuc PCA reporters has previously
shown to be reversible (Remy and Michnick, 2006). However, in a
bimolecular fluorescence complementation (BiFC) assay, which is
using complementary fragments of fluorescent reporter proteins, the
reporter proteins tend to lock the interacting proteins together
(Kodama and Hu, 2012). Moreover, given that 0.1% Triton X-100 is
unlikely to dissolve aggregated or fibrillar forms of tau, and, at this
concentration, all of the tau–GLuc1/2 PCA signal was lost from the
conditioned medium samples, it seems that the aggregated tau
reporters are incapable of generation of luminescence. In this regard,
our GLuc PCA would be similar to the previously reported tau BiFC
assay that showed a reduced signal upon tau aggregation (Chun
et al., 2007). Thus, based on available evidence, we conclude that
the tau–GLuc PCA assay is capable of detection of secreted and
internalized tau species that are mostly in dimeric form.
In our system, more than 99% of secreted tau was found in
vesicle-free form with only a minor fraction pelleted together with
ectosomes and exosomes. It is possible that vesicle-free tau is
overrepresented owing to post-secretion release of tau from
microvesicles such as exosomes (Barten et al., 2011; Kim et al.,
2010b; Saman et al., 2012). Interestingly, we noted that vesicle2009
Journal of Cell Science
Fig. 5. Effect of selected LOAD risk genes on tau secretion and uptake. (A) Levels of intracellular tau dimers. HEK293T cells were co-transfected with tauGLuc1/2 PCA reporters and indicated siRNAs. No alterations in intracellular tau dimerization were observed. Control cells were transfected with 5 nM control
siRNA. Two control siRNAs were used, and their average effect is reported as the control. (B) Cellular release of tau dimers. HEK293T cells were transfected as in A.
LDH release was used to normalize tau secretion values. (C) The effect of gene silencing on cellular uptake of tau dimers. HEK293T cells were transfected
with indicated siRNAs and exposed to conditioned medium containing the tau–GLuc1/2 dimers. (D) Tau dimer release in CHME-5 cells co-transfected with
control, TREM2 and CD33 siRNA. Results are mean±s.e.m. (n=3). *P<0.05, **P<0.01, ***P<0.001 (ANOVA).
Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
Fig. 6. FRMD4A modulates cellular release of tau through cytohesins and Arf6. (A) FRMD4A–HA (top) and FRMD4A–GFP (bottom) localization in transiently
transfected HEK293T cells. The intense vesicle-like staining pattern suggests that FRMD4A is linked to membrane trafficking in HEK293T cells. Scale bar: 10 µm.
(B) FRMD4A–GFP and tau–GLuc2 coexpression in HEK293T does not reveal significant colocalization. Tau localization was revealed by tau-5 immunostaining
and nuclei were counterstained with Hoechst 33342. Arrowheads indicate FRMD4A-containing puncta in tau-enriched areas near the plasma membrane. Scale
bar: 10 µm. (C) Western blot analysis showing that FRMD4A siRNA reduced the expression of FRMD4A–HA protein. Cells were transfected with FRMD4A–HA
and FRMD4A siRNA as in Fig. 5. (D) Overexpression of FRMD4A in HEK293T cells promotes secretion of tau–GLuc1/2 reporters. FRMD4A plasmid was
transfected at 0, 10 ng, 30 ng and 50 ng per well (the total plasmid amount with the tau–GLuc1/2 reporters was 100 ng). Values are relative to mock-transfected
cells with endogenous levels of FRMD4A. (E) Inhibition of cytohesin activity by addition of SecinH3 at the indicated concentrations to the culture medium reduces
FRMD4A-stimulated tau secretion in HEK293T cells overexpressing FRMD4A and tau–GLuc1/2 reporters. (F) SecinH3 increases intracellular tau dimer levels
and has a subtle effect on secretion in HEK293T cells expressing tau–GLuc1/2 reporters (and endogenous FRMD4A). (G) Overexpression of wild-type Arf6
strongly enhances tau secretion, which is effectively blocked by Arf6 siRNA. (H) The effect of the dominant-negative mutant (T27N) and constitutively active
mutant (Q79L) of Arf6 on tau secretion. RLU, relative light units. Results are mean±s.e.m. (n=3). *P<0.05, **P<0.01, ***P<0.001; n.s., not significant (ANOVA).
bound tau is more actively internalized than vesicle-free tau. As tau
internalized via different routes might have a different intracellular
fate, future studies are needed for addressing specific cellular uptake
mechanisms of vesicle-bound versus vesicle-free extracellular tau
species.
Although the tau secretion assay was highly sensitive, in the
uptake assay, the levels of internalized tau were quite low. This
2010
might be partially explained by rapid re-secretion of internalized tau
in HEK293T cells. Macropinocytosis is an endocytic process
used for bulk uptake of macrosolutes and appears to be a major
route of entry for extracellular tau fibrils (Holmes et al., 2013).
Different from endosomes, macropinosomes themselves undergo
rapid exocytosis making their traffic bidirectional and dependent on
regulated coordination of endocytic and exocytic events (Falcone
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Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
Fig. 7. Polarity signaling by aPKCζ and Par6
stimulate tau secretion. (A) aPKCζ overexpression
promotes tau–GLuc1/2 reporter secretion, which is
partially inhibited by expression of the ceramidebinding C-terminus of aPKCζ (C20ζ; amino acids
405–592 of aPKCζ). C20ζ expression alone does not
significantly alter tau secretion. (B) Inhibition of
cytohesin activity by SecinH3 does not reduce tau
secretion stimulated by overexpression of aPKCζ in
HEK293T cells. (C) Overexpression of wild-type Par6
but not the inactive Par6(S345A) promotes tau
secretion but has no effect on intracellular tau dimers
in HEK293T cells. (D) SecinH3 does not suppress the
tau secretion induced by Par6 overexpression. RLU,
relative light units. Results are mean±s.e.m. (n=3).
**P<0.01, ***P<0.001; n.s., not significant (ANOVA).
Strittmatter et al., 1994). Unexpectedly, genes functionally
connected to endocytic pathways and modification of tau
pathology, such as BIN1 (Chapuis et al., 2013) and PICALM
(Xiao et al., 2012), did not affect tau secretion or uptake
significantly. Instead, CD2AP, FRMD4A, TREM2 and CD33
knockdown caused a significant decrease in tau secretion. TREM2
and CD33 are predominantly expressed in myelomonocytic cells,
and their expression level in HEK293T cells is low. Moreover, their
proximal signaling partners, such as DAP12 (also known as
Fig. 8. Reduced FRMD4A level or cytohesin activity promotes secretion of endogenous tau in primary cortical neurons. (A) Mouse cortical neurons
were transduced with lentivirus encoding for GFP (Lenti-GFP) or shRNA against FRMD4A (Lenti-shFRMD4A) or were left untreated (control) at 21 DIV. At 2 days
post transduction, mRNA levels of FRMD4A were analyzed by qPCR and normalized to the GAPDH mRNA levels. (B) The effect of FRMD4A silencing on tau
secretion in cortical neurons. Mouse cortical neurons were prepared and transduced in the same way as in A. Medium was collected 3 days after transduction.
ELISA was used to analyze the tau level in cleared (cell-debris-free) conditioned medium. (C) Mouse cortical neurons were incubated with different concentrations
of SecinH3 or DMSO (control) at 21 DIV. Medium was collected 3 days later. ELISA was used to study the tau level in cleared conditioned medium. Results
are mean±s.e.m. (n=3). *P<0.05, ***P<0.001; n.s., not significant (ANOVA).
2011
Journal of Cell Science
et al., 2006). This might explain the relative inefficiency of tau
uptake and the observed re-secretion of the tau reporters in our
system.
Avila et al. recently hypothesized that, given that several of the
proteins encoded by the top LOAD risk genes interact with tau
(ApoE, BIN1, clusterin and PICALM), these proteins potentially
modify cell-to-cell propagation of tau (Avila et al., 2015). In our in
vitro study, ApoE siRNA affected uptake of tau. This might be
related to the tau-binding property of ApoE (Fleming et al., 1996;
TYROBP), might be lacking from cells that are not of myeloid
origin, limiting or altering their function in commonly used cell
lines like HEK293T. The fact that knockdown of TREM2 or CD33
in a microglial cell line, with higher endogenous expression levels
of both genes, failed to show any effects on tau secretion suggests
that the HEK293T findings might be false-positive hits, possibly
related to off-target effects of siRNA than TREM2 and CD33
function. This also shows that although the in vitro screening system
has certain benefits, functional verification of hits is important.
Using a specific haplotype-based genome-wide association
approach, FRMD4A was identified as a genetic susceptibility
factor for LOAD (Lambert et al., 2013). The functional
connections between FRMD4A protein and Alzheimer’s disease
pathophysiology are currently poorly understood. Single-nucleotide
polymorphisms (SNPs) within the FRMD4A locus are associated
with alterations in the plasma amyloid β peptide (Aβ) levels and the
Aβ42 to Aβ40 ratio in three independent populations from patients not
displaying dementia (Lambert et al., 2013). We recently reported that
the expression of FRMD4A declines in relation to increasing
neurofibrillary pathology in Alzheimer’s disease patients, and
that FRMD4A is functionally linked to both APP metabolism and
tau phosphorylation status in vitro (Martiskainen et al., 2015). Our
current results clearly show that FRMD4A levels in cells are
connected to the level of tau secretion. In non-neuronal
cells, decreased FRMD4A levels reduce the ability of cells to
secrete tau, which might lead to intracellular accumulation,
hyperphosphorylation and toxicity of tau (Gendreau and Hall,
2013; Hall and Saman, 2012). However, in a more physiological and
disease-relevant context, in mature cortical neurons, reduced
FRMD4A levels and cytohesin inhibition, strongly promoted the
secretion of endogenous tau. The difference in the behavior between
our model systems might be explained by the highly specialized and
very tightly regulated secretion machinery of neurons (Südhof,
2013). Thus, reduced FRMD4A levels, as observed in the LOAD
patient brains (Martiskainen et al., 2015), might drive tau secretion
and accelerate disease progression.
FRMD4A regulates epithelial cell polarity by connecting the
Par3–Par6–aPKCζ complex to Arf6 activation through cytohesins
(Ikenouchi and Umeda, 2010). Par polarity complex signaling plays
a crucial role in neuronal polarization (Insolera et al., 2011) but also
in membrane trafficking, including vesicular secretion (Balklava
et al., 2007). Interestingly, cytohesin-1 has been shown to facilitate
synaptic transmission in Xenopus laevis neuromuscular junction,
most likely by making more presynaptic vesicles available for
fusion at the plasma membrane through a direct interaction with
Munc13-1 (also known as Unc13a) (Ashery et al., 1999; Neeb et al.,
1999). By contrast, in hippocampal neurons, Arf6 silencing has
recently been reported to increase synaptic exocytosis, and both
Arf6 silencing and cytohesin inhibition by SecinH3 results in an
increase in the number of docked synaptic vesicles (Tagliatti et al.,
2016). As neuronal tau release appears to be related to plasma
membrane fusion of presynaptic vesicles (Pooler et al., 2013;
Yamada et al., 2014), it seems plausible that FRMD4A, cytohesin
and Arf6 levels and activity in neurons serve as regulators of tau
secretion. Our results thus establish a previously unknown
connection between the activity of the Par6–aPKCζ–FRMD4A–
cytohesin–Arf6 signaling pathway and tau secretion. Interestingly,
inhibition of cytohesin activity has recently been shown to enhance
autophagic flux and to reduce the burden of misfolded SOD1 in
amyotrophic lateral sclerosis (ALS) models (Zhai et al., 2015). It
remains to be seen whether FRMD4A–cytohesin signaling plays a
more general role in the maintenance of neuronal proteostasis.
2012
Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
Polarized delivery of proteins and lipids to specific subdomains
of the plasma membrane is important to a wide range of biological
processes such as epithelial cell polarization and neuronal
synaptogenesis. Our results suggest that the release of tau from
cells is linked to cell polarity signaling through the Par6–aPKC
complex. Defining the molecular mechanisms that regulate tau
secretion will help understanding of how tau pathology propagates
in Alzheimer’s disease and other tauopathies.
MATERIALS AND METHODS
DNA constructs and siRNA
The split Gaussia princeps luciferase (GLuc) system used in this study has
been previously described (Remy and Michnick, 2006). The human
cDNAs for tau (isoform 0N4R) and CD2AP were purchased from Thermo
Scientific. The FRMD4A–GFP plasmid was a gift from Junichi
Ikenouchi (Kyushu University, Fukuoka, Japan) (Ikenouchi and Umeda,
2010), pcDNA3/HA-Arf6 was a gift from Thomas Roberts (Dana-Farber
Cancer Institute, Harvard Medical School, Boston, MA) (Addgene plasmid
# 10834) (Furman et al., 2002), and pCMV5B-Flag-Par6 wt (Addgene
plasmid # 11748) and pMEP5-Flag Par6 S345A (Addgene plasmid # 24648)
were gifts from Jeff Wrana (Department of Molecular Genetics, University of
Toronto, Toronto, Canada) (Ozdamar et al., 2005). aPKCζ cDNA was
acquired from the ORFeome library by the Genome Biology Unit at the
University of Helsinki, and C20ζ (amino acids 405–592) was cloned into the
pcDNA6-V5/His expression plasmid (Invitrogen). shRNA clones (in
pLKO.1) for human TREM2 and CD33, and mouse FRMD4A were
acquired from the TRC1.0 library by the Functional Genomics Unit
Biomedicum Helsinki. All plasmids were sequenced to confirm their identity.
Three siRNAs per each LOAD risk gene and two control siRNAs were
purchased from Invitrogen (Ambion Silencer Select Predesigned siRNA).
Gene-silencing efficiency of siRNAs was determined using qPCR, and the
two most effective siRNAs per target gene were selected for further
experiments (Martiskainen et al., 2015).
Cell culture and transfection
Human embryonic kidney 293T cells (HEK293T) were cultured in
Dulbecco’s modified Eagle’s medium [DMEM with 10% (v/v) FBS
(Gibco, Invitrogen)] and 1% (v/v) L-glutamine-penicillin-streptomycin
solution (Lonza) at 37°C, in 5% CO2 and water-saturated air. Transfection of
HEK293T cells was performed using JetPei and Jetprime reagents
(Polyplus) according to manufacturer’s instructions. Human microglial
CHME-5 cells (Janabi et al., 1995) were cultured and transfected with
JetPrime. Mouse primary cortical neurons were prepared and cultured as
described previously (Nykänen et al., 2012). Neurons were transduced with
lentiviruses after a medium change at 21 DIV. At 3 days post transduction,
the medium was collected for analysis.
Lentivirus production
Four shRNA clones targeting FRMD4A were tested by transient transfection
in N2A mouse neuroblastoma cells. Based on qPCR analysis, one clone was
selected for production of lentiviral particles. Lentiviruses were produced,
stored and used in neuron cultures as described previously (Kysenius et al.,
2012).
Protein-fragment complementation assay
PCA was performed as previously described (Martiskainen et al., 2015).
HEK293T cells were plated on poly-L-lysine-coated white-walled 96-well
plates (Perkin Elmer) at a density of 10,000 cells per well. GLuc reporter
plasmids and siRNA were transfected (100 ng of total plasmid DNA, siRNA
at 5 nM) at 24 h post plating. The culture medium was changed to PhenolRed-free DMEM (Gibco, Invitrogen) without serum 30 min before the
measurement. The PCA signal was read with a Wallac 1420 Victor3
fluorescence multiplate reader (PerkinElmer) or Varioskan Flash multiplate
reader (Thermo Scientific) 48 h post plating by injecting 25 μl of native
coelenterazine (Nanolight Technology) per well (final concentration
20 μM). For a standard experimental condition, four replicate wells were
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Tau secretion assay
At 16 h before measurement, cells transfected with tau–GLuc1/2
reporters were washed once with PBS and changed to Phenol-Red-free
DMEM (Gibco, Invitrogen) without serum (140 μl per well). At 30 min
before measurement, the plate was spun at 200–300 g for 3–5 min using a
swing bucket rotor (Eppendorf, centrifuge 5810) and conditioned PhenolRed-free DMEM was recollected. A total of 75 μl of this conditioned
medium was used for measuring the PCA signal in conditioned medium
(secreted tau dimers), and 50 µl was used for lactate dehydrogenase
(LDH) release measurement (Promega CytoTox 96® Assay, G1781)
according to the manufacturer’s instructions. After collection of
conditioned medium, the cells were changed to 75 μl of fresh PhenolRed-free DMEM and the PCA signal was detected as described for a
standard PCA (intracellular tau dimers). PCA signal in the conditioned
medium was normalized by dividing with the corresponding LDH level
from the same well. For the RNAi screen of tau secretion, tau–GLuc1,
tau–GLuc2 and LOAD risk gene siRNAs (at 5 nM) were co-transfected
into HEK293T cells.
Tau uptake assay
Conditioned medium (Phenol-Red-free DMEM) was collected from
HEK293T cells transfected with tau–GLuc reporters after 24 h
conditioning and cleared by centrifugation at 3000 g for 30 min to remove
cell debris. The level of tau–GLuc1/2 dimers in the medium was determined
by PCA. Untransfected naïve HEK293T cells on 96-well plates were washed
once with pre-warmed PBS and changed to conditioned medium containing
tau–Gluc1/2. After 4 h incubation, the medium was completely removed by
gently pipetting and the cells were washed once with PBS, then incubated
with 20 µg/ml heparin (Sigma) for 5 min to remove cell-surface-associated
tau. Heparin solution was removed, cells were washed with PBS and 75 µl of
Phenol-Red-free DMEM was added to the wells and the cellular PCA signal
was measured as described above. For the RNAi screen of tau uptake,
siRNAs against LOAD risk genes were transfected into HEK293T cells
using JetPrime, and after 24 h cells were changed to fully supplemented
DMEM. Next, at 44 h post plating, the medium was replaced with tau–
GLuc1/2-conditioned medium and incubated for 4 h. Cells were washed and
processed for PCA detection as described above.
Immunofluorescence imaging
Immunofluorescence imaging was performed as previously described
(Kysenius et al., 2012). Cells fixed on glass coverslips were incubated with
tau-5 (Invitrogen, cat. no. AHB0042, 1:600) and anti-HA (HA-7, Sigma,
cat. no. H3663, 1:600) antibodies. After PBS washes, coverslips were
incubated with Alexa-Fluor-568-conjugated anti-mouse-IgG secondary
antibody (Invitrogen, 1:2000). Nuclei were stained with Hoechst 33342
(Invitrogen) and coverslips were mounted with ProLong Gold anti-fade
reagent (Invitrogen). Images were taken with a Zeiss AxioImager M1
epifluorescence microscope.
Western blotting
Western blotting was performed as previously described (Nykänen et al.,
2012). Cells grown on poly-L-lysine-coated six-well plates and transfected
with 3 μg of total DNA per well were washed twice with ice-cold PBS
at 48 h post transfection. Then, cells were lysed and equal amounts of lysate
were resolved on 4–12% gradient Bis-Tris gels (Novex, Invitrogen) under
reducing conditions. Proteins were transferred onto PVDF membranes
(GE Healthcare) with semidry blotting (Bio-Rad). Tau-5 (Invitrogen
#AHB0042, 1:1000), anti-HA (HA-7, Sigma #H3663, 1:1000) and antiGAPDH (6C5, Millipore #MAB374, 1:1000) antibodies, horseradishperoxidase-conjugated secondary antibodies and ECL western blotting
detection reagent (Thermo) were used to detect the chemiluminescence
signal. QuantityOne software (Bio-Rad) was used for quantitative analysis
of western blots.
Native PAGE
Conditioned media were collected and concentrated to 100× with Amicon
Ultra-15 Centrifugal Filters (Merck Millipore, UFC903008). Samples were
prepared using the Novex™ Tris-Glycine Native Sample Buffer (LC2673),
and resolved on NuPAGE™ Novex™ 3-8% Tris-Acetate Protein Gels
(EA0375BOX) with an equal volume of sample per well, using Novex™
Tris-Glycine Native Running Buffer (LC2672; Novex, ThermoFisher
Scientific) according to the manufacturer’s instructions. The gel was
blotted and analyzed as described above.
Protein crosslinking
Protein samples from cell lysates and conditioned media were processed
as described above. When needed, conditioned medium was
concentrated by using Amicon Ultra-15 Centrifugal Filters (Merck
Millipore, UFC903008). Samples with equal amounts of total protein
were incubated for 30 min in room temperature with the non-cleavable
and membrane-impermeable crosslinker BS3 [bis(sulfosuccinimidyl)
suberate; Pierce, Thermo] according to the manufacturer’s instructions.
BS3 was pre-diluted in milli-Q H2O, and added to samples at a final
concentration of 5 mM. Tris-HCl ( pH 7.5) was used as quenching buffer
and added to samples at a final concentration of 50 mM for 15 min at
room temperature. Equal volumes of samples were analyzed by western
blotting.
Media fractionation
For separation of larger microvesicles or ectosomes and exosomes, a widely
used method was employed (Théry et al., 2006). Medium was first cleared at
3000 g for 30 min, followed by centrifugation at 20,000 g for 60 min to
pellet the ectosomal fraction of conditioned medium (Sorvall WX Floor
Ultra centrifuge). The supernatant containing the exosomal fraction of the
medium was carefully transferred to a fresh tube without disturbing the
pellet (not visible). The pellet was washed once with PBS and spun again at
20,000 g for 60 min. After gently removing the supernatant, the pellet was
resuspended either in Phenol-Red-free DMEM for PCA measurement, or
PBS or 1.5× Laemmli buffer for western blot analysis. The volume used for
the resuspension of the pellet was adjusted proportionally according to the
amount of medium loaded for centrifugation. The supernatant was
centrifuged at 100,000 g for 70 min to pellet the exosomal fraction
(Beckman Coulter ultracentrifuge with an SW41 Ti rotor). The exosomal
pellet (not visible) was washed with PBS, spun again at 100,000 g for
70 min and resuspended in the same way as the ectosomal fraction. Flotillin1 (BD Transduction Labs #F65020, 1:500) was used as a marker for
ectosomal vesicles (Kowal et al., 2016).
ELISA
Human tau ELISA measurements were performed by using a commercial
total human-specific tau ELISA kit (KHB0041, Novex, ThermoFisher).
HEK293T cells transfected with tau–GLuc reporters were incubated in
DMEM for 24 h. Medium was then collected and centrifuged at 900 g for
10 min at 4°C and the cells were lysed in western blot extraction buffer. The
protein concentration was determined by a BCA protein assay kit (Thermo)
for both lysate and medium. The ELISA values were normalized to cell
lysate total protein concentration values. Mouse tau ELISA measurements
were performed using a commercial mouse-specific tau ELISA kit
(KMB7011, Novex, ThermoFisher).
Statistical analyses
A minimum of three independent repetitions were used for each experiment.
Microsoft Excel and GraphPad Prism software were used for statistical
analyses and generation of graphs. Statistical significance was evaluated
with two-tailed Student’s t-tests and two-way ANOVA, where appropriate,
with the significance threshold set at P<0.05.
Acknowledgements
We thank Prof. Stephan Michnick (Université de Montré al, Canada) for providing the
humanized GLuc plasmids, Prof. Junichi Ikenouchi (Kyushu University, Japan) for
the FRMD4A–GFP plasmid and Dr Mikko Airavaara (University of Helsinki, Finland)
for the CHME-5 cell line.
2013
Journal of Cell Science
used, and three or four independent experiments were performed. GW4869
(Sigma) and SecinH3 (R&D Systems) were dissolved in DMSO, and further
diluted in culture medium.
Journal of Cell Science (2016) 129, 2003-2015 doi:10.1242/jcs.180745
Competing interests
H.J.H. is an employee and shareholder of Herantis Pharma Plc, which is unrelated to
this study.
Author contributions
X.Y., N.-P.N., C.A.B., A.H., M.H., R.-L.U. and H.J.H. designed and performed
experiments, analyzed the data and wrote the manuscript.
Funding
This study was supported by grants from the Academy of Finland (Suomen
Akatemia) [grant numbers 218081, 263762 to H.J.H., 125274 to M.H.]; the Brain and
Mind doctoral program (to X.Y.); the Integrative Life Science doctoral programs (to
C.A.B.); University of Helsinki funds (to H.J.H.); the Finnish Cultural Foundation
(Suomen Kulttuurirahasto) (to N.-P.N., R.-L.U., H.J.H.); a VTR of Kuopio University
Hospital (Kuopion Yliopistollinen Sairaala) [grant number V16001 to M.H.]; the
Sigrid Jusé lius Foundation (Sigrid Jusé liuksen Sä ä tiö ) (to M.H.); and Strategic
Funding of the University of Eastern Finland (Itä -Suomen yliopisto; UEF-Brain,
to M.H.).
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